1. Introduction
Plasmacytoid dendritic cells (pDC) are a rare but essential subset of dendritic cells (DCs) that act as professional type I interferon (IFN) producing cells by effectively inhibiting viral replication and by triggering a strong antiviral state in the host cells. Although they represent only 0.2–0.8% of human peripheral blood mononuclear cells (PBMCs), pDCs produce 200–1000-times more type I IFN than any other white blood cells in response to various viruses and, thus, play a crucial role in antiviral immunity [1]. The robust type I IFN production of pDCs is critical for the control of acute viral infections [2]. However, the overactivity of pDCs and the overproduction of type I IFNs can induce undesirable autoimmune responses, leading to the damage of the body’s own tissues and to the development of autoimmune diseases. Previous studies have shown that pDCs are directly involved in the pathogenesis and pathomechanism of several autoimmune diseases, such as systemic lupus erythematosus (SLE) or psoriasis [3], thus, serving as potential therapeutic targets in these pathologies. Therefore, the type I IFN response of pDCs is tightly regulated, partially through receptor interactions [4], the comprehensive study of which may help to better understand the mechanism of both antiviral responses and autoimmune diseases.
The functionality of pDCs, including their activation and IFN-producing capacity, is mediated through their specific pattern recognition receptors (PRRs). PDCs selectively express the endosomal Toll-like receptor (TLR) 7 and 9 receptors, which are specialized in the recognition of microbial nucleic acids, mainly of viral origin [5], and, thus, are essential to the production of large amounts of type I IFNs [6]. However, pDCs express several other cytosolic sensors and only those that can detect viruses have been well characterized so far. Our research group previously demonstrated that the two major members of the retinoic acid-inducible gene-I (RIG-I)-like receptors (RLR), namely RIG-I and Melanoma Differentiation-Associated gene 5 (MDA5), are also actively functional in human pDCs and involved in the recognition of replicating viruses in the cytosol [7,8]. The cytosolic DNA sensing cyclic GMP-AMP synthase (cGAS)-stimulator of interferon genes (STING) pathway can also be active in pDCs, resulting in type I IFN production [9]. In addition, our research group has also demonstrated that regulatory receptors of the cytosolic nucleotide-binding oligomerization domain (NOD)-like receptor (NLR) family, namely NLR family caspase activation and recruitment domain (CARD) containing 5 (NLRC5) and NLR family member X1 (NLRX1), are also expressed in pDCs and, among others, are involved in the regulation of RLR activity [8]. Nevertheless, the best-characterized function of NLRs, namely their ability to induce inflammasome activation, has not been extensively studied in pDCs yet. Among the NLRs, NLR pyrin domain containing (NLRP) 1, NLRP3, NLRC4 and, in addition to those absent in melanoma 2 (AIM2), interferon-γ inducible protein 16 (IFI16) and pyrin inflammasomes [10] can form multimeric protein complexes that serve as activation platforms for caspase-1, which controls the maturation of the pro-inflammatory cytokines interleukin (IL)-1β and IL-18. Furthermore, several other NLR-family proteins, including NLRP2, NLRP6, NLRP7, NLRP9b and NLRP12, have been proposed to form inflammasome complexes [11,12,13,14,15]. The role of these receptors is extensively characterized in monocytes, macrophages, conventional DCs and in other cell types [16,17,18,19,20] but not in pDCs. So far, among the inflammasome forming receptors, only the AIM2 cytosolic DNA sensor has been found to be active in tumor-associated pDCs [21] indicating that functional inflammasomes can be assembled in pDCs as well.
Among the caspase-1 activating inflammasomes, the NLRP3 inflammasome is the best studied and most characterized. NLRP3 contains an N-terminal pyrin domain (PYD), a central NACHT (NAIP [neuronal apoptosis inhibitory protein]) domain, which is responsible for activation-induced oligomerization through its adenosine triphosphatase (ATPase) activity [22], and a C-terminal leucine-rich repeat (LRR) domain. Canonical NLRP3 activation usually occurs in two steps. First, during the so-called priming phase, cytokine receptors or other PRRs, such as TLRs and NOD receptors, activate the nuclear factor-kappa B (NF-κB) pathway, which induces the expression of NLRP3 inflammasome components and, thus, contributes to the production of the pro-form of IL-1β and IL-18 [23,24,25,26]. The priming also triggers post-translational modifications, which stabilize NLRP3 in a signal-competent but inactive state [27]. The priming phase is followed by the second NLRP3 activation step, which initiates NLRP3 inflammasome oligomerization. This step can be induced by a wide range of factors, including cellular stress signals initiated during the priming phase and by various pathogen-associated molecular patterns (PAMPs) and damage-associated molecular patterns (DAMPs) [26,27,28]. In response to the activation signals, seven NLRP3 receptors oligomerize through the NACHT domains and then the apoptosis-associated speck-like protein containing CARD (ASC/PYCARD) adaptor protein interacts with NLRP3 through PYD-PYD interaction that facilitates the formation of the helical ASC filament core. Subsequently, via CARD-CARD interaction, ASC recruits pro-caspase-1 and enables its activation through self-cleavage. Thereafter, active caspase-1 cleaves pro-IL-1β and pro-IL-18 and results in the secretion of their biologically active mature forms [27,28]. The inflammatory cytokines IL-1β and IL-18, generated through NLRP3 activation, play a central role in antibacterial and antifungal inflammatory responses [29,30,31].
Nevertheless, it is also known that NLRP3 polymorphism results in the abnormal activation of NLRP3 inflammasome and the increased secretion of IL-1β and IL-18 by innate immune cells induces systemic inflammation that eventually culminates in chronic tissue damage and in the development of autoinflammatory conditions [32]. Moreover, NLRP3-triggered IL-1β can affect lymphocytes in many different ways; thus, it can serve as an important link for NLR-triggered adaptive immune responses as well. Among others, it promotes B cell proliferation and antibody production and increases T cell survival and polarization, which may also promote the differentiation of autoreactive T helper (Th) 1 and Th17 cells [33]. Therefore, several autoimmune diseases, including SLE, psoriasis, multiple sclerosis (MS), rheumatoid arthritis (RA) or inflammatory bowel diseases (IBD), can be associated with NLRP3 overactivity [33,34,35,36].
Thus, increased activity of both the type I IFN pathway and the IL-1β secretory pathway may lead to autoimmune pathologies in which pDCs may play a key role [37,38,39]. However, it is well known that the two pathways interfere with each other. In particular, type I IFNs inhibit NLRP3 inflammasome-dependent IL-1β production through different mechanisms [40,41,42], which might explain why the body’s antibacterial defense mechanism is weakened and more prone to bacterial superinfections following severe viral infections [43,44,45,46,47]. In addition, IL-1β can also inhibit the type I IFN pathway in multiple ways [48,49,50] that represents a mutually negative interaction between the two pathways. Nevertheless, the interplay between the NLRP3 inflammasome-dependent IL-1β and type I IFN pathway has not been studied in human pDCs yet. Since pDCs are known for their ability to produce massive amounts of type I IFNs [4], we hypothesize that the potential NLRP3-dependent release of IL-1β by pDCs might be initiated during those immune responses when the high IFN-I-producing ability of pDCs is not dominant. In recent years, increasing evidence has indicated that pDCs are more complex than “virus-specific” immune cells. In addition to playing a prominent role in combating viral infections, pDCs are also involved in inflammatory immune responses against various bacteria [51,52,53,54] and fungi [55,56,57,58,59,60]. As mentioned above, these antibacterial and antifungal responses are often coordinated by inflammatory cytokines released through NLRP3 inflammasome activation [61,62,63,64,65].
Therefore, we aimed to explore the baseline and activation-induced expression levels of NLRP3 inflammasome components in human pDCs and we sought to identify those exogenous and endogenous signals, which might induce the assembly of NLRP3 inflammasomes and the subsequent secretion of IL-1 family cytokines in human pDCs. Furthermore, we wanted to explore how the activity of the type I IFN pathway affects NLRP3 inflammasome activation and what type of interaction might exist between the type I IFN and IL-1β pathways in pDCs. Thus, in our work, we investigated the NLRP3 pathway activity in pDCs by using activation signals with high type I IFN-inducing capacity and under pathological conditions with elevated type I IFN signature that might reveal which immunological responses might promote or suppress the NLRP3-mediated inflammatory pathways in pDCs in vivo.
2. Results
2.1. Investigating the Expression Profile of NLRP3 Pathway Components in a Human pDC Cell Line
In our experiments, we first explored the baseline and activation-induced expression profile of NLRP3 pathway components in the GEN2.2 human pDC cell line at the mRNA level by quantitative polymerase chain reaction (qPCR) (Supplementary Figure S1A–E) and at the protein level by Western blot (Figure 1A,B). Our results show that the NLRP3 receptor, the ASC adaptor protein and the pro-form of caspase-1 are constitutively expressed both at the mRNA (Supplementary Figure S1A–C) and the protein levels (Figure 1A,B), whereas the cleaved, active form of caspase-1 is undetectable at the protein level in resting pDCs (data not shown). IL-1β is only marginally expressed at the mRNA level (Supplementary Figure S1D) and while its pro-form is barely detectable at the protein level (Figure 1A,B), its cleaved form is undetectable in unstimulated pDCs (data not shown). Although low levels of IL-18 could be detected at the mRNA level in resting pDCs (Supplementary Figure S1E), its pro-form was not detectable at the protein level (data not shown). IL-1α was not present either at the mRNA or protein level in non-activated pDCs (data not shown).
Next, GEN2.2 cells were activated with various synthetic TLR agonists, which modulated the expression levels of NLRP3 pathway components to different extents. The greatest differences were seen in the effects of the TLR9 ligands, CpG-A and CpG-B. Although these unmethylated oligodeoxynucleotide (ODN) sequences act through the same receptor, CpG-A encounters TLR9 in early endosomes and mostly results in type I IFN secretion, whereas CpG-B is preferentially trafficked to late endosomes and, thus, it is a more potent inducer of NF-κB activation and pro-inflammatory cytokine production [66]. CpG-A exposure significantly decreased NLRP3 expression, both at the mRNA and protein level, whereas CpG-B did not affect its mRNA and protein levels, as compared to unstimulated cells (Supplementary Figure S1A and Figure 1A,B). The level of the NLRP3 adaptor protein ASC was not altered by CpG-A treatment, while a 24 h treatment with CpG-B significantly upregulated its expression at the mRNA level; however, that increase was not detectable at the protein level (Supplementary Figure S1B and Figure 1A,B). Both TLR9 agonists enhanced caspase-1 expression; however, a significant increase was detected only in response to a 24 h exposure to CpG-B, both at the mRNA and protein levels (Supplementary Figure S1C and Figure 1A,B). The major difference between the two ligands was observed in their ability to induce IL-1β production. While CpG-B significantly increased IL-1β production in pDCs at 3 and 6 h, CpG-A was not able to elicit IL-1β expression (Supplementary Figure S1D and Figure 1A,B). Although CpG-B significantly upregulated the expression of IL-18 at the mRNA level, the increase was only about one-tenth of the relative expression of IL-1β and probably, therefore, we were not able to detect IL-18 at the protein level in activated pDCs (Supplementary Figure S1E). Interestingly, the TLR7 agonist imiquimod induced similar changes in the expression of NLRP3 pathway components as CpG-B, with the only difference in IL-1β levels, which was significantly higher not only at 3 and 6 h but also at 12 and 24 h of treatment, as compared to unstimulated cells (Supplementary Figure S1A–E and Figure 1A,B). These results suggest that different activation signals exhibit distinct IL-1β production kinetics and that pro-IL-1β protein levels are already detectable within 3 h after activation of pDCs.
Multiple lines of evidence indicate that NLRP3 inflammasome-mediated inflammatory responses are of great importance in the control of bacterial and fungal infections. Several bacteria and bacteria-released components, such as various bacterial toxins, provide potent activation signals for inflammasomes [67]. Thus, in our following experiments, pDCs were activated with live pathogenic Escherichia coli (E. coli), and non-pathogenic bacteria (Bacillus subtilis, Lactobacillus rhamnosus), and opportunistic fungi (Candida albicans). Among the tested microbes, only E. coli was able to induce a significant increase in the IL-1β mRNA expression, with peaks at 3 and 6 h that were similar in extent to those observed after CpG-B activation (Supplementary Figure S2A). Furthermore, E. coli also provided the strongest activation signal for the secretion of tumor necrosis factor (TNF) and IL-6 pro-inflammatory cytokines and the IL-8 chemokine when compared to the other microbial stimuli (Supplementary Figure S2B). Based on these results, we decided to stimulate pDCs with E. coli to investigate the mRNA (Supplementary Figure S3) and protein (Figure 2A,B) level expression of NLRP3 pathway components. Similar to CpG-B and imiquimod, E. coli stimulation enhanced pro-IL-1β expression as early as 3 and 6 h following activation, while it increased pro-caspase-1 expression as late as 12 and 24 h following bacterial stimuli. Further, we found that exposure to E.coli did not affect NLRP3 and ASC protein levels (Figure 2A,B) and E. coli exposure alone did not induce the cleaved form of caspase-1 or IL-1β (data not shown).
All these data imply that in pDCs, mainly Gram-negative, pathogenic bacteria are capable of inducing the expression of the pro-form of IL-1β. However, in sharp contrast to myeloid cells, such as monocytes with high NLRP3 activity, priming signals alone are not sufficient to induce the production of the cleaved, bioactive form of IL-1β in pDCs.
2.2. Assessment of Mature IL-1β Secretion in a Human pDC Cell Line
Next, we wanted to know whether inactive pro-IL-1β could be cleaved and converted into its bioactive, mature form in pDCs. As mentioned above, NLRP3 inflammasome activation generally requires two signals, a primary “priming” signal and a secondary activation signal [26]. The secondary signal ensures the assembly and activation of the NLRP3 inflammasome, which induces the self-cleavage and, thus, the activation of pro-caspase-1 that eventually initiates the cleavage of pro-IL-1β [68]. Numerous secondary signals, including various DAMPs and PAMPs, are known to induce the assembly of the NLRP3 inflammasome [27]. Since we observed that TLR activation alone was not sufficient enough to generate the cleaved form of IL-1β in human pDCs, we applied various secondary activation signals, including adenosine triphosphate (ATP), uric acid sodium salt (MSU), aluminum hydroxide (Alum), the mitochondrial (reactive oxygen species) ROS generator antimycin A [69] and nigericin after priming with CpG-B. Thereafter, we measured the concentration of secreted IL-1β in the cell supernatants in the presence or absence of fetal bovine serum (FBS) in a time-dependent manner (Supplementary Figure S4A). We investigated IL-1β production in the absence of FBS to exclude the ATPase activity of the serum (Supplementary Figure S4A). ATP is rapidly degraded by the transmembrane ecto-ATPases. First, CD39 converts ATP to AMP, which is then dephosphorylated to adenosine by CD73 [70,71]. In addition, the soluble active form of both ectonucleotidases can also be found in the serum [71,72,73,74]; thus, the hydrolysis of nucleotides can take place in the serum as well [75]. Interestingly, among the tested NLRP3 activators, only nigericin, a bacterial toxin, which acts as a potassium ionophore [76], was found to be a potent secondary signal leading to NLRP3 activation in pDCs (Supplementary Figure S4A). In macrophages, ATP is one of the strongest NLRP3 activators; however, our results demonstrated that ATP is not able to induce IL-1β secretion in pDCs. This might be explained by the lack of the ATP-recognizing receptor P2X purinoceptor 7 (P2X7), which is not even inducible by TLR stimulation in pDCs (Supplementary Figure S4B,C). Based on these results, we used nigericin as a secondary signal in our further experiments. Similar to priming with CpG-B, pretreatment with imiquimod and E. coli resulted in significant IL-1β secretion in combination with nigericin. Nevertheless, activation signals, including CpG-A (Figure 3A), Bacillus subtilis, Lactobacillus rhamnosus and Candida albicans (Figure 3B), which were not able to induce the pro-form of IL-1β, did not induce the cleaved form of IL-1β, even in the presence of nigericin. Similar to priming alone (Figure 3A,B, Supplementary Figure S4A), secondary signals alone, including nigericin, were not sufficient to produce cleaved IL-1β in pDCs (data not shown).
In parallel experiments, we utilized the specific NLRP3 inhibitor MCC950 to clarify whether IL-1β secretion by pDCs is indeed NLRP3 inflammasome dependent. As the specific NLRP3 inhibitor almost completely blocked IL-1β secretion by pDCs (Figure 3A,B), we can conclude that mature IL-1β production by pDCs is mainly NLRP3 dependent. In addition, we found that the caspase-1 specific inhibitor Z-YVAD-FMK also significantly reduced the release of mature IL-1β by pDCs (Supplementary Figure S5A). In line with that, we also detected lower cleaved-caspase-1 levels in the cells when the NLRP3 was activated in the presence of the above mentioned inhibitors (Supplementary Figure S5B,C).
In summary, our results suggest that only the combination of specific priming and secondary signals can induce NLRP3 inflammasome activity in human pDCs.
2.3. Analysis of NLRP3 Pathway Activity in Primary Human pDCs
After mapping the expression profile of NLRP3 pathway components in the GEN2.2 human pDC cell line and identifying activation signals that can activate the NLRP3 pathway in these cells, we were curious to see whether a similar activation profile could be detected in primary human pDCs as well. For our experiments, we first collected peripheral blood samples from healthy blood donors, then isolated mononuclear cells from the blood samples by Ficoll-Plaque Plus gradient centrifugation and assessed the expression of NLRP3 pathway components within the gated pDC cell population through flow cytometry using cell surface and intracellular staining. To define the pDC cell population, we first identified the pDC population based on the side scatter (SSC) parameter and blood dendritic cell antigen (BDCA) 4 positivity that showed a homogeneous BDCA4+ population below an approximate SSC value of 200 (Supplementary Figures S6 and S7). Based on SSC and forward scatter (FSC) parameters, the gated BDCA4-positive population is not uniform; thus, we performed a second gating step, where a uniform cell population within the BDCA4 population was gated below approximately 200 on the SSC axis and in the 400–600 region of FSC (Supplementary Figures S6 and S7). Without a second gating step, the BDCA4-positive population also showed some positivity for Linage marker (CD14, CD19, CD56, CD3, CD16 and CD20) (Supplementary Figure S6A), CD11c (Supplementary Figure S6B), CD2 (Supplementary Figure S6C), CD5 (Supplementary Figure S6D), AXL (Supplementary Figure S7A) and CD33 (Supplementary Figure S7B), which are not pDC-specific markers. Furthermore, without a second gating step, only about 90% of the BDCA4-positive population is positive for CD123 (Supplementary Figure S7C), also indicating some degree of contamination with other cell types. However, with a second gating based on SSC-FSC parameters, the positivity/percentage of non-pDC-specific markers within the BDCA4+ population can be significantly reduced (Supplementary Figures S6 and S7). The highest positivity for the non-pDC specific-markers within the BDCA4+ population is shown by those cells, which are located above approximately 600 on the FSC axis (Supplementary Figures S6 and S7). Thus, we suppose that these cells are likely to be more than just possibly clumped pDCs with higher FSC, i.e., size values. Thus, in our further experiments, we used a second gating based on SSC-FSC parameters in addition to BDCA4 positivity to define the pDC population, on which we further examined the expression of NLRP3 pathway components.
Representative dot plots in Figure 4 show that NLRP3, ASC and pro-caspase-1 are expressed constitutively almost in the entire pDC population (Figure 4A). However, ASC protein levels were above 95% in all the donors tested; NLRP3 and pro-caspase-1 levels represented a broader expression range, with some donors showing lower expression values (Figure 4B). At the same time, cleaved-caspase-1, pro-IL-1β and cleaved-IL-1β levels were barely detectable in unstimulated pDCs (Figure 4A,B).
Next, we investigated whether the cleaved form of caspase-1 and the pro-form and cleaved form of IL-1β can be induced in primary pDCs upon activation (Figure 5). The TLR9 ligands CpG-A and CpG-B and the TLR7 agonist imiquimod used alone did not alter pro-caspase-1 levels (Figure 5A) and were not able to induce the cleaved form of caspase-1 (Figure 5B). However, in combination with nigericin, both CpG-B and imiquimod significantly increased cleaved caspase-1 levels in cells, although it is important to note that their efficacy was highly donor dependent (Figure 5B). As observed in the pDC cell line (Figure 3A), pro-IL-1β was mainly detectable by stimulation with CpG-B or imiquimod. The cleaved form of IL-1β was induced only with CpG-B or imiquimod priming following nigericin treatment. On the contrary, CpG-A was found to be a weak activation signal for the induction of both the pro- and cleaved forms of IL-1β in primary pDCs (Figure 5C,D). Similar to the cleaved caspase-1 levels, we detected donor-dependent variations in the extent of IL-1β induction as well (Figure 5C,D). Due to the specific Golgi-independent secretion profile of IL-1β, the intracellular staining process was performed without the use of a protein transport inhibitor [77,78]. However, based on our preliminary results with primary pDCs, 1 h nigericin treatment after TLR priming proved to be the most effective and showed the highest positivity for the cleaved form of IL-1β within the pDC population (data not shown). Using the same experimental conditions, we also validated the intracellular localization of the cleaved form of IL-1β and caspase-1 in pDCs by fluorescence confocal microscopy as well (Supplementary Figure S8).
These results suggest that similar activation signals are required for NLRP3 activation in primary pDCs and in the GEN2.2 human pDC cell line.
2.4. Analysis of NLRP3 Pathway Activity in the Presence of Type I IFNs in pDCs
We hypothesized that the ability of the two TLR9 agonists (CpG-A and CpG-B) to induce IL-1β release by pDCs to a different extent is due to their distinct type I IFN inducing potential [79]. When using the same concentration of the two ligands, CpG-A resulted in a strong and pro-longed secretion of IFN-α (Supplementary Figure S9A), whereas CpG-B induced only very little IFN-α production in GEN2.2 cells (Supplementary Figure S9A). Although both TLR9 ligands could induce the secretion of the pro-inflammatory cytokines IL-6 and TNF, CpG-B resulted in higher cytokine concentrations compared to CpG-A (Supplementary Figure S9B). These results suggest that the major difference between CpG-A and CpG-B is that they have a very different type I IFN-inducing capacity. Thus, we propose that the strong type I IFN triggering capacity of CpG-A may be responsible for its limited potential to induce IL-1β release by human pDCs. In other cell types, a substantial body of evidence suggests that activation of the type I IFN pathway can inhibit the NLRP3-dependent IL-1β pathway by enhancing the expression of several negative regulatory molecules, which inhibit IL-1β formation at the mRNA level, block secondary signals required for NLRP3 activation or directly interact with and, thus, inhibit the assembly of NLRP3 inflammasome components [40,41,80]. Therefore, we activated pDCs with CpG-B in the presence of IFN-α and found that it was able to inhibit pro-IL-1β production, both at the mRNA (Figure 6A) and protein (Figure 6B) levels after 3 and 6 h of CpG-B stimulation. Furthermore, cleaved IL-1β concentrations were also significantly lower when IFN-α was added to cells prior to CpG-B and nigericin treatment (Figure 6C). Thus, it can be concluded that type I IFNs inhibit NLRP3-dependent IL-1β pathway activity in pDCs. Interestingly, in the presence of IL-1β, CpG-A-induced type I IFN production was also significantly reduced, both at the mRNA and protein levels (Supplementary Figure S10), suggesting a mutual negative interaction between the type I IFN and IL-1β pathways.
2.5. Assessing the NLRP3 Activity in pDCs in the Presence of Viruses with High Type I IFN Inducing Capacity
Next, we wanted to investigate the extent to which viruses with strong type I IFN inducing capacity can induce pro-IL-1β production in human pDCs when compared to bacterial stimuli (Supplementary Figure S11). Thus, GEN2.2 cells were treated with the RNA virus Vesicular Stomatitis Virus (VSV), the DNA virus Herpes Simplex Virus (HSV) and the pathogenic bacterium E. coli, which is a good IL-1β inducer, as our previous results showed. Both RNA and DNA viruses greatly enhanced type I IFN production compared to E. coli (Supplementary Figure S11A). Viral exposure did not induce significant pro-IL-1β production, which is in high contrast with E. coli, which is a strong inducer of pro-IL-1β after 3 and 6 h of treatment (Supplementary Figure S11B).
We then investigated how E. coli-induced IL-1β production of pDCs is affected by the presence of viruses. Therefore, the GEN2.2 pDC cell line was pretreated with VSV or HSV for 3 h, when pDCs already produce considerable levels of IFNs (Supplementary Figure S11A) and then exposed to E. coli for 3 or 6 h. Our results showed that pretreatment with viruses significantly reduced E. coli-induced IL-1β mRNA expression (Figure 7A) as well as pro-IL-1β protein levels (Figure 7B). Moreover, viral exposure substantially suppressed the release of mature IL-1β by pDCs upon co-treatment with E.coli and nigericin (Figure 7C). It is important to highlight, however, that viral pretreatment did not affect the E. coli-induced production of TNF, IL-6 and IL-8 (Supplementary Figure S11C).
Subsequently, we repeated our experiments with primary human pDCs and measured IL-1β levels by intracellular staining using flow cytometry. PBMCs from healthy donors were treated with VSV, HSV and E. coli for 2.5 h. In the gated primary pDC population, we found that only E. coli treatment resulted in significant pro-IL-1β induction, while VSV and HSV did not induce any changes compared to unstimulated cells (Figure 8A). Furthermore, 1 h exposure to nigericin was able to upregulate cleaved IL-1β levels upon E.coli pretreatment, whereas it did not induce detectable changes upon prior exposure to viruses (Figure 8B). In addition, neither E. coli nor the viruses induced the cleavage of IL-1β in the absence of nigericin. These results suggest that the NLRP3-dependent IL-1β pathway is barely inducible in human pDCs upon viral exposure.
Furthermore, we found that similar to the pDC cell line, viral pretreatment dampened bacteria-induced IL-1β production in primary pDCs as well. Prior exposure to VSV or HSV viruses significantly suppressed the E. coli-induced pro-IL-1β protein levels (Figure 8C) and the E. coli and nigericin co-treatment mediated production of cleaved IL-1β (Figure 8D). These results suggest that bacteria-induced IL-1β production by pDCs can be inhibited in the presence of RNA and DNA viruses, probably due to the inhibitory effects of virus-induced type I IFNs on the NLRP3-dependent IL-1β pathway.
2.6. Analysis of NLRP3-Dependent IL-1β Pathway Activity in pDCs from Psoriasis Patients Associated with High IFN Signature
Finally, we wanted to explore how IL-1β production by human pDCs is affected under pathological conditions, when cells are exposed to high levels of type I IFNs. To this end, we investigated IL-1β production in pDCs from patients with plaque-type psoriasis, an autoimmune disease associated with excessive type I IFN production and pDC overactivation [81]. Significantly higher levels of IFN-α (Figure 9A) and pro-inflammatory cytokines, including IL-1β, were measured in serum samples from patients with psoriasis compared to healthy donors (Figure 9B). Further, we found that the pDC proportion is significantly lower in PBMCs from psoriatic patients compared with healthy volunteers (Figure 9C) that might be explained by the migration and accumulation of pDCs into the inflamed skin lesions of patients [81]. In addition, we found higher NLRP3, ASC, caspase-1 and IL1B mRNA levels in PBMCs from psoriasis patients compared with healthy individuals (Figure 9D–G). Whereas NLRP3 protein levels were significantly lower in pDCs from psoriatic patients compared to those from healthy controls, we could not detect any differences in the baseline protein levels of ASC and caspase-1 between the two groups (Figure 9H). Cleaved caspase-1, pro-IL-1β and cleaved IL-1β are only marginally expressed by unstimulated cells from both psoriatic and healthy individuals (Figure 9H) and in line with our previous experiments, CpG-A treatment did not affect their expression in pDCs from either psoriatic patients or healthy individuals (Figure 9I). On the contrary, both CpG-B and imiquimod resulted in significantly lower induction of cleaved-caspase-1, pro-IL-1β and cleaved IL-1β in pDCs from psoriatic patients compared to pDCs from healthy donors (Figure 9J,K).
Thus, it is likely that the IL-1β pathway is inhibited in pDCs from patients due to high exposure to type I IFNs. This hypothesis is also supported by data obtained from studying the expression of IFN-inducible regulatory molecules, which inhibit NLRP3-dependent IL-1β secretion. Binding of type I IFNs to their receptors activate the transcription factor signal transducer and activator of transcription (STAT)1, which enhances the expression and activity of several regulatory molecules that can inhibit the NLRP3 pathway at multiple levels [40,41,42]. Such negative regulators include cholesterol-25-hydroxylase (CH25H), IL-10, interleukin-1 receptor antagonist (IL-1RA), inducible nitric oxide synthase (iNOS), suppressor of cytokine signaling (SOCS) 1, PYRIN domain-only proteins (POP) and CARD-only proteins (COP) [40,41,42]. Our results show that activation signals, which induce high type I IFN production, such as CpG-A, highly upregulate the expression of CH25H, SOCS1 and COP1 in human pDCs. Thus, CpG-A is a potent inducer of NLRP3 inhibitory molecules in contrast to CpG-B (Figure 10A). Furthermore, we found that these suppressor proteins were also expressed at significantly higher levels in PBMCs from psoriasis patients compared to those from healthy controls (Figure 10B). Thus, it is possible that, in the presence of high type I IFN levels, CH25H inhibits IL-1β transcription at the mRNA level, SOCS1 inhibits secondary signals required for NLRP3 activation and COP1 inhibits NLRP3-mediated activation of caspase-1 in psoriatic patients [82,83,84] that, altogether, might be responsible for the dampened IL-1β production by patients’ pDCs.
Finally, we also compared the expression of NLRP3 pathway components in the CD14+ monocyte population from psoriatic and healthy individuals, since inflammatory cytokines produced in excess by circulating monocytes also play an important pathological role in psoriasis [85,86,87]. The ability of monocytes to produce type I IFNs is much lower than that of pDCs [88,89,90,91], yet we still wondered whether NLRP3 activity is also hindered by type I IFNs in the monocyte fraction of psoriatic patients. In the steady state, both monocytes and pDCs express NLRP3 and ASC at similar levels (Supplementary Figure S12A) and although we previously found that pDCs show almost 100% positivity for pro-caspase-1 (Figure 4 and Figure 9H), its expression is almost 100-fold higher in monocytes compared to pDCs (Supplementary Figure S12A), indicating a much higher caspase-1 activity in monocytes. Psoriatic patients exhibit a higher percentage of monocytes in peripheral blood compared with healthy individuals (Supplementary Figure S12B). In contrast to pDCs, NLRP3 protein levels were comparable between the monocyte fractions of psoriatic patients and healthy controls (Supplementary Figure S12C). However, monocytes of both psoriatic patients and healthy individuals display high donor-dependent variations in the protein levels of ASC. We detected significantly elevated ASC expression in the monocytes of psoriasis patients compared with healthy controls (Supplementary Figure S12C). The major difference between the pDC and monocyte populations was that high levels of cleaved caspase-1 can be detected in monocytes from psoriatic patients, even without an extra activation signal, while both the pro- and cleaved forms of IL-1β were at marginal levels (Supplementary Figure S12C). While activation (CpG-A, CpG-B, imiquimod and nigericin) significantly decreased the levels of caspase-1, pro-IL-1β and cleaved IL-1β in pDCs of psoriatic patients compared with healthy controls (Figure 9H–K), it did not affect the monocyte fractions of the two groups (Supplementary Figure S12D). Moreover, in contrast to pDCs, monocytes displayed increased expression of caspase-1, pro-IL-1β and cleaved IL-1β upon CpG-A exposure as well (Supplementary Figure S12D) that might be explained by the poor ability of monocytes to induce type I IFN production in response to these activation signals. All these results suggest that either the low baseline caspase-1 levels or the excessive type I IFN production, which inhibits NLRP3 activity, might be responsible for the reduced NLRP3 pathway activity and IL-1β production in human pDCs.
3. Discussion
Due to their unique capacity to rapidly produce massive amounts of type I IFNs, human pDCs are considered as the master regulators of antiviral responses [4,92] and are also involved in the pathogenesis and pathomechanism of various human diseases. Deficiency in type I IFN production by pDCs might lead to persistent viral infections [93,94] or tumor growth due to the lack of IFN-induced anti-tumor activity [95,96], whereas pDC overactivation can result in the development of autoimmune pathologies associated with a high IFN signature [97,98]. Thus, pDC research has primarily focused on PRRs, which provoke type I IFN responses by pDCs, while few data are available regarding the role of the cytosolic inflammasome-forming NLRP3 receptors and the effector functions of NLRP3-triggered inflammatory cytokines, such as IL-1β and IL-18, in pDC-mediated immune responses.
In 2009, Crozat and colleagues published that both mouse and human pDCs have low antibacterial activity, as they found that NLRs involved in antibacterial innate immunity, including NLRP3, are expressed at low mRNA levels by pDCs compared to BDCA1+ DCs [99]. Among the human blood DC subtypes, caspase-1 mRNA expression was high in BDCA1+ DCs, whereas it was barely detectable in human pDCs and BDCA3+ DCs [99]. Later, this observation was validated at the protein level by Worah and colleagues [100], who found that neither resting pDCs nor R848-activated pDCs nor BDCA3 + DCs had detectable caspase-1 protein levels compared to BDCA1+ DCs (also known as CD1c + DCs and recently referred to as cDC2), which showed high caspase-1 expression, both at baseline and after activation [100]. Another study from last year also identified BDCA1 + DCs as potent IL-1β producers in contrast to pDCs and BDCA3 + DCs (also known as cDC1) [101]. All these studies assume that pDCs, due to their low caspase-1 levels, do not possess inflammasome activity. However, it is important to highlight that these studies compared the pro-caspase-1 protein levels [100] and IL-1β secretion [101] of pDCs to BDCA1 + DCs; thus, the weaker signals of pDCs might be covered by the strong signals of BDCA1 + DCs.
Nevertheless, a great body of evidence indicates that pDCs are not only “virus-specific” immune cells, as they may play a role in immune responses against bacteria and fungi as well. In particular, pDCs exposed to various bacteria undergo a maturation process and can induce antigen-specific responses as well [51,52,53]. Interestingly, much more is known about the immune response of pDCs against fungi and the mechanism of their antifungal activity is also widely explored [55,56,57,58,59,60]. These data demonstrate that pDC functions are much more diverse than previously thought and that they may be involved in immune responses against pathogens other than viruses as well. However, to date, there are no data pertaining to the role of the NLRP3-dependent IL-1β pathway in the antibacterial or antifungal activities of pDCs.
Therefore, we first explored whether NLRP3 activity can be detected in the human GEN2.2 pDC cell line, which phenotypically and functionally exhibits the characteristics of primary human pDCs [102]. In this cell line, we were able to detect the NLRP3 receptor, the ASC adaptor protein and the pro-caspase-1 enzyme, both at the mRNA and protein levels in resting and activated states. However, among the inflammatory cytokines associated with NLRP3 activity, only the pro-form of IL-1β was detectable both at the mRNA and protein levels in activated cells. IL-18 expression was very low in both resting and activated cells at the mRNA level and was not detectable at the protein level. Although some studies suggest that IL-18 production by mouse pDCs may contribute to NK cell activation and antigen-specific T cell responses upon viral infection, these studies, like ours, failed to detect IL-18 at the protein level in pDCs [103,104]. Furthermore, although the precursor of IL-1α is constitutively present in almost all cell types under physiological conditions [105], we could not detect IL-1α levels in pDCs under any of the tested conditions. Based on literature data, it is hypothesized that a specific cytokine environment and a combination of stimulation signals are required to induce IL-1α production in pDCs, since IL-1α production has so far only been described in tumor-associated pDCs, which are exposed to the effects of tumor-derived immunosuppressive environment [21]. Furthermore, the IL-1α expression was found to depend on AIM2 and not NLRP3 inflammasome activity [21]. These findings suggest that IL-1β may play the major role in the NLRP3-mediated antimicrobial immune responses of human pDCs.
It is also important to emphasize that we found that distinct activation signals induce different levels of pro-IL-1β expression in pDCs. For example, CpG-B, a ligand for the endosomal TLR9 effectively induces pro-IL-1β, whereas CpG-A, another TLR9 agonist, is not able to do so. This observation is in agreement with literature data showing that different TLR agonists may have distinct IL-1β induction profiles [106]. Furthermore, our results suggest that pro-IL-1β is induced early in pDCs following activation, similar to monocytes and macrophages, which are the main sources of bioactive IL-1β in the myeloid cell compartment [107,108,109,110]. However, the distinct TLR activation signals differed not only in their pro-IL-1β induction ability but also in their pro-IL-1β production kinetics. While pro-IL-1β production reached a peak at 3–6 h after CpG-B stimulation, the TLR7 agonist imiquimod showed prolonged pro-IL-1β production kinetics. Imiquimod has previously been described to mediate complex activation signals in cells and to have TLR7-independent effects as well [111,112,113]. It induces ROS production via the quinone oxidoreductase (NQO) 2 and mitochondrial complex I that may result in K+ efflux-independent NLRP3 activation through the NIMA-related kinase (NEK) 7 adaptor protein [106]. In addition to inducing NLRP3 assembly as a secondary signal, ROS also function as a priming signal and enhance NLRP3 and pro-IL-1β expression by increasing the activity of the NF-κB signaling pathway [114,115]. Thus, it is likely that the ROS-inducing effect of imiquimod may also contribute to the prolonged pro-IL-1β production kinetics in pDCs. Of note, macrophages differentiated from monocytes using various cytokines also exhibit different IL-1β production kinetics [107], suggesting that the type of activation signals has a strong influence on the kinetic profile of IL-1β.
The TLR agonists CpG-B and imiquimod rapidly induced pro-IL-1β production, whereas enhanced pro-caspase-1 protein levels at later incubation time points, mainly at 24 h, when pro-IL-1β induction has already subsided in pDCs. A similar upregulation of pro-caspase-1 levels was observed in CD1c+ DCs after overnight stimulation with R848 [100], whereas in monocytes and macrophages, constitutively high pro-caspase-1 levels were detected independently of the activation signals [107,116]. These data suggest that re-exposing pDCs to TLR activation after 24 h may result in higher NLRP3 inflammasome activity due to significantly higher caspase-1 levels. However, we were not able to test our hypothesis due to the very short lifespan of human pDCs under in vitro conditions.
In general, two activation signals are required for classical, canonical NLRP3 activation [68]. First, the priming signal enhances NLRP3 and pro-IL-1β expression via the NF-κB pathway [23] as well as through the post-translational modification of NLRP3 [117,118] and primes the assembly of inflammasomes, which is then effectively activated by a secondary signal, including whole pathogens, PAMPs or DAMPs [27]. However, an alternative form of NLRP3 activation can be observed in some cell types, such as human monocytes, in which the priming signal alone may also result in NLRP3-dependent mature IL-1β production [119,120]. Furthermore, it has also been described that appropriate secondary signals alone can also evoke classical NLRP3 activation in monocytes [20]. The non-canonical inflammasome promotes pyroptosis and IL-1α release via triggering caspase-4/5 (caspase-11 in mice) activation in a caspase-1 independent manner [41]. Our results showed that in human pDCs, treatment with synthetic TLR ligands alone is insufficient to induce actual NLRP3 activation and mature IL-1β release. It is widely accepted that the TLR4 agonist lipopolysaccharide (LPS), a cell-wall component in Gram-negative bacteria, alone is able to activate NLRP3 inflammasome in monocytes, independently of a second signal [119]. Non-canonical inflammasome activation can also be triggered by cytosolic LPS that induces pyroptotic cell death upon binding to caspase-4/5/11 [41]. In our experiments, we found that the Gram-negative bacteria E. coli provides the strongest priming signal for human pDCs when compared to Gram-positive bacteria strains and the opportunistic fungi Candida albicans. However, similar to treatments with synthetic TLR ligands, E. coli alone did not induce mature IL-1β release, which is likely due to the fact that human pDCs, unlike mouse pDCs, do not express TLR4 [5,121].
Thus, we investigated which secondary signals might induce NLRP3 assembly in the human GEN2.2 pDC cell line following priming and found, that, of the secondary signals we tested, only the potassium ionophore and bacterial toxin, nigericin [76], was able to induce detectable levels of mature IL-1β already after 1 h of treatment. This may suggest that canonical NLRP3 inflammasome activation in pDCs requires potassium efflux. Interestingly, we found that, pDCs do not express the ATP sensing P2X7 receptor, which, in contrast, is highly expressed by monocytes, macrophages and monocyte-derived DCs; thus, it is likely that this potent endogenous danger signal does not function as an NLRP3 activator in pDCs [107,122,123].
After we determined the stimulatory conditions for NLRP3 activation in the human pDC cell line, we repeated our experiments with primary pDCs as well. Recently, it has become apparent that peripheral blood pre-DCs, which can serve as potential precursors for both cDC1 and cDC2 blood DCs, also expresses pDC-specific markers, including CD123, BDCA2 (CD303) and BDCA4 (CD304) proteins, that are commonly used to isolate pDCs [124]. Furthermore, additional markers, such as CD2 [125], CD5 [126], AXL [127] and CD33 [128] proteins, are currently being used to monitor the composition or the purity of the pDC population or even to sort pDCs. Thus, magnetic cell sorting based on BDCA4 expression requires an additional sorting step using a combination of various cell surface markers [54,129,130]. Thus, lately, pDCs have been generally sorted as Lin-CD11c-CD4+CD2-CD5-AXL- cells [131]. In the present study, to avoid cellular stress caused by sorting, which could potentially affect the redox status, metabolic state and viability of cells [132], we identified the pDC population within PBMCs and assessed the activity of NLRP3 pathway components by intracellular staining using flow cytometry. Previously, our laboratory has described that without using any other cell surface markers, BDCA4 positivity combined with light scatter parameters alone is suitable to identify pDCs in peripheral blood [133]. In the present study, we also showed that a second gating based on light scatter parameters applied after gating for BDCA4 can achieve a highly clear pDC population and is adequate to exclude the CD33+ pre-DC population, too.
In the gated primary pDC population, we observed a similar NLRP3 activation pattern, as previously seen in GEN2.2 cells, i.e., CpG-B and imiquimod were shown to be the strongest priming signals for pro-IL-1β induction and, in combination with nigericin, for mature IL-1β production, compared to CpG-A. Similarly, priming or a secondary signal alone could not induce detectable levels of bioactive IL-1β in primary pDCs. In contrast to our results, some literature data demonstrate that primary pDCs produce detectable levels of IL-1β, even in the absence of secondary signals. One study showed that primary pDCs secrete low levels of IL-1β (approximately 20–35 pg/mL) after a 24 h imiquimod (R837) treatment, [134] and another study found that upon co-culture with epithelial cells, pDCs can serve as a source of IL-1β [135]. Furthermore, the latter study showed IL-1β concentrations as high as 100–200 pg/mL in the supernatants of untreated pDC that would suggest a constantly active IL-1β secretion pathway in resting pDCs [135]; however, that is hard to imagine in the absence of activation-induced pro-IL-1β. Of note, in both papers, a one-step magnetic cell separation based on BDCA4 positivity was used to isolate primary pDCs without any additional sorting steps [134,135], which implies inadvertent contamination with pre-DCs based on recent DC classification models [124]. This contamination may cause false-positive results, especially when experiments target functions majorly associated with myeloid DC activity, such as IL-1β or IL-12 production, and not the unique type I IFN producing capacity of pDCs [136]. For instance, IL-12 production detected in human pDC cultures is a result of contamination with pre-DCs [124]. However, there are currently no data about the IL-1β releasing activity of the pre-DC population. In addition, a recent study also used intracellular labeling and flow cytometry to detect IL-1β in PBMC and demonstrated IL-1β positivity in a gated pDC population after 4 h of CL-087 (TLR7 ligand) treatment without using secondary activation [88]. However, it should be pointed out that the anti-IL-1β antibody used by the authors can detect both the pro- and mature form of the cytokine, according to the manufacturer’s protocol; thus, it is likely that the pro-form caused the positivity for IL-1β [88]. Furthermore, the CD123 and CD303 (BDCA2) markers used to identify pDCs in PBMC are not enough to exclude the presence of contaminating DC populations [92,124].
Our further results also highlighted that TLR ligands, which induce a high type I IFN response, such as CpG-A, are unable to induce IL-1β production in pDCs, in contrast to CpG-B. Although both CpG-A and CpG-B activate TLR9, the two ODN sequences elicit different responses by pDCs due to their structural differences. CpG-A ODNs are able to form higher-order multimeric structures due to their palindromic sequence and poly(G) motifs, whereas CpG-B ODNs form linear structures and lack the potential to form multimers [79]. Therefore, CpG-A molecules are retained in early endosomes and lead to high levels of type I IFN secretion in pDCs via activation of the transcription factor interferon regulatory factor (IRF) 7. On the contrary, monomeric CpG-B is rapidly transported to late endosomes, where it mainly facilitates pro-inflammatory cytokine production via NF-κB activation and exhibits a very low potential to induce type I IFN production in pDCs. Therefore, we hypothesized that the strong ability of pDCs to produce type I IFN may also contribute to the low NLRP3 inflammasome activity, as compared to myeloid cells. Indeed, we found that, when pDCs were pretreated with recombinant human IFN-α or viruses inducing type I IFNs, the potent NLRP3 activators of pDCs, including CpG-B or E. coli, were unable to induce large amounts of IL-1β production. Studies using other cell types also indicate that type I IFNs can inhibit NLRP3 activation [40,41,80]. It is also known that bacterial superinfections are common after viral infections that may be partly due to the inhibitory effect of the virus-triggered IFN pathway on the bacteria-induced IL-1β pathway [41]. Interestingly, vice versa, IL-1β can also inhibit the secretion of type I IFNs by enhancing the production of eicosanoid lipid mediators, such as prostaglandin E2 [48]. In line with that, we observed that the presence of IL-1β inhibits CpG-A-mediated IFN-α production in pDCs. All these data indicate that viral superinfections can also develop after severe bacterial infections. It is interesting to note, for example, that IFN-α/β therapy for viral hepatitis was ineffective in 60% of cases that could be due to the IL-1β-mediated inflammation in these patients. It was demonstrated using a hepatic cell model system that the antagonistic effect of IL-1β on the antiviral activity of IFN-α/β is owing to their potential to inhibit IFN-α/β-activated STAT1 and downregulate the expression of antiviral proteins [49]. It has also been observed that ASC and caspase-1-deficient DCs and macrophages have increased levels of type I IFNs [137] and NLRP3 or caspase-1-deficient mice also exhibited a greater type I IFN response [138].
Interactions between type I IFN and IL-1β pathways may play an important role not only during pathogen-induced inflammation, but also in the regulation of the pathomechanisms of various autoimmune diseases. Furthermore, the inhibitory effect of type I IFNs on NLRP3 inflammasome activity may also be an important therapeutic option in the treatment of certain pathologies. For example, in patients with MS with increased NLRP3 activity, IFN-β therapy could suppress the increased activity of the inflammasome that might help to reduce the patients’ symptoms [83]. Both pDCs and NLRP3 receptor overexpression play a role in the pathogenesis and pathomechanism of various autoimmune diseases. Numerous single nucleotide polymorphisms (SNPs) of NLRP3, which are mainly gain-of-function mutations, have been described, for example, in SLE, IBD, MS, RA and psoriasis [139,140]. In addition, pDCs may also play a role in the pathogenesis of psoriasis, since self-nucleic acids released by dying cells in complex with overproduced LL37 cationic antimicrobial peptides induce the persistent activation and excessive type I IFN production of pDCs, which promotes the development of T cell-mediated autoimmune responses [141,142]. Therefore, psoriasis is characterized by a high IFN signature [81]. In the present work, we showed that pDCs from psoriasis patients have significantly lower activation-induced NLRP3 activity compared to healthy subjects, underlying our hypothesis that pDCs with high type I IFN activity have low NLRP3 activity due to the inhibitory effects of type I IFNs on the NLRP3 pathway.
By binding to their receptors, type I IFNs can activate the STAT1 transcription factor, which can increase the expression of several negative regulatory molecules, including CH25H, IL-10, IL1RA, iNOS, SOCS1, POP or COP molecules, which either inhibit IL-1β formation at the mRNA level or suppress secondary signals required for NLRP3 activation or directly interact with NLRP3 inflammasome components and inhibit their assembly [40,41,80]. Of these inhibitory mechanisms, IFN-induced IL-10 inhibition is unlikely to occur in pDCs, as data suggest that pDCs are unable to produce IL-10 [143]. Furthermore, pDCs are also not characterized by nitric oxide (NO) synthesis, as they have very low levels of iNOS and, thus, it is unlikely that NO would inhibit NLRP3 through nitrosylation [144]. However, we found that in human pDCs, the expression of CH25H, SOCS1 and COP1 is significantly increased in the presence of high IFN response-inducing activation signals and we found that the levels of these inhibitory molecules are significantly higher in pDCs from psoriasis patients with high type I IFN levels compared with those from healthy controls. Therefore, we suppose that CH25H inhibits IL-1β transcription, SOCS1 blocks NLRP3 activation and COP1 suppresses NLRP3-dependent activation of caspase-1 in pDCs with high type I IFN pathway activity [82,83,84].
In addition, we found that the overall expression of NLRP3, ASC, IL-1β and caspase-1 is higher in the peripheral blood of psoriatic patients compared to normal controls, implying that overactivation of the NLRP3 inflammasome may also contribute to psoriasis-associated inflammatory responses [85,145,146,147]. In addition, examining the CD14+ monocyte population of patients, we also observed elevated baseline cleaved caspase-1 expression, as compared to healthy controls. It is well known that monocytes have a higher and presumably constant caspase-1 activity compared with macrophages [116,148]. When we compared the levels of NLRP3 pathway components in pDCs and monocytes, we found that the frequency of NLRP3, ASC and pro-caspase-1-positive cells was similar between the two cell populations. Interestingly, the level of pro-caspase-1 expression is significantly higher in monocytes compared to pDCs that supports the idea that the caspase-1-dependent IL-1β production capacity of pDCs may indeed be much lower compared to myeloid cells. However, there is no difference in the expression values of NLRP3 and ASC between the two cell types.
Furthermore, in contrast to pDCs, monocytes from psoriasis patients do not show a reduced NLRP3 activity in response to the same activation signals. The reason behind this might be that the NLRP3 activity of monocytes is not affected as strongly as of pDCs by the inhibitory effects of type I IFNs, since their capacity to produce type I IFNs is several orders of magnitude lower compared to pDCs [1,149]. This is also supported by our findings demonstrating that in contrast to pDCs, CpG-A was able to induce pro-IL-1β, cleaved IL-1β and cleaved caspase-1 expression in monocytes. Several studies have already shown that TLR activation does not or only very slightly induces type I IFN release by monocytes [88,89,90,91]. Although literature data suggest that activated monocytes from psoriasis patients show significantly higher NLRP3 activity than healthy controls and that also contributes to the disease pathology [85,86,87], we could not detect differences in NLRP3 activity between the two groups. It is likely that in our present experiments, we were unable to detect increased NLRP3 activity in patients’ monocytes because we used activation signals tailored to pDCs and, though monocytes express TLR7 [150] and TLR9 [151,152,153] receptors, these cells cannot be strongly stimulated through them. Furthermore, the secretion [154,155] and the constant activity [116,148] of caspase-1 in monocytes also complicate intracellular protein analysis by flow cytometry.
In conclusion, we revealed that human pDCs also express NLRP3 pathway components, the expression of which is differentially affected by distinct activation signals. Furthermore, we show that NLRP3 is functional in these cells, as mature IL-1β secretion can be induced in human pDCs by using a combination of priming and specific secondary activation signals. Nevertheless, we also demonstrated that NLRP3 activity in pDCs is much lower than that of other myeloid cells, due to their low baseline caspase-1 expression and high type I IFN pathway activity. In fact, activation stimuli that induce a high type I IFN response in pDCs also increase the expression of various regulatory molecules, inhibiting NLRP3-mediated IL-1β secretion. Thus, the IL-1β-mediated immune response of pDCs may predominantly prevail under conditions that are not associated with increased type I IFN pathway activity. Our results also indicate that the interplay between the type I IFN and IL-1β pathways is an important regulator of both pathogen-induced and sterile autoimmune inflammatory reactions.
4. Materials and Methods
4.1. GEN2.2 Cell Line
The human pDC cell line (GEN2.2) [102] used in our experiments was provided by Dr. Joel Plumas and Dr. Laurence Chaperot (Research and Development Laboratory, French Blood Bank Rhône-Alpes, Grenoble, France) and was deposited with the CNCM (French National Collection of Microorganism Cultures) under the number CNCMI-2938. GEN2.2 cells were grown on a layer of mitomycin C (Sigma-Aldrich, St. Louis, MO, USA, Cat. No. M4287)-treated murine MS5 feeder cells (Leibniz Institute DSMZ-German Collection of Microorganisms and Cell Cultures, Braunschweig, Germany, Cat. No. ACC 441) in RPMI 1640 medium (Sigma-Aldrich, Cat. No. R8758) supplemented with 10% heat-inactivated FBS (Life Technologies Corporation, Carlsbad, CA, USA, Cat. No. 10270-106), 100 U/mL penicillin, 100 μg/mL streptomycin (both from Biosera, Nuaille, France, Cat. No. XC-A4122/100) and 5% non-essential amino acids (Life Technologies Corporation, Cat. No. 11140050). For experiments, the GEN2.2 cells were removed from the feeder layer and seeded on 24-well plates at a concentration of 5 × 105 cells/500 μL in complete RPMI 1640 medium (Sigma-Aldrich). Cell lines were grown and incubated at 37 °C in a 5% CO2 humidified atmosphere.
4.2. Collection of Human Blood Samples and Isolation of PBMCs
Patient blood samples were provided to us by the Laboratory of Regenerative Medicine and Cellular Pharmacology (Department of Dermatology and Allergology, University of Szeged, Szeged, Hungary). The collection of peripheral blood samples complied with the guidelines of the Helsinki Declaration and was approved by the National Public Health and Medical Officer Service (NPHMOS) and the National Medical Research Council (administrative number: 13740-5/2021/EÜIG and 4969; 90/2021-SZTE IKEB, protocol code: PSO-CELL-01) which follows the EU Member States’ Directive 2004/23/EC and GDPR on presumed written consent practice for tissue collection.
Men or women aged 25 to 65 years suffering from plaque psoriasis with a psoriasis area sensitivity index (PASI) greater than 15 were included in the study. Patients who received systemic treatment (biological or traditional) or total body phototherapy were excluded. Peripheral blood of healthy, gender and age-matched donors was used as a control in experiments with psoriasis samples. To characterize the NLRP3 pathway in healthy individuals, 23–55-year-old volunteers were selected for peripheral blood donation.
Then, 25 mL of peripheral blood was collected from psoriatic and healthy donors into 10 mL BD Vacutainer® Plastic whole blood tubes with spray-coated K2EDTA (BD Biosciences, San Jose, CA, USA, Cat. No. 366643). The blood was diluted 1:1 with physiological saline (NaCl 0.9%, B. Braun, Melsungen, Germany) and then PBMCs were separated by Ficoll-Paque Plus (Cytiva Sweden AB, Uppsala, Sweden, Cat. No. 17144003) gradient centrifugation. Freshly isolated PBMCs were seeded in FACS tubes at a density of 1 × 106 cells/ 500 mL RPMI 1640 medium (Sigma-Aldrich) supplemented with 10% heat-inactivated FBS (Life Technologies Corporation), 2 mM L-glutamine, 100 U/mL penicillin and 100 μg/mL streptomycin (all from Biosera).
4.3. Stimulation and Treatments of the Cells
To prime the NLRP3, inflammasome cells were incubated with 1 μM CpG-A (ODN 2216; Hycult Biotech, Uden, The Netherlands, Cat. No. HC4037), 1 μM CpG-B (ODN 2006; Hycult Biotech, Cat. No. HC4039) or 5 μg/mL imiquimod (IMQ) (InvivoGen, San Diego, CA, USA, Cat. No. tlrl-imq) in fresh, complete RPMI 1640 medium for the indicated times. In order to activate the inflammasome secondary activation signals including 20 μM nigericin (InvivoGen, Cat. No. tlrl-nig), 5 mM ATP (Invivogen, Cat. No. tlrl-atpl), 250 µg/mL Alum (Thermo Scientific, Cat. No. 77161), 300 µg/mL MSU (Sigma-Aldrich, Cat. No. 1198-77-2) or antimycin A (0.5 µg/mL, Sigma-Aldrich, Cat. No. A8674) were added to the cells after priming without a washing step and then the cells were incubated for 1, 2, 4 or 6 h.
In separate experiments, cells were primed with Escherichia coli (E. coli) ATCC11775, Bacillus subtilis ATCC6051, Lactobacillus rhamnosus ATCC53103, Candida albicans ATCC10231, Vesicular Stomatitis Virus (VSV; Indiana strain [156]) or Herpes Simplex Virus 1 (HSV; KOS serotype, ATCC-VR-1493) at a MOI of 10 for bacteria and viruses or 0.01 for Candida for the indicated times. Bacteria and Candida were provided by Dr. Walter Pfliegler (Department of Molecular Biotechnology and Microbiology, Faculty of Science and Technology, University of Debrecen, Debrecen, Hungary). Viruses were kindly provided by Dr. Eszter Csoma (Department of Medical Microbiology, Faculty of Medicine, University of Debrecen, Debrecen, Hungary). After priming with microbes, cells were incubated with 20 μM nigericin (InvivoGen, Cat. No. tlrl-nig) for the indicated times. In some experiments cells were pretreated with VSV and HSV for 3 h before E. coli and nigericin (InvivoGen) treatments.
In parallel experiments 1 µM MCC950 (Invivogen, Cat. No. inh-mcc) or 20 µM Z-YVAD-FMK (BioVision Incorporated, Milpitas, CA, USA, Cat. No. 1012-100) was added to the cells in the last 30 min of the priming and then cells were exposed to the secondary signals without any washing step.
The experiments performed with CpG-B were repeated in the presence of 50 μg/mL recombinant human IFN-α (Abcam, Cambridge, UK, Cat. No. ab48750) as well. In detail, IFN-α was added to the cells 30 min before the CpG-B priming and then the cells were exposed to nigericin without a washing step. Similarly, the experiments with CpG-A were repeated in the presence of 10, 50 or 100 ng/mL recombinant human IL-1β (Peprotech, Cat. No. 200-01B). IL-1β was added to the cells 30 min before the CpG-A treatment.
4.4. Generation and Activation of Primary Macrophages
Human heparinized leukocyte-enriched buffy coats were obtained from healthy blood donors drawn at the Regional Blood Center of Hungarian National Blood Transfusion Service (Debrecen, Hungary) in accordance with the written approval of the Director of the National Blood Transfusion Service and the Regional and Institutional Ethics Committee of the University of Debrecen, Faculty of Medicine (Debrecen, Hungary). PBMCs were separated from buffy coats by Ficoll-Paque Plus (Cytiva) gradient centrifugation. Monocytes were purified from PBMCs by positive selection using magnetic cell separation with anti-CD14-conjugated microbeads (Miltenyi Biotech, Bergish Gladbach, Germany, Cat. No. 130-050-201). Monocytes were cultured in 24-well cell culture plates at a density of 5 × 105 cells/500 μL in RPMI 1640 medium (Sigma-Aldrich) supplemented with 10% heat-inactivated FBS (Life Technologies Corporation), 2 mM L-glutamine (Biosera), 100 U/mL penicillin, 100 μg/mL streptomycin (both from Biosera) and 50 ng/mL recombinant human M-CSF (Peprotech, Cat. No. 300-25), then activated with 250 ng/mL Ultrapure LPS, E. coli 0111:B4 (Invivogen, Cat. No. tlrl-3pelps) for the indicated times. Cells were incubated at 37 °C in a 5% CO2 humidified atmosphere.
4.5. Flow Cytometric Analysis
PBMCs were stained with anti-CD14-FITC (BioLegend, San Diego, USA, Cat. No. 301804) and anti-BDCA4-APC (CD304, Neuropilin-1, BioLegend, Cat. No. 354506), then were fixed and permeabilized with BD Cytofix/CytopermTM Plus Fixation/Permeabilization Kit (BD Biosciences, San Diego, CA, USA, Cat. No.554714) according to the manufacturer’s instructions. After washing the cells were incubated with anti-NLRP3 (clone D2P5E, Cat. No. 13158S), anti-ASC (clone E1E3I; Cat. No. 13833S), anti-IL-1β (clone D3U3E; Cat. No. 12703S), anti-cleaved IL-β (Asp116; clone D3A3Z; Cat. No. 83186S), anti-caspase-1 (clone D7F10; Cat. No. 3866S) and anti-cleaved caspase-1 (Asp297; clone D57A2; Cat. No. 4199S) antibodies (all from Cell Signaling, Danvers, MA, USA) for 30 min. After washing the cells were incubated with PE-conjugated IgG1 secondary antibody (Cat. No. 406421; BioLegend) for 30 min. As an isotype control rabbit IgG (Cell Signaling, clone DA1E, Cat. No. 3900S) was used. As a final step, cells were taken up in 2% paraformaldehyde (Alfa Aesar, Haverhill, MA, USA, Cat. No. J61899). Fluorescence intensities were measured with FACSCalibur flow cytometer (BD Biosciences) and data were analyzed with FlowJo software (TreeStar, Ashland, OR, USA). Throughout data acquisition, 600,000 events were acquired from each sample containing 1,000,000 stained cells. Threshold of FSC was set to 150 to exclude cell debris. Monocytes were identified as CD14-positive cells. pDCs were first recognized as being BDCA4 positive. After this step, the distribution of the cells within the BDCA4+ gate was analyzed by back gating on the light scatter parameters to exclude non-pDCs. BDCA4+ cells in the region 400–600 of FSC were identified as pDCs.
To analyze the phenotype of gated pDCs the following antibodies were used: LIN-FITC (BD Biosciences, Cat. No. 340546), CD2-FITC (Immunotech-Beckman Coulter, Marseille, France, Cat. No. PN IM0442), CD5-PE (PharMingen-BD Biosciences, Cat. No. 555353), CD11c-PE (Immunotech-Beckman Coulter, Cat. No. PN IM1760U), AXL-Alexa FluorTM 488 (R&D Systems Minneapolis, MN, USA, Cat. No. FAB154G), CD33-FITC (eBioscience, Cat.No. 11-0337-42) and CD123-PE-Cy7 (Biolegend, Cat. No. 301804).
4.6. Confocal Microscopy
Activated PBMCs were stained with anti-BDCA4-APC (CD304, Neuropilin-1, BioLegend, Cat. No. 354506) for 30 min at 4 °C then were fixed and permeabilized with BD Cytofix/CytopermTM Plus Fixation/Permeabilization Kit (BD Biosciences) according to the manufacturer’s instructions. After washing cells were incubated with anti-cleaved IL-1β (Asp116; clone D3A3Z; Cat. No. 83186S) or anti-cleaved caspase-1 (Asp297; clone D57A2; Cat. No. 4199S) antibodies (all from Cell Signaling) for 30 min at 4 °C. After washing cells were incubated with PE-conjugated IgG1 secondary antibody (Cat. No. 406421; BioLegend) for 30 min at 4 °C. As an isotype control rabbit IgG (Cell Signaling, clone DA1E, Cat. No. 3900S) was used. Stained cells were dissolved in Mowiol® 4–88 mounting media (Sigma-Aldrich, Cat. No. 81381).
For confocal microscopy 100,000 cells were pipetted on 8-well μ-Slides (chambered coverslip, ibidi GmbH). Cells were visualized immediately by a Zeiss LSM880 confocal microscope. BDCA4-APC was excited at 633 nm and IgG1-PE was excited at 543 nm. Fluorescence emission was detected through 650 to 670 nm and 560 to 615 nm band-pass filters. Images were taken in multi-track mode to prevent cross-talk. Image stacks of 1024 × 1024 pixel, 1.5 μm thick optical sections were obtained with a 40× C-Apochromat water immersion objective (NA = 1.2).
4.7. Quantitative Real-Time PCR
Total RNA was isolated from 5 × 105 GEN2.2 cells or 1 × 106 PBMCs using Tri Reagent (Molecular Research Center, Inc., Cincinnati, OH, USA, Cat. No. TR118). Total RNA was treated with DNase I (Thermo Fisher Scientific, Waltham, MA, USA, Cat. No. AM2222) to exclude amplification of genomic DNA then reverse transcribed into cDNA using the High-Capacity cDNA RT Kit of Applied Biosystems (Thermo Fisher Scientific, Cat. No. 4374966). Gene expression assays were purchased from Thermo Fisher Scientific for NLRP3 (Assay ID: Hs00918082_m1, Cat. No. 4331182), IL-1β (Assay ID: HS00174097_m1, Cat. No. 4331182), IL-18 (Assay ID: Hs01038788_m1, Cat. No. 4331182), IL-1α (Assay ID: Hs00174092_m1, Cat. No.), caspase-1 (Assay ID: Hs00354836_m1, Cat. No. 4331182), PYCARD/ASC (Assay ID: Hs00203118_m1, Cat. No. 4331182), P2X7 (Assay ID: Hs00175721_m1, Cat. No. 4331182), CH25H (Assay ID: Hs02379634_s1, Cat. No. 4331182), SOCS1 (Assay ID: Hs00705164_s1, Cat. No. 4331182), CARD16 (Assay ID: Hs00430993_m1, Cat. No. 4331182), IL1RN (Assay ID: Hs00893626_m1, Cat. No. 4331182), NOS1 (Assay ID: Hs00167223_m1, Cat. No. 4331182) and Integrated DNA Technologies (Coralville, IA, USA) for IFNA1 (Assay ID: Hs.PT.49a.3184790.g) and PPIA (cyclophilin A; Assay ID: Hs.PT.58v.38887593.g). Quantitative PCR was performed using the ABI StepOne Real-Time PCR System (Thermo Fisher Scientific) and cycle threshold values were determined using the StepOne v2.1 Software (Thermo Fisher Scientific). The relative amount of mRNA was obtained by normalizing to the PPIA housekeeping gene in each experiment.
4.8. Western Blotting
For Western blotting 5 × 105 GEN2.2 cells were lysed in Laemmli buffer, heated at 100 °C for 10 min, separated on 10 or 15% SDS-PAGE then electro-transferred to nitrocellulose membranes (Bio-Rad Laboratories GmbH, Munich, Germany). Non-specific binding sites were blocked with 5% non-fat dry milk diluted in TBS Tween buffer (50 mM Tris, 0.5 M NaCl, 0.05% Tween-20, pH 7.4). Membranes were probed with the anti-NLRP3 (clone D2P5E, Cat. No. 13158S), anti-ASC (clone E1E3I; Cat. No. 13833S), anti-IL-1β (clone D3U3E; Cat. No. 12703S) and anti-caspase-1 (clone D7F10; Cat. No. 3866S) (all from Cell Signaling). Beta-actin was used as a loading control (Santa Cruz Biotechnology, clone C4; Cat. No. sc-47778). The bound primary antibodies were conjugated with anti-mouse (Bio-Rad, Cat. No. 1721011) or anti-rabbit (GE Healthcare, Cat. No. NA934) horseradish peroxidase-conjugated secondary antibodies at a dilution of 1:5000 and 1:10,000, respectively, and were visualized by the ECL system using SuperSignal West Pico or Femto chemiluminescent substrate (Thermo Fisher Scientific, Rockford, IL, United States) and X-ray film exposure. Densitometric analysis of immunoreactive bands was performed using Image Studio Lite Software version 5.2 (LI-COR Biosciences, Lincoln, NE, United States).
4.9. ELISA
Cell culture supernatants were collected at the indicated time points and the IL-1β (Cat. No.557953), TNF (Cat. No. 555212), IL-6 (Cat. No. 555220) and IL-8 (Cat. No. 555244) levels were determined by the BD OptEIA human ELISA kits (all from BD Biosciences, San Diego, CA, USA). IFN-α levels were measured by the VeriKineTM Human Interferon Alpha ELISA kit (PBL Interferon Sources, Piscataway, NJ, USA). Assays were performed according to the manufacturer’s instructions. Absorbance measurements were carried out by a Synergy HT microplate reader (Bio-Tek Instruments, Winooski, VT, USA) at 450 nm.
4.10. Statistical Analysis
Data are expressed as the mean ± SD and analyzed by ANOVA, followed by Bonferroni post hoc test or paired Student t test. Data analyses were performed using GraphPad Prism v.6 software (GraphPad Software Inc., La Jolla, CA, USA). Differences were considered to be statistically significant at p < 0.05.
5. Conclusions
In the current study, we focused on pDCs, which are generally protective immune cells and specialized for the elimination of invading viruses. However, pDCs can play a deleterious role in the pathogenesis of various autoimmune disorders, when the overactivated pDCs respond to self-molecules of the body and facilitate immune responses against healthy tissues, leading to chronic inflammation and extensive tissue damage. The activation of pDCs is primarily mediated by their well-known pattern recognition receptors; however, currently, little is known about the expression of inflammasome-forming receptors in pDCs so far. A growing body of evidence indicates that the excessive activation of inflammasomes can also contribute to the development of various autoimmune diseases. Moreover, there remains controversy in the scientific literature over whether or not inflammasomes and the IL-1β pathway are functional in pDCs. Our present findings demonstrate that the NLPR3 inflammasome can be active in pDCs; however, a specific combination of priming and secondary signals is required for the NLRP3-depedent IL-1β production of pDCs. Nevertheless, compared to the high type I IFN producing capacity of pDCs, their IL-1β secretion is overshadowed by that of other myeloid cell types due to the inhibitory effects of type I IFNs on NLRP3 activity. Therefore, a deeper insight into the regulatory mechanisms of this process would allow us to better understand the features of pDCs under various conditions and especially in pDC-associated disorders.
K.P., D.B. and T.F. designed the research, performed experiments, analyzed and interpreted data and wrote the manuscript. W.P., Á.S. and E.C. performed experiments and participated in data analysis. A.S., T.T. and L.K. provided conceptual insight and revised the manuscript. K.P., Z.V. and A.B. contributed with essential reagents. All authors have read and agreed to the published version of the manuscript.
Patient blood samples were provided to us by the Laboratory of Regenerative Medicine and Cellular Pharmacology (Department of Dermatology and Allergology, University of Szeged). The collection of peripheral blood samples complied with the guidelines of the Helsinki Declaration and was approved by the National Public Health and Medical Officer Service (NPHMOS) and the National Medical Research Council (administrative number: 13740-5/2021/EÜIG and 4969; 90/2021-SZTE IKEB, protocol code: PSO-CELL-01), which follows the EU Member States’ Directive 2004/23/EC and GDPR on presumed written consent practice for tissue collection.
Informed consent was obtained from all subjects involved in this study to publish this paper.
The data presented in this study are available in the article’s Figures and in
GEN2.2 cells used in this study were generously provided by Joel Plumas and Laurence Chaperot of Research and Development Laboratory, EFS Rhônes-Alpes, 29 Av Maquis du Gresivaudan, BP 35, 38701 La Tronche, France. We would like to thank Angéla Berki-Pál for her valuable assistance during the laboratory work. The authors would like to thank the patients and healthy individuals who agreed to participate in this study.
The authors declare no conflict of interest.
Publisher’s Note: MDPI stays neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Enlarge this image.Figure 1. Distinct TLR agonists have different effects on the expression of NLRP3 inflammasome pathway components in the human GEN2.2 pDC cell line. GEN2.2 cells were treated with 1 μM CpG-A, 1 μM CpG-B or 5 μg/mL IMQ in a time-dependent manner (A,B). The expression of NLRP3, ASC, pro-caspase-1 and pro-IL-1β was measured at the protein level by Western blotting. Representative blots are shown in (A). Data are shown as mean ± SD from 5 independent experiments in panel (B). Data were analyzed using one-way ANOVA followed by Bonferroni’s post hoc test. * p < 0.05, ** p < 0.01, *** p < 0.001 vs. control (ctrl). IMQ: imiquimod.
Enlarge this image.Figure 2. Pathogenic bacteria influence the expression of NLRP3 inflammasome pathway components in the human GEN2.2 pDC cell line. GEN2.2 cells were treated with E. coli (MOI 10) in a time-dependent manner (A,B). The expression of NLRP3, ASC, pro-caspase-1 and pro-IL-1β was measured at the protein level by Western blotting. Representative blots are shown in (A). Data are shown as mean ± SD from 5 independent experiments in (B). Data were analyzed using one-way ANOVA followed by Bonferroni’s post-hoc test. * p < 0.05, ** p < 0.01 vs. control (ctrl). EC: E. coli.
Enlarge this image.Figure 3. A secondary stimulus is required for the secretion of NLRP3-dependent IL-1β in the human GEN2.2 pDC cell line. GEN2.2 cells were pretreated with 1 μM CpG-A, 1 μM CpG-B or 5 μg/mL IMQ for 3 h, then 20 μM nigericin was added to the cells in a time-dependent manner (A). In parallel experiments, cells were incubated in the presence of 1 μM MCC950 (specific NLRP3 inhibitor) for the last 30 min of TLR stimulation prior to nigericin exposure (A). In similar experiments, GEN2.2 cells were primed with live E. coli (MOI 10), Bacillus subtilis (MOI 10), Lactobacillus rhamnosus (MOI 10) and Candida albicans (MOI 0.01), then nigericin was added to the cells in a time-dependent manner (B). Similarly, in a parallel experiment, cells were incubated with MCC950 for the last 30 min of the microbial stimulation prior to nigericin treatment (B). IL-1 β secretion was measured by ELISA (A,B). Data are represented as mean ± SD of 6 individual experiments and were analyzed using one-way ANOVA followed by Bonferroni’s post-hoc test. ** p < 0.01, *** p < 0.0001, **** p < 0.0001 vs. control (ctrl), # p < 0.05, ## p < 0.01, ### p < 0.0001, #### p < 0.0001. ND: not determined, IMQ: imiquimod, NIG: nigericin, EC: Escherichia coli, BS: Bacillus subtilis, LR: Lactobacillus rhamnosus, CA: Candida albicans.
Enlarge this image.Figure 4. The baseline expression of NLRP3 inflammasome pathway components in primary human pDCs. The NLRP3, ASC, pro-caspase-1, cleaved caspase-1, pro-IL-1β and cleaved IL-1β expressions in primary human pDCs gated from PBMCs were measured using intracellular flow cytometry. Representative dot plots are shown in (A). Green dots indicate isotype controls and red dots show the specific proteins (A). Data are represented as mean ± SD of 22 individual experiments and analyzed using one-way ANOVA followed by Bonferroni’s post-hoc test (B). SSC: side scatter.
Enlarge this image.Figure 5. TLR ligands differ in their IL-1β inducing capacity in primary human pDCs. PBMCs were separated from peripheral blood of healthy donors, then the cells were analyzed by flow cytometry for pDCs. PBMCs were primed with 1 μM CpG-A or 1 μM CpG-B or 5 μg/mL IMQ for 2.5 h (A–D). In parallel, 20 μM nigericin was applied for 1 h to induce the NLRP3-dependent cleavage of caspase-1 and IL-1β, where it is indicated (B,D). The percentage of pro-caspase-1 (A), cleaved caspase-1 (B), pro-IL-1β (C) and cleaved IL-1β (D) -positive cells was determined within the pDC population using intracellular flow cytometry. Representative dot plots are shown in (A–D). Green dots indicate isotype controls and red dots show the specific proteins (A–D). Data are represented as means ± SD of 22 individual experiments and analyzed using one-way ANOVA followed by Bonferroni’s post-hoc test. **** p < 0.0001 vs. control (ctrl). IMQ: imiquimod, NIG: nigericin, SSC: side scatter.
Enlarge this image.Figure 6. IFN-α pretreatment inhibits the IL-1β production in the human GEN2.2 pDC cell line. Cells were pretreated with 50 μg/mL recombinant IFN-α for 30 min, then activated with 1 μM CpG-B for 3 or 6 h (A,C). To induce IL-1β secretion CpG-B-treated cells were incubated in the presence of 20 μM nigericin for 4 h (C). The expression of IL1B was determined at the mRNA level by qPCR (A) and at the protein level by Western blotting (B) and ELISA (C). A representative blot is shown in (B). Bar graphs represent the mean ± SD of 6 independent experiments. Data were analyzed using one-way ANOVA followed by Bonferroni’s post-hoc test. * p < 0.05, ** p < 0.01, *** p < 0.001 vs. control (ctrl), # p < 0.05, ## p < 0.01, ### p < 0.001. IFN: interferon, ND: not determined, NIG: nigericin.
Enlarge this image.Figure 7. Viral pretreatment inhibits the IL-1β production in the human GEN2.2 cell line. GEN2.2 cells were incubated in the presence of VSV or HSV at a MOI of 10 for 3 h. Then cells were activated with E. coli (MOI 10) for 3 or 6 h (A–C). To induce IL-1β secretion E. coli-treated cells were incubated in the presence of 20 μM nigericin in a time-dependent manner (C). The expression of IL1B was determined at the mRNA level by qPCR (A) and at the protein level by Western blotting (B) and ELISA (C). A representative blot is shown in (B). Bar graphs represent the mean ± SD of 4 independent experiments. Data were analyzed using one-way ANOVA followed by Bonferroni’s post-hoc test. * p < 0.05, ** p < 0.01, **** p < 0.0001 vs. control (ctrl), # p < 0.05, ## p < 0.01, ### p < 0.001, #### p < 0.0001. VSV: Vesicular Stomatitis Virus, HSV: Herpes Simplex Virus, EC: Escherichia coli, NIG: nigericin, ND: not determined.
Enlarge this image.Figure 8. VSV or HSV pretreatment inhibits the IL-1β production in primary human pDCs. PBMCs were separated from peripheral blood of healthy individuals, then the cells were analyzed by flow cytometry for pDCs. PBMCs were incubated in the presence of E. coli, VSV or HSV at a MOI of 10 (A). After priming, cells were incubated in the presence of 20 μM nigericin for 1 h, where it is indicated (B). In parallel experiments cells were pretreated with VSV or HSV (MOI 10) for 3 h and then activated with E. coli (MOI 10) for an additional 3 h (C). To induce the cleavage of IL-1β, nigericin was added to the cells for an additional 1 h (D). The percentage of pro-IL-1β (A,C) and cleaved IL-1β (B,D) -positive pDCs was measured using intracellular flow cytometry. Representative dot plots are shown in (A–D). Green dots indicate isotype controls and red dots show the specific proteins (A–D). Data are represented as means ± SD of 4 individual experiments and analyzed using one-way ANOVA followed by Bonferroni’s post-hoc test. **** p < 0.0001 vs. control (ctrl), ## p < 0.01, #### p < 0.0001. VSV: Vesicular Stomatitis Virus, HSV: Herpes Simplex Virus, EC: E. coli, NIG: nigericin, SSC: side scatter.
Enlarge this image.Figure 9. Characteristics of psoriasis patients. Peripheral blood was taken from healthy volunteers and psoriasis patients then PBMCs were separated using Ficoll-Paque gradient centrifugation and blood plasma was stored at -70 °C until analysis. The plasma concentration of IFN-α (A), IL-1β, TNF-α and IL-6 (B) was measured by ELISA. The percentage of pDCs was determined by flow cytometry (C). The baseline expression level of NLRP3 (D), ASC (E), caspase-1 (F) and IL1B (G) was measured by qPCR in PBMCs. In some experiments PBMCs were left untreated (H) or activated with 1 μM CpG-A, 1 μM CpG-B or 5 μg/mL IMQ for 2.5 h (I–K), then stimulated with 20 μM nigericin for 1 h to induce the NLRP3-dependent cleavage of IL-1β and caspase-1 (I–K). The baseline (H) and the activation induced (I–K) expression of NLRP3 inflammasome pathway components was measured in the gated pDC population by intracellular flow cytometry. Bar graphs represent the mean ± SD of 14 independent experiments. Data were analyzed using paired Student t test (A–F) and two-way ANOVA followed by Bonferroni’s post hoc test (H–K). * p < 0.05, ** p < 0.01, *** p < 0.001, **** p < 0.0001 vs. healthy control. ND: not determined, IMQ: imiquimod, NIG: nigericin.
Enlarge this image.Figure 10. Various NLRP3 pathway inhibitors are induced by the powerful type I IFN inducer TLR9 ligands and show elevated levels in psoriasis patients. GEN2.2 cells were treated with 1 μM CpG-A or 1 μM CpG-B in a time-dependent manner and the expression of CH25H, SOCS1 and COP1 was measured by qPCR (A). PBMCs were isolated from the peripheral blood of healthy volunteers and psoriasis patients and the relative expression of CH25H, SOCS1 and COP1 was determined by qPCR (B). Bar graphs represent the mean ± SD of 4–14 independent experiments. Data were analyzed using one-way ANOVA followed by Bonferroni’s post hoc test (A) or paired Student t test (B). * p < 0.05, ** p < 0.01, *** p < 0.001, **** p < 0.0001 vs. control (ctrl) or healthy control.
Supplementary Materials
The following supporting information can be downloaded at:
References
1. Siegal, F.P.; Kadowaki, N.; Shodell, M.; Fitzgerald-Bocarsly, P.A.; Shah, K.; Ho, S.; Antonenko, S.; Liu, Y.J. The nature of the principal type 1 interferon-producing cells in human blood. Science; 1999; 284, pp. 1835-1837. [DOI: https://dx.doi.org/10.1126/science.284.5421.1835]
2. Lande, R.; Gilliet, M. Plasmacytoid dendritic cells: Key players in the initiation and regulation of immune responses. Ann. N. Y. Acad. Sci.; 2010; 1183, pp. 89-103. [DOI: https://dx.doi.org/10.1111/j.1749-6632.2009.05152.x]
3. Ronnblom, L.; Eloranta, M.L.; Alm, G.V. Role of natural interferon-alpha producing cells (plasmacytoid dendritic cells) in autoimmunity. Autoimmunity; 2003; 36, pp. 463-472. [DOI: https://dx.doi.org/10.1080/08916930310001602128]
4. Bencze, D.; Fekete, T.; Pazmandi, K. Type I Interferon Production of Plasmacytoid Dendritic Cells under Control. Int. J. Mol. Sci.; 2021; 22, 4190. [DOI: https://dx.doi.org/10.3390/ijms22084190]
5. Kadowaki, N.; Ho, S.; Antonenko, S.; Malefyt, R.W.; Kastelein, R.A.; Bazan, F.; Liu, Y.J. Subsets of human dendritic cell precursors express different toll-like receptors and respond to different microbial antigens. J. Exp. Med.; 2001; 194, pp. 863-869. [DOI: https://dx.doi.org/10.1084/jem.194.6.863]
6. Bao, M.; Liu, Y.J. Regulation of TLR7/9 signaling in plasmacytoid dendritic cells. Protein Cell; 2013; 4, pp. 40-52. [DOI: https://dx.doi.org/10.1007/s13238-012-2104-8] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/23132256]
7. Szabo, A.; Magyarics, Z.; Pazmandi, K.; Gopcsa, L.; Rajnavolgyi, E.; Bacsi, A. TLR ligands upregulate RIG-I expression in human plasmacytoid dendritic cells in a type I IFN-independent manner. Immunol. Cell Biol.; 2014; 92, pp. 671-678. [DOI: https://dx.doi.org/10.1038/icb.2014.38]
8. Fekete, T.; Bencze, D.; Szabo, A.; Csoma, E.; Biro, T.; Bacsi, A.; Pazmandi, K. Regulatory NLRs Control the RLR-Mediated Type I Interferon and Inflammatory Responses in Human Dendritic Cells. Front. Immunol.; 2018; 9, 2314. [DOI: https://dx.doi.org/10.3389/fimmu.2018.02314]
9. Deb, P.; Dai, J.; Singh, S.; Kalyoussef, E.; Fitzgerald-Bocarsly, P. Triggering of the cGAS-STING Pathway in Human Plasmacytoid Dendritic Cells Inhibits TLR9-Mediated IFN Production. J. Immunol.; 2020; 205, pp. 223-236. [DOI: https://dx.doi.org/10.4049/jimmunol.1800933] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/32471881]
10. Zheng, D.; Liwinski, T.; Elinav, E. Inflammasome activation and regulation: Toward a better understanding of complex mechanisms. Cell Discov.; 2020; 6, 36. [DOI: https://dx.doi.org/10.1038/s41421-020-0167-x] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/32550001]
11. Minkiewicz, J.; de Rivero Vaccari, J.P.; Keane, R.W. Human astrocytes express a novel NLRP2 inflammasome. Glia; 2013; 61, pp. 1113-1121. [DOI: https://dx.doi.org/10.1002/glia.22499] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/23625868]
12. Khare, S.; Dorfleutner, A.; Bryan, N.B.; Yun, C.; Radian, A.D.; de Almeida, L.; Rojanasakul, Y.; Stehlik, C. An NLRP7-containing inflammasome mediates recognition of microbial lipopeptides in human macrophages. Immunity; 2012; 36, pp. 464-476. [DOI: https://dx.doi.org/10.1016/j.immuni.2012.02.001]
13. Vladimer, G.I.; Weng, D.; Paquette, S.W.; Vanaja, S.K.; Rathinam, V.A.; Aune, M.H.; Conlon, J.E.; Burbage, J.J.; Proulx, M.K.; Liu, Q. et al. The NLRP12 inflammasome recognizes Yersinia pestis. Immunity; 2012; 37, pp. 96-107. [DOI: https://dx.doi.org/10.1016/j.immuni.2012.07.006]
14. Levy, M.; Thaiss, C.A.; Zeevi, D.; Dohnalova, L.; Zilberman-Schapira, G.; Mahdi, J.A.; David, E.; Savidor, A.; Korem, T.; Herzig, Y. et al. Microbiota-Modulated Metabolites Shape the Intestinal Microenvironment by Regulating NLRP6 Inflammasome Signaling. Cell; 2015; 163, pp. 1428-1443. [DOI: https://dx.doi.org/10.1016/j.cell.2015.10.048] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/26638072]
15. Zhu, S.; Ding, S.; Wang, P.; Wei, Z.; Pan, W.; Palm, N.W.; Yang, Y.; Yu, H.; Li, H.B.; Wang, G. et al. Nlrp9b inflammasome restricts rotavirus infection in intestinal epithelial cells. Nature; 2017; 546, pp. 667-670. [DOI: https://dx.doi.org/10.1038/nature22967] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/28636595]
16. Sefik, E.; Qu, R.; Junqueira, C.; Kaffe, E.; Mirza, H.; Zhao, J.; Brewer, J.R.; Han, A.; Steach, H.R.; Israelow, B. et al. Inflammasome activation in infected macrophages drives COVID-19 pathology. Nature; 2022; 606, pp. 585-593. [DOI: https://dx.doi.org/10.1038/s41586-022-04802-1]
17. Lei-Leston, A.C.; Murphy, A.G.; Maloy, K.J. Epithelial Cell Inflammasomes in Intestinal Immunity and Inflammation. Front. Immunol.; 2017; 8, 1168. [DOI: https://dx.doi.org/10.3389/fimmu.2017.01168]
18. Hatscher, L.; Amon, L.; Heger, L.; Dudziak, D. Inflammasomes in dendritic cells: Friend or foe?. Immunol. Lett.; 2021; 234, pp. 16-32. [DOI: https://dx.doi.org/10.1016/j.imlet.2021.04.002]
19. Jha, S.; Brickey, W.J.; Ting, J.P. Inflammasomes in Myeloid Cells: Warriors Within. Microbiol. Spectr.; 2017; 5, [DOI: https://dx.doi.org/10.1128/microbiolspec.MCHD-0049-2016] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/28102121]
20. Gritsenko, A.; Yu, S.; Martin-Sanchez, F.; Diaz-Del-Olmo, I.; Nichols, E.M.; Davis, D.M.; Brough, D.; Lopez-Castejon, G. Priming Is Dispensable for NLRP3 Inflammasome Activation in Human Monocytes In Vitro. Front. Immunol.; 2020; 11, 565924. [DOI: https://dx.doi.org/10.3389/fimmu.2020.565924] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/33101286]
21. Sorrentino, R.; Terlizzi, M.; Di Crescenzo, V.G.; Popolo, A.; Pecoraro, M.; Perillo, G.; Galderisi, A.; Pinto, A. Human lung cancer-derived immunosuppressive plasmacytoid dendritic cells release IL-1alpha in an AIM2 inflammasome-dependent manner. Am. J. Pathol.; 2015; 185, pp. 3115-3124. [DOI: https://dx.doi.org/10.1016/j.ajpath.2015.07.009]
22. Duncan, J.A.; Bergstralh, D.T.; Wang, Y.; Willingham, S.B.; Ye, Z.; Zimmermann, A.G.; Ting, J.P. Cryopyrin/NALP3 binds ATP/dATP, is an ATPase, and requires ATP binding to mediate inflammatory signaling. Proc. Natl. Acad. Sci. USA; 2007; 104, pp. 8041-8046. [DOI: https://dx.doi.org/10.1073/pnas.0611496104]
23. Bauernfeind, F.G.; Horvath, G.; Stutz, A.; Alnemri, E.S.; MacDonald, K.; Speert, D.; Fernandes-Alnemri, T.; Wu, J.; Monks, B.G.; Fitzgerald, K.A. et al. Cutting edge: NF-kappaB activating pattern recognition and cytokine receptors license NLRP3 inflammasome activation by regulating NLRP3 expression. J. Immunol.; 2009; 183, pp. 787-791. [DOI: https://dx.doi.org/10.4049/jimmunol.0901363]
24. Franchi, L.; Eigenbrod, T.; Nunez, G. Cutting edge: TNF-alpha mediates sensitization to ATP and silica via the NLRP3 inflammasome in the absence of microbial stimulation. J. Immunol.; 2009; 183, pp. 792-796. [DOI: https://dx.doi.org/10.4049/jimmunol.0900173]
25. Xing, Y.; Yao, X.; Li, H.; Xue, G.; Guo, Q.; Yang, G.; An, L.; Zhang, Y.; Meng, G. Cutting Edge: TRAF6 Mediates TLR/IL-1R Signaling-Induced Nontranscriptional Priming of the NLRP3 Inflammasome. J. Immunol.; 2017; 199, pp. 1561-1566. [DOI: https://dx.doi.org/10.4049/jimmunol.1700175]
26. Motta, V.; Soares, F.; Sun, T.; Philpott, D.J. NOD-like receptors: Versatile cytosolic sentinels. Physiol. Rev.; 2015; 95, pp. 149-178. [DOI: https://dx.doi.org/10.1152/physrev.00009.2014]
27. Swanson, K.V.; Deng, M.; Ting, J.P. The NLRP3 inflammasome: Molecular activation and regulation to therapeutics. Nat. Rev. Immunol.; 2019; 19, pp. 477-489. [DOI: https://dx.doi.org/10.1038/s41577-019-0165-0]
28. Groslambert, M.; Py, B.F. Spotlight on the NLRP3 inflammasome pathway. J. Inflamm. Res.; 2018; 11, pp. 359-374. [DOI: https://dx.doi.org/10.2147/JIR.S141220]
29. Dinarello, C.A. Overview of the IL-1 family in innate inflammation and acquired immunity. Immunol. Rev.; 2018; 281, pp. 8-27. [DOI: https://dx.doi.org/10.1111/imr.12621]
30. Gabay, C.; Lamacchia, C.; Palmer, G. IL-1 pathways in inflammation and human diseases. Nat. Rev. Rheumatol.; 2010; 6, pp. 232-241. [DOI: https://dx.doi.org/10.1038/nrrheum.2010.4]
31. Miller, L.S.; Pietras, E.M.; Uricchio, L.H.; Hirano, K.; Rao, S.; Lin, H.; O’Connell, R.M.; Iwakura, Y.; Cheung, A.L.; Cheng, G. et al. Inflammasome-mediated production of IL-1beta is required for neutrophil recruitment against Staphylococcus aureus in vivo. J. Immunol.; 2007; 179, pp. 6933-6942. [DOI: https://dx.doi.org/10.4049/jimmunol.179.10.6933] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/17982084]
32. Masumoto, J.; Zhou, W.; Morikawa, S.; Hosokawa, S.; Taguchi, H.; Yamamoto, T.; Kurata, M.; Kaneko, N. Molecular biology of autoinflammatory diseases. Inflamm. Regen.; 2021; 41, 33. [DOI: https://dx.doi.org/10.1186/s41232-021-00181-8] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/34635190]
33. Shaw, P.J.; McDermott, M.F.; Kanneganti, T.D. Inflammasomes and autoimmunity. Trends Mol. Med.; 2011; 17, pp. 57-64. [DOI: https://dx.doi.org/10.1016/j.molmed.2010.11.001]
34. Li, Z.; Guo, J.; Bi, L. Role of the NLRP3 inflammasome in autoimmune diseases. Biomed. Pharmacother.; 2020; 130, 110542. [DOI: https://dx.doi.org/10.1016/j.biopha.2020.110542] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/32738636]
35. Zhang, Y.; Yang, W.; Li, W.; Zhao, Y. NLRP3 Inflammasome: Checkpoint Connecting Innate and Adaptive Immunity in Autoimmune Diseases. Front. Immunol.; 2021; 12, 732933. [DOI: https://dx.doi.org/10.3389/fimmu.2021.732933] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/34707607]
36. Yi, Y.S. Role of inflammasomes in inflammatory autoimmune rheumatic diseases. Korean J. Physiol. Pharmacol.; 2018; 22, pp. 1-15. [DOI: https://dx.doi.org/10.4196/kjpp.2018.22.1.1]
37. Crow, M.K.; Olferiev, M.; Kirou, K.A. Type I Interferons in Autoimmune Disease. Annu. Rev. Pathol.; 2019; 14, pp. 369-393. [DOI: https://dx.doi.org/10.1146/annurev-pathol-020117-043952]
38. Chasset, F.; Dayer, J.M.; Chizzolini, C. Type I Interferons in Systemic Autoimmune Diseases: Distinguishing Between Afferent and Efferent Functions for Precision Medicine and Individualized Treatment. Front. Pharmacol.; 2021; 12, 633821. [DOI: https://dx.doi.org/10.3389/fphar.2021.633821]
39. Di Domizio, J.; Cao, W. Fueling autoimmunity: Type I interferon in autoimmune diseases. Expert Rev. Clin. Immunol.; 2013; 9, pp. 201-210. [DOI: https://dx.doi.org/10.1586/eci.12.106]
40. Guarda, G.; Braun, M.; Staehli, F.; Tardivel, A.; Mattmann, C.; Forster, I.; Farlik, M.; Decker, T.; Du Pasquier, R.A.; Romero, P. et al. Type I interferon inhibits interleukin-1 production and inflammasome activation. Immunity; 2011; 34, pp. 213-223. [DOI: https://dx.doi.org/10.1016/j.immuni.2011.02.006]
41. Labzin, L.I.; Lauterbach, M.A.; Latz, E. Interferons and inflammasomes: Cooperation and counterregulation in disease. J. Allergy Clin. Immunol.; 2016; 138, pp. 37-46. [DOI: https://dx.doi.org/10.1016/j.jaci.2016.05.010] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/27373324]
42. Kopitar-Jerala, N. The Role of Interferons in Inflammation and Inflammasome Activation. Front. Immunol.; 2017; 8, 873. [DOI: https://dx.doi.org/10.3389/fimmu.2017.00873] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/28791024]
43. Lee, B.; Robinson, K.M.; McHugh, K.J.; Scheller, E.V.; Mandalapu, S.; Chen, C.; Di, Y.P.; Clay, M.E.; Enelow, R.I.; Dubin, P.J. et al. Influenza-induced type I interferon enhances susceptibility to gram-negative and gram-positive bacterial pneumonia in mice. Am. J. Physiol. Lung Cell. Mol. Physiol.; 2015; 309, pp. L158-L167. [DOI: https://dx.doi.org/10.1152/ajplung.00338.2014]
44. Robinson, K.M.; Choi, S.M.; McHugh, K.J.; Mandalapu, S.; Enelow, R.I.; Kolls, J.K.; Alcorn, J.F. Influenza A exacerbates Staphylococcus aureus pneumonia by attenuating IL-1beta production in mice. J. Immunol.; 2013; 191, pp. 5153-5159. [DOI: https://dx.doi.org/10.4049/jimmunol.1301237] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/24089191]
45. Kudva, A.; Scheller, E.V.; Robinson, K.M.; Crowe, C.R.; Choi, S.M.; Slight, S.R.; Khader, S.A.; Dubin, P.J.; Enelow, R.I.; Kolls, J.K. et al. Influenza A inhibits Th17-mediated host defense against bacterial pneumonia in mice. J. Immunol.; 2011; 186, pp. 1666-1674. [DOI: https://dx.doi.org/10.4049/jimmunol.1002194] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/21178015]
46. Robinson, K.M.; McHugh, K.J.; Mandalapu, S.; Clay, M.E.; Lee, B.; Scheller, E.V.; Enelow, R.I.; Chan, Y.R.; Kolls, J.K.; Alcorn, J.F. Influenza A virus exacerbates Staphylococcus aureus pneumonia in mice by attenuating antimicrobial peptide production. J. Infect. Dis.; 2014; 209, pp. 865-875. [DOI: https://dx.doi.org/10.1093/infdis/jit527]
47. Li, W.; Moltedo, B.; Moran, T.M. Type I interferon induction during influenza virus infection increases susceptibility to secondary Streptococcus pneumoniae infection by negative regulation of gammadelta T cells. J. Virol.; 2012; 86, pp. 12304-12312. [DOI: https://dx.doi.org/10.1128/JVI.01269-12]
48. Mayer-Barber, K.D.; Andrade, B.B.; Oland, S.D.; Amaral, E.P.; Barber, D.L.; Gonzales, J.; Derrick, S.C.; Shi, R.; Kumar, N.P.; Wei, W. et al. Host-directed therapy of tuberculosis based on interleukin-1 and type I interferon crosstalk. Nature; 2014; 511, pp. 99-103. [DOI: https://dx.doi.org/10.1038/nature13489]
49. Tian, Z.; Shen, X.; Feng, H.; Gao, B. IL-1 beta attenuates IFN-alpha beta-induced antiviral activity and STAT1 activation in the liver: Involvement of proteasome-dependent pathway. J. Immunol.; 2000; 165, pp. 3959-3965. [DOI: https://dx.doi.org/10.4049/jimmunol.165.7.3959]
50. Kohase, M.; Zhang, Y.H.; Lin, J.X.; Yamazaki, S.; Sehgal, P.B.; Vilcek, J. Interleukin-1 can inhibit interferon-beta synthesis and its antiviral action: Comparison with tumor necrosis factor. J. Interferon Res.; 1988; 8, pp. 559-570. [DOI: https://dx.doi.org/10.1089/jir.1988.8.559]
51. Veckman, V.; Julkunen, I. Streptococcus pyogenes activates human plasmacytoid and myeloid dendritic cells. J. Leukoc. Biol.; 2008; 83, pp. 296-304. [DOI: https://dx.doi.org/10.1189/jlb.0707457] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/17965337]
52. Parcina, M.; Wendt, C.; Goetz, F.; Zawatzky, R.; Zahringer, U.; Heeg, K.; Bekeredjian-Ding, I. Staphylococcus aureus-induced plasmacytoid dendritic cell activation is based on an IgG-mediated memory response. J. Immunol.; 2008; 181, pp. 3823-3833. [DOI: https://dx.doi.org/10.4049/jimmunol.181.6.3823] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/18768836]
53. Williams, N.L.; Morris, J.L.; Rush, C.M.; Ketheesan, N. Plasmacytoid dendritic cell bactericidal activity against Burkholderia pseudomallei. Microbes Infect.; 2015; 17, pp. 311-316. [DOI: https://dx.doi.org/10.1016/j.micinf.2014.12.007] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/25532693]
54. Raieli, S.; Trichot, C.; Korniotis, S.; Pattarini, L.; Soumelis, V. TLR1/2 orchestrate human plasmacytoid predendritic cell response to gram+ bacteria. PLoS Biol.; 2019; 17, e3000209. [DOI: https://dx.doi.org/10.1371/journal.pbio.3000209]
55. Romani, L.; Bistoni, F.; Gaziano, R.; Bozza, S.; Montagnoli, C.; Perruccio, K.; Pitzurra, L.; Bellocchio, S.; Velardi, A.; Rasi, G. et al. Thymosin alpha 1 activates dendritic cells for antifungal Th1 resistance through toll-like receptor signaling. Blood; 2004; 103, pp. 4232-4239. [DOI: https://dx.doi.org/10.1182/blood-2003-11-4036] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/14982877]
56. Ramirez-Ortiz, Z.G.; Specht, C.A.; Wang, J.P.; Lee, C.K.; Bartholomeu, D.C.; Gazzinelli, R.T.; Levitz, S.M. Toll-like receptor 9-dependent immune activation by unmethylated CpG motifs in Aspergillus fumigatus DNA. Infect. Immun.; 2008; 76, pp. 2123-2129. [DOI: https://dx.doi.org/10.1128/IAI.00047-08] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/18332208]
57. Dan, J.M.; Wang, J.P.; Lee, C.K.; Levitz, S.M. Cooperative stimulation of dendritic cells by Cryptococcus neoformans mannoproteins and CpG oligodeoxynucleotides. PLoS ONE; 2008; 3, e2046. [DOI: https://dx.doi.org/10.1371/journal.pone.0002046]
58. Ramirez-Ortiz, Z.G.; Lee, C.K.; Wang, J.P.; Boon, L.; Specht, C.A.; Levitz, S.M. A nonredundant role for plasmacytoid dendritic cells in host defense against the human fungal pathogen Aspergillus fumigatus. Cell Host Microbe; 2011; 9, pp. 415-424. [DOI: https://dx.doi.org/10.1016/j.chom.2011.04.007]
59. Loures, F.V.; Rohm, M.; Lee, C.K.; Santos, E.; Wang, J.P.; Specht, C.A.; Calich, V.L.; Urban, C.F.; Levitz, S.M. Recognition of Aspergillus fumigatus hyphae by human plasmacytoid dendritic cells is mediated by dectin-2 and results in formation of extracellular traps. PLoS Pathog.; 2015; 11, e1004643. [DOI: https://dx.doi.org/10.1371/journal.ppat.1004643]
60. Hole, C.R.; Leopold Wager, C.M.; Mendiola, A.S.; Wozniak, K.L.; Campuzano, A.; Lin, X.; Wormley, F.L., Jr. Antifungal Activity of Plasmacytoid Dendritic Cells against Cryptococcus neoformans In Vitro Requires Expression of Dectin-3 (CLEC4D) and Reactive Oxygen Species. Infect. Immun.; 2016; 84, pp. 2493-2504. [DOI: https://dx.doi.org/10.1128/IAI.00103-16] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/27324480]
61. Van de Veerdonk, F.L.; Joosten, L.A.; Netea, M.G. The interplay between inflammasome activation and antifungal host defense. Immunol. Rev.; 2015; 265, pp. 172-180. [DOI: https://dx.doi.org/10.1111/imr.12280]
62. Skeldon, A.; Saleh, M. The inflammasomes: Molecular effectors of host resistance against bacterial, viral, parasitic, and fungal infections. Front. Microbiol.; 2011; 2, 15. [DOI: https://dx.doi.org/10.3389/fmicb.2011.00015]
63. Tavares, A.H.; Burgel, P.H.; Bocca, A.L. Turning Up the Heat: Inflammasome Activation by Fungal Pathogens. PLoS Pathog.; 2015; 11, e1004948. [DOI: https://dx.doi.org/10.1371/journal.ppat.1004948] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/26204108]
64. Vladimer, G.I.; Marty-Roix, R.; Ghosh, S.; Weng, D.; Lien, E. Inflammasomes and host defenses against bacterial infections. Curr. Opin. Microbiol.; 2013; 16, pp. 23-31. [DOI: https://dx.doi.org/10.1016/j.mib.2012.11.008] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/23318142]
65. Brewer, S.M.; Brubaker, S.W.; Monack, D.M. Host inflammasome defense mechanisms and bacterial pathogen evasion strategies. Curr. Opin. Immunol.; 2019; 60, pp. 63-70. [DOI: https://dx.doi.org/10.1016/j.coi.2019.05.001] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/31174046]
66. Hanagata, N. CpG oligodeoxynucleotide nanomedicines for the prophylaxis or treatment of cancers, infectious diseases, and allergies. Int. J. Nanomed.; 2017; 12, pp. 515-531. [DOI: https://dx.doi.org/10.2147/IJN.S114477] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/28144136]
67. Kim, J.J.; Jo, E.K. NLRP3 inflammasome and host protection against bacterial infection. J. Korean Med. Sci.; 2013; 28, pp. 1415-1423. [DOI: https://dx.doi.org/10.3346/jkms.2013.28.10.1415]
68. Latz, E.; Xiao, T.S.; Stutz, A. Activation and regulation of the inflammasomes. Nat. Rev. Immunol.; 2013; 13, pp. 397-411. [DOI: https://dx.doi.org/10.1038/nri3452]
69. Agod, Z.; Fekete, T.; Budai, M.M.; Varga, A.; Szabo, A.; Moon, H.; Boldogh, I.; Biro, T.; Lanyi, A.; Bacsi, A. et al. Regulation of type I interferon responses by mitochondria-derived reactive oxygen species in plasmacytoid dendritic cells. Redox Biol.; 2017; 13, pp. 633-645. [DOI: https://dx.doi.org/10.1016/j.redox.2017.07.016]
70. Zimmermann, H. Extracellular metabolism of ATP and other nucleotides. Naunyn Schmiedebergs Arch. Pharmacol.; 2000; 362, pp. 299-309. [DOI: https://dx.doi.org/10.1007/s002100000309] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/11111825]
71. Zimmermann, H.; Zebisch, M.; Strater, N. Cellular function and molecular structure of ecto-nucleotidases. Purinergic Signal.; 2012; 8, pp. 437-502. [DOI: https://dx.doi.org/10.1007/s11302-012-9309-4]
72. Schneider, E.; Rissiek, A.; Winzer, R.; Puig, B.; Rissiek, B.; Haag, F.; Mittrucker, H.W.; Magnus, T.; Tolosa, E. Generation and Function of Non-cell-bound CD73 in Inflammation. Front. Immunol.; 2019; 10, 1729. [DOI: https://dx.doi.org/10.3389/fimmu.2019.01729]
73. Diaz-Garcia, E.; Garcia-Tovar, S.; Alfaro, E.; Zamarron, E.; Mangas, A.; Galera, R.; Ruiz-Hernandez, J.J.; Sole-Violan, J.; Rodriguez-Gallego, C.; Van-Den-Rym, A. et al. Role of CD39 in COVID-19 Severity: Dysregulation of Purinergic Signaling and Thromboinflammation. Front. Immunol.; 2022; 13, 847894. [DOI: https://dx.doi.org/10.3389/fimmu.2022.847894]
74. Morello, S.; Capone, M.; Sorrentino, C.; Giannarelli, D.; Madonna, G.; Mallardo, D.; Grimaldi, A.M.; Pinto, A.; Ascierto, P.A. Soluble CD73 as biomarker in patients with metastatic melanoma patients treated with nivolumab. J. Transl. Med.; 2017; 15, 244. [DOI: https://dx.doi.org/10.1186/s12967-017-1348-8]
75. Coade, S.B.; Pearson, J.D. Metabolism of adenine nucleotides in human blood. Circ. Res.; 1989; 65, pp. 531-537. [DOI: https://dx.doi.org/10.1161/01.RES.65.3.531]
76. Greaney, A.J.; Leppla, S.H.; Moayeri, M. Bacterial Exotoxins and the Inflammasome. Front. Immunol.; 2015; 6, 570. [DOI: https://dx.doi.org/10.3389/fimmu.2015.00570] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/26617605]
77. Eder, C. Mechanisms of interleukin-1beta release. Immunobiology; 2009; 214, pp. 543-553. [DOI: https://dx.doi.org/10.1016/j.imbio.2008.11.007] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/19250700]
78. Pizzirani, C.; Ferrari, D.; Chiozzi, P.; Adinolfi, E.; Sandona, D.; Savaglio, E.; Di Virgilio, F. Stimulation of P2 receptors causes release of IL-1beta-loaded microvesicles from human dendritic cells. Blood; 2007; 109, pp. 3856-3864. [DOI: https://dx.doi.org/10.1182/blood-2005-06-031377] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/17192399]
79. Hanagata, N. Structure-dependent immunostimulatory effect of CpG oligodeoxynucleotides and their delivery system. Int. J. Nanomed.; 2012; 7, pp. 2181-2195. [DOI: https://dx.doi.org/10.2147/IJN.S30197]
80. Stehlik, C.; Dorfleutner, A. COPs and POPs: Modulators of inflammasome activity. J. Immunol.; 2007; 179, pp. 7993-7998. [DOI: https://dx.doi.org/10.4049/jimmunol.179.12.7993]
81. Nestle, F.O.; Conrad, C.; Tun-Kyi, A.; Homey, B.; Gombert, M.; Boyman, O.; Burg, G.; Liu, Y.J.; Gilliet, M. Plasmacytoid predendritic cells initiate psoriasis through interferon-alpha production. J. Exp. Med.; 2005; 202, pp. 135-143. [DOI: https://dx.doi.org/10.1084/jem.20050500]
82. Reboldi, A.; Dang, E.V.; McDonald, J.G.; Liang, G.; Russell, D.W.; Cyster, J.G. Inflammation. 25-Hydroxycholesterol suppresses interleukin-1-driven inflammation downstream of type I interferon. Science; 2014; 345, pp. 679-684. [DOI: https://dx.doi.org/10.1126/science.1254790]
83. Inoue, M.; Williams, K.L.; Oliver, T.; Vandenabeele, P.; Rajan, J.V.; Miao, E.A.; Shinohara, M.L. Interferon-beta therapy against EAE is effective only when development of the disease depends on the NLRP3 inflammasome. Sci. Signal.; 2012; 5, ra38. [DOI: https://dx.doi.org/10.1126/scisignal.2002767] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/22623753]
84. Druilhe, A.; Srinivasula, S.M.; Razmara, M.; Ahmad, M.; Alnemri, E.S. Regulation of IL-1beta generation by Pseudo-ICE and ICEBERG, two dominant negative caspase recruitment domain proteins. Cell Death Differ.; 2001; 8, pp. 649-657. [DOI: https://dx.doi.org/10.1038/sj.cdd.4400881] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/11536016]
85. Verma, D.; Fekri, S.Z.; Sigurdardottir, G.; Bivik Eding, C.; Sandin, C.; Enerback, C. Enhanced Inflammasome Activity in Patients with Psoriasis Promotes Systemic Inflammation. J. Investig. Dermatol.; 2021; 141, pp. 586-595.E5. [DOI: https://dx.doi.org/10.1016/j.jid.2020.07.012] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/32896537]
86. Yu, N.; Peng, C.; Chen, W.; Sun, Z.; Zheng, J.; Zhang, S.; Ding, Y.; Shi, Y. Circulating Metabolomic Signature in Generalized Pustular Psoriasis Blunts Monocyte Hyperinflammation by Triggering Amino Acid Response. Front. Immunol.; 2021; 12, 739514. [DOI: https://dx.doi.org/10.3389/fimmu.2021.739514] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/34567002]
87. Costa, M.C.; Paixao, C.S.; Viana, D.L.; Rocha, B.O.; Saldanha, M.; da Mota, L.M.H.; Machado, P.R.L.; Pagliari, C.; de Oliveira, M.F.; Arruda, S. et al. Mononuclear Phagocyte Activation Is Associated With the Immunopathology of Psoriasis. Front. Immunol.; 2020; 11, 478. [DOI: https://dx.doi.org/10.3389/fimmu.2020.00478] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/32269570]
88. Bender, A.T.; Tzvetkov, E.; Pereira, A.; Wu, Y.; Kasar, S.; Przetak, M.M.; Vlach, J.; Niewold, T.B.; Jensen, M.A.; Okitsu, S.L. TLR7 and TLR8 Differentially Activate the IRF and NF-kappaB Pathways in Specific Cell Types to Promote Inflammation. Immunohorizons; 2020; 4, pp. 93-107. [DOI: https://dx.doi.org/10.4049/immunohorizons.2000002] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/32086319]
89. Congy-Jolivet, N.; Cenac, C.; Dellacasagrande, J.; Puissant-Lubrano, B.; Apoil, P.A.; Guedj, K.; Abbas, F.; Laffont, S.; Sourdet, S.; Guyonnet, S. et al. Monocytes are the main source of STING-mediated IFN-alpha production. EBioMedicine; 2022; 80, 104047. [DOI: https://dx.doi.org/10.1016/j.ebiom.2022.104047] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/35561451]
90. Kim, T.H.; Kim, C.W.; Oh, D.S.; Jung, H.E.; Lee, H.K. Monocytes Contribute to IFN-beta Production via the MyD88-Dependent Pathway and Cytotoxic T-Cell Responses against Mucosal Respiratory Syncytial Virus Infection. Immune Netw.; 2021; 21, e27. [DOI: https://dx.doi.org/10.4110/in.2021.21.e27] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/34522440]
91. de Marcken, M.; Dhaliwal, K.; Danielsen, A.C.; Gautron, A.S.; Dominguez-Villar, M. TLR7 and TLR8 activate distinct pathways in monocytes during RNA virus infection. Sci. Signal.; 2019; 12, pp. 941-954. [DOI: https://dx.doi.org/10.1126/scisignal.aaw1347] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/31662487]
92. Reizis, B. Plasmacytoid Dendritic Cells: Development, Regulation, and Function. Immunity; 2019; 50, pp. 37-50. [DOI: https://dx.doi.org/10.1016/j.immuni.2018.12.027] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/30650380]
93. Aiello, A.; Giannessi, F.; Percario, Z.A.; Affabris, E. The involvement of plasmacytoid cells in HIV infection and pathogenesis. Cytokine Growth Factor Rev.; 2018; 40, pp. 77-89. [DOI: https://dx.doi.org/10.1016/j.cytogfr.2018.03.009] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/29588163]
94. Cervantes-Barragan, L.; Lewis, K.L.; Firner, S.; Thiel, V.; Hugues, S.; Reith, W.; Ludewig, B.; Reizis, B. Plasmacytoid dendritic cells control T-cell response to chronic viral infection. Proc. Natl. Acad. Sci. USA; 2012; 109, pp. 3012-3017. [DOI: https://dx.doi.org/10.1073/pnas.1117359109] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/22315415]
95. Li, S.; Wu, J.; Zhu, S.; Liu, Y.J.; Chen, J. Disease-Associated Plasmacytoid Dendritic Cells. Front. Immunol.; 2017; 8, 1268. [DOI: https://dx.doi.org/10.3389/fimmu.2017.01268] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/29085361]
96. Zhou, B.; Lawrence, T.; Liang, Y. The Role of Plasmacytoid Dendritic Cells in Cancers. Front. Immunol.; 2021; 12, 749190. [DOI: https://dx.doi.org/10.3389/fimmu.2021.749190] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/34737750]
97. Ye, Y.; Gaugler, B.; Mohty, M.; Malard, F. Plasmacytoid dendritic cell biology and its role in immune-mediated diseases. Clin. Transl. Immunol.; 2020; 9, e1139. [DOI: https://dx.doi.org/10.1002/cti2.1139]
98. Panda, S.K.; Kolbeck, R.; Sanjuan, M.A. Plasmacytoid dendritic cells in autoimmunity. Curr. Opin. Immunol.; 2017; 44, pp. 20-25. [DOI: https://dx.doi.org/10.1016/j.coi.2016.10.006]
99. Crozat, K.; Vivier, E.; Dalod, M. Crosstalk between components of the innate immune system: Promoting anti-microbial defenses and avoiding immunopathologies. Immunol. Rev.; 2009; 227, pp. 129-149. [DOI: https://dx.doi.org/10.1111/j.1600-065X.2008.00736.x]
100. Worah, K.; Mathan, T.S.M.; Vu Manh, T.P.; Keerthikumar, S.; Schreibelt, G.; Tel, J.; Duiveman-de Boer, T.; Skold, A.E.; van Spriel, A.B.; de Vries, I.J.M. et al. Proteomics of Human Dendritic Cell Subsets Reveals Subset-Specific Surface Markers and Differential Inflammasome Function. Cell Rep.; 2016; 16, pp. 2953-2966. [DOI: https://dx.doi.org/10.1016/j.celrep.2016.08.023]
101. Hatscher, L.; Lehmann, C.H.K.; Purbojo, A.; Onderka, C.; Liang, C.; Hartmann, A.; Cesnjevar, R.; Bruns, H.; Gross, O.; Nimmerjahn, F. et al. Select hyperactivating NLRP3 ligands enhance the TH1- and TH17-inducing potential of human type 2 conventional dendritic cells. Sci. Signal.; 2021; 14, pp. 16-32. [DOI: https://dx.doi.org/10.1126/scisignal.abe1757] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/33906973]
102. Chaperot, L.; Blum, A.; Manches, O.; Lui, G.; Angel, J.; Molens, J.P.; Plumas, J. Virus or TLR agonists induce TRAIL-mediated cytotoxic activity of plasmacytoid dendritic cells. J. Immunol.; 2006; 176, pp. 248-255. [DOI: https://dx.doi.org/10.4049/jimmunol.176.1.248] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/16365416]
103. Barr, D.P.; Belz, G.T.; Reading, P.C.; Wojtasiak, M.; Whitney, P.G.; Heath, W.R.; Carbone, F.R.; Brooks, A.G. A role for plasmacytoid dendritic cells in the rapid IL-18-dependent activation of NK cells following HSV-1 infection. Eur. J. Immunol.; 2007; 37, pp. 1334-1342. [DOI: https://dx.doi.org/10.1002/eji.200636362] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/17407097]
104. Lousberg, E.L.; Diener, K.R.; Fraser, C.K.; Phipps, S.; Foster, P.S.; Chen, W.; Uematsu, S.; Akira, S.; Robertson, S.A.; Brown, M.P. et al. Antigen-specific T-cell responses to a recombinant fowlpox virus are dependent on MyD88 and interleukin-18 and independent of Toll-like receptor 7 (TLR7)- and TLR9-mediated innate immune recognition. J. Virol.; 2011; 85, pp. 3385-3396. [DOI: https://dx.doi.org/10.1128/JVI.02000-10] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/21248035]
105. Cavalli, G.; Colafrancesco, S.; Emmi, G.; Imazio, M.; Lopalco, G.; Maggio, M.C.; Sota, J.; Dinarello, C.A. Interleukin 1alpha: A comprehensive review on the role of IL-1alpha in the pathogenesis and treatment of autoimmune and inflammatory diseases. Autoimmun. Rev.; 2021; 20, 102763. [DOI: https://dx.doi.org/10.1016/j.autrev.2021.102763]
106. Gross, C.J.; Mishra, R.; Schneider, K.S.; Medard, G.; Wettmarshausen, J.; Dittlein, D.C.; Shi, H.; Gorka, O.; Koenig, P.A.; Fromm, S. et al. K(+) Efflux-Independent NLRP3 Inflammasome Activation by Small Molecules Targeting Mitochondria. Immunity; 2016; 45, pp. 761-773. [DOI: https://dx.doi.org/10.1016/j.immuni.2016.08.010]
107. Budai, M.M.; Tozser, J.; Benko, S. Different dynamics of NLRP3 inflammasome-mediated IL1beta production in GM-CSF- and M-CSF-differentiated human macrophages. J. Leukoc. Biol.; 2017; 101, pp. 1335-1347. [DOI: https://dx.doi.org/10.1189/jlb.3A0716-300RR]
108. Ipseiz, N.; Pickering, R.J.; Rosas, M.; Tyrrell, V.J.; Davies, L.C.; Orr, S.J.; Czubala, M.A.; Fathalla, D.; Robertson, A.A.; Bryant, C.E. et al. Tissue-resident macrophages actively suppress IL-1beta release via a reactive prostanoid/IL-10 pathway. EMBO J.; 2020; 39, e103454. [DOI: https://dx.doi.org/10.15252/embj.2019103454]
109. Piccini, A.; Carta, S.; Tassi, S.; Lasiglie, D.; Fossati, G.; Rubartelli, A. ATP is released by monocytes stimulated with pathogen-sensing receptor ligands and induces IL-1beta and IL-18 secretion in an autocrine way. Proc. Natl. Acad. Sci. USA; 2008; 105, pp. 8067-8072. [DOI: https://dx.doi.org/10.1073/pnas.0709684105]
110. Kovacs, E.G.; Alatshan, A.; Budai, M.M.; Czimmerer, Z.; Biro, E.; Benko, S. Caffeine Has Different Immunomodulatory Effect on the Cytokine Expression and NLRP3 Inflammasome Function in Various Human Macrophage Subpopulations. Nutrients; 2021; 13, 2409. [DOI: https://dx.doi.org/10.3390/nu13072409]
111. Schon, M.; Bong, A.B.; Drewniok, C.; Herz, J.; Geilen, C.C.; Reifenberger, J.; Benninghoff, B.; Slade, H.B.; Gollnick, H.; Schon, M.P. Tumor-selective induction of apoptosis and the small-molecule immune response modifier imiquimod. J. Natl. Cancer Inst.; 2003; 95, pp. 1138-1149. [DOI: https://dx.doi.org/10.1093/jnci/djg016] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/12902443]
112. Kanneganti, T.D.; Ozoren, N.; Body-Malapel, M.; Amer, A.; Park, J.H.; Franchi, L.; Whitfield, J.; Barchet, W.; Colonna, M.; Vandenabeele, P. et al. Bacterial RNA and small antiviral compounds activate caspase-1 through cryopyrin/Nalp3. Nature; 2006; 440, pp. 233-236. [DOI: https://dx.doi.org/10.1038/nature04517] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/16407888]
113. Riol-Blanco, L.; Ordovas-Montanes, J.; Perro, M.; Naval, E.; Thiriot, A.; Alvarez, D.; Paust, S.; Wood, J.N.; von Andrian, U.H. Nociceptive sensory neurons drive interleukin-23-mediated psoriasiform skin inflammation. Nature; 2014; 510, pp. 157-161. [DOI: https://dx.doi.org/10.1038/nature13199] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/24759321]
114. Elliott, E.I.; Sutterwala, F.S. Initiation and perpetuation of NLRP3 inflammasome activation and assembly. Immunol. Rev.; 2015; 265, pp. 35-52. [DOI: https://dx.doi.org/10.1111/imr.12286] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/25879282]
115. Long, Y.; Liu, X.; Tan, X.Z.; Jiang, C.X.; Chen, S.W.; Liang, G.N.; He, X.M.; Wu, J.; Chen, T.; Xu, Y. ROS-induced NLRP3 inflammasome priming and activation mediate PCB 118- induced pyroptosis in endothelial cells. Ecotoxicol. Environ. Saf.; 2020; 189, 109937. [DOI: https://dx.doi.org/10.1016/j.ecoenv.2019.109937]
116. Netea, M.G.; Nold-Petry, C.A.; Nold, M.F.; Joosten, L.A.; Opitz, B.; van der Meer, J.H.; van de Veerdonk, F.L.; Ferwerda, G.; Heinhuis, B.; Devesa, I. et al. Differential requirement for the activation of the inflammasome for processing and release of IL-1beta in monocytes and macrophages. Blood; 2009; 113, pp. 2324-2335. [DOI: https://dx.doi.org/10.1182/blood-2008-03-146720]
117. Juliana, C.; Fernandes-Alnemri, T.; Kang, S.; Farias, A.; Qin, F.; Alnemri, E.S. Non-transcriptional priming and deubiquitination regulate NLRP3 inflammasome activation. J. Biol. Chem.; 2012; 287, pp. 36617-36622. [DOI: https://dx.doi.org/10.1074/jbc.M112.407130] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/22948162]
118. Song, N.; Liu, Z.S.; Xue, W.; Bai, Z.F.; Wang, Q.Y.; Dai, J.; Liu, X.; Huang, Y.J.; Cai, H.; Zhan, X.Y. et al. NLRP3 Phosphorylation Is an Essential Priming Event for Inflammasome Activation. Mol. Cell; 2017; 68, pp. 185-197.E6. [DOI: https://dx.doi.org/10.1016/j.molcel.2017.08.017] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/28943315]
119. Gaidt, M.M.; Ebert, T.S.; Chauhan, D.; Schmidt, T.; Schmid-Burgk, J.L.; Rapino, F.; Robertson, A.A.; Cooper, M.A.; Graf, T.; Hornung, V. Human Monocytes Engage an Alternative Inflammasome Pathway. Immunity; 2016; 44, pp. 833-846. [DOI: https://dx.doi.org/10.1016/j.immuni.2016.01.012] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/27037191]
120. Gaidt, M.M.; Hornung, V. Alternative inflammasome activation enables IL-1beta release from living cells. Curr. Opin. Immunol.; 2017; 44, pp. 7-13. [DOI: https://dx.doi.org/10.1016/j.coi.2016.10.007]
121. Zhang, W.; An, E.K.; Hwang, J.; Jin, J.O. Mice Plasmacytoid Dendritic Cells Were Activated by Lipopolysaccharides Through Toll-Like Receptor 4/Myeloid Differentiation Factor 2. Front. Immunol.; 2021; 12, 727161. [DOI: https://dx.doi.org/10.3389/fimmu.2021.727161] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/34603298]
122. Ohradanova-Repic, A.; Machacek, C.; Fischer, M.B.; Stockinger, H. Differentiation of human monocytes and derived subsets of macrophages and dendritic cells by the HLDA10 monoclonal antibody panel. Clin. Transl. Immunol.; 2016; 5, e55. [DOI: https://dx.doi.org/10.1038/cti.2015.39]
123. Ferrari, D.; La Sala, A.; Chiozzi, P.; Morelli, A.; Falzoni, S.; Girolomoni, G.; Idzko, M.; Dichmann, S.; Norgauer, J.; Di Virgilio, F. The P2 purinergic receptors of human dendritic cells: Identification and coupling to cytokine release. FASEB J.; 2000; 14, pp. 2466-2476. [DOI: https://dx.doi.org/10.1096/fj.00-0031com]
124. See, P.; Dutertre, C.A.; Chen, J.; Gunther, P.; McGovern, N.; Irac, S.E.; Gunawan, M.; Beyer, M.; Handler, K.; Duan, K. et al. Mapping the human DC lineage through the integration of high-dimensional techniques. Science; 2017; 7, 69. [DOI: https://dx.doi.org/10.1126/science.aag3009]
125. Matsui, T.; Connolly, J.E.; Michnevitz, M.; Chaussabel, D.; Yu, C.I.; Glaser, C.; Tindle, S.; Pypaert, M.; Freitas, H.; Piqueras, B. et al. CD2 distinguishes two subsets of human plasmacytoid dendritic cells with distinct phenotype and functions. J. Immunol.; 2009; 182, pp. 6815-6823. [DOI: https://dx.doi.org/10.4049/jimmunol.0802008] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/19454677]
126. Burgueno-Bucio, E.; Mier-Aguilar, C.A.; Soldevila, G. The multiple faces of CD5. J. Leukoc. Biol.; 2019; 105, pp. 891-904. [DOI: https://dx.doi.org/10.1002/JLB.MR0618-226R] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/30676652]
127. Lemke, G.; Rothlin, C.V. Immunobiology of the TAM receptors. Nat. Rev. Immunol.; 2008; 8, pp. 327-336. [DOI: https://dx.doi.org/10.1038/nri2303] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/18421305]
128. Crocker, P.R.; Paulson, J.C.; Varki, A. Siglecs and their roles in the immune system. Nat. Rev. Immunol.; 2007; 7, pp. 255-266. [DOI: https://dx.doi.org/10.1038/nri2056]
129. Hagen, S.H.; Henseling, F.; Hennesen, J.; Savel, H.; Delahaye, S.; Richert, L.; Ziegler, S.M.; Altfeld, M. Heterogeneous Escape from X Chromosome Inactivation Results in Sex Differences in Type I IFN Responses at the Single Human pDC Level. Cell Rep.; 2020; 33, 108485. [DOI: https://dx.doi.org/10.1016/j.celrep.2020.108485] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/33296655]
130. Onodi, F.; Bonnet-Madin, L.; Meertens, L.; Karpf, L.; Poirot, J.; Zhang, S.Y.; Picard, C.; Puel, A.; Jouanguy, E.; Zhang, Q. et al. SARS-CoV-2 induces human plasmacytoid predendritic cell diversification via UNC93B and IRAK4. J. Exp. Med.; 2021; 218, e20201387. [DOI: https://dx.doi.org/10.1084/jem.20201387]
131. Alculumbre, S.G.; Saint-Andre, V.; Di Domizio, J.; Vargas, P.; Sirven, P.; Bost, P.; Maurin, M.; Maiuri, P.; Wery, M.; Roman, M.S. et al. Diversification of human plasmacytoid predendritic cells in response to a single stimulus. Nat. Immunol.; 2018; 19, pp. 63-75. [DOI: https://dx.doi.org/10.1038/s41590-017-0012-z] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/29203862]
132. Llufrio, E.M.; Wang, L.; Naser, F.J.; Patti, G.J. Sorting cells alters their redox state and cellular metabolome. Redox Biol.; 2018; 16, pp. 381-387. [DOI: https://dx.doi.org/10.1016/j.redox.2018.03.004] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/29627745]
133. Magyarics, Z.; Csillag, A.; Pazmandi, K.; Rajnavolgyi, E.; Bacsi, A. Identification of plasmacytoid pre-dendritic cells by one-color flow cytometry for phenotype screening. Cytometry A; 2008; 73, pp. 254-258. [DOI: https://dx.doi.org/10.1002/cyto.a.20529]
134. Yu, C.F.; Peng, W.M.; Oldenburg, J.; Hoch, J.; Bieber, T.; Limmer, A.; Hartmann, G.; Barchet, W.; Eis-Hubinger, A.M.; Novak, N. Human plasmacytoid dendritic cells support Th17 cell effector function in response to TLR7 ligation. J. Immunol.; 2010; 184, pp. 1159-1167. [DOI: https://dx.doi.org/10.4049/jimmunol.0901706]
135. Rodriguez Rodrigues, C.; Cabrini, M.; Remes Lenicov, F.; Sabatte, J.; Ceballos, A.; Jancic, C.; Raiden, S.; Ostrowski, M.; Silberstein, C.; Geffner, J. Epithelial cells activate plasmacytoid dendritic cells improving their anti-HIV activity. PLoS ONE; 2011; 6, e28709. [DOI: https://dx.doi.org/10.1371/journal.pone.0028709] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/22163327]
136. Fitzgerald-Bocarsly, P.; Feng, D. The role of type I interferon production by dendritic cells in host defense. Biochimie; 2007; 89, pp. 843-855. [DOI: https://dx.doi.org/10.1016/j.biochi.2007.04.018]
137. Corrales, L.; Woo, S.R.; Williams, J.B.; McWhirter, S.M.; Dubensky, T.W., Jr.; Gajewski, T.F. Antagonism of the STING Pathway via Activation of the AIM2 Inflammasome by Intracellular DNA. J. Immunol.; 2016; 196, pp. 3191-3198. [DOI: https://dx.doi.org/10.4049/jimmunol.1502538] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/26927800]
138. Yu, X.; Du, Y.; Cai, C.; Cai, B.; Zhu, M.; Xing, C.; Tan, P.; Lin, M.; Wu, J.; Li, J. et al. Inflammasome activation negatively regulates MyD88-IRF7 type I IFN signaling and anti-malaria immunity. Nat. Commun.; 2018; 9, 4964. [DOI: https://dx.doi.org/10.1038/s41467-018-07384-7]
139. Yang, C.A.; Chiang, B.L. Inflammasomes and human autoimmunity: A comprehensive review. J. Autoimmun.; 2015; 61, pp. 1-8. [DOI: https://dx.doi.org/10.1016/j.jaut.2015.05.001]
140. Kim, Y.K.; Shin, J.S.; Nahm, M.H. NOD-Like Receptors in Infection, Immunity, and Diseases. Yonsei Med. J.; 2016; 57, pp. 5-14. [DOI: https://dx.doi.org/10.3349/ymj.2016.57.1.5]
141. Wang, A.; Bai, Y. Dendritic cells: The driver of psoriasis. J. Dermatol.; 2020; 47, pp. 104-113. [DOI: https://dx.doi.org/10.1111/1346-8138.15184]
142. Lande, R.; Botti, E.; Jandus, C.; Dojcinovic, D.; Fanelli, G.; Conrad, C.; Chamilos, G.; Feldmeyer, L.; Marinari, B.; Chon, S. et al. The antimicrobial peptide LL37 is a T-cell autoantigen in psoriasis. Nat. Commun.; 2014; 5, 5621. [DOI: https://dx.doi.org/10.1038/ncomms6621]
143. Boonstra, A.; Rajsbaum, R.; Holman, M.; Marques, R.; Asselin-Paturel, C.; Pereira, J.P.; Bates, E.E.; Akira, S.; Vieira, P.; Liu, Y.J. et al. Macrophages and myeloid dendritic cells, but not plasmacytoid dendritic cells, produce IL-10 in response to MyD88- and TRIF-dependent TLR signals, and TLR-independent signals. J. Immunol.; 2006; 177, pp. 7551-7558. [DOI: https://dx.doi.org/10.4049/jimmunol.177.11.7551]
144. Morita, R.; Uchiyama, T.; Hori, T. Nitric oxide inhibits IFN-alpha production of human plasmacytoid dendritic cells partly via a guanosine 3’,5’-cyclic monophosphate-dependent pathway. J. Immunol.; 2005; 175, pp. 806-812. [DOI: https://dx.doi.org/10.4049/jimmunol.175.2.806]
145. Johansen, C.; Moeller, K.; Kragballe, K.; Iversen, L. The activity of caspase-1 is increased in lesional psoriatic epidermis. J. Invest. Dermatol.; 2007; 127, pp. 2857-2864. [DOI: https://dx.doi.org/10.1038/sj.jid.5700922]
146. Tervaniemi, M.H.; Katayama, S.; Skoog, T.; Siitonen, H.A.; Vuola, J.; Nuutila, K.; Sormunen, R.; Johnsson, A.; Linnarsson, S.; Suomela, S. et al. NOD-like receptor signaling and inflammasome-related pathways are highlighted in psoriatic epidermis. Sci. Rep.; 2016; 6, 22745. [DOI: https://dx.doi.org/10.1038/srep22745]
147. Ciazynska, M.; Olejniczak-Staruch, I.; Sobolewska-Sztychny, D.; Narbutt, J.; Skibinska, M.; Lesiak, A. The Role of NLRP1, NLRP3, and AIM2 Inflammasomes in Psoriasis: Review. Int. J. Mol. Sci.; 2021; 22, 5898. [DOI: https://dx.doi.org/10.3390/ijms22115898]
148. Kahlenberg, J.M.; Dubyak, G.R. Differing caspase-1 activation states in monocyte versus macrophage models of IL-1beta processing and release. J. Leukoc. Biol.; 2004; 76, pp. 676-684. [DOI: https://dx.doi.org/10.1189/jlb.0404221]
149. Ito, T.; Kanzler, H.; Duramad, O.; Cao, W.; Liu, Y.J. Specialization, kinetics, and repertoire of type 1 interferon responses by human plasmacytoid predendritic cells. Blood; 2006; 107, pp. 2423-2431. [DOI: https://dx.doi.org/10.1182/blood-2005-07-2709] [PubMed: https://www.ncbi.nlm.nih.gov/pubmed/16293610]
150. Azar, P.; Mejia, J.E.; Cenac, C.; Shaiykova, A.; Youness, A.; Laffont, S.; Essat, A.; Izopet, J.; Passaes, C.; Muller-Trutwin, M. et al. TLR7 dosage polymorphism shapes interferogenesis and HIV-1 acute viremia in women. JCI Insight; 2020; 5, e136047. [DOI: https://dx.doi.org/10.1172/jci.insight.136047]
151. Lacerte, P.; Brunet, A.; Egarnes, B.; Duchene, B.; Brown, J.P.; Gosselin, J. Overexpression of TLR2 and TLR9 on monocyte subsets of active rheumatoid arthritis patients contributes to enhance responsiveness to TLR agonists. Arthritis Res. Ther.; 2016; 18, 10. [DOI: https://dx.doi.org/10.1186/s13075-015-0901-1]
152. Juarez, E.; Nunez, C.; Sada, E.; Ellner, J.J.; Schwander, S.K.; Torres, M. Differential expression of Toll-like receptors on human alveolar macrophages and autologous peripheral monocytes. Respir. Res.; 2010; 11, 2. [DOI: https://dx.doi.org/10.1186/1465-9921-11-2]
153. Fiola, S.; Gosselin, D.; Takada, K.; Gosselin, J. TLR9 contributes to the recognition of EBV by primary monocytes and plasmacytoid dendritic cells. J. Immunol.; 2010; 185, pp. 3620-3631. [DOI: https://dx.doi.org/10.4049/jimmunol.0903736]
154. Shamaa, O.R.; Mitra, S.; Gavrilin, M.A.; Wewers, M.D. Monocyte Caspase-1 Is Released in a Stable, Active High Molecular Weight Complex Distinct from the Unstable Cell Lysate-Activated Caspase-1. PLoS ONE; 2015; 10, e0142203. [DOI: https://dx.doi.org/10.1371/journal.pone.0142203]
155. Mitra, S.; Wewers, M.D.; Sarkar, A. Mononuclear Phagocyte-Derived Microparticulate Caspase-1 Induces Pulmonary Vascular Endothelial Cell Injury. PLoS ONE; 2015; 10, e0145607. [DOI: https://dx.doi.org/10.1371/journal.pone.0145607]
156. Bacsi, A.; Ebbesen, P.; Szabo, J.; Beck, Z.; Andirko, I.; Csoma, E.; Toth, F.D. Pseudotypes of vesicular stomatitis virus-bearing envelope antigens of certain HIV-1 strains permissively infect human syncytiotrophoblasts cultured in vitro: Implications for in vivo infection of syncytiotrophoblasts by cell-free HIV-1. J. Med. Virol.; 2001; 64, pp. 387-397. [DOI: https://dx.doi.org/10.1002/jmv.1063]
© 2022 by the authors. Licensee MDPI, Basel, Switzerland. This article is an open access article distributed under the terms and conditions of the Creative Commons Attribution (CC BY) license (https://creativecommons.org/licenses/by/4.0/). Notwithstanding the ProQuest Terms and Conditions, you may use this content in accordance with the terms of the License.
Details
; Szöőr, Árpád 4 ; Csoma, Eszter 5 ; Szántó, Antónia 6 ; Tarr, Tünde 6 ; Bácsi, Attila 2
; Kemény, Lajos 7
; Veréb, Zoltán 7 ; Pázmándi, Kitti 2 1 Department of Immunology, Faculty of Medicine, University of Debrecen, 4032 Debrecen, Hungary; Doctoral School of Molecular Cell and Immune Biology, University of Debrecen, 4032 Debrecen, Hungary
2 Department of Immunology, Faculty of Medicine, University of Debrecen, 4032 Debrecen, Hungary
3 Department of Molecular Biotechnology and Microbiology, Faculty of Science and Technology, University of Debrecen, 4032 Debrecen, Hungary
4 Department of Biophysics and Cell Biology, Faculty of Medicine, University of Debrecen, 4032 Debrecen, Hungary
5 Department of Medical Microbiology, Faculty of Medicine, University of Debrecen, 4032 Debrecen, Hungary
6 Division of Clinical Immunology, Faculty of Medicine, University of Debrecen, 4032 Debrecen, Hungary
7 Regenerative Medicine and Cellular Pharmacology Laboratory, Department of Dermatology and Allergology, Faculty of Medicine, University of Szeged, 6720 Szeged, Hungary