Drosophila Host Model Reveals New Enterococcus faecalis Quorum-Sensing Associated Virulence Factors

Abstract

Enterococcus faecalis V583 is a vancomycin-resistant clinical isolate which belongs to the hospital-adapted clade, CC2. This strain harbours several factors that have been associated with virulence, including the fsr quorum-sensing regulatory system that is known to control the expression of GelE and SprE proteases. To discriminate between genes directly regulated by Fsr, and those indirectly regulated as the result of protease expression or activity, we compared gene expression in isogenic mutants of V583 variously defective in either Fsr quorum sensing or protease expression. Quorum sensing was artificially induced by addition of the quorum signal, GBAP, exogenously in a controlled manner. The Fsr regulon was found to be restricted to five genes, gelE, sprE, ef1097, ef1351 and ef1352. Twelve additional genes were found to be dependent on the presence of GBAP-induced proteases. Induction of GelE and SprE by GBAP via Fsr resulted in accumulation of mRNA encoding lrgAB, and this induction was found to be lytRS dependent. Drosophila infection was used to discern varying levels of toxicity stemming from mutations in the fsr quorum regulatory system and the genes that it regulates, highlighting the contribution of LrgAB and bacteriocin EF1097 to infection toxicity. A contribution of SprE to infection toxicity was also detected. This work brought to light new players in E. faecalis success as a pathogen and paves the way for future studies on host tolerance mechanisms to infections caused by this important nosocomial pathogen.

About the Authors:

Neuza Teixeira

Affiliations ITQB Instituto de Tecnologia Química e Biológica, Universidade Nova de Lisboa, Oeiras, Portugal, Departments of Ophthalmology, and Microbiology and Immunobiology, Harvard Medical School, Boston, Massachusetts, United States of America, CEDOC Faculdade de Ciências Médicas, Universidade Nova de Lisboa, Lisboa, Portugal

Sriram Varahan

Affiliation: Division of Biology, Kansas State University, Manhattan, Kansas, United States of America

Matthew J. Gorman

Current address: The Division of Biology and Biomedical Sciences, Washington University at St. Louis, St. Louis, Missouri, United States of America

Affiliation: Division of Biology, Kansas State University, Manhattan, Kansas, United States of America

Kelli L. Palmer

Current address: Department of Molecular and Cell Biology, University of Texas at Dallas, Richardson, Texas, United States of America

Affiliation: Departments of Ophthalmology, and Microbiology and Immunobiology, Harvard Medical School, Boston, Massachusetts, United States of America

Anna Zaidman-Remy

Affiliation: CEDOC Faculdade de Ciências Médicas, Universidade Nova de Lisboa, Lisboa, Portugal

Ryoji Yokohata

Affiliation: Department of Bioscience and Biotechnology, Faculty of Agriculture, Graduate School, Kyushu University, Fukuoka, Japan

Jiro Nakayama

Affiliation: Department of Bioscience and Biotechnology, Faculty of Agriculture, Graduate School, Kyushu University, Fukuoka, Japan

Lynn E. Hancock

Affiliation: Division of Biology, Kansas State University, Manhattan, Kansas, United States of America

António Jacinto

Affiliation: CEDOC Faculdade de Ciências Médicas, Universidade Nova de Lisboa, Lisboa, Portugal

Michael S. Gilmore

Affiliation: Departments of Ophthalmology, and Microbiology and Immunobiology, Harvard Medical School, Boston, Massachusetts, United States of America

Maria de Fátima Silva Lopes

* E-mail: [email protected]

Affiliations ITQB Instituto de Tecnologia Química e Biológica, Universidade Nova de Lisboa, Oeiras, Portugal, IBET Instituto de Biologia Experimental e Tecnológica, Oeiras, Portugal

Introduction

Drosophila melanogaster is used increasingly as a model for identifying virulence factors of pathogenic microbes, and for elucidating their effects on the host [1]. The fruit fly presents several advantages, such as small size, short life cycle, short generation time, a fully sequenced genome and pre-existing libraries of genetic mutants. In addition, its immune system shares similarities with the mammalian immune system, including genes and pathways. In particular, the Toll and Imd pathways in D. melanogaster have parallels in the mammalian Toll-like (TLR) and interlleukin-1 (IL-1) receptor families, and the mammalian tumour necrosis factor signalling pathway [2]. In 2007, Cox and Gilmore characterized the microbiome of this host and showed that Enterococcus sp. and naturally colonize its alimentary canal; and that cytolysin, a toxin expressed by some strains of Enterococcus faecalis, contributes to death of the flies when colonized [3]. It is also known that E. faecalis are able to kill the flies and induce the Toll pathway after infection by septic injury, and that haemocytes (Drosophila circulating cells that function as phagocytes) also play a role in flýs defence against these bacteria [4], [5].

Enterococci are Gram-positive bacteria commonly found in gastrointestinal tract consortia, but are also adapted to survive and persist in the environment. In contrast to their benign role as members of the gut flora, select lineages of several enterococcal species have become leading causes of antibiotic resistant nosocomial infection, causing infections of the urinary tract, bloodstream, intra-abdominal and pelvic regions, and surgical sites [6].

E. faecalis, the species most frequently associated with nosocomial infections [7], possesses a number of traits that exacerbate the effects of infection. Fsr (Enterococcus faecalis sensor regulator) a two-component, quorum sensing regulatory system, was first described in 2000 by Qin et al. as a paralog of the Agr system in Staphylococcus aureus [7]. Despite similarities, Agr is functionally distinct from Fsr as it uses the RNAIII riboregulator [8]. The fsr operon comprises four genes: fsrA, fsrB, fsrC and fsrD [9]. The last encodes an auto-inducing cyclic peptide named gelatinase biosynthesis-activating pheromone (GBAP), and this peptide is processed and exported out of the cell by FsrB. Accumulation of GBAP outside cells is sensed by the FsrC histidine kinase, leading to the activation of the response regulator FsrA. Activated FsrA induces expression of the fsrBDC genes forming an auto regulatory circuit that results in a rapid, exponential increase in GBAP signalling. Expression of a second operon is induced by FsrA consisting of two cistrons gelE-sprE. The first cistron, gelE, encodes gelatinase, an extracellular zinc metalloprotease, and the second, sprE, encodes a serine protease [7], [10]. Several studies provided evidence that both Fsr and the proteases independently contribute to the pathogenicity of E. faecalis in different infection models [11], [12], [13], [14], [15], [16], [17]. The proteases have also been shown to be involved in biofilm formation [18], in translocation across intestinal T84 cells [19], in degradation of antimicrobial peptides (AMPs) from the immune system of Galleria mellonella [20], in autolysis regulation [21] and as regulators of Ace surface protein exposure on the surface of E. faecalis cells [22], [23].

The exact mechanisms by which Fsr and its regulated proteases contribute to toxicity of infection are not known. This has been confounded in part by unexplained variation in experimental results. In 2005, Singh et al. tested fsrB and gelE mutants in E. faecalis strain OG1RF in a rat endocarditis model. Deletion of the proteases led to a greater decrease in endocarditis severity than deletion of fsrB. In the absence of fsrB, the gelE expression was reduced, and the authors postulated that was the reason for the smaller attenuation of fsrB mutant [15]. In contrast, studies examining the role of these traits in rabbit endophtalmitis [13], [14], murine and C. elegans infection [11], [12], and in a G. mellonella infection model [17] all found that fsrB deletion led to a greater attenuation than deletion of the proteases. These last results raised the possibility that Fsr could be affecting directly or indirectly more genes or their products than just the proteases. Bourgogne et al. compared gene expression in OG1RF with an isogenic fsrB deletion mutant, and provided some evidence that Fsr regulates more than gelE and sprE protease genes [24]. While it is known that host substrates, such as complement components C3, C3a and C5a are targeted by GelE [20], [25], [26], little is known regarding a functional role for SprE in production of host injury and death.

To decipher the role of Fsr-regulated genes in virulence, we used a clonal-complex (CC) 2 strain [27], E. faecalis V583, the first vancomycin enterococcal isolate in the US, which was obtained from a chronic bloodstream infection [28]. E. faecalis CC2 is the leading multidrug resistant hospital adapted clade [27], [29]. To rigorously characterize the Fsr regulon, we compared gene expression in isogenic mutants in Fsr genes and each of the Fsr-regulated protease genes using microarrays and purified GBAP. D. melanogaster was used to examine the individual contribution to virulence of SprE protease and other genes found to be part of the Fsr regulon (or related to it, including EF1097, LrgAB and the two-component system LytRS).

Results

In order to precisely identify genes for which expression is altered when GBAP reaches effective quorum sensing concentration, we used a fsrB mutant, which is unable to produce GBAP, but is able to sense it [30]. We also used single and double protease mutants in the fsrB mutant background in order to identify any genes for which expression is indirectly controlled by Fsr through its regulation of protease levels. Table 1 shows key changes in gene expression in V583ΔfsrB, V583ΔfsrBΔgelE, V583ΔfsrBΔsprE and V583ΔfsrBΔgelEΔsprE after 10 min of GBAP exposure. Besides genes previously known, or predicted, to be regulated by Fsr through GBAP (gelE, sprE and ef1097) [7], [10], [24], 15 additional genes were differentially regulated by GBAP addition collectively in all four mutants (Table 1). In contrast to previous results using oligo-array study [24], the current approach employed a statistically more robust technology [31] and isolated the effects of only Fsr quorum sensing through the use of mutants and the exogenous quorum molecule.

[Figure omitted. See PDF.]

Table 1. Genes differentially expressed upon addition of GBAP to V583ΔfsrB, V583ΔfsrBΔgelE, V583ΔfsrBΔsprE and V583ΔfsrBΔgelEΔsprE strains.

https://doi.org/10.1371/journal.pone.0064740.t001

Fsr Dependent Genes

As expected, V583ΔfsrB responded to GBAP by substantially increasing the expression of gelE (ef1818) (fold change 63) and sprE (ef1817) (fold change 59). To a lesser extent, fsrC (ef1820) (fold change 3) transcript abundance was also increased. As shown in Table 1, mutation of each protease gene did not affect the expression of the other genes in the fsr or gelE-sprE operons, showing that the presence of the deletions in these operons did not have polar effects on transcript abundance of the remaining protease gene (V583ΔfsrBΔgelE expresses wild type levels of sprE, and V583ΔfsrBΔsprE expresses wild type levels of gelE). In accordance to previous results by others [24], fsrA expression was not affected by GBAP. Genes for which expression was affected by GBAP in all the four mutants are therefore under the direct control of FsrA and not influenced by indirect activities of the proteases on secondary regulators. In addition to Fsr and protease genes, ef1097 was induced by GBAP addition showing transcript abundance changes (fold change 31) similar to those observed for the protease genes. Transcripts of the ef1352 gene where more abundant upon GBAP induction, but exhibited an increase of a lower magnitude (fold change 5).

To determine whether a specific promoter motif could be identified upstream of genes found to be regulated by Fsr through its quorum sensing, we compared known [32] and putative promoter regions. The V583 promotor regions of ef1097, gelE and fsrB possess a predicted FsrA binding motif [32]. However, this motif does not occur upstream of ef1351. This raises the possibility that induction of ef1351–ef1352 in our experiments may be related to increased expression of the only gene which was also induced in the four mutants, but not independently controlled, ef1097. Alternatively, direct FsrA regulation mechanisms may be more complex than previously suspected.

Genes Dependent on Simultaneous Fsr and Proteases Activation

Some genes were found to be affected by the presence or absence of proteases, indicating an indirect regulatory pathway. Those only affected if sprE was absent (ef1815, ef1816); those affected only if either one of the proteases was absent (ef0893); those for which mRNA levels were altered only when both proteases were absent (ef0411, ef0563, ef0891, ef0892, ef1218); those for which mRNA accumulated only in the presence of both proteases (ef3193 and ef3194) and those affected in the absence of only the gelE gene (ef0468, ef0776). These last two genes might respond to the high expression levels of sprE in a way yet to be determined. Overall, the twelve genes affected by the combined activation of Fsr and the proteases are putatively involved in different cellular processes, such as regulation, cell-wall metabolism and transport, and some are even of unknown function. Currently available data does not allow us to further clarify the connection between these genes and the Fsr-GelE-SprE system.

LytRS System is Required for GBAP Induction of lrgAB Genes

EF3193–EF3194 correspond to the lrgAB genes which, in S. aureus, are described to be involved in repression of murein hydrolase activity, decreased autolysis and increased tolerance to penicillin [33]. In S. aureus these genes are regulated by the LytRS two-component regulatory system, located immediately upstream of the lrgAB genes [34]. There is no data about the function of lrgAB genes in E. faecalis but it is known that they are also located downstream of lytRS homologs, which suggests that in V583 lrgAB are regulated by LytRS. In our experiments, ef3193-3194 mRNA was more abundant upon GBAP induction only in the fsrB mutant, suggesting that these genes are not responding directly to FsrA activation, but probably to increased protease GelE and SprE expression, which only occurs when GBAP is added to the fsrB mutant. In order to test the hypothesis that the large increase in lrgAB abundance was the result of GBAP induction via the LytRS system, we deleted this two-component system from the fsrB mutant strain and compared the expression of lrgAB genes in the ΔfsrBΔlytRS and fsrB mutants (Figure 1). We found that GBAP is only able to induce lrgAB genes if LytRS is functional. These results were not observed in previous studies of fsr regulation in OG1RF [24]. None of the E. faecalis ΔlytRS or ΔlrgAB mutant strains showed different antibiotic resistance profiles (Table S1) nor gelatinase activities when compared to the wild-type strain (data not shown). Low level expression of lrgAB genes was observed in the ΔfsrBΔlytRS mutant (Figure S1), which points either to a low constitutive expression of those genes or to the existence of another regulator(s) able to modulate their expression.

[Figure omitted. See PDF.]

Figure 1. LytRS is required for GBAP induction of lrgAB genes.

The semi-quantitative RT-PCR shows expression of lrgAB genes in the VI13 (ΔfsrB mutant) and KS19 (ΔfsrBΔlytRS mutant), in the presence of GBAP. Expression of gelE and gdh were used as positive and negative controls, respectively, of Fsr induction by GBAP and of RNA concentration, respectively. The RNA used for this analysis was previously treated with RNase-free DNase I to remove contaminating DNA.

https://doi.org/10.1371/journal.pone.0064740.g001

Fsr and the Proteases Affect D. melanogaster Tolerance to E. faecalis Infection

To test the functional importance of genes found to be directly and indirectly dependent on Fsr, we then tested the virulence of the fsr-related mutants in a D. melanogaster injection model. We first compared the ability of the triple mutant V583ΔfsrBΔgelEΔsprE, to the single V583ΔfsrB mutant, and the V583 parental strain, to kill Drosophila. The fate of both the host (percentage of survival) and the bacteria (number of CFU) was followed for 24 h. In our assay, 50% of the flies were killed by the wild type strain 10 hours post-injection and after 14 h nearly all flies were dead (Figure 2A). For the same period of infection, the triple mutant V583ΔfsrBΔgelEΔsprE strain only killed 15% of the infected flies. 24 h post-injection, the triple mutant V583ΔfsrBΔgelEΔsprE was significantly attenuated (see Table S2 for detailed statistical analysis). These results show that the Fsr system and the proteases it regulates contribute measurably to toxicity in this model.

[Figure omitted. See PDF.]

Figure 2. Drosophila survival rates upon infection with E. faecalis strains.

75 Oregon R (5- to 7-day-old) male adult flies, raised at 25°C, were divided in tubes of 25 flies each, and infected, by septic injury onto the thorax with a thin needle, with V583 (A, B, D) and VE14089 derived strains (C). Data is representative of three independent experiments (225 flies per strain). Curves assigned with an * are significantly different (p<0.0001) from the respective wild-type -infected curve, as determined by log-rank analysis (Table S2).

https://doi.org/10.1371/journal.pone.0064740.g002

The survival curve of flies infected with the wild type strain shows two different killing rates: until 8 h, V583 strain is able to kill around 3 flies/hour; after this time, and until 12 h, V583 kills flies at a much higher rate, 15 flies/hour. At 8 h post infection, V583 cells reach the cell density considered to be able to induce the activation of the Fsr system in broth culture [9], [35]. Although there is no data on the in vivo Fsr expression during E. faecalis growth inside the host, we cannot exclude the possibility that the increased killing rate after 8 h is due to induced expression of the proteases.

In order to dissect the contribution of fsr-regulated genes to the lethality of infection, we tested these genes separately by infecting the flies with single deletion mutants (Figure 2B). Deletion of both proteases, either in the double protease mutant or in the triple mutant, led to a greater attenuation of virulence then deletion of fsrB (p<0.0001, Table S2). Consistent with previous demonstrations that in an fsrB mutant strain, proteases are still expressed [15], we observed an attenuation of the virulence in the triple mutant over that of the fsrB mutant, suggesting that low level expression of both proteases is enough to induce increased killing of the flies by the fsrB mutant. Absence of gelE alone produced the lowest attenuation of E. faecalis virulence, differing significantly (p<0.0001, Table S2) from the effect of the absence of sprE gene alone, which was attenuated to a similar level achieved by deletion of fsrB (Table S2). This result points to SprE as having a major role in E. faecalis virulence in the Drosophila model. All strains grew similarly inside Drosophila (Figure S2).

ef1097 Contributes to Toxicity in D. melanogaster Infection

The large increase in ef1097 mRNA abundance upon GABP addition, and the fact that it has been previously associated with Fsr system in another E. faecalis strain [24], led us to delete this gene to test its role in E. faecalis virulence. This mutant was constructed in VE14089, a plasmid cured derivative strain of V583, previously reported in G. mellonella to be less virulent than parental V583 strain [36]. Our results confirm that strain VE14089 is less virulent than V583 in the D. melanogaster model as well (compare control in Figure 2A and 2C). Previously, we compared the toxicity of V583ΔfsrBΔgelEΔsprE and V583ΔgelEΔsprE strains in the fly (Figure 2A and 2B). Both strains express ef1097, and therefore, the role of this protein was not assessed. Figure 2C clearly shows that deletion of ef1097 reduces killing of the flies by E. faecalis, therefore providing evidence for a role of this bacteriocin in E. faecalis toxicity in the fly. As deletion of ef1097 did not affect the gelatinase production ability of V583 strain (results not shown), the reduction of toxicity does not appear to be due to an effect on expression of fsr or the proteases it regulates.

LrgAB and LytRS Contribute Differently to Death of D. melanogaster

LytRS appears to induce lrgAB expression upon addition of GBAP to the fsrB mutant strain (Figure 1). Interestingly, lytRS was previously found to be strongly induced during infection of G. mellonella, and proposed to contribute to E. faecalis VE14089 virulence in the same model [37]. The importance of LytRS was therefore tested in Drosophila infection. Our results (Figure 2D) did not show a significant difference in the fly survival (Table S2) following infection with the lytRS mutant as compared to wild type. Our results cannot be compared to those of Hanin et al. [37] as both the strains and the infection protocols used were different.

lgrAB are still expressed in the lytRS mutant. We thus wondered if complete abolishment of its expression would have a more pronounced effect on D. melanogaster toxicity than that of its regulator LytRS. The lrgAB mutant strain was significantly reduced in toxicity for D. melanogaster (Figure 2D, Table S2). This result highlights the relevance of the lrgAB operon in infection by E. faecalis and constitutes the first report on such a role for this operon in this species.

Discussion

Assessing the basis for virulence of an opportunistic pathogen, such as E. faecalis, is difficult because it is invariably subtle and multifactorial. Research on this topic in recent years has concluded that the sole presence of a gene predicted to induce virulence in a strain does not necessarily imply that the same gene may lead to the same host fate in a different E. faecalis strains [17], [38]. Besides the genome background and the host, the manner in which the microbe is introduced also play a roles in determining whether or not a factor contributes to toxicity. D. melanogaster has been used as a model host to study pathogenesis because it provides easy handling, fast results, a fully sequenced genome, pre-existing libraries of genetic mutants, the possibility to play on the host side and similarities with the mammal immune system. In this work, we show that it can be used to discern varying levels of toxicity stemming from mutations in the fsr quorum regulatory system and the genes that it regulates.

In a representative of the hospital endemic lineage CC2, V583, the Fsr regulon is largely restricted to the five genes, namely gelE, sprE, ef1097, ef1351 and ef1352 found to be directly dependent on GBAP-induced Fsr activation, and twelve additional genes found to be dependent on GBAP induction of the proteases. Among these are genes coding for proteins involved in cell-wall, transport and regulatory functions. These genes are thus candidates to link the Fsr-proteases activity with the phenotypes known to be associated to their impairment, namely biofilm formation, adhesion and translocation to/in host-cells, autolysis and host damage and death. This contrasts with previous findings in the more commensal background, OG1RF, which was tested using an X-mer based oligonucleotide array with fewer controls and less redundancy than the Affymetrix microarrays used here. Our experiment assayed the first ten minutes after a burst of GBAP aiming to get clear, measurable and immediate changes in expression, whereas the study by Bourgogne et al [24] followed the changes in expression of an fsrB mutant spanning different growth stages. Their experimental design likely allowed for further events of differential expression to take place. Whether the differences in results stem from differences in strains, or differences in techniques and experimental approaches used, is not currently known.

In the present study, we found that induction of GelE and SprE by GBAP via the fsr regulator resulted in accumulation of mRNA encoding lrgAB, and that this induction was lytRS dependent, indicating a functional relationship between Fsr and LytRS regulons. In S. aureus, autolysis is positively regulated by Agr, a paralog of Fsr, that positively regulates LrgAB [39]. Unlike S. aureus, in E. faecalis FsrA does not regulate lrgAB genes directly, but does so indirectly. Both GelE and SprE have previously been shown to play a role in autolysis regulation in E. faecalis, respectively promoting and repressing it [40]. GelE is known to proteolytically activate AtlA [21], a major autolysin. Recently, GelE was also found to control the levels of SalB, a protein with no evident peptidoglycan hydrolytic activity, but affecting the levels of proteins involved in cell-wall synthesis and cell division [41]. A salB mutant in OG1-RF strain showed anomalous cell-division and increased autolysis [41]. Given the current knowledge, we could speculate that autolysis regulation could constitute the functional link, found in this study, between Fsr and LytRS. Future studies should address the mechanism behind GelE-SprE regulation of autolytic activities in E. faecalis and how they affect the expression of lrgAB operon through LytRS regulation.

EF1097 protein, found by Bourgogne et al. 2006 [24] to be dependent on Fsr regulation in E. faecalis OG1RF, was here confirmed to be true also for the V583 strain. In 2007, Swe et al. [42] suggested that ef1097 gene encodes a precursor of antimicrobial proteins with similarities to the streptococcin SA-M57 in S. aureus. EF1097 is conserved in all E. faecalis strains (Table S3). Finding this bacteriocin to be similarly regulated in distinct E. faecalis strains, namely OG1RF and V583, suggests this is a common feature in the species. QS-activated bacteriocin production may constitute a means to kill surrounding and competing bacteria thus providing competitive advantage to E. faecalis when colonizing or infecting a host. The Fsr homologue in S. aureus, Agr, is known to regulate the expression of pro-inflammatory peptides, the phenol-soluble modulins (PSM), in a RNAIII independent way [43]. Several roles in pathogenesis have been attributed to these amphipathic peptides [44], including antimicrobial activity [45], biofilm formation, maturation and detachment [46], and cytolytic ability to neutrophils and other human cells [47]. Although the role of EF1097 is not as extensively studied as that of PSMs, their shared features, namely quorum-sensing induction and role in virulence, should direct further studies on EF1097 role in E. faecalis biology and interaction with the host.

Despite the inexistence of clues on the EF1097 mechanism of action, bacteriocins have been shown to produce changes in membrane potential and affect transport of magnesium and amino acids [48]. EF1352, which codes for a putative magnesium-translocating P-type ATPase, was induced in all strains used in the microarrays. However, this operon lacks the previously described FsrA binding motif in its promotor region. It is thus licit to speculate that expression of this operon may be dependent on expression of ef1097, as this is the only Fsr dependent gene with the FsrA motif not deleted and tested in the microarrays assays. Further studies are needed to understand the link between bacteriocin production and induction of an MgtA transporter, although we could hypothesise that EF1097 could induce ion leakage, which in turn, would induce MgtA.

Despite different mortality curves were produced upon infection of Drosophila with the tested mutants, they all grew similarly inside the host. Hosts have two ways to deal with an infection: resistance and tolerance [36], [37]. Resistance is related with pathogen load and with mechanisms used to kill the pathogens: more resistant hosts have fewer pathogens. Tolerance is a consequence of the host ability to overcome the fitness cost imposed upon infection and induction of the immune system and is related to the ability of the host to remain healthy. Tolerance can be defined and measured from the slope of the health-by microbe curve. We plotted the flýs survival against pathogen load, assuming host population survival as a measure of its health (Figure 3), and confirmed that inactivation of Fsr and the two proteases increased flýs tolerance to E. faecalis, whereas flies showed similar resistance towards all studied E. faecalis strains. Mechanisms involved both in tolerance [49], [50] and resistance [5], [51], [52]of Drosophila towards enterococcal infections have been identified. If we understand how the E. faecalis virulence factors studied in this work affect the flýs tolerance mechanisms and responses, we can postulate that future approaches to fight enterococci can be through improving host tolerance, providing an alternative, or complementary, approach to bacterial killing by use of antibiotics.

[Figure omitted. See PDF.]

Figure 3. Drosophila-health by E. faecalis-load curve.

Source data used to construct this figure was obtained from results on Figure 2, only considering time points at which enough flies alive were available. All strains show two different slopes corresponding to different tolerance values, revealing that at some point (pathogen load value) there is a huge decrease in tolerance to E. faecalis. This inflection point corresponds to a lower pathogen load for the wild type strain (105), when compared to the mutant strains (106). For 106 value of pathogen load, the wild type induced only 10% survival in the Drosophila population, as opposed to 90% survival of the Drosophila population infected with the triple mutant.

https://doi.org/10.1371/journal.pone.0064740.g003

GelE is known to be able to degrade several host proteins. Therefore, besides its ability to degrade host immune factors, this protease may be involved in host tissue injury. Recently, GelE has also been implicated in release of Ace protein from the surface of E. faecalis cells in OG1RF strain [22]. In that study, authors showed that deletion of gelE gene increased the number of Ace proteins bound to the surface of the bacterial cells, increasing adherence to collagen. In the insect model G. mellonella, collagen adherence has been shown to be required for invasion and virulence [53]. Although this remains to be proven true for Drosophila, it is licit to speculate that the lower attenuation of the gelE mutant in this insect host model could be due to increased adherence to host cells and proteins. Despite considered to be cell-bound, SprE is also able to degrade host proteins, such as insulin and fibrinogen, but not immune system elements, such as complement from human serum or Cecropin from insect hemolymph [20]. Its major contribution to host death proven in this work needs thus urgent clarification.

This work brought to light new players (Figure 4) in Fsr role in E. faecalis, namely LrgAB operon, which will help unravel the bacterial programmed cell death which, in turn, may help discover new approaches to control this important nosocomial pathogen. Moreover, Drosophila was successfully established as a model to study virulence associated genes in E. faecalis, highlighting LrgAB and EF1097 as novel virulence factors induced by QS. Using Drosophila as a model also allowed us to show that SprE is, per se, a relevant player in host injury and to suggest that E. faecalis success during septic injury is not due to GelE acting as a bacterial defence against the flies AMPs, but that it could rather be through host injury.

[Figure omitted. See PDF.]

Figure 4. GBAP-dependent regulatory network.

Once the GBAP (black disks) concentration outside cells reaches a certain threshold (upper part of the cell), the Fsr system is activated, and the FsrA regulator induces expression of gelE, sprE and ef1097 genes. Both produce proteins which will be located to the cell membrane and cell wall. Although GelE is loosely bound to the cell, it will also be released from it. The induced expression of ef1352, which encodes a putative MgtA protein, by GBAP is likely due to increased amounts of EF1097, predicted to be a bacteriocin. EF1352 could function as an auto-immunity factor against EF1097. The increased level of GelE and SprE proteins in the cell-wall in response to GBAP are proposed to induce changes sensed by LytS protein, which in turn, activates LytR, responsible for induction of lrgAB genes. When no GBAP is produced (lower part of the cell) ef1097 is not expressed, but both GelE and SprE are still produced, although in lower amounts (dotted line). In this situation, lrgAB genes are still expressed, but the increment in their expression during growth in the exponential phase (assayed during microarrays performed without GBAP) is not due to the QS molecule. As we found that lrgAB can still be expressed in a lytRS mutant, we propose that this is not the only regulator able to induce expression of that operon.

https://doi.org/10.1371/journal.pone.0064740.g004

Materials and Methods

Bacterial Strains and Plasmids

Strains and plasmids used in this study are listed in Table 2. E. faecalis strains were grown either in BHI, M17 broth/agar (Oxoid) or Enterococcel Agar (Quilaban) at 37°C, unless a different growth temperature is specified. Escherichia coli strains were grown in LB medium (Sigma) at 37°C with agitation. The following antibiotic concentrations were used: with E. faecalis, tetracycline 30 µg/ml; with E. coli, ampicillin 150 µg/ml and tetracycline 150 µg/ml.

[Figure omitted. See PDF.]

Table 2. Strains, plasmids and primers used in this study.

https://doi.org/10.1371/journal.pone.0064740.t002

Antibiotic Resistance Assay

Resistance to different antibiotics (Ciprofloxacin, Penicillin, Sulphamethoxazole, Vancomycin, Nitrofurantoin, Ofloxacin, Ampicillin, and Ceftriaxone) was determined according to the recommendations of the disk providers (Oxoid) [54], and results were interpreted according to the recommendations of the Clinical and Laboratory Standards Institute (CLSI, formerly NCCLS) (http: //www.clsi.org/).

General DNA Techniques

General molecular biology techniques were performed by standard methods. Restriction enzymes, polymerases and T4 DNA ligase were used according to manufacturers’ instructions. PCR amplification was performed using a Biometra thermocycler. When necessary, PCR products and DNA restriction fragments were purified with purification kits (Macherey-Nagel). Plasmids were purified using the Miniprep kit (Macherey-Nagel). Electrotransformation of E. coli and E. faecalis was carried out as described by Dower et al. (1988) and Dunny et al. (1991), using a Gene Pulser apparatus (Bio-Rad) [55], [56]. Plasmid inserts and mutant sequence were confirmed by sequencing at StabVida (Portugal).

Mutant Construction

E. faecalis V583 mutants (MG01[V583ΔfsrBΔgelE]; MG02[V583ΔfsrBΔsprE]; and MG03[V583ΔfsrBΔgelEΔsprE] were constructed by introducing pVT01(ΔgelE), pVT02(ΔsprE), and pVT03(ΔgelEΔsprE), respectively into the VI13[V583ΔfsrB] strain and selecting for protease gene deletions essentially as described by Thomas et al. 2009 [21]. These strains are still responsive to external GBAP, but are not able to produce the QS molecule, as is the case of VI13[V583ΔfsrB] [30]. Construction of KS17[V583ΔlytSR] and KS18[V583ΔlrgAB] mutants was done similarly to the method described by Thurlow et al. using the marker less deletion vector pLT06 [57]. In brief, flanking regions of lytSR and lrgAB were amplified from E. faecalis V583 chromosomal DNA by PCR with primers LytP1, LytP2, LytP3, LytP4 and LrgP1, LrgP2, LrgP3, LrgP4 respectively (Table 2). The flanking PCR fragments were ligated together following BamHI digestion and reamplified by PCR using the external primers P1 and P4, for both the lytSR and lrgAB deletion constructs. The resulting amplicons were digested with EcoRI and PstI and cloned into similarly digested pLT06 to create pKS103 (ΔlytSR) and pKS104 (ΔlrgAB). The resulting plasmids were confirmed by restriction analysis and sequenced. Plasmids were introduced into E. faecalis V583 by electroporation and selection of the desired mutant was performed as described [57]. To create KS19[V583ΔfsrBΔlytSR], VI13 was transformed with pKS103 (ΔlytSR) and selection for deletion of lytSR was performed as described [57].

E. faecalis V583Δef1097 was constructed essentially as described by Brinster et al. (2007) [58] in strain VE14089 [36]. Briefly, flanking regions of EF1097 were amplified from chromosomal DNA of V583 by PCR with primers EF1097_1, EF1097_2, EF1097_3 and EF1097_4 respectively (Table 2). The two cognate PCR fragments were fused by PCR using the external primers EF1097_1 and EF1097_4 for EF1097, respectively, and the resulting product was cloned into pGEM-T (Promega). The inserted PCR fragment was removed from its cloning vector by restriction enzymes and subsequently cloned into pG+host9 plasmid [59], which was then electroporated into E. faecalis VE14089. The ef1097 single- and double crossover mutants were selected as described by Brinster et al. (2007) [58], [59]. Successful targeted mutations of ef1097 were first identified by PCR screening and were confirmed by sequencing (StabVida, Portugal), and analysed by Vector NTI program (Invitrogen).

RNA Extraction and cDNA Synthesis for Microarrays

E. faecalis strains were grown in BHI, at 37°C, until 0.4 OD (600 nm). At this point, purified GBAP, prepared as previously described [29], was added to a final concentration of 10 nM in the culture. This concentration was previously shown to be able to induce the Fsr system [9], [36]. In order to determine the effect of GBAP induction at a time in growth when we knew, from previous work [35], that the Fsr system was not yet fully activated, we chose 0.4 OD to add GBAP. The quorum-sensing molecule was added to induce the Fsr quorum-sensing system in strains which lack the ability to produce the GBAP molecule, but are still able to sense it. At time zero (immediately after GBAP addition) and after 10 min post-GBAP addition, RNA was extracted from cells and used to synthesize cDNA and perform microarray transcriptional analysis. Experiments without GBAP were also performed. To prepare samples for Affymetrix GeneChip analysis, a previously published protocol was used with few modifications [60]. Briefly, RNA was stabilized with RNA protect (Qiagen) and RNA was isolated with RNeasy columns per the manufacturer's instructions (Qiagen). Samples were treated with RNase-free DNase I (Roche) to remove contaminating DNA, and the absence of contaminating DNA was confirmed by PCR. RNA integrity was verified using agarose gel electrophoresis of glyoxylated samples (Ambion). cDNA was prepared from RNA using Superscript II Reverse Transcriptase (Invitrogen) with random (N6) priming. cDNA was fragmented with dilute DNase I (Roche) and fragments were biotinylated with the BioArray Terminal Labeling Kit (Enzo Life Sciences) prior to hybridization.

Affymetrix GeneChip Analysis

Samples were hybridized to a previously described custom E. faecalis Affymetrix GeneChip [27] and scanned at the University of Iowa DNA Core Facility. All microarray experiments were performed in duplicate. Data was analysed using Affymetrix GeneChip Operating Software, which identifies probe sets with statistically significant hybridization over background (i.e. presence versus absence calls) and among those, identifies probe sets for which hybridization is significantly increased or decreased in pairwise comparisons of microarray experiments. Signal log ratios for differentially expressed probe sets were averaged and converted to fold change values. Only genes with ≥3-fold differential expression were considered. The data discussed in this publication have been deposited in NCBI's Gene Expression Omnibus [61] and are accessible through GEO Series accession number GSE42036 (http: //www.ncbi.nlm.nih.gov/geo/query/acc.cgi?acc=GSE42036).

Semiquantitative RT-PCR

RNA was extracted from strains V583ΔlytRS and V583ΔfsrB grown in BHI broth at 37°C. Briefly, overnight cultured cells were diluted 1∶100 and growth was monitored by following OD600. Cells were collected in the same conditions as those used for RNA extraction for microarrays. Total RNA was extracted and purified with an RNeasy Mini kit (Qiagen). RNA integrity was checked by electrophoresis on a 1% agarose gel (RNase free). cDNA was synthesized using random primers (Roche Diagnostics), 3 mg total RNA and a Transcriptor High Fidelity cDNA Synthesis kit (Roche Diagnostics). Serial dilutions of V583ΔlytRS and V583ΔfsrB cDNA were used for PCR in order to amplify cDNA of lrgA (primers: lrgA, mlrgA), lrgB (primers: lrgB, mlrgB) and gelE (primers: mgel_2, gelE) (Table 2).

D. melanogaster Infection

Oregon R male flies were injected with 50 nl of bacteria at 0.02 OD (600 nm) from one of the strains: V583, V583ΔfsrBΔgelE, V583ΔfsrBΔsprE, V583ΔfsrBΔgelEΔsprE, V583ΔlytRS, V583ΔlrgAB, VE14089 and VE14089Δef1097. As control, flies were injected with the same volume of BHI medium. Male flies were anesthetized with CO2 and the injections were carried out with a pulled glass capillary needle using a nano-injector (Nanoliter 2000, World Precision Instruments). Reproducibility was measured by determining the number of bacteria injected at time zero. Injected flies were placed at 29°C, 65% humidity. Seventy-five flies were assayed for each survival curve, and they were placed in three vials of 25 flies each. Each experiment was repeated three times, making a total of 225 flies tested per strain in each set of three replicates, to ensure high confidence results. Death was recorded at 0, 4, 6, 8, 10, 12, 14 and 24 h hours post-injection. All experiments were performed at least three times. Following challenge with bacteria, six individual flies were collected (at 0 h, 4 h, 8 h, 12 h and 24 h), homogenized, diluted serially, and plated onto Enterococcel agar (Quilaban). E. faecalis CFUs (colony forming units) were determined by testing three groups of six flies for each time point.

Percentage of Similarities between V583 Genome and Other Genomes Published

The percentage of similarities was made with blast program (http: //blast.ncbi.nlm.nih.gov/). The genomes that were used on this analysis were from Broad Institute page (http: //www.broadinstitute.org/annotation/genome/enterococcus_faecalis/MultiHome.html) and compared with V583 genome (http: //www.ncbi.nlm.nih.gov/nuccore/NC_004668.1).

Statistical Analysis

Statistical analysis of Drosophila survival was performed using GraphPad Prism software version 5.03. Survival curves were compared using Log-rank and Gehan-Breslow-Wilcoxon tests. Statistical analysis of Drosophila survival was performed using t-test.

Supporting Information

[Figure omitted. See PDF.]

Figure S1.

lrgAB expression in the absence of GBAP. The semi-quantitative RT-PCR shows expression of lrgAB genes in the VI13 (ΔfsrB mutant) and KS19 (ΔfsrBΔlytRS mutant) strains, in the absence of GBAP. Expression of gelE and gdh were used as negative and positive controls, respectively. The RNA used for this analysis was previously treated with RNase-free DNase I to remove contaminating DNA and PCR was done in order to confirm absence of DNA from the RNA samples analysed.

https://doi.org/10.1371/journal.pone.0064740.s001

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Figure S2.

E. faecalis growth curves in injected flies. Oregon R (5- to 7-day-old) male adult flies, raised at 25°C, were divided in tubes of 25 flies each, and infected, by septic injury onto the thorax with a thin needle, with V583 mutants. Flies were collected at 0, 4, 8, 12, and 24 h. Three groups of six flies for each time point were homogenized and plated in Enterococcel agar and E. faecalis CFUs were determined.

https://doi.org/10.1371/journal.pone.0064740.s002

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Table S1.

https://doi.org/10.1371/journal.pone.0064740.s003

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Table S2.

https://doi.org/10.1371/journal.pone.0064740.s004

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Table S3.

https://doi.org/10.1371/journal.pone.0064740.s005

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Acknowledgments

The authors are grateful to Isabel Marques, from IGC, for her help in enterococcal genome comparison regarding genes directly regulated by Fsr.

Author Contributions

Conceived and designed the experiments: NT MdFSL MSG. Performed the experiments: NT SV MJG RY. Analyzed the data: NT KP AZR MdFSL. Contributed reagents/materials/analysis tools: MSG LEH JN AJ MdFSL. Wrote the paper: NT MdFSL AZR KP LEH JN MSG AJ.

Citation: Teixeira N, Varahan S, Gorman MJ, Palmer KL, Zaidman-Remy A, Yokohata R, et al. (2013) Drosophila Host Model Reveals New Enterococcus faecalis Quorum-Sensing Associated Virulence Factors. PLoS ONE 8(5): e64740. https://doi.org/10.1371/journal.pone.0064740

References

1. Boyer L, Paquette N, Silverman N, Stuart LM (2012) Bacterial effectors: learning on the fly. Adv Exp Med Biol 710: 29–36.

2. Glavis-Bloom J, Muhammed M, Mylonakis E (2012) Of model hosts and man: using Caenorhabditis elegans, Drosophila melanogaster and Galleria mellonella as model hosts for infectious disease research. Adv Exp Med Biol 710: 11–17.

3. Cox CR, Gilmore MS (2007) Native microbial colonization of Drosophila melanogaster and its use as a model of Enterococcus faecalis pathogenesis. Infect Immun 75: 1565–1576.

4. Schneider DS, Ayres JS, Brandt SM, Costa A, Dionne MS, et al. (2007) Drosophila eiger mutants are sensitive to extracellular pathogens. PLoS Pathog 3: e41.

5. Nehme NT, Quintin J, Cho JH, Lee J, Lafarge MC, et al. (2011) Relative roles of the cellular and humoral responses in the Drosophila host defense against three gram-positive bacterial infections. PLoS One 6: e14743.

6. Gilmore MS, Coburn PS, Nallapareddy SR, Murray BE (2002) Enterococcal Virulence. In: Gilmore MS, Clewell DB, Courvalin P, Dunny GM, Murray BE, Rice LB, editor. The Enterococci Pathogenesis, Molecular Biology, and Antibiotic Resistance. Washington D.C.: American Society for Microbiology. 301–354.

7. Qin X, Singh KV, Weinstock GM, Murray BE (2000) Effects of Enterococcus faecalis fsr genes on production of gelatinase and a serine protease and virulence. Infect Immun 68: 2579–2586.

8. Novick RP, Ross HF, Projan SJ, Kornblum J, Kreiswirth B, et al. (1993) Synthesis of staphylococcal virulence factors is controlled by a regulatory RNA molecule. Embo J 12: 3967–3975.

9. Nakayama J, Cao Y, Horii T, Sakuda S, Akkermans AD, et al. (2001) Gelatinase biosynthesis-activating pheromone: a peptide lactone that mediates a quorum sensing in Enterococcus faecalis. Mol Microbiol 41: 145–154.

10. Qin X, Singh KV, Weinstock GM, Murray BE (2001) Characterization of fsr, a regulator controlling expression of gelatinase and serine protease in Enterococcus faecalis OG1RF. J Bacteriol 183: 3372–3382.

11. Garsin DA, Sifri CD, Mylonakis E, Qin X, Singh KV, et al. (2001) A simple model host for identifying Gram-positive virulence factors. Proc Natl Acad Sci U S A 98: 10892–10897.

12. Sifri CD, Mylonakis E, Singh KV, Qin X, Garsin DA, et al. (2002) Virulence effect of Enterococcus faecalis protease genes and the quorum-sensing locus fsr in Caenorhabditis elegans and mice. Infect Immun 70: 5647–5650.

13. Engelbert M, Mylonakis E, Ausubel FM, Calderwood SB, Gilmore MS (2004) Contribution of gelatinase, serine protease, and fsr to the pathogenesis of Enterococcus faecalis endophthalmitis. Infect Immun 72: 3628–3633.

14. Mylonakis E, Engelbert M, Qin X, Sifri CD, Murray BE, et al. (2002) The Enterococcus faecalis fsrB gene, a key component of the fsr quorum-sensing system, is associated with virulence in the rabbit endophthalmitis model. Infect Immun 70: 4678–4681.

15. Singh KV, Nallapareddy SR, Nannini EC, Murray BE (2005) Fsr-independent production of protease(s) may explain the lack of attenuation of an Enterococcus faecalis fsr mutant versus a gelE-sprE mutant in induction of endocarditis. Infect Immun 73: 4888–4894.

16. Jha AK, Bais HP, Vivanco JM (2005) Enterococcus faecalis mammalian virulence-related factors exhibit potent pathogenicity in the Arabidopsis thaliana plant model. Infect Immun 73: 464–475.

17. Gaspar F, Teixeira N, Rigottier-Gois L, Marujo P, Nielsen-LeRoux C, et al. (2009) Virulence of Enterococcus faecalis dairy strains in an insect model: the role of fsrB and gelE. Microbiology 155: 3564–3571.

18. Hancock LE, Perego M (2004) The Enterococcus faecalis fsr two-component system controls biofilm development through production of gelatinase. J Bacteriol 186: 5629–5639.

19. Zeng J, Teng F, Murray BE (2005) Gelatinase is important for translocation of Enterococcus faecalis across polarized human enterocyte-like T84 cells. Infect Immun 73: 1606–1612.

20. Park SY, Kim KM, Lee JH, Seo SJ, Lee IH (2007) Extracellular gelatinase of Enterococcus faecalis destroys a defense system in insect hemolymph and human serum. Infect Immun 75: 1861–1869.

21. Thomas VC, Hiromasa Y, Harms N, Thurlow L, Tomich J, et al. (2009) A fratricidal mechanism is responsible for eDNA release and contributes to biofilm development of Enterococcus faecalis. Mol Microbiol 72: 1022–1036.

22. Pinkston KL, Gao P, Diaz-Garcia D, Sillanpaa J, Nallapareddy SR, et al. (2011) The Fsr quorum-sensing system of Enterococcus faecalis modulates surface display of the collagen-binding MSCRAMM Ace through regulation of gelE. J Bacteriol 193: 4317–4325.

23. Singh KV, Nallapareddy SR, Sillanpaa J, Murray BE (2010) Importance of the collagen adhesin ace in pathogenesis and protection against Enterococcus faecalis experimental endocarditis. PLoS Pathog 6: e1000716.

24. Bourgogne A, Hilsenbeck SG, Dunny GM, Murray BE (2006) Comparison of OG1RF and an isogenic fsrB deletion mutant by transcriptional analysis: the Fsr system of Enterococcus faecalis is more than the activator of gelatinase and serine protease. J Bacteriol 188: 2875–2884.

25. Thurlow LR, Thomas VC, Narayanan S, Olson S, Fleming SD, et al. (2010) Gelatinase contributes to the pathogenesis of endocarditis caused by Enterococcus faecalis. Infect Immun 78: 4936–4943.

26. Park SY, Shin YP, Kim CH, Park HJ, Seong YS, et al. (2008) Immune evasion of Enterococcus faecalis by an extracellular gelatinase that cleaves C3 and iC3b. J Immunol 181: 6328–6336.

27. McBride SM, Fischetti VA, Leblanc DJ, Moellering RC Jr, Gilmore MS (2007) Genetic diversity among Enterococcus faecalis. PLoS ONE 2: e582.

28. Sahm DF, Kissinger J, Gilmore MS, Murray PR, Mulder R, et al. (1989) In vitro susceptibility studies of vancomycin-resistant Enterococcus faecalis. Antimicrob Agents Chemother 33: 1588–1591.

29. Willems RJ, Hanage WP, Bessen DE, Feil EJ (2011) Population biology of Gram-positive pathogens: high-risk clones for dissemination of antibiotic resistance. FEMS Microbiol Rev 35: 872–900.

30. Teixeira N, Santos S, Marujo P, Yokohata R, Iyer VS, et al. (2012) The incongruent gelatinase genotype and phenotype in Enterococcus faecalis are due to shutting off the ability to respond to the gelatinase biosynthesis-activating pheromone (GBAP) quorum-sensing signal. Microbiology 158: 519–528.

31. Woo Y, Affourtit J, Daigle S, Viale A, Johnson K, et al. (2004) A comparison of cDNA, oligonucleotide, and Affymetrix GeneChip gene expression microarray platforms. J Biomol Tech 15: 276–284.

32. Del Papa MF, Perego M (2011) Enterococcus faecalis virulence regulator FsrA binding to target promoters. J Bacteriol 193: 1527–1532.

33. Groicher KH, Firek BA, Fujimoto DF, Bayles KW (2000) The Staphylococcus aureus lrgAB operon modulates murein hydrolase activity and penicillin tolerance. J Bacteriol 182: 1794–1801.

34. Sharma-Kuinkel BK, Mann EE, Ahn JS, Kuechenmeister LJ, Dunman PM, et al. (2009) The Staphylococcus aureus LytSR two-component regulatory system affects biofilm formation. J Bacteriol 191: 4767–4775.

35. Nakayama J, Cao Y, Horii T, Sakuda S, Nagasawa H (2001) Chemical synthesis and biological activity of the gelatinase biosynthesis-activating pheromone of Enterococcus faecalis and its analogs. Biosci Biotechnol Biochem 65: 2322–2325.

36. Rigottier-Gois L, Alberti A, Houel A, Taly JF, Palcy P, et al. (2011) Large-scale screening of a targeted Enterococcus faecalis mutant library identifies envelope fitness factors. PLoS One 6: e29023.

37. Hanin A, Sava I, Bao Y, Huebner J, Hartke A, et al. (2010) Screening of in vivo activated genes in Enterococcus faecalis during insect and mouse infections and growth in urine. PLoS One 5: e11879.

38. Gaspar FB, Montero N, Akary E, Teixeira N, Matos R, et al. (2012) Incongruence between the cps type 2 genotype and host-related phenotypes of an Enterococcus faecalis food isolate. Int J Food Microbiol 158: 120–125.

39. Fujimoto DF, Brunskill EW, Bayles KW (2000) Analysis of genetic elements controlling Staphylococcus aureus lrgAB expression: potential role of DNA topology in SarA regulation. J Bacteriol 182: 4822–4828.

40. Thomas VC, Thurlow LR, Boyle D, Hancock LE (2008) Regulation of autolysis-dependent extracellular DNA release by Enterococcus faecalis extracellular proteases influences biofilm development. J Bacteriol 190: 5690–5698.

41. Shankar J, Walker RG, Wilkinson MC, Ward D, Horsburgh MJ (2012) SalB inactivation modulates culture supernatant exoproteins and affects autolysis and viability in Enterococcus faecalis OG1RF. J Bacteriol 194: 3569–3578.

42. Swe PM, Heng NC, Ting YT, Baird HJ, Carne A, et al. (2007) ef1097 and ypkK encode enterococcin V583 and corynicin JK, members of a new family of antimicrobial proteins (bacteriocins) with modular structure from Gram-positive bacteria. Microbiology 153: 3218–3227.

43. Queck SY, Jameson-Lee M, Villaruz AE, Bach TH, Khan BA, et al. (2008) RNAIII-independent target gene control by the agr quorum-sensing system: insight into the evolution of virulence regulation in Staphylococcus aureus. Mol Cell 32: 150–158.

44. Periasamy S, Chatterjee SS, Cheung GY, Otto M (2012) Phenol-soluble modulins in staphylococci: What are they originally for? Commun Integr Biol 5: 275–277.

45. Joo HS, Cheung GY, Otto M (2011) Antimicrobial activity of community-associated methicillin-resistant Staphylococcus aureus is caused by phenol-soluble modulin derivatives. J Biol Chem 286: 8933–8940.

46. Periasamy S, Joo HS, Duong AC, Bach TH, Tan VY, et al. (2012) How Staphylococcus aureus biofilms develop their characteristic structure. Proc Natl Acad Sci U S A 109: 1281–1286.

47. Kretschmer D, Nikola N, Durr M, Otto M, Peschel A (2012) The virulence regulator Agr controls the staphylococcal capacity to activate human neutrophils via the formyl peptide receptor 2. J Innate Immun 4: 201–212.

48. Uratani Y, Hoshino T (1984) Pyocin R1 inhibits active transport in Pseudomonas aeruginosa and depolarizes membrane potential. J Bacteriol 157: 632–636.

49. Rakoff-Nahoum S, Paglino J, Eslami-Varzaneh F, Edberg S, Medzhitov R (2004) Recognition of commensal microflora by toll-like receptors is required for intestinal homeostasis. Cell 118: 229–241.

50. Leendertse M, Willems RJ, Giebelen IA, van den Pangaart PS, Wiersinga WJ, et al. (2008) TLR2-dependent MyD88 signaling contributes to early host defense in murine Enterococcus faecium peritonitis. J Immunol 180: 4865–4874.

51. Lemaitre B, Reichhart JM, Hoffmann JA (1997) Drosophila host defense: differential induction of antimicrobial peptide genes after infection by various classes of microorganisms. Proc Natl Acad Sci U S A 94: 14614–14619.

52. Brun S, Vidal S, Spellman P, Takahashi K, Tricoire H, et al. (2006) The MAPKKK Mekk1 regulates the expression of Turandot stress genes in response to septic injury in Drosophila. Genes Cells 11: 397–407.

53. Abranches J, Miller JH, Martinez AR, Simpson-Haidaris PJ, Burne RA, et al. (2011) The collagen-binding protein Cnm is required for Streptococcus mutans adherence to and intracellular invasion of human coronary artery endothelial cells. Infect Immun 79: 2277–2284.

54. Lopes Mde F, Ribeiro T, Martins MP, Tenreiro R, Crespo MT (2003) Gentamicin resistance in dairy and clinical enterococcal isolates and in reference strains. J Antimicrob Chemother 52: 214–219.

55. Dower WJ, Miller JF, Ragsdale CW (1988) High efficiency transformation of E. coli by high voltage electroporation. Nucleic Acids Res 16: 6127–6145.

56. Dunny GM, Lee LN, LeBlanc DJ (1991) Improved electroporation and cloning vector system for gram-positive bacteria. Appl Environ Microbiol 57: 1194–1201.

57. Thurlow LR, Thomas VC, Hancock LE (2009) Capsular polysaccharide production in Enterococcus faecalis and contribution of CpsF to capsule serospecificity. J Bacteriol 191: 6203–6210.

58. Brinster S, Furlan S, Serror P (2007) C-terminal WxL domain mediates cell wall binding in Enterococcus faecalis and other gram-positive bacteria. J Bacteriol 189: 1244–1253.

59. Maguin E, Prevost H, Ehrlich SD, Gruss A (1996) Efficient insertional mutagenesis in lactococci and other gram-positive bacteria. J Bacteriol 178: 931–935.

60. Schuster M, Lostroh CP, Ogi T, Greenberg EP (2003) Identification, timing, and signal specificity of Pseudomonas aeruginosa quorum-controlled genes: a transcriptome analysis. J Bacteriol 185: 2066–2079.

61. Edgar R, Domrachev M, Lash AE (2002) Gene Expression Omnibus: NCBI gene expression and hybridization array data repository. Nucleic Acids Res 30: 207–210.

62. Hancock L, Perego M (2002) Two-component signal transduction in Enterococcus faecalis. J Bacteriol 184: 5819–5825.

63. Grant SG, Jessee J, Bloom FR, Hanahan D (1990) Differential plasmid rescue from transgenic mouse DNAs into Escherichia coli methylation-restriction mutants. Proc Natl Acad Sci U S A 87: 4645–4649.

64. Law J, Buist G, Haandrikman A, Kok J, Venema G, et al. (1995) A system to generate chromosomal mutations in Lactococcus lactis which allows fast analysis of targeted genes. J Bacteriol 177: 7011–7018.

65. Thurlow LR, Thomas VC, Fleming SD, Hancock LE (2009) Enterococcus faecalis capsular polysaccharide serotypes C and D and their contributions to host innate immune evasion. Infect Immun 77: 5551–5557.