Identification and characterization of PhoP regulon members in Yersinia pestis biovar Microtus
- Yingli Li†1,
- He Gao†1,
- Long Qin†1,
- Bei Li1,
- Yanping Han1,
- Zhaobiao Guo1,
- Yajun Song1,
- Junhui Zhai1,
- Zongmin Du1,
- Xiaoyi Wang1,
- Dongsheng Zhou1Email author and
- Ruifu Yang1Email author
© Li et al; licensee BioMed Central Ltd. 2008
Received: 21 December 2007
Accepted: 27 March 2008
Published: 27 March 2008
The transcription regulator PhoP has been shown to be important for Y. pestis survival in macrophages and under various in vitro stresses. However, the mechanism by which PhoP promotes bacterial intracellular survival is not fully understood. Our previous microarray analysis suggested that PhoP governed a wide set of cellular pathways in Y. pestis. A series of biochemical experiments were done herein to study members of the PhoP regulon of Y. pestis biovar Microtus.
By using gel mobility shift assay and quantitative RT-PCR, a total of 30 putative transcription units were characterized as direct PhoP targets. The primer extension assay was further used to determine the transcription start sites of 18 PhoP-dependent promoters and to localize the -10 and -35 elements. The DNase I footprinting was used to identify the PhoP-binding sites within 17 PhoP-dependent promoters, enabling the identification of PhoP box and matrix that both represented the conserved signals for PhoP recognition in Y. pestis. Data presented here providing a good basis for modeling PhoP-promoter DNA interactions that is crucial to the PhoP-mediated transcriptional regulation.
The proven direct PhoP targets include nine genes encoding regulators and 21 genes or operons with functions of detoxification, protection against DNA damages, resistance to antimicrobial peptides, and adaptation to magnesium limitation. We can presume that PhoP is a global regulator that controls a complex regulatory cascade by a mechanism of not only directly controlling the expression of specific genes, but also indirectly regulating various cellular pathways by acting on a set of dedicated regulators. These results help us gain insights into the PhoP-dependent mechanisms by which Y. pestis survives the antibacterial strategies employed by host macrophages.
Plague, caused by Yersinia pestis, is one of the most dangerous, infectious diseases in the world . Y. pestis has the ability of survival and growth within naïve macrophages both in vivo and in vitro [2, 3]. It has been shown that Y. pestis is a facultative intracellular parasite that resides and grows within host macrophages during the early stages of infection . Many virulence factors of Y. pestis have been tested for their ability to promote resistance to macrophage killing: pesticin, Pla, the pigmentation phenotype, and the plasmid pCD1-encoded type III secretion system, but they are all shown not to be required for bacterial survival in macrophages [2, 5–7]. Besides the two-component regulatory system PhoP-PhoQ  and the rip operon , the determinants which allow the pathogen's survival and growth in the macrophages are still poorly understood.
A low Mg2+ concentration is indicative of an intracellular environment as seen in macrophages, while a high Mg2+ concentration denotes extracellular fluids . PhoQ, an inner membrane-bound sensor-kinase, is inactive when bound with Mg2+; however, when the extracellular Mg2+ concentration drops, Mg2+ dissociates from PhoQ, leaving it activated. PhoQ then phosphorylates PhoP that either activates or represses transcription of specific target genes . As a transcription factor, PhoP controls its target genes through binding to their promoter DNA regions. A 17 bp PhoP box sequence, which consists of a direct repeat of the hexanucleotide consensus (T/G)GTTTA, has been shown to be the conservative signals of the PhoP-binding sites in Escherichia coli [12, 13]. This is essentially in agreement with the heptanucleotide consensus (T/G)GTTTA(A/T) sequence proposed in Salmonella enterica .
A phoP null mutant of Y. pestis shows a reduced ability to survive in macrophages and under in vitro conditions of low pH, oxidative stress, high osmolarity and antimicrobial peptides [8, 15]. The mean lethal dose of this phoP mutant in mice is increased 75-fold in comparison with that of the wild-type strain . In our previous work , cDNA microarray was used to determine the expression profile of a Y. pestis phoP null mutant grown under low Mg2+ conditions, enabling the genome-wide screening for PhoP-dependent genes in Y. pestis.
In the present work, a total of 30 transcription units were characterized as the direct targets of PhoP. It was shown that PhoP was a global regulator governing a complex regulatory cascade in Y. pestis. The subsequent determination of transcription start sites, -10/-35 elements, and PhoP-binding sites enabled the mapping of PhoP-DNA interactions, and helped to model the PhoP-mediated transcriptional regulation. Various genes of protective or adaptive functions, identified to be under the direct and positive control of PhoP, might contribute to Y. pestis's escape from the antibacterial strategies employed by host macrophages.
The wild-type (WT) strain 201 was isolated from Microtus brandti in the Inner Mongolia, China. It has an LD50 of less than 10 cells for mice by subcutaneous challenge. Strain 201 belongs to a newly established Y. pestis biovar Microtus, which is supposed to be avirulent to humans, although this biovar is highly lethal to mice . The phoP null mutant of Y. pestis  was generated by using the one-step inactivation method based on the lambda phage recombination with the helper plasmid pKD46 .
Bacterial growth and RNA isolation
Bacterial growth and RNA isolation were essentially the same as those described previously . A chemically defined TMH medium  was used for cultivating the bacteria. Both the WT strain and the phoP null mutant were pre-cultivated at 26°C in the TMH medium containing 20 mM MgCl2 to an OD620 of about 0.6. Bacteria were harvested, washed twice with the TMH medium containing 10 μM MgCl2, and then 1:20 diluted into the fresh 10 μM Mg2+ TMH medium. Both the strains were grown at 26°C until reaching the middle exponential growth phase (an OD620 of about 0.6) and then the cell cultures were transferred to 37°C for 1 h before harvest for RNA isolation.
Immediately before being harvested, bacterial cells were mixed with RNAprotect Bacteria Reagent (Qiagen) to minimize RNA degradation. Total RNA was isolated by using the TRIzol Reagent (Invitrogen). RNA quality was monitored by agarose gel electrophoresis and RNA quantity was measured by spectrophotometer.
Preparation of His-PhoP
The entire coding region of the phoP gene of strain 201 was cloned into plasmid pET28a (Novagen). The recombinant plasmids encoding a His-PhoP fusion protein were transformed into E. coli BL21 (DE3) cells (Novagen). Expression of His-PhoP was induced by addition of 1 mM isopropyl-beta-D-thiogalactoside. The recombinant protein was purified under native conditions with a QIAexpressionist™ Ni-NTA affinity chromatography (Qiagen). All steps in the isolation procedure were performed at 4°C. The purified, eluted protein was concentrated to a final concentration of about 1.0 mg ml-1 with the Amicon Ultra-15 (Millipore). The protein purity was verified by SDS-PAGE.
Preparation of polyclonal antibody against His-PhoP
The six-week-old New Zealand white rabbits were immunized with the His-PhoP protein (100 μg/rabbit) emulsified with the Freund's complete adjuvant through the subcutaneous route, followed by the boost immunization every two weeks for another three times with the mixture of PhoP/Freund's incomplete adjuvant. The specific antibody in the serum was monitored by indirect ELISA. The blood was collected by the carotid bleeding under callisection and the serum was separated for IgG purification by the method of saturated ammonium sulfate. The purity of the antibody was verified by SDS-PAGE and its quantity was measured by UV spectrometry.
Gel mobility shift assay (EMSA)
Primers (Additional file 1) were designed to amplify 400 to 500 bp region upstream of the start codon of each gene tested. EMSA was performed using the Gel Shift Assay Systems (Promega). The 5' ends of DNA were labeled using [γ-32P] ATP and T4 polynucleotide kinase. DNA binding was performed in a 10 μl reaction volume containing binding buffer [1 mM MgCl2, 0.5 mM EDTA, 0.5 mM DTT, 50 mM NaCl, 10 mM Tris-HCl (pH 7.5) and 0.05 mg/ml poly-(dI-dC)], labeled DNA (1000 to 2000 c.p.m/μl) and increasing amount of the His-PhoP protein. We included three controls in each EMSA experiment: i) specific DNA competitor (unlabeled promoter region of the same gene); ii) nonspecific DNA competitor [unlabeled promoter region of purK, one of the negative controls (see below)]; and iii) the supershift control (the antibody against His-PhoP was added for supershift by formation of DNA-PhoP-antibody complex). After incubation at room temperature for 30 min, the products were loaded onto a native 4% (w/v) polyacrylamide gel and electrophoresed in 0.5×TBE buffer for about 30 min at 220 V. Radioactive species were detected by autoradiography after exposure to Kodak film at -70°C.
Real-time quantitative RT-PCR
Gene-specific primers (Additional file 1) were designed to produce a 150 to 200 bp amplicon for each gene. The contaminated DNA was removed from each 5 to 10 μg of total RNA by using the Ambion's DNA-free™ Kit. cDNA was generated by using 5 μg of total RNA and 3 μg of random hexamer primers. Real-time PCR was performed in triplicate using independent cultures and RNA preparations through the LightCycler system (Roche) together with the SYBR Green master mix, and with 1:25 dilution of cDNA as templates. To ensure that there was no contamination of genomic DNA, negative controls were performed by using 'cDNA' generated without reverse transcriptase as templates. Reactions containing primer pairs without template were also included as blank controls. 16S rRNA was used as an internal control for each RNA preparation. On the basis of the standard curves of 16S rRNA expression, the relative mRNA level was determined by calculating the threshold cycle (ΔCt) of each gene by the classic ΔCt method . The RT-PCR data of 16S rRNA gene was used to normalize that of all the other genes. The transcriptional variation of the WT strain and the phoP null mutant for each gene was then calculated. A mean ratio of two was taken as the cutoff of statistical significance.
An oligonucleotide primer (Additional file 1) was designed to be complementary to the RNA transcript of each gene from a suitable position (generally 80 to 150 bp downstream of the translation start site). Primer extension assay was performed using the Primer Extension System-AMV Reverse Transcriptase kit (Promega). The extension primers were end-labeled with [γ-32P] ATP. Three nanograms of each end-labeled primer were annealed with 10 to 30 μg of total RNA and extended according to the manufacturer's protocol. The same labeled primer was also used for sequencing with the fmol® DNA Cycle Sequencing System (Promega). The products were concentrated and subjected to electrophoresis in a 6% polyacrylamide/8 M urea gel. The result was detected by autoradiography (Kodak film).
DNase I footprinting
To obtain each promoter DNA fragment with a single 32P-labeled end, PCR amplification was performed with the promoter-specific primer pairs (see Additional file 1), in which either the sense or the antisense primer was end-labeled. The PCR products were purified by using MinElute reaction cleanup columns (Qiagen). Increasing amount of His-PhoP was incubated with the labeled DNA fragment (2 to 5 pmol) for 30 min at room temperature in a final volume of 10 μl containing binding buffer same as EMSA. Before DNA digestion, 10 μl of Ca2+/Mg2+ solution (5 mM CaCl2 and 10 mM MgCl2) was added, followed by incubation for 1 min at room temperature. Then, the optimized RQ1 RNase-Free DNase I (Promega) was added to the reaction mixture, and the mixture was incubated at room temperature for 50 to 90s. The reaction was quenched by adding 9 μl of the stop solution (200 mM NaCl, 30 mM EDTA and 1% SDS) for 1 min at room temperature. The partially digested DNA samples were extracted with phenol/chloroform, precipitated with ethanol, and analyzed in a 6% polyacrylamide/8M urea gel. Protected regions were identified by comparison with the sequence ladders. For sequencing, the fmol® DNA Cycle Sequencing System (Promega) was used. The results were detected as described above.
Computational promoter analysis
The 500 bp region upstream of the start codon of each gene tested was retrieved with the retrieve-seq tool . By using the FUZZNUC program , the E. coli PhoP box was matched within the PhoP sites as determined by DNase I footprinting. Homologues of the PhoP box identified from the PhoP sites were then collected and displayed by the WebLogo program  to generate a sequence logo; additionally, the position count matrixes were built from them by using the consensus-matrix and convert-matrix tools .
Direct targets of PhoP
The comparison of mRNA profile of the WT Y. pestis with that of the phoP null mutant under the Mg2+-limiting condition  identified an array of 706 PhoP-dependent genes. This analysis had the difficulty in distinguishing between direct targets and indirect ones of PhoP. In the present study, the following genes (87 genes in total) were picked out from the above 706 ones for EMSA: i) those responsible for stress-adaptive or regulatory function; and ii) those with a homologue of E. coli PhoP box sequence in their promoter-proximal regions (with a cutoff of 2 bp mismatch). The EMSA was conducted to test the binding of His-PhoP to the 400 to 500 bp region upstream of the translation start site for each gene. Accordingly, a total of 30 transcription units gave the stable, positive results of EMSA (Table 2 and Additional file 3). To ensure the specificity of EMSA, two additional genes (purK and atpG) were included as negative controls. For selection of them as negative controls, the patser-matrix tool  was employed to match the PhoP matrix (see below) within their promoter regions, and both of them gave a very low value of weight score (a greater number of this score corresponds to a higher probability of presence of a PhoP-binding site).
1 The gene IDs were derived from the genome annotation of Y. pestis CO92. Putative transcription units (30 in total) were boxed, and the vertical arrows indicated the transcriptional organization.
2 The mRNA expression in the phoP null mutant was compared with that in the WT strain grown under low Mg2+ condition.
3 The data were present as the mean change of mRNA level for each gene under the paired growth conditions. The positive number stood for fold increased, while minus decreased.
4 There was the discrepancy between the data determined by RT-PCR and microarray (a total of three genes); the subsequent primer extension assay verified the rationality of the RT-PCR results.
5'ND' indicated 'not done'.
The microarray analysis was able to semi-quantitatively identify genes under either positive or negative control by PhoP. However, microarray results are influenced by various factors, and thereby should be validated by at least one traditional method . Accordingly, the real-time quantitative RT-PCR, using the same RNA preparations as the microarray analysis, was performed to validate the microarray data in Additional file 2. Except for three genes (metJ, fruR and astC), RT-PCR and microarray data showed a good agreement. Since RT-PCR and microarray gave the contradictory results for the above three genes, the further primer extension assay (Additional file 4) was conducted by using the same RNA preparations, which showed the creditability of the RT-PCR data (Additional file 2 and Additional file 5). Thereby, the positive or negative regulation of each selected gene by the PhoP was elucidated as shown in Additional file 2.
Taken together, we identified a total of 30 transcription units whose transcription was PhoP-dependent in response to Mg2+ limitation, and these units should be the direct PhoP targets.
Transcription start sites of direct PhoP targets
In addition to the above three genes (metJ, fruR and astC), we still performed the primer extension assay on another 15 genes (Additional file 4). These genes encoded either stress-adaptive or regulatory functions. A single primer extension product was detected for 12 of them. Two or more primer extension products were detected for katA, uspB, pmrE, oppA,phoP and slyA. Since the shorter extension products might represent the premature stops due to difficulties of polymerase in passing difficult sequences, only the longest product was chosen for the identification of each gene's transcription start site.
Accordingly, a transcription start site was identified for each of the above 18 genes, indicating a PhoP-dependent promoter was transcribed for each of them. The nucleotide number of each transcription start site was taken as '+1', and accordingly the promoter -10 and -35 elements for RNA polymerase(RNAP) recognition were predicted (see below).
The PhoP-binding sites
To precisely determine the PhoP-binding sites of target genes, DNase I footprinting assay was performed on 17 PhoP-dependent promoter DNA regions (both coding and noncoding strands) (Additional file 6). DNase I footprinting results confirmed the direct binding of His-PhoP to these promoter regions in vitro. For each DNA fragment tested, His-PhoP protected at least one distinct region against DNase I digestion in a dose-dependent pattern. The size of footprint ranged from 25 to 62 bases with an average of 35 bases. These footprint regions were considered as the PhoP-binding sites. Interestingly, the phoP promoter region had two separated PhoP binding sites, while sodB had three (Additional file 6). Additionally, the uspA and uspB genes shared a single PhoP binding site (see below). In total, 19 PhoP-binding sites were detected for the 17 PhoP-regulated genes analyzed.
The His tag fused in the recombinant PhoP protein is positively charged, while DNA probe in the footprinting experiments is negatively charged. One may argue that there would be the possibility of nonspecific binding between His tag and DNA probe. Accordingly, the PCR-generated upstream DNA fragments of two genes sodC and oppA were employed as negative controls (Additional file 7). The DNA probes used here did not harbor the predicted PhoP box, compared with the corresponding ones in Additional file 6. No His-PhoP protected region was detected for the DNA probes tested, indicating the specificity of DNase I footprinting experiments.
The PhoP regulatory motif in Y. pestis
Organization of PhoP-dependent promoters
PhoP-dependent genes and direct PhoP targets
Experiments of lacZ reporter fusion in S. typhimurium [26, 27] and E. coli  have shown that the PhoP regulatory protein affects more than 40 different genes, termed PhoP-activated and PhoP-repressed genes. By comparison of gene expression profiles between a wild-type strain and the isogenic mutant of phoP grown under low Mg2+ conditions, cDNA microarray enables the genome-wide identification of PhoP-dependent genes in both E. coli [12, 29] and S. typhimurium . The lacZ fusion experiments can demonstrate whether the promoter activity of an upstream DNA fragment is dependent on PhoP, while microarray analysis can screen for genes whose transcription is affected by the mutation of phoP gene. Both of them cannot answer whether a gene is a direct or indirect target of PhoP.
Protein-DNA binding experiments, including EMSA, DNase I footprinting and chromatin immunoprecipitation, can be used to detect the direct target genes of PhoP. Accordingly, at least 22 transcription units have been proven to be the direct PhoP targets in S. typhimurium and/or E. coli (summarized in Additional file 8). In the present work, we identify a total of 30 transcription units under the direct control of PhoP in Y. pestis by using EMSA, DNase I footprinting, real-time RT-PCR and primer extension. Only three analogues (slyA , phoP [12, 14] and mgtCB ) of them have been previously reported in S. typhimurium and/or E. coli. In addition, DNase I footprinting has demonstrated the binding of the Salmonella PhoP protein to the upstream DNA fragments of the Y. pestis pmrF and pmrE operons , which was confirmed in this study by using the Y. pestis PhoP protein. Thus, the present study disclosed 25 'novel' direct targets of PhoP, which encoded a wide range of functions including oxidative defense, universal stress response, synthesis and modification of LPS, oligopeptide transport, peptidoglycan remodeling, regulators, and various/unknown functions (Additional file 2).
The Mg2+-responsive PhoP is a global transcriptional regulator in Y. pestis
Genomic transcriptional profiling of the phoP null mutant of Y. pestis in response to low Mg2+ stimulus revealed at least 706 PhoP-dependent genes, representing approximately 16% of the total protein-coding capacity of the Y. pestis genome . These genes are distributed among almost all the functional classes according to the genome annotation of Y. pestis CO92 (see Additional file 9). In our present work, the detected 30 direct PhoP targets including nine genes (YPO0010, YPO0414, YPO0736, YPO1279,metJ, fruR, lacI, phoP and slyA) that encode broad regulatory functions (Additional file 2).
The general features of Y. pestis PhoP can be summarized as follows: i) it regulates a large number of genes that belong to a wide set of functional classes; ii) it not only directly controls the expression of specific genes, but also indirectly regulates various cellular pathways by acting on a set of local regulators; and iii) it functions as either an activator or a repressor depending on the target promoters. A conclusion could be postulated that the Mg2+-responsive PhoP is a global transcriptional regulator that governs a complex of regulatory cascades in Y. pestis.
PhoP-promoter DNA interactions for transcriptional regulation
As shown above, Y. pestis PhoP binds to DNA regions at various positions from the RNA polymerase-binding site (-10 and -35 elements), i.e., upstream, overlapping or downstream of the promoter -35 elements (Figure 2). Thus, the PhoP-dependent promoters identified herein could be grouped into the following three categories: i) Class I promoters, which can be found in the mgtC, katA, sodB(Site1), uspB, uspA, pagP, oppA, YPO0010 and phoP promoters, contain PhoP-binding sites upstream of the promoter -35 element. Class I PhoP-dependent promoters may have a class I regulation that depends on the RNA polymerase α subunit C-terminal domain (αCTD) for function ; ii) Class II promoters containing PhoP-binding sites overlapping the DNA binding site of RNAP are found in the ahpC, sodA, sodB(Site2),pmrE and pmrH promoters. There may be a class II regulation for these promoters, which requires the RNA polymerase σ subunit C-terminal domain (σCTD) or the α-subunit surface for function; and iii) Class III promoters, downstream of the DNA binding site of RNAP, are seen in the sodB(Site3), sodC, metJ, fruR and slyA promoters. Although unusual, this kind of promoter have been found in Salmonella, where SlyA binds downstream of the transcription start sites of ugtL and slyA [31, 35].
Two PhoP-binding sites, site 1 and site 2, were identified within the phoP promoter (Additional file 6). Fifteen pmol of PhoP gave a complete protection on the site 1, while for the site 2, 25 pmol of PhoP still showed an incomplete protection (Additional file 6). It has been proposed that the doses of DNA-binding transcription factor required for the transcriptional activation of its target genes are related to their binding affinity . Accordingly, the PhoP's affinity to site 1 was stronger than that to site 2. Both site 1 and site 2 are located upstream of the -35 element.
We defined the PhoP sites within a collection of 17 PhoP-dependent promoters in Y. pestis. A relatively larger collection of PhoP-binding sites here promoted us to perform the sequence alignment, leading to the identification of a PhoP box (very similar to those in E. coli and S. enterica) as well as the position count matrix (Figure 1). All of them represent the conserved signals for PhoP recognition in Y. pestis. The box is a contiguous oligonucleotide, and thus it can not show much of the information originally presented in these PhoP sites. Representation of consensus patterns with the position count matrix is able to give a full description of the uneven composition in each position, i.e., some nucleotides occurred much more frequently than others. Thus, the matrixes presented here will over-represent the PhoP-recognized DNA binding sites in Y. pestis more accurately than the classic 18 bp box sequence.
The determination of PhoP regulatory motifs in Y. pestis promoted us to identify additional genes potentially under the direct control of the PhoP. Briefly, the 500 bp fragment upstream of each PhoP-dependent gene determined by cDNA microarray was scanned with the position count matrix in Figure 1(c) by using the patser-matrix tool . This analysis generated a weight score for each promoter DNA. A greater value of this score corresponds to a higher probability of presence of a PhoP-binding site. When seven was taken as the cutoff value, a total of 88 genes or possible operons, which could be assigned into nine functional categories, were picked out as the potential direct PhoP targets (see Additional file 10). Searching the upstream regions of genes for the PhoP consensus sequences can help us identify the candidate targets regulated directly by the PhoP. However, the mere presence of a PhoP consensus does not necessarily mean that the PhoP must bind and regulate the target. Either EMSA or DNase I footprinting is required to determine whether it is a functional target for PhoP-specific binding.
PhoP-regulated functions likely contribute to intracellular growth of Y. pestis
Y. pestis is considered as a facultative intracellular pathogen that is capable of surviving and growing within macrophages during its early stage of infection. When Y. pestis cells are phagocytosed by a macrophage, they are usually found in a vacuole, the phagolysosome . The phagolysosome has evolved an array of mechanisms to kill or inhibit the evading bacteria, including the activated oxygen species, an acidic pH as low as 4.0, the abundant antimicrobial peptides, and the limited availability of Mg2+.
Disruption of the phoP gene renders Y. pestis more sensitive to low pH, oxidative stress and antimicrobial peptides that are found to be killing mechanisms for invading pathogen by macrophage [8, 15]. When the phoP gene of Y. pestis strain 201 used in this study was disrupted using a lambda Red recombination system , similar phenotypes of this phoP null mutant were also observed (data not shown).
Herein, a combined use of microarray, EMSA, RT-PCR, primer extension, and DNase I footprinting demonstrated that the PhoP could directly mediate the transcriptional activation of transcription units encoding functions that are protective against or adaptive to the killing mechanisms used by host macrophages: i) five genes (sodA, sodB, sodC,katA, and ahpC) encoding detoxification enzymes for scavenging oxidative stress; ii) two (uspA and uspB) playing roles in protection against DNA damage ; iii) three (pmrHFIJKLM, pmrE and pagP) for LPS modification enzymes that play key roles in the bacterial resistance to antimicrobial peptides; and iv) mgtCB encoding a major Mg2+ transport system. In particular, the later two groups of genes has been shown to be regulated by the PhoP and required for the intra-macrophage survival of S. typhimurium, a classic facultative intracellular pathogen [11, 40]. In addition, it has been reported that the pmrE and the mgtC function independently to promote early survival of Y. pestis in the macrophage phagosomes .
The above data lead us to an assumption that, in Y. pestis, the PhoP responds to the low Mg2+ signal in host macrophages and mediates the transcriptional activation of various protective or adaptive functions. These functions, together, most likely make Y. pestis escape from macrophage-induced killing mechanisms. Further biochemical and phenotypic investigations on these candidate genes should be implemented to validate this hypothesis.
A total of 30 transcription units (single-genes or putative operons) were characterized as direct PhoP targets in the present work, of which 25 appeared to be disclosed for the first time. In particular, 11 of them encoded various protective or adaptive functions (Mg2+ transport, oxidative defense, universal stress response, and synthesis and modification of LPS), and they were positively controlled by PhoP, providing an array of candidate genes for future investigation on their contribution to the intracellular survival of Y. pestis in host macrophages. Additional nine of them encoded broad regulatory functions. Accordingly, the Mg2+-responsive PhoP could be proposed as a global regulator that governs a complex of regulatory cascade in Y. pestis.
Transcription start sites, promoter -10/-35 elements, and PhoP-binding sites were dissected within the upstream DNA regions of 17 PhoP-dependent genes or operons, providing a good basis for mapping PhoP-promoter DNA interactions and for modeling PhoP-mediated transcriptional regulation. Alignment of the detecting PhoP sites generated the PhoP regulatory motif of Y. pestis, in formats of both a continuous oligonucleotide (PhoP box) and the position count matrix, which would be useful for computational searching of additional, potential PhoP targets, even within the whole genome. Biovar Microtus strain 201 used in this study is highly lethal to mice, but avirulent to humans. Results obtained from this biovar should have their relevance for human-pathogenic strains. However, remodeling of regulatory cascades/networks likely contributes to the phenotypic divergences of difference biovars [17, 42]. Further attempts should be conducted to investigate the differences or similarities between human-virulent and -avirulent Y. pestis isolates concerning PhoP-mediated regulation.
Financial supports for this work came from the National Natural Science Foundation of China (No. 30600353) and the National Natural Science Foundation of China for Distinguished Young Scholars (No. 30525025).
- Perry RD, Fetherston JD: Yersinia pestis--etiologic agent of plague. Clin Microbiol Rev. 1997, 10 (1): 35-66.PubMedPubMed CentralGoogle Scholar
- Pujol C, Bliska JB: The ability to replicate in macrophages is conserved between Yersinia pestis and Yersinia pseudotuberculosis. Infect Immun. 2003, 71 (10): 5892-5899. 10.1128/IAI.71.10.5892-5899.2003.PubMedPubMed CentralView ArticleGoogle Scholar
- Pujol C, Bliska JB: Turning Yersinia pathogenesis outside in: subversion of macrophage function by intracellular yersiniae. Clin Immunol. 2005, 114 (3): 216-226. 10.1016/j.clim.2004.07.013.PubMedView ArticleGoogle Scholar
- Lukaszewski RA, Kenny DJ, Taylor R, Rees DG, Hartley MG, Oyston PC: Pathogenesis of Yersinia pestis infection in BALB/c mice: effects on host macrophages and neutrophils. Infect Immun. 2005, 73 (11): 7142-7150. 10.1128/IAI.73.11.7142-7150.2005.PubMedPubMed CentralView ArticleGoogle Scholar
- Straley SC, Harmon PA: Growth in mouse peritoneal macrophages of Yersinia pestis lacking established virulence determinants. Infect Immun. 1984, 45 (3): 649-654.PubMedPubMed CentralGoogle Scholar
- Cornelis GR, Boland A, Boyd AP, Geuijen C, Iriarte M, Neyt C, Sory MP, Stainier I: The virulence plasmid of Yersinia, an antihost genome. Microbiol Mol Biol Rev. 1998, 62 (4): 1315-1352.PubMedPubMed CentralGoogle Scholar
- Charnetzky WT, Shuford WW: Survival and growth of Yersinia pestis within macrophages and an effect of the loss of the 47-megadalton plasmid on growth in macrophages. Infect Immun. 1985, 47 (1): 234-241.PubMedPubMed CentralGoogle Scholar
- Oyston PC, Dorrell N, Williams K, Li SR, Green M, Titball RW, Wren BW: The response regulator PhoP is important for survival under conditions of macrophage-induced stress and virulence in Yersinia pestis. Infect Immun. 2000, 68 (6): 3419-3425. 10.1128/IAI.68.6.3419-3425.2000.PubMedPubMed CentralView ArticleGoogle Scholar
- Pujol C, Grabenstein JP, Perry RD, Bliska JB: Replication of Yersinia pestis in interferon gamma-activated macrophages requires ripA, a gene encoded in the pigmentation locus. Proc Natl Acad Sci U S A. 2005, 102 (36): 12909-12914. 10.1073/pnas.0502849102.PubMedPubMed CentralView ArticleGoogle Scholar
- Groisman EA: The ins and outs of virulence gene expression: Mg2+ as a regulatory signal. Bioessays. 1998, 20 (1): 96-101. 10.1002/(SICI)1521-1878(199801)20:1<96::AID-BIES13>3.0.CO;2-3.PubMedView ArticleGoogle Scholar
- Groisman EA: The pleiotropic two-component regulatory system PhoP-PhoQ. J Bacteriol. 2001, 183 (6): 1835-1842. 10.1128/JB.183.6.1835-1842.2001.PubMedPubMed CentralView ArticleGoogle Scholar
- Minagawa S, Ogasawara H, Kato A, Yamamoto K, Eguchi Y, Oshima T, Mori H, Ishihama A, Utsumi R: Identification and molecular characterization of the Mg2+ stimulon of Escherichia coli. J Bacteriol. 2003, 185 (13): 3696-3702. 10.1128/JB.185.13.3696-3702.2003.PubMedPubMed CentralView ArticleGoogle Scholar
- Yamamoto K, Ogasawara H, Fujita N, Utsumi R, Ishihama A: Novel mode of transcription regulation of divergently overlapping promoters by PhoP, the regulator of two-component system sensing external magnesium availability. Mol Microbiol. 2002, 45 (2): 423-438. 10.1046/j.1365-2958.2002.03017.x.PubMedView ArticleGoogle Scholar
- Lejona S, Aguirre A, Cabeza ML, Garcia Vescovi E, Soncini FC: Molecular characterization of the Mg2+-responsive PhoP-PhoQ regulon in Salmonella enterica. J Bacteriol. 2003, 185 (21): 6287-6294. 10.1128/JB.185.21.6287-6294.2003.PubMedPubMed CentralView ArticleGoogle Scholar
- Hitchen PG, Prior JL, Oyston PC, Panico M, Wren BW, Titball RW, Morris HR, Dell A: Structural characterization of lipo-oligosaccharide (LOS) from Yersinia pestis: regulation of LOS structure by the PhoPQ system. Mol Microbiol. 2002, 44 (6): 1637-1650. 10.1046/j.1365-2958.2002.02990.x.PubMedView ArticleGoogle Scholar
- Zhou D, Han Y, Qin L, Chen Z, Qiu J, Song Y, Li B, Wang J, Guo Z, Du Z, Wang X, Yang R: Transcriptome analysis of the Mg2+-responsive PhoP regulator in Yersinia pestis. FEMS Microbiol Lett. 2005, 250 (1): 85-95. 10.1016/j.femsle.2005.06.053.PubMedView ArticleGoogle Scholar
- Zhou D, Tong Z, Song Y, Han Y, Pei D, Pang X, Zhai J, Li M, Cui B, Qi Z, Jin L, Dai R, Du Z, Wang J, Guo Z, Huang P, Yang R: Genetics of metabolic variations between Yersinia pestis biovars and the proposal of a new biovar, microtus. J Bacteriol. 2004, 186 (15): 5147-5152. 10.1128/JB.186.15.5147-5152.2004.PubMedPubMed CentralView ArticleGoogle Scholar
- Datsenko KA, Wanner BL: One-step inactivation of chromosomal genes in Escherichia coli K-12 using PCR products. Proc Natl Acad Sci U S A. 2000, 97 (12): 6640-6645. 10.1073/pnas.120163297.PubMedPubMed CentralView ArticleGoogle Scholar
- Straley SC, Bowmer WS: Virulence genes regulated at the transcriptional level by Ca2+ in Yersinia pestis include structural genes for outer membrane proteins. Infect Immun. 1986, 51 (2): 445-454.PubMedPubMed CentralGoogle Scholar
- Huggett J, Dheda K, Bustin S, Zumla A: Real-time RT-PCR normalisation; strategies and considerations. Genes Immun. 2005, 6 (4): 279-284. 10.1038/sj.gene.6364190.PubMedView ArticleGoogle Scholar
- van Helden J: Regulatory sequence analysis tools. Nucleic Acids Res. 2003, 31 (13): 3593-3596. 10.1093/nar/gkg567.PubMedPubMed CentralView ArticleGoogle Scholar
- Olson SA: EMBOSS opens up sequence analysis. European Molecular Biology Open Software Suite. Brief Bioinform. 2002, 3 (1): 87-91. 10.1093/bib/3.1.87.PubMedView ArticleGoogle Scholar
- Crooks GE, Hon G, Chandonia JM, Brenner SE: WebLogo: a sequence logo generator. Genome Res. 2004, 14 (6): 1188-1190. 10.1101/gr.849004.PubMedPubMed CentralView ArticleGoogle Scholar
- Zhou D, Yang R: Global analysis of gene transcription regulation in prokaryotes. Cell Mol Life Sci. 2006, 63 (19-20): 2260-2290. 10.1007/s00018-006-6184-6.PubMedView ArticleGoogle Scholar
- Parkhill J, Dougan G, James KD, Thomson NR, Pickard D, Wain J, Churcher C, Mungall KL, Bentley SD, Holden MT, Sebaihia M, Baker S, Basham D, Brooks K, Chillingworth T, Connerton P, Cronin A, Davis P, Davies RM, Dowd L, White N, Farrar J, Feltwell T, Hamlin N, Haque A, Hien TT, Holroyd S, Jagels K, Krogh A, Larsen TS, Leather S, Moule S, O'Gaora P, Parry C, Quail M, Rutherford K, Simmonds M, Skelton J, Stevens K, Whitehead S, Barrell BG: Complete genome sequence of a multiple drug resistant Salmonella enterica serovar Typhi CT18. Nature. 2001, 413 (6858): 848-852. 10.1038/35101607.PubMedView ArticleGoogle Scholar
- Soncini FC, Garcia Vescovi E, Solomon F, Groisman EA: Molecular basis of the magnesium deprivation response in Salmonella typhimurium: identification of PhoP-regulated genes. J Bacteriol. 1996, 178 (17): 5092-5099.PubMedPubMed CentralGoogle Scholar
- Belden WJ, Miller SI: Further characterization of the PhoP regulon: identification of new PhoP-activated virulence loci. Infect Immun. 1994, 62 (11): 5095-5101.PubMedPubMed CentralGoogle Scholar
- Kato A, Tanabe H, Utsumi R: Molecular characterization of the PhoP-PhoQ two-component system in Escherichia coli K-12: identification of extracellular Mg2+-responsive promoters. J Bacteriol. 1999, 181 (17): 5516-5520.PubMedPubMed CentralGoogle Scholar
- Oshima T, Aiba H, Masuda Y, Kanaya S, Sugiura M, Wanner BL, Mori H, Mizuno T: Transcriptome analysis of all two-component regulatory system mutants of Escherichia coli K-12. Mol Microbiol. 2002, 46 (1): 281-291. 10.1046/j.1365-2958.2002.03170.x.PubMedView ArticleGoogle Scholar
- Monsieurs P, De Keersmaecker S, Navarre WW, Bader MW, De Smet F, McClelland M, Fang FC, De Moor B, Vanderleyden J, Marchal K: Comparison of the PhoPQ regulon in Escherichia coli and Salmonella typhimurium. J Mol Evol. 2005, 60 (4): 462-474. 10.1007/s00239-004-0212-7.PubMedView ArticleGoogle Scholar
- Shi Y, Latifi T, Cromie MJ, Groisman EA: Transcriptional control of the antimicrobial peptide resistance ugtL gene by the Salmonella PhoP and SlyA regulatory proteins. J Biol Chem. 2004, 279 (37): 38618-38625. 10.1074/jbc.M406149200.PubMedView ArticleGoogle Scholar
- Winfield MD, Latifi T, Groisman EA: Transcriptional regulation of the 4-amino-4-deoxy-L-arabinose biosynthetic genes in Yersinia pestis. J Biol Chem. 2005, 280 (15): 14765-14772. 10.1074/jbc.M413900200.PubMedView ArticleGoogle Scholar
- Ishihama A: Functional modulation of Escherichia coli RNA polymerase. Annu Rev Microbiol. 2000, 54: 499-518. 10.1146/annurev.micro.54.1.499.PubMedView ArticleGoogle Scholar
- Niu W, Kim Y, Tau G, Heyduk T, Ebright RH: Transcription activation at class II CAP-dependent promoters: two interactions between CAP and RNA polymerase. Cell. 1996, 87 (6): 1123-1134. 10.1016/S0092-8674(00)81806-1.PubMedPubMed CentralView ArticleGoogle Scholar
- Norte VA, Stapleton MR, Green J: PhoP-responsive expression of the Salmonella enterica serovar typhimurium slyA gene. J Bacteriol. 2003, 185 (12): 3508-3514. 10.1128/JB.185.12.3508-3514.2003.PubMedPubMed CentralView ArticleGoogle Scholar
- Zwir I, Shin D, Kato A, Nishino K, Latifi T, Solomon F, Hare JM, Huang H, Groisman EA: Dissecting the PhoP regulatory network of Escherichia coli and Salmonella enterica. Proc Natl Acad Sci U S A. 2005, 102 (8): 2862-2867. 10.1073/pnas.0408238102.PubMedPubMed CentralView ArticleGoogle Scholar
- Fujita M, Gonzalez-Pastor JE, Losick R: High- and low-threshold genes in the Spo0A regulon of Bacillus subtilis. J Bacteriol. 2005, 187 (4): 1357-1368. 10.1128/JB.187.4.1357-1368.2005.PubMedPubMed CentralView ArticleGoogle Scholar
- Straley SC, Harmon PA: Yersinia pestis grows within phagolysosomes in mouse peritoneal macrophages. Infect Immun. 1984, 45 (3): 655-659.PubMedPubMed CentralGoogle Scholar
- Kvint K, Nachin L, Diez A, Nystrom T: The bacterial universal stress protein: function and regulation. Curr Opin Microbiol. 2003, 6 (2): 140-145. 10.1016/S1369-5274(03)00025-0.PubMedView ArticleGoogle Scholar
- Groisman EA, Mouslim C: Sensing by bacterial regulatory systems in host and non-host environments. Nat Rev Microbiol. 2006, 4 (9): 705-709. 10.1038/nrmicro1478.PubMedView ArticleGoogle Scholar
- Grabenstein JP, Fukuto HS, Palmer LE, Bliska JB: Characterization of phagosome trafficking and identification of PhoP-regulated genes important for survival of Yersinia pestis in macrophages. Infect Immun. 2006, 74 (7): 3727-3741. 10.1128/IAI.00255-06.PubMedPubMed CentralView ArticleGoogle Scholar
- Achtman M, Morelli G, Zhu P, Wirth T, Diehl I, Kusecek B, Vogler AJ, Wagner DM, Allender CJ, Easterday WR, Chenal-Francisque V, Worsham P, Thomson NR, Parkhill J, Lindler LE, Carniel E, Keim P: Microevolution and history of the plague bacillus, Yersinia pestis. Proc Natl Acad Sci U S A. 2004, 101 (51): 17837-17842. 10.1073/pnas.0408026101.PubMedPubMed CentralView ArticleGoogle Scholar
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