RpoS integrates CRP, Fis, and PhoP signaling pathways to control Salmonella Typhi hlyE expression
© Jofré et al.; licensee BioMed Central Ltd. 2014
Received: 3 December 2013
Accepted: 21 May 2014
Published: 31 May 2014
SPI-18 is a pathogenicity island found in some Salmonella enterica serovars, including S. Typhi. SPI-18 harbors two ORFs organized into an operon, hlyE and taiA genes, both implicated in virulence. Regarding the hlyE regulation in S. Typhi, it has been reported that RpoS participates as transcriptional up-regulator under low pH and high osmolarity. In addition, CRP down-regulates hlyE expression during exponential growth. Previously, it has been suggested that there is another factor related to catabolite repression, different from CRP, involved in the down-regulation of hlyE. Moreover, PhoP-dependent hlyE up-regulation has been reported in bacteria cultured simultaneously under low pH and low concentration of Mg2+. Nevertheless, the relative contribution of each environmental signal is not completely clear. In this work we aimed to better understand the regulation of hlyE in S. Typhi and the integration of different environmental signals through global regulators.
We found that Fis participates as a CRP-independent glucose-dependent down-regulator of hlyE. Also, Fis and CRP seem to exert the repression over hlyE through down-regulating rpoS. Moreover, PhoP up-regulates hlyE expression via rpoS under low pH and low Mg2+ conditions.
All these results together show that, at least under the tested conditions, RpoS is the central regulator in the hlyE regulatory network, integrating multiple environmental signals and global regulators.
The genus Salmonella includes two species, Salmonella bongori and Salmonella enterica. S. enterica is comprised of six subspecies where only a small fraction of the subspecies I serovars are involved in infections of humans and other warm-blooded animals [1, 2]. Most of these Salmonella serovars are “generalists”, infecting a wide range of hosts and causing different symptoms. This is the case for S. enterica serovar Typhimurium (S. Typhimurium) and S. enterica serovar Enteritidis (S. Enteritidis) . In contrast, some serovars are able to infect a specific host, causing typhoid-like disease . These include S. enterica serovar Typhi (S. Typhi), which infects only humans.
S. enterica infection begins with ingestion of contaminated water or food. Some environmental conditions found in the gut induce the expression of virulence factors that participate in the intestinal invasion and colonization, including genes found in the Salmonella Pathogenicity Island 1 (SPI-1) . Among these conditions, high osmolarity, microaerobiosis and response to bile seem to be the most important signals at this stage of the infection [5, 6]. Some S. enterica serovars, such as S. Typhi in humans, can enter the host bloodstream, disseminate and survive inside the macrophages by expressing a different subset of genes, including SPI-2 genes . The most important conditions found at this stage of the infection include nutrient depletion (especially Mg2+) and low pH . It is thought that Salmonella virulence factors are specifically expressed at determined stages of the infection. Nevertheless, at present it is more obvious that several virulence factors are not restricted to a unique stage of the infection. For example, SipA, encoded by SPI-1 enhances entry efficiency to intestinal epithelial cells by promoting actin polymerization, but also contributes to proliferation of Salmonella inside macrophages .
The SPI-18 is a pathogenicity island found in a subset of S. enterica serovars able to produce a systemic disease in humans, including S. Typhi; but absent in generalist serovars such as S. Typhimurium . The SPI-18 harbors only two ORFs organized into an operon, the taiA – hlyE genes [10, 11]. TaiA is a novel invasin involved in increased phagocytosis of the bacteria by macrophages . On the other hand, HlyE (also called ClyA or SheA) is a well characterized hemolysin that is exported in outer membrane vesicles . Human infections by S. Typhi cause a specific antibody response to HlyE, indicating effective toxin production during the normal infective cycle . Moreover, heterologous expression of S. Typhi hlyE in S. Typhimurium improves the colonization of deep organs in mice .
Regarding hlyE regulation in S. Typhi, previously it has been reported that RpoS participates as a transcriptional positive regulator under low pH and high osmolarity . In addition, the global regulator CRP, implicated in catabolite repression, down-regulates hlyE expression during exponential growth. Nevertheless, addition of glucose to the growth medium results in a decrease of hlyE mRNA in S. Typhi Δcrp mutant, suggesting that there is another factor related to catabolite repression, different from CRP, involved in down-regulation of hlyE in S. Typhi . PhoP-dependent up-regulation of hlyE was reported when bacteria were cultured simultaneously under low pH and low concentration of Mg2+. Nevertheless, the relative contribution of each environmental signal is not clear.
In this work we wanted to better understand the regulation of hlyE in S. Typhi and the integration of different environmental signals through global regulators. We found that Fis participates as a CRP-independent glucose-dependent down-regulator of hlyE in S. Typhi. Moreover, Fis and CRP seem to exert the repression over hlyE via down-regulating rpoS. On the other hand, PhoP up-regulates hlyE expression via rpoS under low pH and low Mg2+ conditions. All these results together show that, at least under the tested conditions, RpoS is the central regulator in the hlyE regulatory network, integrating multiple environmental signals.
Fis participates in the repression of hlyE at transcriptional level
To corroborate whether an increase in the hlyE transcript due to the absence of fis in LB and in LB + glucose resulted in increased HlyE-associated hemolytic activity, erythrocyte damage produced by whole bacterial lysates of S. Typhi WT and Δfis mutants grown in LB or LB + glucose was compared by quantifying the release of hemoglobin. We used PBS and 5% sodium deoxycholate to obtain the value for 0% and 100% hemolysis respectively, as previously described . As shown in Figure 1B and C, the Δcrp mutant appeared to be more hemolytic that the WT strain only when cultured in LB (control). As previously reported, this effect is abolished in presence of glucose . On the other hand, the Δfis mutant appeared also to be more hemolytic than the WT strain. However, unlike the effect observed with the Δcrp mutant, the presence of glucose was unable to revert the hemolysis to the WT level in the Δfis strain, consistently with the results obtained with RT-PCR (Figure 1A). S. Typhi Δcrp ΔhlyE and S. Typhi Δfis ΔhlyE exhibited no hemolysis in any condition (data not shown). To corroborate the data obtained by RT-PCR and by the determination of the hemolytic activity, we constructed the S. Typhi hlyE-3xFLAG strain by placing a 3xFLAG at the C-terminus of hlyE. This procedure led to subsequent detection of the FLAG-tagged proteins via Western blotting as previously described . Then, we constructed the S. Typhi hlyE-3xFLAG Δcrp and S. Typhi hlyE-3xFLAG Δfis derivatives by electrotransforming with gDNA from single mutants as described . These strains were used to determine the HlyE accumulation. As shown in Figure 1D, all the results obtained by RT-PCR were confirmed by Western blot. These results together show that fis participates in the repression of hlyE at transcriptional level.
Glucose increases transcription of fis
As stated above, the effect of Δcrp mutant on hlyE transcriptional level is relieved when glucose is added into the culture medium, suggesting that a second repressor is activated in some way under a glucose-rich medium. Considering that Fis also participates as an hlyE repressor and considering that glucose is unable to relief the Δfis effect in the hlyE transcription (Figure 1A), we inferred that glucose might increase the transcription of fis. In order to test this hypothesis, we performed a RT-PCR to detect the fis transcript of S. Typhi cultured to OD600 = 0.4 in LB or LB + glucose. As shown in Figure 1E, the presence of glucose increased fis transcription compared with bacteria grown in standard LB. This result supports the fact that glucose increases the fis expression, thereby contributing to the repression of hlyE.
CRP and Fis participate in the repression of hlyE transcription by repressing rpoS transcription
PhoPQ two-component regulatory system participates in hlyE induction via rpoS
All these results together strongly suggest that RpoS is essential for hlyE transcription under all the conditions tested. On the other hand, phoPQ participates in hlyE induction under pH 5.0 and low Mg2+ in an RpoS-dependent manner.
As previously reported, CRP participates in the hlyE repression. Nevertheless, the mechanism involved in such repression has not been elucidated . The absence of obvious CRP DNA-binding boxes at the promoter region of taiA – hlyE operon , and the fact that we were unable to find direct binding between CRP-cAMP and the taiA – hlyE promoter region, suggests that CRP might be acting indirectly, more likely regulating other transcriptional regulators. Here, we present genetic evidence indicating that CRP exerts down-regulation of hlyE by repressing rpoS (Figures 1 and 2), one of the most important hlyE activators in S. Typhi . CRP has been also described as an RpoS repressor in other bacterial species. For instance, E. coli Δcrp is remarkably resistant to hydrogen peroxide and acid stress, due to an elevated catalase activity attributable to enhanced accumulation of the alternate sigma factor RpoS . On the other hand, it has been reported that rpoS expression is repressed by direct binding of CRP-cAMP to its promoter region in Vibrio vulnificus. In that same work, the authors suggest that CRP could repress RpoS expression in S. enterica by direct binding arguing that S. enterica rpoS promoter presents similar CRP binding boxes than V. vulnificus. Nevertheless, the available studies of S. enterica include experiments performed only with S. Typhimurium, and the data are controversial. Cheng and Sun demonstrated direct binding of CRP to the rpoS promoter region in S. Typhimurium, where it is able to bind to two sites in this sequence. Both sites are conserved in S. Typhi rpoS promoter, suggesting a direct binding by CRP. Moreover, the authors showed that base-substitutions performed in the CRP-binding sites at the rpoS promoter region, led to a decreased rpoS transcription, concluding that CRP is an rpoS up-regulator . Nevertheless, this result can be also explained by the fact that the base-substitution may be affecting unknown overlapped regulators’ binding sites. On the other hand, Hirsch and Elliott showed that S. Typhimurium rpoS-lacZ Δcrp exhibited twice more β-galactosidase activity compared with the otherwise isogenic strain S. Typhimurium rpoS-lacZ, suggesting that CRP is an RpoS repressor , supporting our findings in S. Typhi. In addition, CRP has been described as a pleiotropic factor in S. enterica implicated in carbon source utilization, synthesis of flagella, reduced growth rate, and attenuation of virulence, among other functions [29–32]. This versatility can be explained, at least in part, by the fact that CRP is regulating rpoS.
As previously stated, hlyE presents a CRP-independent down-regulation when glucose is present in the culture medium, suggesting the presence of another glucose-dependent down-regulator . In this work, we found that fis participates in hlyE repression especially in presence of glucose (Figure 1). It has been stated that Fis regulates gene expression by increasing/decreasing its level in E. coli. In this work, we found that glucose induces the fis expression in S. Typhi, suggesting that Fis is also regulated by its level in S. enterica (Figure 1E). On the other hand, Fis precludes the RpoS accumulation by repressing the rpoS transcription (Figure 2). Hirsch and Elliott showed that fis represses rpoS expression by direct binding in S. Typhimurium , supporting our observations. As with CRP, Fis might participate in down-regulation of hlyE via RpoS, and this regulation could be exerted directly due to the presence of several putative Fis binding boxes in S. Typhi rpoS promoter (Figure 2C). Considering that crp and fis deletions seem to produce additive effects in hlyE transcription (Figure 1A), these two repressors probably act through different pathways to repress the hlyE expression (Figure 4).
We also explored the relative participation of rpoS and phoPQ in the up-regulation of hlyE under pH 5.0 and low Mg2+ concentrations. We found that RpoS is essential for hlyE expression under all the tested conditions, strongly suggesting that RpoS accumulation is the most relevant event in hlyE regulation. Moreover, both rpoS and phoPQ are necessary to achieve a complete induction of hlyE under low pH in S. Typhi, where the phoPQ-dependent induction occurs via RpoS. The induction pathway of RpoS by low pH is not fully understood. One component of induction is RpoS stabilization, where PhoPQ participates by serving as a transcriptional activator of the iraP (yaiB) gene in S. Typhimurium. IraP enhances RpoS stability by interacting with RssB, the protein that normally delivers RpoS to the ClpXP protease for degradation , supporting the fact that phoPQ requires rpoS to induce hlyE expression (Figure 4). On the other hand, it has been reported that mutant strains unable to degrade RpoS still exhibited induction under acid shock in S. enterica. Moreover, rpoS translation is enhanced under low pH . This phenomenon can explain the fact that rpoS is able to partially induce hlyE transcription under pH 5.0, independently of the presence of phoPQ (Figure 3A).
In the case of the hlyE induction under low Mg2+ concentrations, we found that phoPQ is essential to increase hlyE transcript in an rpoS-dependent manner. In S. enterica RpoS accumulates when bacteria are grown under low Mg2+ conditions . This process requires PhoPQ, which is specifically activated under low Mg2+ by increasing the transcription of iraP, as previously reported [33, 35]. It is possible that PhoPQ is participating in the increase of hlyE transcription under low Mg2+ via IraP-dependent RpoS stabilization. Nevertheless, in the case of low Mg2+ we found that rpoS is unable to induce an increased transcription of hlyE in a ΔphoPQ background. Previous studies reported that low Mg2+ concentrations are unable to induce RpoS accumulation in a ΔphoPQ background , supporting our results.
In this paper we showed that RpoS is the most important activator of hlyE expression. According to our results, RpoS sits atop a hierarchical network that integrates diverse environmental and physiological cues. PhoPQ, CRP, and Fis fine-tune these global inputs to precisely control the dosage of HlyE, but also the time in the infection cycle in which this gene is expressed. For HlyE, the amount of protein produced can determine the function. For instance, sublytic concentrations of HlyE affect the Ca2+ homeostasis in epithelial cells by induction of slow, intracellular Ca2+ oscillations, while increased concentrations act cytolytically . Thus, HlyE belongs to the novel group of pore-forming toxins shown to elicit such biphasic responses . On the other hand, HlyE apparently is participating in different stages of the infective process. Previously, it has been reported that S. Typhi hlyE mutants are impaired in invasion of human epithelial cells HEp-2 in vitro. Consistently, other pore-forming hemolysins play critical roles in invasion of eukaryotic epithelial cells [37–39]. These data show that hlyE could participate in the intestinal stage of the S. Typhi infection. On the other hand, HlyE is capable to reduce or control bacterial growth, as hlyE deletion enhanced S. Typhi survival within macrophages without affecting cytotoxicity , suggesting that this cytolysin could also be participating in the systemic dissemination of bacteria inside macrophages. In addition, hlyE increase their expression when bacteria were cultured under high osmolarity, a condition normally associated to the gut [14, 40], but also when bacteria were cultured under low Mg2+ concentrations or low pH (Figure 3), conditions found inside the macrophages [41, 42]. RpoS, PhoP, CRP and Fis may be important for the proper hlyE expression inside macrophages, since the RpoS and PhoP respective regulons are activated inside these cells; and both crp and fis expression is repressed in the same environment [41, 43]. Furthermore, hlyE induction by high osmolarity is RpoS dependent , reinforcing the fact that this sigma factor is an integrator of different signaling pathways. All this evidence together strongly suggests that HlyE is not circumscribed to a single stage of the infective process, as previously proposed . This work show that hlyE presents a complex regulation network involving different environmental signals and global regulators, presumably because this gene is actually participating in different stages of the S. Typhi infections process.
We studied the hlyE regulation in S. Typhi using genetic approaches. All our results together show that, at least under the tested conditions, RpoS is the most important up-regulator in the hlyE regulatory network. RpoS integrates multiple environmental signals and global regulators, including CRP, Fis, and PhoP signaling pathways, to control S. Typhi hlyE expression.
Bacterial strains, media and culture conditions
A clinical isolate of S. Typhi, named STH2370, was obtained from the Infectious Diseases Hospital Lucio Córdova in Santiago, Chile. S. Typhi STH2370 strain was grown to an optical density at 600 nm (OD600) of 1.4, and frozen as a primary stock. S. Typhi STH2370 and derivative strains were grown routinely in liquid culture in Luria-Bertani (LB) broth (Bacto tryptone, 10 g/liter; bacto yeast extract, 5 g/liter; NaCl, 5 g/liter) at 37°C, with aeration provided by shaking. When required, medium was supplemented with chloramphenicol (20 μg/ml), ampicillin (100 μg/ml), gentamicin (20 μg/ml) or glucose (0.4% w/v). LB medium was solidified by the addition of agar (15 g/l). The culture medium was modified in order to simulate the environmental conditions during S. Typhi infection process. To determine the effect of glucose in gene expression, bacteria were grown in LB buffered at pH 7.0 to an OD600 = 0.35, washed three times with PBS prior to be resuspended with LB buffered at pH 7.0 (control) or LB buffered at pH 7.0 + 0.4% w/v glucose. To determine the effect of low pH in gene expression, bacteria were grown in LB buffered at pH 7.0 to an OD600 = 0.35, washed three times with PBS prior to be resuspended with LB buffered at pH 7.0 (control) or LB buffered at pH 5.0 with buffer citrate. To determine the effect of low Mg2+ in gene expression, bacteria were grown in LB buffered at pH 7.0 to an OD600 = 0.35, washed three times with PBS prior to be resuspended with M9 10 mM Mg2+(control) or M9 10 μM Mg2+. In all the cases, bacteria were incubated 1 h at 37°C with shaking prior to isolate total RNA or total proteins of each strain. It is important to underline that all the strain tested are in logarithmic phase at OD600 = 0.35 when cultured in LB buffered at pH 7.0.
Construction of S. Typhi mutant strains
Primers used in this study
Primers used for the red/swap technique []
crp (H1 + P1)
crp (H2 + P2)
fis (H1 + P1)
fis (H2 + P2)
rpoS (H1 + P1)
rpoS (H2 + P2)
phoP (H1 + P1)
phoQ (H2 + P2)
Primers for epitope tagging (3xFLAG) 
Primers used for cloning
Primers for mRNA detection by RT-PCR
PCR amplifications for plasmid construction were performed using an Eppendorf thermal cycler and Taq (Fermentas) DNA polymerase. Reaction mixtures contained 1x PCR buffer, 1.5 mM MgCl2, each dNTP (200 mM), primers (1 mM), 100 ng of template DNA, and 2 U of Taq DNA polymerase. Standard conditions for amplification were 30 cycles at 96°C for 40 s, 60°C for 45 s, and 72°C for 2 min, followed by a final extension step at 72°C for 10 min. Template S. Typhi STH2370 chromosomal DNA was prepared as described . For complementing S. Typhi ΔrpoS or S. Typhi ΔphoPQ, we constructed the pBRPOS and pBPHOPQ plasmids by cloning the PCR product generated with RPOS-C + RPOS-NP or PHOPQ-C + PHOPQ-NP, respectively, into pBBR5. For complementing S. Typhi Δcrp or S. Typhi Δfis, we constructed the pTCRP and pTFIS plasmids by cloning the PCR product generated with CRP-C + CRP-NP or FIS-C + FIS-NP, respectively, into pCR TOPO 2.1 TA (Invitrogen) according to the manufacturer’s instructions. In all the cases, the cloned amplicons contained the ORF and the corresponding promoter region.
RNA isolation, reverse transcription and real-time quantitative PCR (RT-PCR)
Total mRNA from the strains grown under the tested conditions was extracted using TRIzol reagents (Invitrogen) as described by the manufacturer. RNA was precipitated with isopropanol for 10 min at room temperature, washed with ice cold 70% v/v ethanol and resuspended in DEPC-treated water prior to treatment with DNase I to remove any trace of DNA. Purity of extracted RNA was determined by spectrometry. Reverse transcription was performed on 2 μg of DNase-treated RNA using Superscript II RT (Invitrogen) at 50°C for 50 min followed by 70°C for 10 min in 20 μl with 2.5 mM of the corresponding reverse primer (RT-HLYE-C, RT-RPOS-C and RT-FIS-C for hlyE, rpoS and fis mRNA detection, respectively). The 16sRV reverse primer for 16 s mRNA by quantitative detection was used under each condition to normalize against a reference transcript. Relative quantification of each mRNA was performed using Brilliant II SYBR Green QPCR Master Reagent Kit and the Mx3000P detection system (Stratagene). The reaction mixture was carried out in a final volume of 20 μl containing 1 μl of diluted cDNA (1:1000), 0.24 μl of each primer (120 nM) (RT-HLYE-C + RT-HLYE-N for hlyE mRNA detection, RT-RPOS-C + RT-RPOS-N for rpoS mRNA detection, RT-FIS-C + RT-FIS-N for fis mRNA detection and 16sFW + 16sRV for 16 s mRNA detection), 10 μl of 10X Master Mix, 0.14 μl of diluted ROX (1:200) and 8.38 μl of nuclease-free H2O. The reaction was performed under the following conditions: 10 min at 95°C followed by 40 cycles of 30 s at 95°C, 30 s at 53°C and 45 s at 72°C. Finally a melting cycle from 53 to 95°C was performed to check for amplification specificity. Amplification efficiency was calculated from a standard curve constructed by amplifying serial dilutions of RT-PCR products for each gene. These values were used to obtain the fold change in expression for the gene of interest normalized with 16 s levels as previously described . Experiments were performed in three biological and technical replicates for each culture condition. When appropriate, the statistical significance of differences in the relative expression data was determined using the one way ANOVA test.
3xFLAG fusion proteins were immunodetected by the use of anti-FLAG M2 mAbs from Sigma. Strains carrying the epitope-tagged gene were grown under the conditions described above and washed twice with 100 mM Tris–HCl pH 8.0. Bacterial pellets were resuspended with 100 mM Tris–HCl and sonicated 60 s on ice. Then, the samples were mixed with 1 volume of Laemmli buffer . Suspensions were incubated at 98°C for 5 min. The resulting lysates were quickly centrifuged to remove cell debris and used, straight or suitably diluted, for SDS-PAGE. Twenty μg of bacterial proteins, previously quantified following the Bradford method , were resolved by SDS-PAGE and then transferred to poly (vinylidenedifluoride) membranes and probed with mAbs (1:1.000) and horseradish peroxidase-conjugated goat antimouse IgG [1:5.000 (Sigma)]. Detection was performed by enhanced chemioluminescence (ECL, Amersham Pharmacia).
Hemolytic activity quantification
S. Typhi and derivative strains were grown under the tested conditions, the OD600 was recorded, and the cultures were chilled to 4°C. Samples of each strain were washed twice with PBS, resuspended in 1 ml of PBS and then sonicated for 60 s on ice. This suspension was gently mixed with 1 volume of sheep erythrocytes (109 cells/ml) previously washed twice with PBS, and incubated 30 min at 37°C without shaking. To measure the hemolytic activity, samples were cleared by centrifugation and the OD545 was determined. Instead of the bacterial suspension, PBS or 5% sodium deoxycholate (DC) were used as reference hemolysis values for 0 and 100%, respectively. The arbitrary hemolytic units were calculated using the formula: (OD545Sample – OD545PBS)/(OD545DC – OD545PBS).
This work was supported by FONDECYT (Fondo Nacional de Desarrollo Científico y Tecnológico, Government of Chile) Grants 1110120 (GCM) and 11121506 (JAF) and UNAB-Grant DI-13-11/I (MRJ) and DI-222-12/N (JAF); MRJ is a MECESUP fellow program “Fortalecimiento del programa de Doctorado en Biociencias Moleculares” Grant UAB-0802. AAH is a FONDECYT Postdoctoral, fellow Grant 3130523.
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