Coxiella burnetii Phagocytosis Is Regulated by GTPases of the Rho Family and the RhoA Effectors mDia1 and ROCK

Abstract

The GTPases belonging to the Rho family control the actin cytoskeleton rearrangements needed for particle internalization during phagocytosis. ROCK and mDia1 are downstream effectors of RhoA, a GTPase involved in that process. Coxiella burnetii, the etiologic agent of Q fever, is internalized by the host´s cells in an actin-dependent manner. Nevertheless, the molecular mechanism involved in this process has been poorly characterized. This work analyzes the role of different GTPases of the Rho family and some downstream effectors in the internalization of C. burnetii by phagocytic and non-phagocytic cells. The internalization of C. burnetii into HeLa and RAW cells was significantly inhibited when the cells were treated with Clostridium difficile Toxin B which irreversibly inactivates members of the Rho family. In addition, the internalization was reduced in HeLa cells that overexpressed the dominant negative mutants of RhoA, Rac1 or Cdc42 or that were knocked down for the Rho GTPases. The pharmacological inhibition or the knocking down of ROCK diminished bacterium internalization. Moreover, C. burnetii was less efficiently internalized in HeLa cells overexpressing mDia1-N1, a dominant negative mutant of mDia1, while the overexpression of the constitutively active mutant mDia1-ΔN3 increased bacteria uptake. Interestingly, when HeLa and RAW cells were infected, RhoA, Rac1 and mDia1 were recruited to membrane cell fractions. Our results suggest that the GTPases of the Rho family play an important role in C. burnetii phagocytosis in both HeLa and RAW cells. Additionally, we present evidence that ROCK and mDia1, which are downstream effectors of RhoA, are involved in that process.

About the Authors:

Romina P. Salinas

Contributed equally to this work with: Romina P. Salinas, Rodolfo M. Ortiz Flores

Affiliation: Instituto de Histología y Embriología, Facultad de Ciencias Médicas, Universidad Nacional de Cuyo—CONICET, Mendoza, 5500, Argentina

Rodolfo M. Ortiz Flores

Contributed equally to this work with: Romina P. Salinas, Rodolfo M. Ortiz Flores

Affiliation: Instituto de Histología y Embriología, Facultad de Ciencias Médicas, Universidad Nacional de Cuyo—CONICET, Mendoza, 5500, Argentina

Jesús S. Distel

Affiliation: Instituto de Histología y Embriología, Facultad de Ciencias Médicas, Universidad Nacional de Cuyo—CONICET, Mendoza, 5500, Argentina

Milton O. Aguilera

Affiliation: Instituto de Histología y Embriología, Facultad de Ciencias Médicas, Universidad Nacional de Cuyo—CONICET, Mendoza, 5500, Argentina

María I. Colombo

Affiliation: Instituto de Histología y Embriología, Facultad de Ciencias Médicas, Universidad Nacional de Cuyo—CONICET, Mendoza, 5500, Argentina

Walter Berón

* E-mail: [email protected]

Affiliation: Instituto de Histología y Embriología, Facultad de Ciencias Médicas, Universidad Nacional de Cuyo—CONICET, Mendoza, 5500, Argentina

Introduction

The dynamic remodeling of actin cytoskeleton is intimately involved in essential cellular processes such as cell adhesion and motility [1], apoptosis [2], endocytosis and phagocytosis [3].

The small GTPases of the Rho family regulate a wide range of cellular activities including cell cycle, morphogenesis, gene transcription, cell adhesion and motility, and vesicular trafficking [4–6]. Some of these functions are tightly associated with the actin cytoskeleton dynamics. The best characterized members of the Rho family are RhoA, Rac1, and Cdc42 which, during cell motility, regulate the formation of stress fibers, lamellipodia and filopodia, respectively, [7,8]. Rho GTPases and the actin cytoskeleton are known to be involved in macropinocytosis and clathrin-dependent and independent endocytosis [3,9,10], and also in endoplasmic reticulum (ER)-Golgi transport during cell secretion [3,11,12].

To form actin filaments, actin nucleation requires factors that can be classified into three groups: the Arp2/3 complex and its nucleation promoting factors, formins, and the tandem-monomer-binding nucleators [13]. The factors mDia1 and mDia2 are members of a subset of formins known as Diaphanous-related formins (Drfs), which have the ability to nucleate and polymerize linear actin filaments [14,15]. At the plasma membrane, both mDia1 and mDia2 can form lamellipodia and filopodia [16,17]. Within the cytoplasm, mDia1 gives rise to stress fibers [18,19] and mDia2 controls the actin dynamics that contributes to vesicle movement [20]. The factors mDia1 and mDia2 have been demonstrated to be involved in actin dynamics leading to the formation of the phagocytic cup in macrophages [21]. In particular, mDia binds directly to both profilin and RhoA, which are recruited around phagocytic cups that are induced by fibronectin-coated beads, suggesting that RhoA regulates actin polymerization by targeting profilin through p140mDia beneath the specific region of plasma membranes [22]. In addition, the interaction of IQGAP with mDia1 is required for phagocytosis and phagocytic cup formation. Moreover, IQGAP mediates the localization of the actin filament nucleator mDia1 [23].

The three Rho isoforms (A, B and C) have several common effectors such as mDia and Rho-kinases (ROCK) 1 and 2, which are both essential for stress fibers formation and focal adhesion organization during cell movement [24,25]. The activation of Rho-kinase also modulates contractile ring formation during cytokinesis [26]. ROCK1 appears to be essential for the formation of stress fibers, whereas ROCK2 appears to be necessary for phagocytosis and cell contraction, both of which are dependent on the phosphorylation of the myosin light chain (MLC) and the MLC phosphatase [27–29].

Phagocytosis is the process developed by cells to engulf particulate material such as apoptotic cells, cell debris and, even, inert particles. Moreover, phagocytosis represents a crucial event that triggers host’s defense mechanisms against invading pathogens. Nevertheless, several pathogens have acquired different strategies to evade these mechanisms to survive and multiply within the host´s cell [30,31]. The phagocytic process is initiated by a recognition step in which ligands on the particle surface bind receptors on the membrane of host’s cells [32]. The ligand-receptor interaction leads to actin cytoskeleton and membrane rearrangements that permit, in the first place, particle engulfment and, in the second, particle sequestration into a phagosome which precedes maturation into a phagolysosome [33,34].

The GTPases of the Rho family control the actin cytoskeleton rearrangements needed for particle internalization by the phagocytes [35]. Fcγ and complement receptor-mediated phagocytosis, also termed Type I and Type II phagocytosis respectively, have been described in macrophages. Cdc42 and Rac1 are activated early in FcγR-mediated phagocytosis, mostly at the rims of the cup [36,37]. Firstly, Cdc42 activates and accumulates preferentially in the tips of the extending pseudopodia [37]. Soon afterwards, after Cdc42 activation and during closure, Rac1 is activated and localized throughout the phagocytic cup, while Rac2 is activated later on, mostly at the base of the cup [37,38]. RhoA seems to be primarily involved in CR3-mediated phagocytosis [36,39]. Even though some reports support the hypothesis that RhoA is unnecessary in FcγR-mediated phagocytosis [21,36,40], others suggest otherwise [41,42].

Coxiella burnetii, the causative agent of human Q fever, is an obligate intracellular bacterium found in a wide range of hosts, including livestock and humans. In the case of humans, they acquire the primary infection via the inhalation of contaminated aerosols [43,44]. Infected animals excrete C. burnetii in milk, urine and feces, and the bacteria are dispersed together with the amniotic fluids and the placenta during animal birthing. C. burnetii can survive long periods in the environment, since it is highly resistant to heat, drying and common disinfectants. C. burnetii infects mainly monocytes/macrophages, but it can also infect a wide variety of host cells in vitro [45]. This bacterium resides in an acidic parasitophorous vacuole (PV), which has late endosome-lysosome characteristics [46–49]. Recently it has been shown that the PV also interacts with the autophagic pathway, acquiring autophagosomal features [46,48,50]. Interestingly, we have shown that the PV biogenesis is regulated by actin and Rho family GTPases [51]. More recently, we have demonstrated that cortactin is involved in C. burnetii entry into the host´s cells [52].

It has been demonstrated that cytochalasin D inhibits C. burnetii uptake [53–55] and that the C3 exotransferase of Clostridium botulinum, a GTPase Rho inhibitor, inhibits membrane protrusion when the cells are infected with C. burnetii [56]. Yet, the role that the actin cytoskeleton of the host´s cell plays in the C. burnetii entry process remains to be fully characterized.

This report describes the involvement of the GTPases of the Rho family, and the effectors ROCK and mDia1 in C. burnetii internalization into HeLa and RAW cells. We observed that the overexpression of dominant negative mutants of RhoA, Rac1 and Cdc42 in HeLa cells inhibited bacterium uptake, thereby suggesting that these three GTPases are important for internalization. Similar results were obtained when specific siRNA to RhoA and Rac1 were used. We also analyzed the role of ROCK in internalization using a specific inhibitor, and by silencing the protein with a siRNA. Both treatments diminished C. burnetii internalization. Furthermore, we studied the participation of mDia1 in that process and found that the overexpression of a negative mutant of mDia1 reduced C. burnetii uptake. In summary, our results indicate that the GTPases of the Rho family and the RhoA effectors mDia1 and ROCK regulate the internalization of C. burnetii.

Materials and Methods

Materials

Dulbecco’s Modified Eagle's Medium (D-MEM), fetal bovine serum (FBS), penicillin and streptomycin were obtained from Gibco BRL/Life Technologies (Buenos Aires, Argentina). Plasmids encoding EGFP-Rac1, -Cdc42 and -RhoA dominant negative mutants were kindly provided by Dr Philippe Chavrier (Centre National de la Recherche Scientifique/Institut Curie, Paris, France) and Mark R. Phillips (Laboratory of Molecular Rheumatology, NYU, School of Medicine, USA). Plasmids encoding EGFP-mDia1 WT, and the truncated forms -mDia1-ΔN3 and -mDia1-N1 were kindly provided by Dr. Fernandez-Borja (The Netherlands Cancer Institute, Division of Tumor Biology, The Netherlands). Small interfering RNAs (siRNAs) against RhoA (1129127), Rock1 (1130663) and Rac1 (1126011) were purchased from Bioneer (Alameda, USA). The monoclonal anti-RhoA antibody was purchased from Santa Cruz Biotechnology (California, USA); and the monoclonal anti-Rac1 antibody, the monoclonal anti-mDia1 and anti-actin Ab-5 were purchased from BD (Buenos Aires, Argentina). The monoclonal anti-E cadherin antibody (Cell Signaling Technology) was a gift of Dr. Ciocca (Laboratorio de Oncología, IMBECU-CONICET, Mendoza, Argentina). Secondary antibodies were purchased from Jackson ImmunoResearch Laboratories, Inc. (West Grove, PA, USA The rabbit polyclonal anti-Coxiella antiserum was kindly provided by Dr Robert Heinzen (Rocky Mountain Laboratories, NIAID, NIH, Hamilton, MT, USA). Toxin B, from Clostridium difficile, and the inhibitor Y27632 were from Merck-Calbiochem® (Buenos Aires, Argentina). Phalloidin-FITC and the protease inhibitor cocktail were from Sigma-Aldrich (Buenos Aires, Argentina).

Cell culture

HeLa cells (Asociación Banco Argentino de Células, Buenos Aires, Argentina) were grown in DMEM supplemented with 10% heat-inactivated FBS, 2.2 g/l sodium bicarbonate, 2 mM glutamine, 100 IU/ml penicillin and 100 μg/ml streptomycin, pH 7, at 37°C under a 5% CO₂ atmosphere. RAW cells were grown in RPMI supplemented with 10% heat-inactivated FBS, 2.2 g/l sodium bicarbonate, 2 mM glutamine, 100 IU/ml penicillin and 100 μg/ml streptomycin, pH 7, at 37°C under a 5% CO₂ atmosphere.

Propagation of phase II C. burnetii

Clone 4 phase II Nine Mile strain of C. burnetii which are infective for cells in culture but not for mammals, were provided by Ted Hackstadt (Rocky Mountain Laboratories, NIAID, NIH, Hamilton, MT, USA) and handled in a biosafety level II facility. Non-confluent Vero cells were cultured in T25 flasks at 37°C under a 5% CO₂ atmosphere in DMEM supplemented with 5% FBS, 0.22 g/l sodium bicarbonate and 20 mM Hepes, pH 7 (MfbH). Cultures were infected with C. burnetii phase II suspensions for 6 days at 37°C under a 5% CO₂ atmosphere. In order to prepare cell lysates, cells were frozen at -70°C, then thawed at 37°C, scraped and passed 20 times through a 27-gauge needle connected to a syringe. Cell lysates were centrifuged at 800 x g for 10 min at 4°C. Supernatants were centrifuged at 24,000 x g for 30 min at 4°C, and pellets containing C. burnetii were resuspended in phosphate-buffered saline (PBS; 10 mM sodium phosphate, 0.9% NaCl), aliquoted and frozen at -70°C.

Infection of HeLa and RAW cells with C. burnetii

Cells (5 x 10⁵) were seeded on sterile glass coverslips placed in 24-well plates and grown overnight in MfbH medium. For infection, a 5 μl aliquot of C. burnetii suspension was added per well (Multiplicity of infection: 20–40). Cells were incubated for different lengths of time at 37°C under a 5% CO₂ atmosphere. Cells were fixed and processed for indirect immunofluorescence.

Subcellular fractionation

HeLa cells were cultured in 60-mm dishes and infected as described above for different lengths of time. Cells were washed with cold PBS and homogenization buffer HB (250 mM sucrose, 3 mM imidazole, pH 7.4), and scraped in HB containing protease inhibitors and 0.5 mM EDTA. Scraped cells were homogenized using a Dounce type homogenizer with a Teflon pestle. The homogenate was centrifuged at 13000 xg for 15 sec at 4°C. An aliquot of the supernatant (postnuclear supernatant) was frozen at -20°C (total fraction: T) and the rest was centrifuged at 100,000 x g for 30 min at 4°C. The supernatant obtained and the pellet represented the cytosolic (C) and membrane (M) fractions, respectively. Both fractions were analyzed by SDS-PAGE and Western blot.

Immunofluorescence

Cells were fixed with 2% paraformaldehyde in PBS for 10 min at 37°C, washed with PBS and blocked with 50 mM NH₄Cl in PBS. After washing, cells were incubated with a rabbit antiserum against C. burnetii (1:1000) and a donkey anti-rabbit secondary antiserum conjugated to Cy5 diluted 1:600 in PBS containing 0.5% BSA (non-permeabilizing conditions). In this condition, only extracellular bacteria were stained in white pseudo color. After washing, cells were incubated with the same rabbit antiserum against C. burnetii (1:1000) and a donkey anti-rabbit secondary antibody conjugated to Cy3 diluted 1:600 in PBS containing 0.5% BSA and 0.05% saponin (permeabilizing conditions). Under these conditions, the white-labeled extracellular bacteria were stained in red pseudo color, thus the extracellular one acquired both white and red pseudo colors, while the intracellular ones were only stained in red pseudo color. F-actin was stained with phalloidin-FITC. Coverslips were mounted with Mowiol (Sigma-Aldrich, Buenos Aires, Argentina) and examined under fluorescence microscopy (FV1000 Olympus Confocal Microscope and the FV 10-ASW 1.7 software, Olympus, Japan).

Cell transfection

HeLa cells were transfected for 6 h with 2 μg/ml pEGFP empty vector or pEGFP plasmids expressing the fusion proteins of EGFP with the dominant negative mutants RhoA N19, Rac1 N17 or Cdc42 N17, mDia1 WT or the truncated forms mDia1-ΔN3 and mDia1-N1. Cell transfection was carried out using Lipofectamine® 2000 (Invitrogen, Buenos Aires, Argentina), according to the manufacturer’s instructions. After 6 h of transfection, cells were washed and incubated for 18 h in MfbH medium at 37°C under a 5% CO₂ atmosphere The siRNA transfection was performed employing Lipofectamine® 2000 according to the manufacturer’s instructions (Bioneer, Alameda, USA).

Western blotting

HeLa and RAW cells were cultured in 60 mm dishes and infected as described earlier for different lengths of time. After infection, cells were washed with PBS, scraped into ice-cold lysis buffer (50 mM Tris-HCl, pH 7.2, 1% Triton X-100, 0.5% deoxycholate, 0.1% SDS, 50 mM NaCl, 10 mM MgCl₂, 2 mM Na₃VO₄, 10 mM NaF, 0.5 mg/ml DTT, 2 mM EDTA) supplemented with a protease inhibitor cocktail and kept on ice for 20 min. Lysates were clarified by centrifugation at 2000 x g for 15 min at 4°C. Clarified lysates were transferred to clean tubes, mixed with Laemmli buffer and boiled for 5 min. Samples were resolved by SDS-PAGE and the proteins transferred to nitrocellulose membranes using standard procedures. Membranes were blocked for 2 h at 4°C in Tween-Tris-buffered saline (TTBS; 0.1% Tween 20, 100 mM Tris/HCl, 0.9% NaCl) supplemented with 5% BSA, then incubated overnight at 4°C with the appropriate primary antibodies. Membranes were washed three times with TTBS and then incubated for 2 h at room temperature with appropriate peroxidase-conjugated secondary antibodies. Membranes were washed again with TTBS and developed using the ECL Western blotting system (GE Healthcare) according to the supplier’s recommendations. Anti-actin and anti-E cadherin antibodies were used as loading controls. Band densitometry was carried out using ImageJ software (NIH, USA).

Fluorescence microscopy

Cells were analyzed by fluorescence microscopy using an FV1000 Olympus Confocal Microscope and the FV 10-ASW 1.7 software (Olympus, Japan). Images were processed using ImageJ software. Cell boundaries were marked with dotted lines in all figures showing experiments performed with transfected cells.

Statistical analysis

Differences between conditions were tested by one-way analysis of variance (ANOVA) and Dunnett’s post hoc tests or Student’s t single group test. Differences were considered significant at p < 0.05.

Results

Clostridium difficile toxin B, an inhibitor of Rho family GTPases, diminishes the internalization of C. burnetii by phagocytic and non-phagocytic cells

It is well known that to accomplish internalization into the host´s cells, several pathogens modulate the GTPases of the Rho family [57]. In previous works, we have demonstrated that actin and Rho GTPases are involved in the intracellular trafficking of C. burnetii [51]. However, comprehensive studies regarding the role of these GTPases in C. burnetii entry into host cells are scarce. Clostridium difficile toxin B is a pharmacological tool used to study Rho GTPases function. This toxin is a protein that monoglucosylates RhoA, Rac1 and Cdc42, leading to their irreversible inactivation [58,59].

To determine the role of Rho GTPases in the internalization of C. burnetii, RAW and HeLa cells (phagocytic and non-phagocytic cells, respectively), were infected for 4 h at 37°C in the presence of different toxin B concentrations. Cells were fixed, processed for indirect immunofluorescence and analyzed by confocal microscopy to evaluate cell morphology and the number of intracellular bacteria. F-actin was stained with phalloidin-FITC. Control cells (DMSO-treated) the typical HeLa cell morphology with typical cortical actin, filopodia and stress fibers (Fig 1A, panel a). As expected, the toxin altered HeLa morphology mainly at high concentrations, a condition under which cells became rounded and lost the typical actin structure (Fig 1A, panel p). In the inset panels of Fig 1A, intracellular bacteria are shown in red pseudo color (yellow arrowheads) while the extracellular ones are shown in red and white pseudo colors (arrows). The number of intracellular bacteria was lower in cells treated with toxin B as compared to the control (Fig 1A, insets, and B). Toxin treatment inhibited C. burnetii internalization in a dose-dependent manner. Similar results were observed when RAW cells were infected (Fig 2). Even though the toxin-treated RAW cells exhibited milder changes in their shapes as compared to non-treated cells (Fig 2A), they lost the typical actin structures and were less efficient in C. burnetii internalization (Fig 2A, insets, and 2B). Treatment with increasing concentrations of toxin B did not affect significantly the number of total bacteria associated to HeLa (Fig 1C) or RAW (Fig 2C) cell surfaces. These findings would indicate that the progressive inhibition of the bacterium internalization is not due to a defective in bacterial cell adherence.

[Figure omitted. See PDF.]

Fig 1. Clostridium difficile toxin B diminishes the internalization of C. burnetii by HeLa cells.

(A) HeLa cells were infected with C. burnetii for 4 h at 37°C in the presence of 0.05% DMSO (control, panels a-e) or with different concentrations of Clostridium difficile toxin B (panels f-t). Cells were fixed and processed for indirect immunofluorescence to determine C. burnetii internalization and F-actin distribution as described in Materials and Methods. Cells were analyzed by confocal microscopy. Micrographs of representative cells are shown. Cells were incubated sequentially with an antibody against C. burnetii and an appropriate secondary antibody conjugated to Cy5 (white pseudo color) under non-permeabilizing conditions. Under this condition, extracellular bacteria were stained in white pseudo color (panels c, h, m, and r). Then, cells were re-incubated with the same anti-C. burnetii antibody and an appropriate secondary antibody conjugated to Cy3 (red pseudo color) under permeabilizing conditions. Under this condition total bacteria were stained in red pseudo color (panels b, g, l, and q). In the merged images (panels d, i, n and s) and the insets of the merged images (panels e, j, o, and t), extracellular C. burnetii is shown in white and red pseudo colors (arrows), while intracellular C. burnetii is shown in red pseudo color (yellow arrowheads). F-actin was labeled with phalloidin-FITC (green, panels a, f, k, and p). Bars scale: 5 μm. (B) Quantification of C. burnetii internalized in control and toxin-treated HeLa cells. (C) Quantification of total C. burnetii associated to control and treated HeLa cells. Between 100 and 120 cells and 1200 and 1600 bacteria were counted in each experiment. Results are expressed as means ± SE of three independent experiments. *p < 0.05, **p < 0.01 compared to the DMSO treatment (one-way ANOVA and Dunnett's post hoc test). ns: non-significant differences between groups (p > 0.05).

https://doi.org/10.1371/journal.pone.0145211.g001

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Fig 2. Clostridium difficile toxin B diminishes internalization of C. burnetii by RAW macrophages.

(A) RAW cells were infected with C. burnetii for 4 h at 37°C in the presence of 0.05% DMSO (control, panels a-e) or different concentrations of Clostridium difficile toxin B (panels f-t). Cells were fixed and processed for indirect immunofluorescence to determine C. burnetii internalization and F-actin distribution as described in Materials and Methods. Cells were analyzed by confocal microscopy. Micrographs of representative cells are shown. As indicated in Fig 1, extracellular and total bacteria were stained in white pseudo color (panels c, h, m, and r) and red pseudo color (panels b, g, l, and q), respectively. In the merged images (panels d, i, n, and s) and the insets of the merged images (panels e, j, o, and t), extracellular C. burnetii is shown in white and red pseudo colors (arrows), while intracellular C. burnetii is shown in red pseudo color (yellow arrowheads). F-actin was labeled with phalloidin-FITC (green). Bar scale: 10 μm. (B) Quantification of C. burnetii internalized in control and toxin-treated RAW cells. (C) Quantification of total C. burnetii associated to control or toxin-treated cells. Between 100 and 120 cells and 1200 and 1600 bacteria were counted in each experiment. Results are expressed as means ± SE of three independent experiments. **p < 0.01, ***p < 0.001, compared to DMSO treatment (one-way ANOVA and Dunnett's post hoc test). ns: non-significant differences between groups (p > 0.05).

https://doi.org/10.1371/journal.pone.0145211.g002

These results suggest that the GTPases belonging to the Rho family play a role in C. burnetii entry into both phagocytic and non-phagocytic cells.

RhoA and Rac1 GTPases are recruited to the membrane fraction obtained from HeLa cells infected with C. burnetii

It is known that the GTPases of the Rho family regulate the actin cytoskeleton reorganization beneath the plasma membrane of the host´s cells in contact with particles or microorganisms to be engulfed during phagocytosis [60,61]. GTPases cycle between an active state (GTP-bound) and an inactive one (GDP-bound). It is also known that in the GTP-bound form, GTPases are recruited to membranes and initiate intracellular signal cascades that regulate different cell functions [62,63].

We suggest that C. burnetii estimulates recruitment of Rho GTPases to the host´s cell membrane during phagocytosis. To test our hypotesis, HeLa cells were infected for different periods of time, lysed and cetrifuged to obtain membrane and cytosolic fractions. Postnuclear supernatant (T: total fraction), cytosol (C) and membrane (M) fractions were analyzed by SDS-PAGE and Western blot. Fig 3A and 3B depicts that RhoA recruitment to the membrane fraction increased after 30 min and peaked after 60 min of infection. After this timepoint, the levels of Rho membrane association decreased to basal levels. This result suggests that RhoA is activated during C. burnetii-host´s cell interaction. Interestingly, when the Rac1 membrane recuitment was analyzed, as shown in Fig 3C and 3D, the maximum level was observed after 30 min of infection, sugesting that Rac1 is also activated, though earlier than RhoA. The membrane recruitment of Cdc42 during infection was also analyzed, but unfortunately the antibody against Cdc42 used was unable to detect the protein even in the total fraction (data not shown). Similar results were obtained in HeLa cells incubated with heat-killed C. burnetii (S1 Fig). Therefore, the same signaling cascade can be activated by live and heat-killed C. burnetii during phagocytosis.

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Fig 3. RhoA and Rac1 are recruited to a membrane fraction obtained from cells infected with C. burnetii.

HeLa cells were infected with C. burnetii for different lengths of time, lysed and centrifuged to obtain postnuclear supernatant, membrane and cytosolic fractions as described in Materials and Methods. (A) Postnuclear supernatant (T: total), cytosol (C) and membrane (M) fractions were analyzed by SDS-PAGE and Western blot using antibodies against RhoA and Rac1. Anti-actin and anti-E cadherin antibodies were used as loading controls. (B) Quantification of RhoA or Rac1 recruitment to the membrane fraction. The band intensities corresponding to RhoA, Rac1, E cadherin and actin were measured by the ImageJ software, and the band intensity ratio between RhoA and E cadherin, and Rac1 and E cadherin in the membrane fractions was calculated. Results are expressed as means ± SE from at least three independent experiments. Mean values were compared with the 0 min infection condition by Student’s t test for single group mean (*p < 0.05, ***p < 0.001). ns: non-significant differences between groups (p > 0.05). RU: Relative Units.

https://doi.org/10.1371/journal.pone.0145211.g003

Internalization of C. burnetii by HeLa cells is inhibited by overexpression of Rho GTPases dominant negative mutants or by silencing these proteins

The inhibitory effect of toxin B in C. burnetii internalization and recruitment of Rho GTPases to a membrane fraction obtained from infected cells suggests that Rho GTPases are activated during infection. An experimental approach to assess the requirement for the active forms of Rho GTPases during the bacterium entry consists in overexpressing the dominant negative mutants of these proteins. HeLa cells were transfected with pEGFP-RhoA N19, pEGFP-Cdc42 N17 or pEGFP-Rac1 N17 and then infected for 4 h at 37°C. Cells were fixed and processed as mentioned before to evaluate the number of intracellular bacteria. As displayed in Fig 4A, the overexpressed dominant negative mutants featured a diffused distribution in the cytoplasm (Fig 4A, panels f, k and p).

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Fig 4. C. burnetti internalization is inhibited by overexpression of the dominant negative mutants of Rho GTPases.

(A) HeLa cells were transfected with pEGFP (panels a-e), pEGFP-RhoA N19 (panels f-j), pEGFP-Cdc42 N17 (panels k-o), or pEGFP-Rac1 N17 (panels p-t). Cells were infected for 4 h at 37°C with C. burnetii and subsequently fixed and processed for immunofluorescence to determine the levels of C. burnetii internalization as described in Materials and Methods. Cells were analyzed by confocal microscopy. Representative micrographs are presented. As indicated in Fig 1, extracellular and total bacteria were stained in white pseudo color (panels c, h, m, and r) and red pseudo color (panels b, g, l, and q), respectively. In the merged images (panels d, i, n, and s) and the insets of the merged images (panels e, j, o, and t), extracellular C. burnetii is shown in white and red pseudo colors (arrows), while intracellular C. burnetii is shown in red pseudo color (yellow arrowheads). Bars scale: 5 μm. (B) Quantification of C. burnetii internalized by transfected HeLa cells. (C) Quantification of total C. burnetii associated to HeLa cells. Between 40 and 60 cells and between 400 and 600 bacteria were counted in each experiment. Results are expressed as means ± SE of three independent experiments. *p < 0.05, **p < 0.01 compared to the EGFP control (one-way ANOVA and Dunnett's post hoc test). ns: non-significant differences between groups (p > 0.05).

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In HeLa cells overexpressing EGFP, a larger number of intracellular bacteria (red pseudo color, yellow arrowheads) was observed in relation to the extracellular ones (red and white pseudo colors, arrows) (Fig 4A, panel e). In HeLa cells overexpressing the dominant negative mutants of the three Rho GTPases, a significant inhibition of C. burnetii internalization was observed (Fig 4A, panels j, o and t, and B). Total bacteria associated to the cells was not significantly different among the tested constructs (Fig 4C), thus indicating that the low percentage of internalized bacteria is not due to a defective bacterial adherence to cells. The strongest inhibitory effect was observed in cells overexpressing the dominant negative mutant of RhoA (i.e., RhoA N19). These results suggest that the active forms of RhoA, Cdc42 and Rac1 are important for the entry of C. burnetii into host´s cells.

To confirm the role of RhoA and Rac1 in the internalization process, these proteins were knocked down by specific siRNAs. HeLa cells were transfected with siRNAs against RhoA and Rac1 and then infected for 4 h at 37°C. Cells were either lysed to analyze the depletion levels of RhoA and Rac1 proteins (see Fig 5D) or fixed and processed as mentioned above in order to evaluate the number of intracellular bacteria. The number of intracellular bacteria (red pseudo color, yellow arrowheads) was lower in HeLa cells transfected with Rac1 (Fig 5A, panels c and d, and B) and RhoA (Fig 5A, panels e and f, and B) siRNAs as compared to that observed in cells transfected with the scramble siRNA (Fig 5A, panels a and b, and B). The depletion of the endogenous RhoA or Rac1 proteins diminished C. burnetii internalization without significantly affecting the number of total bacteria associated to HeLa cells. This finding suggests that the inhibition of the bacterium internalization is not explained by a defect in bacteria adherence to the cells (Fig 5C). These inhibitory effects are in agreement with those produced by the overexpression of the dominant negative mutants RhoA N19 and Rac1 N17.

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Fig 5. Knockdown of Rho GTPases and Rock inhibits internalization of C. burnetii.

(A) HeLa cells were co-transfected with pEGFP and a scramble (panels a and b), Rac1 (panels c and d), RhoA (panels e and f) or ROCK (panels g and h) siRNAs or the RhoA/Rac1 siRNA combination (panels i and j). Cells were infected for 4 h at 37°C with C. burnetii and then fixed and processed for immunofluorescence to determine C. burnetii internalization as described in Materials and Methods. Cells were analyzed by confocal microscopy. Representative micrographs of cells are presented. As indicated in Fig 1, in the merged images (panels a, c, e, g, and i) and the insets of the merged images (panels d, d, f, h, and j), extracellular C. burnetii is shown in white and red pseudo colors (arrows), while intracellular C. burnetii is shown in red pseudo color (yellow arrowheads). Scale bar: 5 μm. (B) Quantification of C. burnetii internalized by transfected HeLa cells. (C) Quantification of total C. burnetii associated to HeLa cells. Between 40 and 60 cells and between 400 and 600 bacteria were counted in each experiment. Results are expressed as means ± SE of three independent experiments. ***p < 0.001, compared to scramble siRNA (one-way ANOVA and Dunnett's post hoc test). ns: non-significant differences between groups (p > 0.05). (D) Lysates of cotransfected HeLa cells were analyzed by SDS-PAGE and Western blot using antibodies against Rac1, RhoA and ROCK. An anti-actin antibody was used as loading control. Scr: scramble siRNA.

https://doi.org/10.1371/journal.pone.0145211.g005

To test the possibility of a combined effect that would further inhibit C. burnetii entry, HeLa cells were cotransfected with siRNAs targeted to RhoA and Rac1 and then infected for 4 h at 37°C. Cells were fixed and processed as described above to evaluate the number of intracellular bacteria. The level of C. burnetii internalization in cells depleted for both RhoA and Rac1 (Fig 5A, panels i and j, and B) was similar (Fig 5A, panels e and f, and B). The number of total bacteria associated to HeLa cells did not change significantly (Fig 5C) indicating that the low percentage of internalized bacteria does not result from a defective bacterial adherence to cells. These results suggest that there is no additive effect of RhoA and Rac1 on C. burnetii internalization and that these GTPases participate in two parallel pathways. However, this hypothesis should be confirmed.

ROCK, an effector of RhoA, is involved in the internalization of C. burnetii

It is known that during cell adhesion and migration, RhoA regulates stress fiber formation and contraction through the ROCK-dependent phosphorylation of the myosin light chain [64,65]. ROCK has also been demonstrated to be involved in phagocytosis [28,29]. Taking into account the recruitment of RhoA at the membranous fraction in cells infected with C. burnetii (Fig 3A and 3B), the role of RhoA in C. burnetii internalization (Fig 4A and 4B), and that ROCK is a downstream effector of RhoA, we decided to assess if this kinase participates in the bacterium uptake. One strategy to assess this issue was to diminish the cell synthesis of ROCK. To this end, HeLa cells were transfected with siRNA against ROCK and then infected for 4 h at 37°C. Cells were either lysed to analyze the depletion levels of ROCK protein (see Fig 5D) or fixed and processed as outlined above to evaluate the number of intracellular bacteria. The number of intracellular bacteria (red pseudo color, yellow arrowheads) was lower in HeLa cells transfected with ROCK siRNAs (Fig 5A, panels g and h, and B) in relation to the number of bacteria observed in cells transfected with the scramble siRNA (Fig 5A, panels a and b, and B). The depletion of the endogenous ROCK protein decreased C. burnetti internalization without significantly affecting the number of total bacteria associated to cells. This evidences that the inhibition of the bacterium internalization is not due to a defect in bacterial cell adherence (Fig 5C). These results suggest that ROCK plays a key role in the internalization of C. burnetii.

The other experimental approach to assess the role of ROCK in the uptake of C. burnetii was to inhibit the kinase by a specific inhibitor. To this end, HeLa or RAW cells were pre-incubated with different concentrations of Y27632, a ROCK inhibitor, and then infected for 4 h at 37°C. Cells were fixed and processed as described earlier so as to evaluate the number of intracellular bacteria. As displayed in Fig 6A and 6B, Y27632 inhibited C. burnetii internalization in a dose-dependent manner without affecting the total bacteria associated to the cells (Fig 6C), thus indicating that the adhesion of the bacteria to the cell surface is not affected by the inhibitor. As expected, the inhibitor altered the stress fibers formation (Fig 6A). Similar results were obtained using RAW cells (Fig 6D–6F). These results suggest that ROCK participates in the internalization of C. burnetii regardless of the cell lines used (e.g. epithelial cells or macrophages).

[Figure omitted. See PDF.]

Fig 6. The specific inhibitor of ROCK, Y27632, diminishes C. burnetii internalization by HeLa or RAW cells.

(A) HeLa or (D) RAW cells were infected with C. burnetii for 4 h at 37°C in the presence of 0.05% DMSO (control, A, panel a; D, panel a) or different concentrations of Y27632 (A, panels b-d; D, panels b-d). Cells were fixed and processed for indirect immunofluorescence to determine C. burnetii internalization and F-actin distribution as described in Materials and Methods. Cells were analyzed by confocal microscopy. Representative micrographs of cells are presented. F-actin was labeled with phalloidin-FITC (green). Representative micrographs of cells are presented. As indicated in Fig 1, in the merged images (A, panels a, b, c, and d; D, panels a, b, c, and d), extracellular C. burnetii is shown in white and red pseudo colors (arrows), while intracellular C. burnetii is shown in red pseudo color (yellow arrowheads). Between 100 and 120 cells and between 1200 and 1600 bacteria were counted in each experiment. Scale bar: 5 μm (A); 10 μm (D). Quantification of C. burnetii internalized by Y27632-treated HeLa (B) or RAW (E) cells. Quantification of total C. burnetii associated to HeLa (C) or RAW (F) cells. Results are expressed as means ± SE of three independent experiments. ***p < 0.001, compared to DMSO treatment (one-way ANOVA and Dunnett's post hoc test). ns: non-significant differences between groups (p > 0.05).

https://doi.org/10.1371/journal.pone.0145211.g006

The factor mDia1, an effector of RhoA, is recruited to the membrane fraction obtained from HeLa cells infected with C. burnetii

The factor mDia1 belongs to the formin family of proteins which behave as actin nucleator factors regulating actin dynamics [14,15]. Upon activation by RhoA, mDia1 is recruited to cell membrane to become functional [22,66]. Therefore, we decided to assess whether mDia1 is recruited to the cell membrane during infection. Then, HeLa cells were infected for different periods of time, lysed and centrifuged to obtain a membrane and a cytosolic fraction. Postnuclear supernatant (T: total fraction), cytosol (C) and membrane (M) fraction were analyzed by SDS-PAGE and Western blot. Fig 7A and 7B, shows that mDia1 recruitment to the membrane fraction increased after 30 min and reached its peak after 60 min of infection, a time point after which the levels of protein association decreased to basal levels. The mDia1 showed similar membrane recruitment kinetics when the experiments were performed with heat-killed C. burnetii (S1 Fig). The latter result strongly suggests that mDia1 is activated during C. burnetii-host´s cell interaction. Interestingly, the infection time of maximum mDia1 recruitment was similar to that observed for RhoA (Fig 3A and 3B).

[Figure omitted. See PDF.]

Fig 7. The factor mDia1 is recruited to membrane fraction obtained from cells infected with C. burnetii.

(A) HeLa cells were infected with C. burnetii for different lengths of time, lysed and centrifuged to obtain postnuclear supernatant, membrane and cytosolic fractions. (A) Postnuclear supernatant (T: total), cytosol (C) and membrane (M) fractions were analyzed by SDS-PAGE and western blot using an antibody against mDia1. Anti-actin and anti-E cadherin antibodies were used as loading controls. (B) Quantification of mDia1 recruitment to membrane fraction. The band intensity of mDia1, E cadherin and actin was measured by the ImageJ software, and band intensity ratio between mDia1 and E cadherin in the membrane fractions was calculated. Results are expressed as means ± SE from at least three independent experiments. Means were compared with the 0 min infection condition by Student’s t test for single group mean (**p < 0.01, ***p < 0.001). ns: non-significant differences between groups (p > 0.05). (RU): Relative Units.

https://doi.org/10.1371/journal.pone.0145211.g007

Internalization of C. burnetii by HeLa cells is stimulated by overexpression of a constitutively active variant of mDia1

The best-studied formins are diaphanous-related formins (DRFs), which are direct effectors of the Rho GTPases family. DRF proteins, such as mDia, have the actin assembly activity in the C-terminal end and the regulatory region in the N-terminal end, which mediates intramolecular interactions with the C terminus to maintain formins in an autoinhibited state [67]. The C-terminal end contains three structural and functional elements: (a) the profilin-binding FH1, (b) the actin-binding FH2, and (c) the diaphanous autoregulatory domain (DAD). The N terminus consists of four distinct structural domains, including (a) the GTPase binding domain (GBD), which binds Rho family GTPases in the GTP-bound state; (b) the diaphanous inhibitory domain (DID), which binds the C-terminal autoinhibitory DAD segment and also interacts with Rho GTPases; (c) the dimerization domain (DD); and (d) a coiled-coil (CC) region. The inactive mDia adopts an autoinhibitory conformation mediated by an intramolecular interaction between the DAD, DID and a part of the GBD domains. Binding of GTP-bound Rho protein (GTP Rho) to the GBD domain promotes formin release from the autoinhibited state [67,68].

To test whether mDia1 plays a role in the internalization process, HeLa cells were transfected with pEGFP-mDia1 wild type (WT), pEGFP-mDia1-N1 or pEGFP-mDia1-ΔN3. The truncated mutants mDia1-N1 (N-terminal Rho-binding domains) and mDia1-ΔN3 (C-terminal FH1 and FH2 domains) function as dominant negative and constitutively active forms, respectively [18]. After transfection, cells were infected for 4 h at 37°C, fixed and processed as specified above to evaluate the number of intracellular bacteria. The different overexpressed constructs of mDia1 (Fig 8A) featured a distribution similar to that reported by Watanabe et al [18]. C. burnetii internalization diminished in cell overexpressing EGFP-mDia1-N1 suggesting that the FH2 and FH3 domains are important for actin cytoskeleton remodeling involved in C. burnetii uptake. In turn, an increase in internalization was observed in cells overexpressing the active EGFP-mDia1-ΔN3 construct (Fig 8A and 8B). The overexpression of all constructs did not significantly affect the amount of total bacteria associated to the cells. This finding evidences that changes in the bacterium internalization process is not due to a defect in bacteria adherence to the cells (Fig 8C).

[Figure omitted. See PDF.]

Fig 8. The overexpression of the dominant negative mutants of mDia1 inhibits internalization of C. burnetii.

(A) HeLa cells were transfected with pEGFP (panels a-e), pEGFP-mDia1 WT (panels f-j), pEGFP-mDia1-N1 (dominant negative form) (panels k-o) or pEGFP-mDia1-ΔN3 (constitutively active form) (panels p-t). Transfected cells were infected for 4 h at 37°C with C. burnetii. Cells were fixed and processed for immunofluorescence to determine C. burnetii internalization as described in Materials and Methods. Cells were analyzed by confocal microscopy. Representative micrographs of cells are presented. As indicated in Fig 1, extracellular and total bacteria were stained in white pseudo color (panels c, h, m, and r) and red pseudo color (panels b, g, l, and q), respectively. In the merged images (panels d, i, n, and s) and the insets of merged images (panels e, j, o, and t), extracellular C. burnetii is shown in white and red pseudo colors (arrows), while intracellular C. burnetii is shown in red pseudo color (yellow arrowheads). Scale bar: 5 μm. (B) Quantification of C. burnetii internalized by transfected HeLa cells. (C) Quantification of total C. burnetii associated to HeLa cells. Between 40 and 60 cells and between 400 and 600 bacteria were counted in each experiment. Results are expressed as means ± SE of three independent experiments. *p < 0.05, **p < 0.01 compared to the EGFP control (one-way ANOVA and Dunnett's post hoc test). ns: non-significant differences between groups (p > 0.05).

https://doi.org/10.1371/journal.pone.0145211.g008

Taken together, these results indicate that the RhoA effector mDia1 is activated and recruited to the membranes upon infection with Coxiella and, in addition, its function is important for C. burnetii entry into host cells.

The overexpression of a constitutively active variant of mDia1 stimulated internalization of C. burnetii in RhoA-depleted HeLa cells

To examine the relationship between mDia91 and RhoA in the internalization process, HeLa cells were cotransfected with siRNAs targeted to RhoA and pEGFP-mDia1 WT or pEGFP-mDia1-ΔN3 (constitutively active form) and then infected for 4 h at 37°C. Cells were fixed and processed as specified above to evaluate the number of intracellular bacteria. The internalization of C. burnetii was found to be diminished in WT EGFP-mDia1 overexpressing cells that were transfected with RhoA siRNA as compared to those transfected with scramble siRNA. Interestingly, the internalization of C. burnetii increased in EGFP-mDia1-ΔN3 overexpressing cells that were transfected with RhoA or scramble siRNAs (Fig 9A and 9B). These results indicate that the constitutively active form of mDia1 restores C. burnetii uptake in cells depleted of RhoA. As expected, once mDia1 is activated, its function can be performed independently of RhoA.

[Figure omitted. See PDF.]

Fig 9. The overexpression of the constitutively active form of mDia1 restored the entry of C. burnetii into RhoA-knocked down HeLa cells.

(A) HeLa cells were cotransfected with pEGFP-mDia1 WT (panels a-j) or pEGFP-mDia1-ΔN3 (constitutively active form) (panels k-t) and scramble siRNA (panels a-e) or RhoA siRNA (panels p-t). Transfected cells were infected for 4 h at 37°C with C. burnetii. Cells were fixed and processed for immunofluorescence to determine C. burnetii internalization as described in Materials and Methods. Cells were analyzed by confocal microscopy. Representative micrographs of cells are presented. As indicated in Fig 1, extracellular and total bacteria were stained in white pseudo color (panels c, h, m, and r) and red pseudo color (panels b, g, l, and q), respectively. In the merged images (panels d, i, n, and s) and the insets of merged images (panels e, j, o, and t), extracellular C. burnetii is shown in white and red pseudo colors (arrows), while intracellular C. burnetii is shown in red pseudo color (yellow arrowheads). Scale bar: 5 μm. (B) Quantification of C. burnetii internalized by cotransfected HeLa cells. (C) Quantification of total C. burnetii associated to HeLa cells. Between 40 and 60 cells and 400 and 600 bacteria were counted in each experiment. Results are expressed as means ± SE of three independent experiments. ***p < 0.001 compared to the EGFP control (one-way ANOVA and Dunnett's post hoc test). ns: non-significant differences between groups (p > 0.05). Scr: scramble siRNA.

https://doi.org/10.1371/journal.pone.0145211.g009

Discussion

Several pathogens are able to modulate the host´s cells functions as an evasion mechanism. During the interaction with host´s cells, the microorganisms can remain adhered to the cell surface or being internalized and then become sequestered into an intracellular vacuole that prevents the fusion with lysosomes. Once internalized, other pathogens lyse the phagosome and multiply within the cytoplasm using host’s actin filaments to disseminate to neighboring cells [69].

It is well known that C. burnetii is a pathogen that transits along the phagocytic pathway interacting with different endosomal compartments, generating a PV with autophagolysosomal characteristics; however, the C. burnetii entry to the host´s cells is a poorly characterized mechanism. Nonetheless, it has previously been demonstrated that C. burnetii NMII and NMI internalization is diminished in fibroblasts and monocytes treated with cytochalasin D, an inhibitor of actin polymerization, suggesting a participation of the actin cytoskeleton in that process [53–55]. In this work, similar results were obtained in HeLa and RAW cells infected with C. burnetii NMII and treated with cytochalasin D (data not shown). Meconi et al. [56] have postulated that monocytes incubated with C. burnetii NMI exhibited dramatic plasma membrane extensions and protrusions associated to actin cytoskeleton reorganization. Conversely, only a few membrane folds were observed in cells incubated with the attenuated C. burnetii NMII [56]. However, the molecular events related to the morphological changes observed in the plasma membrane and the entry of C. burnetii NMI or NMII into monocytes were not analyzed. Interestingly, and despite the more profound changes in the host´s plasma membrane induced by virulent C. burnetii compared to that caused by the avirulent bacterium, the internalization of the latter was more efficient [54]. All together, these observations are in agreement with our experimental model in which discreet plasma membrane extensions stimulated by avirulent C. burnetti are associated with a minor actin cytoskeleton rearrangement that allows effective C. burnetii internalization. Adhesion and invasion of bacteria to the host’s cell can be either an active or a passive process. The active one, termed "triggering mechanism", involves a bacterial type 3 secretion system (T3SS) that injects effectors into the host´s cell cytoplasm to stimulate uncontrolled actin rearrangement ruffles formation and bacteria internalization. The passive process or "zippering mechanism", involves a narrow interaction between bacteria (ligands) and host´s cell (receptors) surfaces, pseudopodia formation and bacterial uptake [70,71]. Cumulative evidence indicates that C. burnetii uses a zipper mechanism to entry into the host´s cell [72]. C. burnetii enters the cell by a sinking process that involves the extension of much lower prominent pseudopodia as compared to other bacteria or IgG-opsonized particles [73,74].

We have previously demonstrated that the formation of C. burnetii containing PV depends on actin and GTPases of the Rho family [51]. More recently, after studying the early interaction between C. burnetii and the host´s cell, we showed that cortactin, a protein that participates in the regulation of actin cytoskeleton dynamics, plays a role in the C. burnetii internalization step [52]. The present study contributes to further understand the role of the GTPases of the Rho family in bacterial pathogenesis. We provide evidence that Rac1, Cdc42 and, particularly, RhoA, and their effectors mDia1 and ROCK, are involved in signal transduction pathways that are involved in the internalization of avirulent C. burnetii into phagocytic and non-phagocytic cells. The use of different cellular models have facilitated important progresses to better understand C. burnetii-host´s cells interaction [75–77], as well as to study the host-cell interplay of other pathogens [78,79]. In this work, RAW and HeLa cell lines were used as professional and non-professional phagocytes, respectively, demonstrating that similar molecular mechanisms are involved in both infection models.

The GTPases of the Rho family, main regulators of actin cytoskeleton dynamics, participate in phagocytosis and invasion of several pathogens [80,81]. Our data demonstrate the role of Rho GTPases in C. burnetii internalization in both HeLa and RAW cells by using C. difficile toxin B, a pharmacological tool used in other experimental models of infection of HeLa cells with Chlamydia trachomatis [82] or Neisseria meningitidis [83]. Meconi et al [56] have demonstrated that monocytes treated with the C3 exotransferase of C. botulinum, an inhibitor of Rho GTPases, drastically diminished the formation of membrane protrusions induced by infection with C. burnetii NMI [56]; however, these authors have not assessed the bacterium internalization. In this study, C. difficile toxin B abrogated C. burnetii uptake in HeLa as well as RAW cells, suggesting that the GTPases of the Rho family have a critical regulatory function in the internalization process.

It has previously been demonstrated that GTPases, when activated, are recruited to membranes from the cytoplasm [62,63,84]. We observed that Rac1 and RhoA associated to a membrane fraction obtained from cells infected with C. burnetii after 30 and 60 min, respectively. This result suggests that the bacterium sequentially activates different members of the Rho GTPases family during infection. By the FRET technique, it has been shown that during IgG-opsonized erythrocytes phagocytosis, Rac1 and Rac2 were activated shortly after Cdc42 activation [37]. More interestingly, during phagocytosis of complement-opsonized zymosan particles, RhoA activation was detected by western blotting after 20 min of internalization [39]. This activation time is similar to the one observed in our C. burnetii infection model. Unfortunately, the antibody against Cdc42 used was unable to detect the protein even in the postnuclear supernatant. Thus, the activation of Cdc42 during C. burnetii infection could not be ruled out.

Interestingly, it has been reported that the activation level of Rho GTPases in cell lines, even in cells strongly stimulated, is often very low, around 5% of the total GTPase pool, to be easily detected by techniques such as western blot [85–88]. Moreover, the cycling of GTPases between membrane and cytoplasm, and their interaction with RhoGDI affects the sensibility of immunostaining experiments as well as GFP-Rho overexpression experiments because a very low fraction of GTPase is activated in a spatio-temporal way in the cell [87,89]. The low recruitment to the membrane and the fast cycling of the Rho proteins may explain the fact that we could not detect the EGFP-mDia1 at the Coxiella entry sites by fluorescent microscopy. Biosensors have been used to visualize, at high resolution, the activation of Rho GTPases in living cells [86,87,90]. The application of these tools in future studies will greatly enhance the ability to analyze and understand the role of GTPase activation during C. burnetii infection.

In the present study, we demonstrated the importance of the active state of Rho GTPases in C. burnetii internalization by using HeLa cells overexpressing dominant negative mutants which significantly decreased the bacterium entry into the cells. A similar experimental approach has been used to evidence the internalization process of other pathogens. Chlamydia caviae internalization is controlled by Cdc42 and Rac1 [80], whereas in the uptake of Chlamydia trachomatis, only Rac1 is involved [82]. These results suggest that the process is highly dependent on bacterium species. However, in some cases, the relationship between uptake and Rho proteins seems to be related to the type of host´s cells. For instance, Listeria entry is Rac-dependent in Vero cells but requires both Rac1 and Cdc42 in Ref52 fibroblasts [91] or mainly Cdc42 in HeLa cells [92]. The internalization of Neisseria meningitidis into COS epithelial cells expressing specific Opa-receptors is mediated by Cdc42 and Rac1, but is independent of RhoA activity [83]. Interestingly, we show herein that the three GTPases are involved in C. burnetii internalization by HeLa cells, thus suggesting that these GTPases may act synergistically during the entry of these bacteria. Burnham et al [93] have reported comparable results during invasion of HeLa cells by Streptococcus. The role of Rho GTPases has also been tested by using specific siRNAs. Our results demonstrate that the level of C. burnetii uptake in cells depleted of RhoA or Rac1 was similar to that observed in cells depleted of the two GTPases. The double-knockdown results suggest that there exists no additive effect between RhoA and Rac1 and that these GTPases participate in two parallel pathways. We believe that these hypotheses remain to be tested, which is difficult to attain, considering the complex crosstalk between the GTPases of the Rho family. It is known that the crosstalk between Rho-GTPase signals that involves formation of complexes between regulators of the same and different GTPases (GAP, GEF, membrane receptors, downstream effectors) hinders the interpretation of physiological cell processes [87,94].

It is noteworthy that the recruitment of mDia1, an effector of RhoA, to membrane fractions of cells infected with C. burnetii suggests that mDia1 acquires an open conformation that exposes the actin nucleation sites, which allows the actin polymerization needed for C. burnetii internalization. This observation is consistent with the stimulation of C. burnetii uptake in cells overexpressing the mDia1 positive mutant ΔN3, which contains the actin nucleation domain, and also with the inhibition of the uptake in cells overexpressing the negative mutant N1 that only contains the Rho binding domain. Other models have shown that this mutant stimulates cell elongation and the formation of parallel thin actin cables, while the negative truncated mutant inhibits actin-fiber formation by sequestering active Rho proteins [18,95]. Thus, it is likely that a similar mechanism is working for Coxiella infection. The participation of mDia1 and related proteins has also been observed in the infection process of other bacterial pathogens. Shigella flexneri and Rickettsia rickettsii utilize mDia1 and Sca2 (formin mimic protein), respectively, to induce actin polymerization and, therefore, intracellular motility and spreading [96,97]. During infection with Vibrio cholerae, VopF, a TTSS effector with formin-like activity, participates in vivo in intestinal colonization and, in vitro, in alterations of actin cytoskeleton and cell morphology in a manner similar to formin [98]. Recently, the role of formin FHOD1 in S. typhimurium entry into HeLa cell has been demonstrated [99].

It has also been shown that mDia1 is recruited to endosomes in HeLa cells suggesting its role in controlling endosomal trafficking [95,100]. Colucci-Guyon et al [21] observed that mDia1, together with actin, was recruited early to the phagocytic cup during CR3-mediated phagocytosis in RAW264.7 macrophages. Interestingly, C. burnetii interacts with CR3 and the αVβ3 integrin of the host’s cells [54]. Therefore, it is tempting to hypothesize that mDia1 may regulate C. burnetii internalization through CR3. Further studies should be conducted to assess this hypothesis.

In this work we have provided evidence that the kinase ROCK is also a key player in C. burnetii internalization, since the process was hampered in cells treated with a ROCK inhibitor, or by silencing the protein with a specific siRNA. These observations are in agreement with the role of ROCK in CR3-mediated phagocytosis in J774.A1 and RAW264.7 macrophages and in Cos-7 fibroblasts [21,28]. Likewise, the Salmonella invasion of non-phagocytic cells was significantly decreased by the ROCK inhibitor Y27632 [101]. More recently, Truong et al [99] have demonstrated the requirement of ROCK II, but not of ROCK I, in S. typhimurium uptake into HeLa cells using specific siRNAs. In our model, employing a similar experimental approach, we demonstrated the role of ROCK I, yet the participation of ROCK II cannot be ruled out if the effect of the general ROCK inhibitor is considered. ROCK has also been involved in the infection of other pathogens such as E. coli K1 [102] that invades brain microvascular endothelial cells, and EHV-1 (equine herpes virus type 1) in a CHO-K1 cell line [103]. Thus, it is evident that ROCK participates in infection processes involving different types of microorganisms comprising not only bacteria but also viruses.

In conclusion, our results indicate that the active forms of RhoA, Cdc42 and Rac1 play an important role and work sequentially in the entry of C. burnetii into the host´s cells, regulating the actin rearrangement needed for this process. It could be speculated that these GTPases may work together in a cooperative manner, but this hypothesis needs to be further tested. Moreover, we report for the first time, that the RhoA effectors mDia1 and ROCK are involved in a signal transduction mechanism that favors C. burnetii uptake, highlighting the importance of these molecules in Coxiella entry into host´s cells.

Supporting Information

[Figure omitted. See PDF.]

S1 Fig. RhoA, Rac1 and mDia1 are recruited to the membrane fraction obtained from HeLa cells infected with heat-killed C. burnetii.

HeLa cells were infected with heat-killed C. burnetii for different lengths of time, lysed and centrifuged to obtain postnuclear supernatant, membrane and cytosolic fractions as described in Materials and Methods. (A) Postnuclear supernatant (T: total), cytosol (C) and membrane (M) fractions were analyzed by SDS-PAGE and Western blot using antibodies against RhoA, Rac1 and mDia1. Anti-actin and anti-E cadherin antibodies were used as loading controls. (B) Quantification of RhoA, Rac1 and mDia1 recruitment to the membrane fraction. The band intensity of RhoA, Rac1, mDia1, E cadherin and actin was measured by the ImageJ software, and band intensity ratio between RhoA and E cadherin, Rac1 and E cadherin, and mDia1 and E cadherin in the membrane fractions was calculated. Results are expressed as means ± SE from at least three independent experiments. Means were compared with the 0 min infection condition by Student’s t test for single group mean (*p < 0.05, ***p < 0.001). ns: indicates non-significant differences between groups (p > 0.05). (RU): Relative Units.

https://doi.org/10.1371/journal.pone.0145211.s001

(TIF)

Acknowledgments

The authors wish thank Philippe Chavrier (Centre National de la Recherche Scientifique/Institut Curie, Paris, France) and Mark R. Phillips (Laboratory of Molecular Rheumatology, NYU, School of Medicine, USA) for providing the plasmids encoding Rho proteins and their mutants, Robert Heinzen (Rocky Mountain Laboratories, NIAID, NIH, Hamilton, MT, USA) for providing the rabbit polyclonal anti-Coxiella antibody, Ted Hackstadt (Rocky Mountain Laboratories, NIAID, NIH, Hamilton, MT, USA) for providing C. burnetii; and Mar Fernandez-Borja (The Netherlands Cancer Institute, Division of Tumour Biology, Amsterdam) for providing the plasmids encoding EGFP-mDia1 and their truncated forms. The authors are also grateful to Alejandra Medero and Tirso Sartor for their help with tissue culture and biochemical techniques.

Author Contributions

Conceived and designed the experiments: RPS RMOF JSD MOA MIC WB. Performed the experiments: RPS RMOF JSD MOA. Analyzed the data: RPS RMOF JSD WB. Wrote the paper: WB.

Citation: Salinas RP, Ortiz Flores RM, Distel JS, Aguilera MO, Colombo MI, Berón W (2015) Coxiella burnetii Phagocytosis Is Regulated by GTPases of the Rho Family and the RhoA Effectors mDia1 and ROCK. PLoS ONE 10(12): e0145211. https://doi.org/10.1371/journal.pone.0145211

References

1. Gardel ML, Schneider IC, Aratyn-Schaus Y, Waterman CM (2010) Mechanical integration of actin and adhesion dynamics in cell migration. Annu Rev Cell Dev Biol 26: 315–333. pmid:19575647

2. Gourlay CW, Ayscough KR (2005) A role for actin in aging and apoptosis. Biochem Soc Trans 33: 1260–1264. pmid:16246093

3. Croise P, Estay-Ahumada C, Gasman S, Ory S (2014) Rho GTPases, phosphoinositides, and actin: a tripartite framework for efficient vesicular trafficking. Small GTPases 5: e29469. 29469 [pii]; pmid:24914539

4. Jaffe AB, Hall A (2005) Rho GTPases: biochemistry and biology. Annu Rev Cell Dev Biol 21: 247–269. pmid:16212495

5. Heasman SJ, Ridley AJ (2008) Mammalian Rho GTPases: new insights into their functions from in vivo studies. Nat Rev Mol Cell Biol 9: 690–701. nrm2476 [pii]; pmid:18719708

6. Chi X, Wang S, Huang Y, Stamnes M, Chen JL (2013) Roles of rho GTPases in intracellular transport and cellular transformation. Int J Mol Sci 14: 7089–7108. ijms14047089 [pii]; pmid:23538840

7. Aspenstrom P, Fransson A, Saras J (2004) Rho GTPases have diverse effects on the organization of the actin filament system. Biochem J 377: 327–337. pmid:14521508

8. Ladwein M, Rottner K (2008) On the Rho'd: the regulation of membrane protrusions by Rho-GTPases. FEBS Lett 582: 2066–2074. pmid:18442478

9. Qualmann B, Mellor H (2003) Regulation of endocytic traffic by Rho GTPases. Biochem J 371: 233–241. pmid:12564953

10. Kaksonen M, Toret CP, Drubin DG (2006) Harnessing actin dynamics for clathrin-mediated endocytosis. Nat Rev Mol Cell Biol 7: 404–414. pmid:16723976

11. Dubois T, Paleotti O, Mironov AA, Fraisier V, Stradal TE, De Matteis MA, et al. (2005) Golgi-localized GAP for Cdc42 functions downstream of ARF1 to control Arp2/3 complex and F-actin dynamics. Nat Cell Biol 7: 353–364. pmid:15793564

12. Matas OB, Fritz S, Luna A, Egea G (2005) Membrane trafficking at the ER/Golgi interface: functional implications of RhoA and Rac1. Eur J Cell Biol 84: 699–707. pmid:16180308

13. Firat-Karalar EN, Welch MD (2011) New mechanisms and functions of actin nucleation. Curr Opin Cell Biol 23: 4–13. S0955-0674(10)00178-X [pii]; pmid:21093244

14. Faix J, Grosse R (2006) Staying in shape with formins. Dev Cell 10: 693–706. S1534-5807(06)00209-7 [pii]; pmid:16740473

15. Schonichen A, Geyer M (2010) Fifteen formins for an actin filament: a molecular view on the regulation of human formins. Biochim Biophys Acta 1803: 152–163. S0167-4889(10)00015-7 [pii]; pmid:20102729

16. Yang C, Czech L, Gerboth S, Kojima S, Scita G, Svitkina T (2007) Novel roles of formin mDia2 in lamellipodia and filopodia formation in motile cells. PLoS Biol 5: e317. 07-PLBI-RA-0359 [pii]; pmid:18044991

17. Goh WI, Lim KB, Sudhaharan T, Sem KP, Bu W, Chou AM, et al. (2012) mDia1 and WAVE2 proteins interact directly with IRSp53 in filopodia and are involved in filopodium formation. J Biol Chem 287: 4702–4714. M111.305102 [pii]; pmid:22179776

18. Watanabe N, Kato T, Fujita A, Ishizaki T, Narumiya S (1999) Cooperation between mDia1 and ROCK in Rho-induced actin reorganization. Nat Cell Biol 1: 136–143. pmid:10559899

19. Hotulainen P, Lappalainen P (2006) Stress fibers are generated by two distinct actin assembly mechanisms in motile cells. J Cell Biol 173: 383–394. jcb.200511093 [pii]; pmid:16651381

20. Wallar BJ, Deward AD, Resau JH, Alberts AS (2007) RhoB and the mammalian Diaphanous-related formin mDia2 in endosome trafficking. Exp Cell Res 313: 560–571. S0014-4827(06)00456-3 [pii]; pmid:17198702

21. Colucci-Guyon E, Niedergang F, Wallar BJ, Peng J, Alberts AS, Chavrier P (2005) A role for mammalian diaphanous-related formins in complement receptor (CR3)-mediated phagocytosis in macrophages. Curr Biol 15: 2007–2012. S0960-9822(05)01212-1 [pii]; pmid:16303559

22. Watanabe N, Madaule P, Reid T, Ishizaki T, Watanabe G, Kakizuka A, et al. (1997) p140mDia, a mammalian homolog of Drosophila diaphanous, is a target protein for Rho small GTPase and is a ligand for profilin. EMBO J 16: 3044–3056. pmid:9214622

23. Brandt DT, Marion S, Griffiths G, Watanabe T, Kaibuchi K, Grosse R (2007) Dia1 and IQGAP1 interact in cell migration and phagocytic cup formation. J Cell Biol 178: 193–200. jcb.200612071 [pii]; pmid:17620407

24. Amano M, Chihara K, Kimura K, Fukata Y, Nakamura N, Matsuura Y, et al. (1997) Formation of actin stress fibers and focal adhesions enhanced by Rho-kinase. Science 275: 1308–1311. pmid:9036856

25. Wheeler AP, Ridley AJ (2004) Why three Rho proteins? RhoA, RhoB, RhoC, and cell motility. Exp Cell Res 301: 43–49. S0014-4827(04)00479-3 [pii]; pmid:15501444

26. Matsumura F (2005) Regulation of myosin II during cytokinesis in higher eukaryotes. Trends Cell Biol 15: 371–377. S0962-8924(05)00130-3 [pii]; pmid:15935670

27. Fox R, Nhan TQ, Law GL, Morris DR, Liles WC, Schwartz SM (2007) PSGL-1 and mTOR regulate translation of ROCK-1 and physiological functions of macrophages. EMBO J 26: 505–515. 7601522 [pii]; pmid:17245434

28. Olazabal IM, Caron E, May RC, Schilling K, Knecht DA, Machesky LM (2002) Rho-kinase and myosin-II control phagocytic cup formation during CR, but not FcgammaR, phagocytosis. Curr Biol 12: 1413–1418. S0960982202010692 [pii]. pmid:12194823

29. Yoneda A, Multhaupt HA, Couchman JR (2005) The Rho kinases I and II regulate different aspects of myosin II activity. J Cell Biol 170: 443–453. jcb.200412043 [pii]; pmid:16043513

30. Alonso A, Garcia-del PF (2004) Hijacking of eukaryotic functions by intracellular bacterial pathogens. Int Microbiol 7: 181–191. im2304028 [pii]. pmid:15492932

31. Alix E, Mukherjee S, Roy CR (2011) Subversion of membrane transport pathways by vacuolar pathogens. J Cell Biol 195: 943–952. jcb.201105019 [pii]; pmid:22123831

32. Underhill DM, Ozinsky A (2002) Phagocytosis of microbes: complexity in action. Annu Rev Immunol 20: 825–852. 103001.114744 [pii]. pmid:11861619

33. Flannagan RS, Jaumouille V, Grinstein S (2012) The cell biology of phagocytosis. Annu Rev Pathol 7: 61–98. pmid:21910624

34. Fairn GD, Grinstein S (2012) How nascent phagosomes mature to become phagolysosomes. Trends Immunol. S1471-4906(12)00053-1 [pii];

35. Niedergang F, Chavrier P (2005) Regulation of phagocytosis by Rho GTPases. Curr Top Microbiol Immunol 291: 43–60. pmid:15981459

36. Caron E, Hall A (1998) Identification of two distinct mechanisms of phagocytosis controlled by different Rho GTPases. Science 282: 1717–1721. pmid:9831565

37. Hoppe AD, Swanson JA (2004) Cdc42, Rac1, and Rac2 display distinct patterns of activation during phagocytosis. Mol Biol Cell 15: 3509–3519. E03-11-0847 [pii]. pmid:15169870

38. Cougoule C, Hoshino S, Dart A, Lim J, Caron E (2006) Dissociation of recruitment and activation of the small G-protein Rac during Fcgamma receptor-mediated phagocytosis. J Biol Chem 281: 8756–8764. M513731200 [pii]; pmid:16434390

39. Kim JG, Moon MY, Kim HJ, Li Y, Song DK, Kim JS, et al. (2012) Ras-related GTPases Rap1 and RhoA collectively induce the phagocytosis of serum-opsonized zymosan particles in macrophages. J Biol Chem 287: 5145–5155. M111.257634 [pii]; pmid:22194606

40. May RC, Caron E, Hall A, Machesky LM (2000) Involvement of the Arp2/3 complex in phagocytosis mediated by FcgammaR or CR3. Nat Cell Biol 2: 246–248. pmid:10783245

41. Hackam DJ, Rotstein OD, Schreiber A, Zhang W, Grinstein S (1997) Rho is required for the initiation of calcium signaling and phagocytosis by Fcgamma receptors in macrophages. J Exp Med 186: 955–966. pmid:9294149

42. Hall AB, Gakidis MA, Glogauer M, Wilsbacher JL, Gao S, Swat W, et al. (2006) Requirements for Vav guanine nucleotide exchange factors and Rho GTPases in FcgammaR- and complement-mediated phagocytosis. Immunity 24: 305–316. S1074-7613(06)00141-5 [pii]; pmid:16546099

43. Woldehiwet Z (2004) Q fever (coxiellosis): epidemiology and pathogenesis. Res Vet Sci 77: 93–100. pmid:15196898

44. Waag DM (2007) Coxiella burnetii: host and bacterial responses to infection. Vaccine 25: 7288–7295. S0264-410X(07)00915-2 [pii]; pmid:17825460

45. Baca OG, Paretsky D (1983) Q fever and Coxiella burnetii: a model for host-parasite interactions. Microbiol Rev 47: 127–149. pmid:6348504

46. Beron W, Gutierrez MG, Rabinovitch M, Colombo MI (2002) Coxiella burnetii localizes in a Rab7-labeled compartment with autophagic characteristics. Infect Immun 70: 5816–5821. pmid:12228312

47. Howe D, Mallavia LP (2000) Coxiella burnetii exhibits morphological change and delays phagolysosomal fusion after internalization by J774A.1 cells. Infect Immun 68: 3815–3821. pmid:10858189

48. Romano PS, Gutierrez MG, Beron W, Rabinovitch M, Colombo MI (2007) The autophagic pathway is actively modulated by phase II Coxiella burnetii to efficiently replicate in the host cell. Cell Microbiol 9: 891–909. pmid:17087732

49. Voth DE, Heinzen RA (2007) Lounging in a lysosome: the intracellular lifestyle of Coxiella burnetii. Cell Microbiol 9: 829–840. pmid:17381428

50. Gutierrez MG, Vazquez CL, Munafo DB, Zoppino FC, Beron W, Rabinovitch M, et al. (2005) Autophagy induction favours the generation and maturation of the Coxiella-replicative vacuoles. Cell Microbiol 7: 981–993. pmid:15953030

51. Aguilera M, Salinas R, Rosales E, Carminati S, Colombo MI, Beron W (2009) Actin dynamics and Rho GTPases regulate the size and formation of parasitophorous vacuoles containing Coxiella burnetii. Infect Immun 77: 4609–4620. IAI.00301-09 [pii]; pmid:19635823

52. Rosales EM, Aguilera MO, Salinas RP, Carminati SA, Colombo MI, Martinez-Quiles N, et al. (2012) Cortactin is involved in the entry of Coxiella burnetii into non-phagocytic cells. PLoS One 7: e39348. PONE-D-11-23416 [pii]. pmid:22761768

53. Baca OG, Klassen DA, Aragon AS (1993) Entry of Coxiella burnetii into host cells. Acta Virol 37: 143–155. pmid:8105658

54. Capo C, Lindberg FP, Meconi S, Zaffran Y, Tardei G, Brown EJ, et al. (1999) Subversion of monocyte functions by coxiella burnetii: impairment of the cross-talk between alphavbeta3 integrin and CR3. J Immunol 163: 6078–6085. ji_v163n11p6078 [pii]. pmid:10570297

55. Dellacasagrande J, Ghigo E, Hammami SM, Toman R, Raoult D, Capo C, et al. (2000) alpha(v)beta(3) integrin and bacterial lipopolysaccharide are involved in Coxiella burnetii-stimulated production of tumor necrosis factor by human monocytes. Infect Immun 68: 5673–5678. pmid:10992470

56. Meconi S, Jacomo V, Boquet P, Raoult D, Mege JL, Capo C (1998) Coxiella burnetii induces reorganization of the actin cytoskeleton in human monocytes. Infect Immun 66: 5527–5533. pmid:9784567

57. Lemichez E, Aktories K (2013) Hijacking of Rho GTPases during bacterial infection. Exp Cell Res 319: 2329–2336. S0014-4827(13)00192-4 [pii]; pmid:23648569

58. Aktories K, Barbieri JT (2005) Bacterial cytotoxins: targeting eukaryotic switches. Nat Rev Microbiol 3: 397–410. nrmicro1150 [pii]; pmid:15821726

59. Genth H, Huelsenbeck J, Hartmann B, Hofmann F, Just I, Gerhard R (2006) Cellular stability of Rho-GTPases glucosylated by Clostridium difficile toxin B. FEBS Lett 580: 3565–3569. S0014-5793(06)00631-4 [pii]; pmid:16730714

60. May RC, Machesky LM (2001) Phagocytosis and the actin cytoskeleton. J Cell Sci 114: 1061–1077. pmid:11228151

61. Patel JC, Hall A, Caron E (2000) Rho GTPases and macrophage phagocytosis. Methods Enzymol 325: 462–473. S0076-6879(00)25466-9 [pii]. pmid:11036627

62. Michaelson D, Philips M (2006) The use of GFP to localize Rho GTPases in living cells. Methods Enzymol 406: 296–315. S0076-6879(06)06022-8 [pii]; pmid:16472666

63. Roberts PJ, Mitin N, Keller PJ, Chenette EJ, Madigan JP, Currin RO, et al. (2008) Rho Family GTPase modification and dependence on CAAX motif-signaled posttranslational modification. J Biol Chem 283: 25150–25163. M800882200 [pii]; pmid:18614539

64. Bhadriraju K, Yang M, Alom RS, Pirone D, Tan J, Chen CS (2007) Activation of ROCK by RhoA is regulated by cell adhesion, shape, and cytoskeletal tension. Exp Cell Res 313: 3616–3623. S0014-4827(07)00322-9 [pii]; pmid:17673200

65. Amano M, Nakayama M, Kaibuchi K (2010) Rho-kinase/ROCK: A key regulator of the cytoskeleton and cell polarity. Cytoskeleton (Hoboken) 67: 545–554.

66. Ramalingam N, Zhao H, Breitsprecher D, Lappalainen P, Faix J, Schleicher M (2010) Phospholipids regulate localization and activity of mDia1 formin. Eur J Cell Biol 89: 723–732. S0171-9335(10)00115-9 [pii]; pmid:20619927

67. Alberts AS (2001) Identification of a carboxyl-terminal diaphanous-related formin homology protein autoregulatory domain. J Biol Chem 276: 2824–2830. M006205200 [pii]. pmid:11035012

68. Li F, Higgs HN (2005) Dissecting requirements for auto-inhibition of actin nucleation by the formin, mDia1. J Biol Chem 280: 6986–6992. M411605200 [pii]; pmid:15591319

69. Cossart P, Roy CR (2010) Manipulation of host membrane machinery by bacterial pathogens. Curr Opin Cell Biol 22: 547–554. S0955-0674(10)00069-4 [pii]; pmid:20542678

70. Pizarro-Cerda J, Cossart P (2006) Bacterial adhesion and entry into host cells. Cell 124: 715–727. S0092-8674(06)00187-5 [pii]; pmid:16497583

71. Swanson JA, Baer SC (1995) Phagocytosis by zippers and triggers. Trends Cell Biol 5: 89–93. S0962892400889564 [pii]. pmid:14732161

72. van Schaik EJ, Chen C, Mertens K, Weber MM, Samuel JE (2013) Molecular pathogenesis of the obligate intracellular bacterium Coxiella burnetii. Nat Rev Microbiol 11: 561–573. nrmicro3049 [pii]; pmid:23797173

73. Allen LA, Aderem A (1996) Molecular definition of distinct cytoskeletal structures involved in complement- and Fc receptor-mediated phagocytosis in macrophages. J Exp Med 184: 627–637. pmid:8760816

74. Kaplan G (1977) Differences in the mode of phagocytosis with Fc and C3 receptors in macrophages. Scand J Immunol 6: 797–807. pmid:561436

75. Hussain SK, Broederdorf LJ, Sharma UM, Voth DE (2010) Host Kinase Activity is Required for Coxiella burnetii Parasitophorous Vacuole Formation. Front Microbiol 1: 137. pmid:21772829

76. McDonough JA, Newton HJ, Klum S, Swiss R, Agaisse H, Roy CR (2013) Host Pathways Important for Coxiella burnetii Infection Revealed by Genome-Wide RNA Interference Screening. MBio 4. mBio.00606-12 [pii];

77. Newton HJ, McDonough JA, Roy CR (2013) Effector Protein Translocation by the Coxiella burnetii Dot/Icm Type IV Secretion System Requires Endocytic Maturation of the Pathogen-Occupied Vacuole. PLoS One 8: e54566. PONE-D-12-31876 [pii]. pmid:23349930

78. Tierrez A, Garcia-del PF (2005) New concepts in Salmonella virulence: the importance of reducing the intracellular growth rate in the host. Cell Microbiol 7: 901–909. CMI540 [pii]; pmid:15953023

79. Pizarro-Cerda J, Kuhbacher A, Cossart P (2012) Entry of Listeria monocytogenes in mammalian epithelial cells: an updated view. Cold Spring Harb Perspect Med 2. 2/11/a010009 [pii];

80. Subtil A, Wyplosz B, Balana ME, Dautry-Varsat A (2004) Analysis of Chlamydia caviae entry sites and involvement of Cdc42 and Rac activity. J Cell Sci 117: 3923–3933. jcs.01247 [pii]. pmid:15265988

81. Patel JC, Galan JE (2008) Investigating the function of Rho family GTPases during Salmonella/host cell interactions. Methods Enzymol 439: 145–158. S0076-6879(07)00411-9 [pii]; pmid:18374162

82. Carabeo RA, Grieshaber SS, Hasenkrug A, Dooley C, Hackstadt T (2004) Requirement for the Rac GTPase in Chlamydia trachomatis invasion of non-phagocytic cells. Traffic 5: 418–425. TRA184 [pii]. pmid:15117316

83. Billker O, Popp A, Brinkmann V, Wenig G, Schneider J, Caron E, et al. (2002) Distinct mechanisms of internalization of Neisseria gonorrhoeae by members of the CEACAM receptor family involving Rac1- and Cdc42-dependent and -independent pathways. EMBO J 21: 560–571. pmid:11847104

84. Bishop AL, Hall A (2000) Rho GTPases and their effector proteins. Biochem J 348 Pt 2: 241–255. pmid:10816416

85. Benard V, Bohl BP, Bokoch GM (1999) Characterization of rac and cdc42 activation in chemoattractant-stimulated human neutrophils using a novel assay for active GTPases. J Biol Chem 274: 13198–13204. pmid:10224076

86. Pertz O, Hahn KM (2004) Designing biosensors for Rho family proteins—deciphering the dynamics of Rho family GTPase activation in living cells. J Cell Sci 117: 1313–1318. 117/8/1313 [pii]. pmid:15020671

87. Pertz O (2010) Spatio-temporal Rho GTPase signaling—where are we now? J Cell Sci 123: 1841–1850. 123/11/1841 [pii]; pmid:20484664

88. Ren XD, Kiosses WB, Schwartz MA (1999) Regulation of the small GTP-binding protein Rho by cell adhesion and the cytoskeleton. EMBO J 18: 578–585. pmid:9927417

89. Michaelson D, Silletti J, Murphy G, D'Eustachio P, Rush M, Philips MR (2001) Differential localization of Rho GTPases in live cells: regulation by hypervariable regions and RhoGDI binding. J Cell Biol 152: 111–126. pmid:11149925

90. Hodgson L, Shen F, Hahn K (2010) Biosensors for characterizing the dynamics of rho family GTPases in living cells. Curr Protoc Cell Biol Chapter 14: Unit-26.

91. Bierne H, Gouin E, Roux P, Caroni P, Yin HL, Cossart P (2001) A role for cofilin and LIM kinase in Listeria-induced phagocytosis. J Cell Biol 155: 101–112. jcb.200104037 [pii]. pmid:11571311

92. Bierne H, Miki H, Innocenti M, Scita G, Gertler FB, Takenawa T, et al. (2005) WASP-related proteins, Abi1 and Ena/VASP are required for Listeria invasion induced by the Met receptor. J Cell Sci 118: 1537–1547. jcs.02285 [pii]; pmid:15769844

93. Burnham CA, Shokoples SE, Tyrrell GJ (2007) Rac1, RhoA, and Cdc42 participate in HeLa cell invasion by group B streptococcus. FEMS Microbiol Lett 272: 8–14. FML768 [pii]; pmid:17517067

94. Duman JG, Mulherkar S, Tu YK, Cheng X, Tolias KF (2015) Mechanisms for spatiotemporal regulation of Rho-GTPase signaling at synapses. Neurosci Lett. S0304-3940(15)00391-2 [pii];

95. Fernandez-Borja M, Janssen L, Verwoerd D, Hordijk P, Neefjes J (2005) RhoB regulates endosome transport by promoting actin assembly on endosomal membranes through Dia1. J Cell Sci 118: 2661–2670. 118/12/2661 [pii]; pmid:15944396

96. Heindl JE, Saran I, Yi CR, Lesser CF, Goldberg MB (2010) Requirement for formin-induced actin polymerization during spread of Shigella flexneri. Infect Immun 78: 193–203. IAI.00252-09 [pii]; pmid:19841078

97. Haglund CM, Choe JE, Skau CT, Kovar DR, Welch MD (2010) Rickettsia Sca2 is a bacterial formin-like mediator of actin-based motility. Nat Cell Biol 12: 1057–1063. ncb2109 [pii]; pmid:20972427

98. Tam VC, Serruto D, Dziejman M, Brieher W, Mekalanos JJ (2007) A type III secretion system in Vibrio cholerae translocates a formin/spire hybrid-like actin nucleator to promote intestinal colonization. Cell Host Microbe 1: 95–107. S1931-3128(07)00044-3 [pii]; pmid:18005688

99. Truong D, Brabant D, Bashkurov M, Wan LC, Braun V, Heo WD, et al. (2013) Formin-mediated actin polymerization promotes Salmonella invasion. Cell Microbiol 15: 2051–2063. pmid:23869992

100. Tominaga T, Sahai E, Chardin P, McCormick F, Courtneidge SA, Alberts AS (2000) Diaphanous-related formins bridge Rho GTPase and Src tyrosine kinase signaling. Mol Cell 5: 13–25. S1097-2765(00)80399-8 [pii]. pmid:10678165

101. Hanisch J, Kolm R, Wozniczka M, Bumann D, Rottner K, Stradal TE (2011) Activation of a RhoA/myosin II-dependent but Arp2/3 complex-independent pathway facilitates Salmonella invasion. Cell Host Microbe 9: 273–285. S1931-3128(11)00096-5 [pii]; pmid:21501827

102. Khan NA, Shin S, Chung JW, Kim KJ, Elliott S, Wang Y, et al. (2003) Outer membrane protein A and cytotoxic necrotizing factor-1 use diverse signaling mechanisms for Escherichia coli K1 invasion of human brain microvascular endothelial cells. Microb Pathog 35: 35–42. S0882401003000901 [pii]. pmid:12860457

103. Frampton AR Jr., Stolz DB, Uchida H, Goins WF, Cohen JB, Glorioso JC (2007) Equine herpesvirus 1 enters cells by two different pathways, and infection requires the activation of the cellular kinase ROCK1. J Virol 81: 10879–10889. JVI.00504-07 [pii]; pmid:17670830