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Perturbation of the two-component signal transduction system, BprRS, results in attenuated virulence and motility defects in Burkholderia pseudomallei

BMC Genomics volume 17, Article number: 331 (2016) Cite this article

Abstract

Background

Burkholderia pseudomallei is the causative agent of melioidosis, a severe invasive disease of humans and animals. Initial screening of a B. pseudomallei signature-tagged mutagenesis library identified an attenuated mutant with a transposon insertion in a gene encoding the sensor component of an uncharacterised two-component signal transduction system (TCSTS), which we designated BprRS.

Results

Single gene inactivation of either the response regulator gene (bprR) or the sensor histidine kinase gene (bprS) resulted in mutants with reduced swarming motility and reduced virulence in mice. However, a bprRS double mutant was not attenuated for virulence and displayed wild-type levels of motility. The transcriptomes of the bprS, bprR and bprRS mutants were compared with the transcriptome of the parent strain K96243. Inactivation of the entire BprRS TCSTS (bprRS double mutant) resulted in altered expression of only nine genes, including both bprR and bprS, five phage-related genes and bpss0686, encoding a putative 5, 10-methylene tetrahydromethanopterin reductase involved in one carbon metabolism. In contrast, the transcriptomes of each of the bprR and bprS single gene mutants revealed more than 70 differentially expressed genes common to both mutants, including regulatory genes and those required for flagella assembly and for the biosynthesis of the cytotoxic polyketide, malleilactone.

Conclusions

Inactivation of the entire BprRS TCSTS did not alter virulence or motility and very few genes were differentially expressed indicating that the definitive BprRS regulon is relatively small. However, loss of a single component, either the sensor histidine kinase BprS or its cognate response regulator BprR, resulted in significant transcriptomic and phenotypic differences from the wild-type strain. We hypothesize that the dramatically altered phenotypes of these single mutants are the result of cross-regulation with one or more other TCSTSs and concomitant dysregulation of other key regulatory genes.

Background

Burkholderia pseudomallei is a highly pathogenic Gram-negative organism and the causative agent of melioidosis, a potentially fatal infectious disease of humans and animals. The bacterium is endemic to tropical regions including South East Asia and Northern Australia; mortality rates resulting from melioidosis remain extremely high, with up to 42 % mortality in the Northeastern region of Thailand and 14 % mortality in Australia’s Northern Territory [1, 2]. Importantly, a 90 % mortality rate is associated with septic shock [3]. In Northern Australia, melioidosis accounts for 32 % of community-acquired bacteraemic pneumonia and 6 % of all bacteraemias [4], while in the Northeastern region of Thailand, the disease accounts for 20 % of all community-acquired septicaemias [5] and is the third most common cause of death from an infectious disease [2]. The complex clinical spectrum of melioidosis, the potentially rapid progression of disease and the fact that B. pseudomallei is innately resistant to a wide range of antimicrobial agents [6–8] makes treatment of this disease difficult.

For B. pseudomallei and most other opportunistic pathogens, the ability to sense external signals is critical for the transition from their environmental niche into the eukaryotic host, as well as for survival within specific niches within the host. Prokaryotic two-component signal transduction systems (TCSTS) constitute a critical set of regulators which act to sense environmental signals and respond by altering gene expression [9–11]. TCSTS generally consist of a membrane-bound sensor kinase (SK) and a cytosolic DNA-binding response regulator (RR) [11]. The SK protein senses extracellular stimuli and responds through the autophosphorylation of a specific histidine residue. This phosphoryl group is then transferred to an aspartate residue on the cytoplasmic RR leading to a conformational change that activates the RR, resulting in the altered expression of a specific set of genes [12]. TCSTS components are promising drug targets as these systems are not present in mammalian cells and inhibitors that target TCSTSs are likely to function in a manner distinct from existing antimicrobial agents, thereby providing an alternative treatment for multidrug resistant bacteria [13]. Moreover, many TCSTS regulate expression of virulence genes and therefore drugs that target TCSTS could reduce virulence without affecting bacterial viability and thus reduce the development of antimicrobial resistance during treatment regimens [14].

The genome of B. pseudomallei strain K96243 encodes more than 60 TCSTS [15] but only a few have been characterized including BPSL2024-5, VirAG, MrgRS and IrlRS. The IrlRS system is involved in the regulation of B. pseudomallei invasion of epithelial cells as well as heavy metal resistance. However, an irlR mutant was not attenuated for virulence in the C57BL/6 mouse, infant diabetic rat and Syrian hamster models [16, 17]. The MrgRS system responds to temperature, with increased expression of mrgR and mrgS observed during growth at 37 °C compared to 25 °C. This system may be involved in pathogenesis, but its role in virulence has not been specifically tested [18]. The VirAG system regulates the expression of the type VI secretion system cluster 1 (T6SS-1) during growth within macrophages. Both a virG mutant and a T6SS-1 mutant were attenuated for virulence [19]. The gene bpsl2025, encoding the SK of a TCSTS, was first identified in an in vivo hamster infection microarray study and a directed bpsl2025 mutant was significantly attenuated in the hamster model (≥3-log increase in ID50) [20].

Here we characterise a TCSTS in B. pseudomallei that we have named BprRS. Inactivation of the entire BprRS system via inactivation of both genes had no effect on virulence or motility and RNA expression analysis of the double bprRS mutant revealed few changes in gene expression. However, inactivation of only one component (either bprR or bprS) led to an attenuated phenotype in both virulence and motility. High-throughput RNA sequencing (RNA-seq) comparing the transcriptomes of the bprS and bprR mutants with the parent strain of B. pseudomallei revealed a large number of expression changes in genes required for chemotaxis, flagella biosynthesis and production of malleilactone. Furthermore, many transcriptional regulators were also differentially expressed in the single gene mutant strains. We propose that the altered phenotypes displayed by the bprR and bprS single mutants are due to the orphaned sensor or the orphaned response regulator (respectively) engaging in cross-talk interactions with one or more of the other B. pseudomallei TCSTS.

Results

Identification of an attenuated B. pseudomallei bprS (bpss0687) signature-tagged transposon mutant

A signature-tagged library of 336 B. pseudomallei K96243 mutants was constructed and screened for reduced in vivo growth in the acute (BALB/c) mouse melioidosis model. Mutants displaying reduced hybridisation in the output pools were tested individually for an in vivo growth defect by competitive growth assays. Five mutants were identified that displayed a statistically significant in vivo growth defect (P < 0.001). Four of the attenuated mutants contained transposon insertions within genes required for the biosynthesis of 1,3-linked 2-O-acetyl-6-deoxy-β-D-manno-heptopyranose capsular polysaccharide (three in wzm2, one in wcbQ). This locus has previously been shown to be important for B. pseudomallei virulence [21, 22]. The fifth attenuated mutant contained a Tn5 insertion within bpss0687 (112 bp from the 3′ end) and this mutant was designated bprS::Tn5 (Fig. 1a). The presence of a single transposon insertion in this mutant was confirmed by Southern blot analysis (data not shown). The ID50 of the B. pseudomallei parent strain K96243 and the bprS::Tn5 mutant was determined in groups of five BALB/c mice following inoculation via the intranasal (i.n.) or intraperitoneal (i.p.) routes of infection. For the i.n. route of infection, the ID50 of the bprS::Tn5 mutant was >1.3 × 107 CFU while the parent strain K96243 was <1.2 × 104 CFU. For the i.p. route of infection, the ID50 of the bprS::Tn5 mutant was >1.6 × 104 CFU compared with <1.2 × 103 CFU for the parent strain K96243. Therefore, the bprS::Tn5 mutant was attenuated for virulence via both infection routes in BALB/c mice. Importantly, the bprS::Tn5 mutant displayed normal in vitro growth in both rich medium (2YT) and minimal medium (M9) indicating that the attenuated phenotype was not due to a general growth defect (data not shown).

Fig. 1
figure 1

Schematic representation of the bprR (bpss0688) and bprS (bpss0687) genes in the B. pseudomallei K96243 wild-type strain and each of the bprS and bprR mutants. Panel a, organisation of the bprRS genes in B. pseudomallei wild-type showing the conserved amino acid domains encoded within each gene. Domains shown are the receiver and effector domains within bprR and, within bprS, the following domains: transmembrane regions 1 and 2 (TMR1 and 2) between which the stimulus-specific region is located, the HAMP (histidine kinases, adenylyl cyclases, methyl-accepting chemotaxis proteins, and phosphatases) signal transduction domain, the HisKA (histidine kinase A) dimerization/phosphoacceptor domain and the HATPase_c (histidine kinase-like ATPase catalytic) domain. The relative position of the insertion in each of the single mutants is shown below the gene schematic. Panel b, schematic representation of the regions remaining in each gene and the relative position of the tetracycline gene cassette in the bprRS double mutant

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Bioinformatic analysis of BPSS0687 revealed that the predicted protein sequence displayed significant amino acid identity to a number of characterised histidine kinases, including QseC from Pseudomonas spp. (92 % coverage, 39 % identity). Several conserved amino acid domains were identified within the predicted SK, including a catalytic histidine kinase-like ATPase, C-terminal domain (HATPase_c), a histidine kinase A domain (HisKA), a HAMP (histidine kinases, adenylyl cyclases, methyl-accepting chemotaxis proteins, and phosphatases) signal transduction domain and two transmembrane regions flanking the predicted stimulus-specific region (Fig. 1a). Located immediately upstream of the histidine kinase gene was a gene encoding a protein with receiver and effector domains typical of a RR (bpss0688). RT-PCR using primers that spanned the two genes indicated that bpss0687 and bpss0688 were co-transcribed (data not shown). Together these data indicate that bpss0687 and bpss0688 encode a cognate TCSTS pair named BprRS.

Generation of directed bprS, bprR and bprRS mutants and associated virulence studies

To confirm that inactivation of bprS led to an attenuated phenotype, a directed bprS mutant was constructed using double-crossover insertional mutagenesis (Fig. 1a). We first compared the growth of the parent strain K96243 and the mutant in BALB/c mice using competitive growth assays. The bprS mutant displayed normal in vitro growth (data not shown) but the in vivo competitive index of the bprS mutant was 0.094 ± 0.08, indicative of an approximately 10-fold reduced growth rate in vivo compared to the parent strain. The attenuated phenotype was then confirmed using virulence trials in BALB/c mice (Fig. 2). Mice infected with the parent strain K96243 displayed signs of illness by 28–50 h (days 2–3) and eight of the nine mice were euthanized by 190 h (day 8) after infection. In contrast, the survival rate in the group infected with the bprS mutant was significantly increased (Fisher’s exact test; P = 0.015), with only two mice developing late stage signs of infection and required euthanasia after 190 h.

Fig. 2
figure 2

Kaplan-Meier survival curves for groups of mice infected intranasally with the B. pseudomallei wild-type or the bprS, bprR or bprRS mutant strains. Mice were infected with the following doses; wild-type strain, 6 × 104 CFU; bprS mutant, 8 × 104 CFU, bprR mutant, 3 × 104 CFU, bprRS mutant 9 × 104 CFU

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To further characterise the BprRS TCSTS, a directed bprR mutant (Fig. 1a) and a bprRS double mutant (Fig. 1b) were also constructed by double-crossover insertional mutagenesis. The bprR mutant was also highly attenuated for virulence (P = 0.003) with only a single mouse showing late-stage disease signs at 150 h (day 6) (Fig. 2). In contrast, the bprRS mutant was not attenuated for virulence as determined by numbers of surviving mice (Fisher’s exact test; P = 0.13) or time to euthanasia (Log-rank Mantel-Cox test; P = 0.062) (Fig. 2). These data clearly show that separate inactivation of BprRS TCSTS SK or the RR resulted in decreased virulence, but inactivation of both genes in the BprRS TCSTS system did not.

Transcriptomic analyses of the bprRS double mutant

TCSTS are critical regulators of bacterial gene expression. To understand why the bprRS mutant was not attenuated for virulence, while the single bprR and bprS mutants were, we analysed the transcriptomes of all three mutant strains and the wild-type strain. Firstly, to identify the genes controlled by the BprRS system we compared the transcriptomes of the bprRS double mutant and the parent strain, K96243. In total, only nine genes were differentially expressed (five with increased and four with decreased expression) in the bprRS double mutant (Table 1). Both the truncated bprR and bprS gene fragments showed increased expression, suggesting that the BprRS TCSTS likely regulates its own expression. Two genes, bpss0686 and bpss0686a, located immediately upstream of the bprRS TCSTS genes but transcribed from the other strand, showed increased expression in the bprRS double mutant (Table 1); these genes were also identified as differentially expressed in the bprS single mutant (Table 2). Bioinformatic analyses of bpss0686a revealed no additional information on the open reading frame and analysis of the RNA-seq data revealed that only a single sequence read of the 13 million sequence reads generated from the parent strain (K96243) matched this region, indicating that bpss0686a may not encode a functional protein, or it is not expressed under the conditions used for bacterial growth. Bioinformatic analysis of bpss0686 revealed that it encoded a putative enzyme belonging to the flavin-utilizing monoxygenase super family and the nitrilotriacetate monoxgenase sub-family. Moreover, the encoded protein had 65 % identity (96 % coverage) to the 5, 10-methylene tetrahydromethanopterin reductase in Methylobacterium extorquens that is required for one carbon metabolism [23]. Five phage-associated genes were also differentially expressed in the bprRS double mutant; four of these showed decreased expression and one, encoding a phage membrane protein (bpss1087), showed increased expression. Three of the phage genes, bpss1087 and bpss1066 (encoding a predicted phage terminase/endonuclease subunits), and bpss1072 (encoding a protein of unknown function), are located on chromosome 2 within a predicted prophage. The remaining two genes differentially expressed in the bprRS double mutant encoded a predicted ATPase (bpsl0145) and a phage membrane protein (bpsl0146) that were within a large region on chromosome 1 also containing a predicted prophage.

Table 1 Genes with differential expression in the bprRS double mutant compared to expression in the wild-type parent strain
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Table 2 Genes with increased expression in either the bprR and/or bprS single mutants
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Transcriptomic analyses of the bprS, bprR single gene mutants

In order to identify gene expression changes that resulted from perturbation of the BprRS system via inactivation of bprS, encoding the SK, or bprR, encoding the RR, we compared the transcriptomes of the bprS and bprR mutants with the wild-type strain. A total of 170 genes were differentially expressed in one or both of the single mutants and 57 genes showed increased expression and 16 reduced expression (≥2-fold change in expression at FDR <0.01) in both the bprS mutant and the bprR mutants (Fig. 3, Tables 2 and 3); thus, these gene lists show a high degree of similarity (Fisher’s exact test; P < 0.001). Moreover, when a slightly less stringent FDR of <0.05 was applied to the initial gene list generated, 103 of the 171 genes identified were differentially expressed in both the bprS mutant and the bprR mutant (87 increased and 16 decreased) (Fig. 3, Tables 2 and 3). Genes identified with increased expression in the bprS and bprR single mutants included many involved in the production of secondary metabolites; bpsl3323-3329 and bpss0689-0690 involved in fatty acid biosynthesis, bpss0692-0698 involved in the degradation of aromatic compounds, and all the genes within the malleilactone biosynthesis locus (bpss0298-bpss0312).

Fig. 3
figure 3

A Venn diagram showing the number of B. pseudomallei genes with increased expression (up arrow) or with reduced expression (down arrow) in each of the bprR, bprS and bprRS double mutants. Genes were identified as differentially expressed if they showed >2-fold expression change (log2 > 1.0) compared to the wild-type strain with a False Discovery Rate (FDR) of <0.01. The total number of genes in each mutant showing increased expression (>2-fold) with a more relaxed FDR of <0.05 are shown in brackets

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Table 3 Genes with decreased expression in the bprR and/or bprS single mutants
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Two genes encoding methyl-accepting chemotaxis proteins (MCPs) (bpsl1829 and tar) and at least 19 genes required for flagella biosynthesis (including fliA encoding the flagella biosynthesis sigma factor) showed increased expression in the bprS single mutant; the majority of these also showed increased expression in the bprR mutant although mostly with FDR values between 0.01 and 0.05 (Tables 2 and 4). Genes involved in antibiotic resistance were also increased in expression and included bpeR (encoding a TetR family regulator), bpeA and bpeB that together encode the resistance-nodulation-division (RND) multidrug efflux pump BpeAB-OprA [24]. Other genes involved in antibiotic resistance that were over-expressed included the gene bpsl2708, encoding a putative metallo-β-lactamase, and penA that encodes a class A β-lactamase conferring resistance to ceftazidime [25, 26]. Three genes (bpss0623, macB and bpss0625) encoding an ABC transporter/type I secretion system predicted to be involved in drug resistance [27] were also over-expressed in the mutants. Genes with decreased expression in both the bprR and bprS mutant included five genes (bpss0515-bpss0520) located within the type 6 secretion system cluster 2 (T6SS-2). This cluster encodes one of six T6SSs produced by B. pseudomallei (designated T6SS-1through to T6SS-6) but only T6SS-1 has been determined to have a role in virulence [28].

Table 4 Regulatory genes differentially expressed in the bprR and/or bprS single mutants
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Importantly, a large number of regulatory genes were identified as differentially expressed when the BprRS system was perturbed by single gene inactivation. Regulatory genes with increased expression in both the bprS and bprR single mutants included fliA and bpeR (discussed above) and malR (bpss0312), encoding a regulator that shares identity (97 %) with MalR in Burkholderia thailandensis, an orphan LuxR homolog that activates the malleilactone biosynthesis genes independently of acyl-homoserine lactone and quorum sensing systems [29, 30]. The genes bprP (bpss1553), encoding a transmembrane regulator, and the adjacent gene bprQ, encoding a transmembrane protein, involved in the control of the BsaN virulence regulon were also over-expressed. Importantly, the BsaN virulence regulon includes genes encoding the type III secretion system locus 3 (TTSS3) [31, 32]. The expression of bpss0799 in both the bprR and bprS single mutants was also increased (Table 4); the encoded protein contains an EAL domain and shares significant identity with cyclic diguanylate phosphodiesterases, which are known to control motility and biofilm formation in a number of bacteria [33]. Other regulatory genes with increased expression but in only the bprR mutant were bpss0797 encoding an IclR family protein, bpss0755 encoding a LysR family protein, and bpsl1564 that encodes a putative transcriptional regulatory protein (Table 4). Only one regulatory gene (bpss00070, encoding an IS30 transposase) had decreased expression in the bprR mutant. Regulatory genes that were reduced in expression but only in the bprS single mutant included bpsl2972, encoding an IclR family protein, and dctD, encoding a C4-dicarboxylate transport transcriptional response regulator (Table 4).

Perturbation of the BprRS TCSTS affects B. pseudomallei motility

In the mutants with a single inactivation in either bprS or bprR, 21 genes involved in flagella biosynthesis were increased in expression, located in four different locations on chromosome 1 (Table 2). In addition, two genes encoding methyl-accepting chemotaxis proteins (bpsl1829 and tar) showed increased expression, and there was decreased expression of the type-1 fimbrial gene, bpsl1801 (Table 3) predicted to be involved in attachment to surfaces. Accordingly, we analysed the bprS mutants (bprS::Tn5 and the bprS directed mutant), the bprR directed mutant, the parent strain K96243, as well as the bprRS double mutant, for their ability to migrate or swarm in a coordinated manner on solid medium. The parent strain K96243 and the bprRS double mutant both demonstrated a capacity for rapid swarming, with the leading edge of the swarming population migrating to the edge of the agar plate (diameter 80 mm) after 18 h at 37 °C (Fig. 4). However, all strains with either bprS or bprR inactivated demonstrated a significantly reduced ability to swarm in a coordinated manner (Fig. 4). To confirm that the reduced swarming motility was due to perturbation of the BprRS system, we complemented the bprS directed mutant with the complete bprRS operon in trans. Interestingly, we were unable to clone either bprS or bprR into the multicopy plasmid pBHR1 alone. Swarming motility was fully restored in the bprS(bprRS) complemented strain, whereas the bprS mutant harbouring empty vector (pBHR1) alone retained the reduced motility phenotype (Fig. 4). These data show that inactivation of a single component in the BprRS TCSTS can reduce the swarming ability of B. pseudomallei.

Fig. 4
figure 4

The B. pseudomallei bprS and bprR mutants display reduced motility. Swarming motility was measured on agar plates grown at 37 °C for 18 h. Panel a, selected images of motility plates and Panel b, quantification of the motility data. Strains are B. pseudomallei wild-type (WT), directed bprS mutant (bprS), bprS transposon mutant (bprS::Tn5), bprR mutant (bprR), bprRS double mutant (bprRS), complemented bprS mutant (bprS(bprRS)), bprS mutant containing empty vector (bprS(pBHR1)) and a non-motile fliC mutant control (panel b only). Data are mean ± SEM. * = P < 0.01

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Discussion

We have identified a putative TCSTS in B. pseudomallei strain K96243 that is encoded by bprS (bpss0687) encoding the SK, and bprR (bpss0688) encoding the RR. Inactivation of the entire BprRS system did not result in changes to virulence or motility, and RNA expression analysis of the bprRS double mutant identified very few genes that were differentially expressed compared to the expression in the parent strain K96243. Genes identified as differentially expressed in the bprRS double mutant included one (bpss0686) adjacent to the bprS gene, encoding a predicted 5, 10-methylene tetrahydromethanopterin reductase that is required for one carbon metabolism [23]. Five genes that encoded phage-related proteins were also identified. Thus, our analysis suggests that the BprRS TCSTS regulon is small but it is possible that under different growth conditions, such as during growth in a host or the environment, other genes may be identified that belong to the BprRS regulon.

In contrast, inactivation of a single component (bprS or bprR) of the BprRS TCSTS resulted in the differential expression of a large number of genes. More than 70 genes were differentially expressed in both the bprS and bprR mutant and included those involved in flagella biosynthesis, malleilactone biosynthesis, antibiotic resistance, chemotaxis and regulation. In addition, phenotypic assays showed that the bprS and bprR mutants displayed reduced growth in mice and reduced swarming motility. Together, these results clearly demonstrate that perturbation of the BprRS system, but not inactivation of the whole system, attenuates B. pseudomallei. We hypothesize that the changes observed as a result of perturbation of the BprRS TCSTS arise through cross-regulation with one or more of the 60 TCSTS encoded on the B. pseudomallei genome [15]. A number of interactions between TCSTS have been identified in Escherichia coli; in vitro phosphorylation assays showed that phosphorylation of RRs by non-cognate SKs was observed for at least 21 pairs [34]. While most E. coli cross-talk interactions are weak [34], strong cross-talk has been observed between a number of systems, including CreC and PhoB and the PmrA/B and QseB/C systems of E. coli [35, 36] Interactions between PhoB, PmrA/B and QseB/C happen at multiple levels including phosphorylation, dephosphorylation and DNA binding. The E. coli QseC SK normally acts to dephosphorylate (and deactivate) its cognate RR QseB, but QseB can be phosphorylated by PmrB at relatively high levels [36] and the binding of both RRs at the qseBC promoter is likely to be required for normal gene expression. In the absence of QseC the phosphorylating activity of PmrB on QseB is uncontrolled, leading to increased expression of the QseBC TCSTS and decreased expression of a range of virulence genes including those involved in pilin and flagellin synthesis. Importantly, while an E. coli qseC mutant was non-motile and attenuated for virulence, the single qseB and the double qseBC mutants showed wild-type virulence and motility [37]. Cross-regulation has been implicated in at least three E. coli TCSTS that affect flagella synthesis and motility, including predicted interactions between ArcAB and another unidentified TCSTS [38]. Therefore, we propose that in the absence of both BprR and BprS (i.e. the bprRS double mutant) only the expression of genes within the BprRS regulon is affected. However, in the absence of BprS, BprR is phosphorylated by one or more, non-cognate sensor kinases and interacts with genes outside the BprRS regulon. Conversely, we predict that in the absence of BprR, BprS phosphorylates one or more, non-cognate response regulators. Moreover, given that a large subset of genes was differentially expressed in both the bprR and bprS mutants, we propose that the majority of cross-talk occurs largely with a single, as yet unidentified, TCSTS cognate pair. This cross-talk then leads to a cascade of dysregulation, including altered expression of genes encoding other regulators.

Phenotypic analysis of the mutants revealed that the bprS and bprR mutants were attenuated for swarming motility. In both mutants many flagella biosynthesis genes showed increased expression compared to the wild-type strain; suggesting that altered motility resulted from incorrect levels of flagella proteins or dysregulated timing of expression. Furthermore, genes within the flagella-associated locus, including fliC encoding the flagella subunit, were not changed in expression compared to that in the parent strain K96243 supporting the proposition that the altered motility of the BprS and BprR mutants may have been affected by an imbalance in the expression of the flagella biosynthesis and structural components. In E. coli and other bacteria, flagella synthesis involves the action of numerous and complex TCSTS interactions, and we predict similar interactions between regulatory factors is also likely to be essential for the co-ordinated movement of B. pseudomallei. The gene bpss0799, encoding a protein with an EAL domain characteristic of cyclic diguanylate phosphodiesterases, was increased in expression in both the bprS and bprR mutants. Cyclic diguanylate phosphodiesterases negatively control levels of bis-(3′-5′)-cyclic dimeric guanosine monophosphate (c-di-GMP) and, together with the positive regulator diguanylate cyclase, initiate the c-di-GMP signalling system in bacteria. The global second messenger c-di-GMP then binds to specific effector molecules that target, and subsequently affect the expression of a wide range of genes involved in cellular functions including motility, biofilm formation and the production of fimbriae [33]. A previous study identified another B. pseudomallei gene (cdpA or bpsl1263) as encoding the cyclic diguanylate phosphodiesterase involved in flagella function and motility [39]. However, our own bioinformatic analysis (data not shown) indicates that bpsl1263 encodes a protein with both an EAL and a GGDEF domain, the latter domain being characteristic of diguanylate cyclases. Other regulatory genes with increased expression in the bprS and bprR mutants included two genes encoding predicted MCPs, bpsl1829 and tar. MCPs are the trans-membrane sensor proteins of the chemotaxis pathway that controls bacterial movement in response to available nutrients or other environmental stimuli [40]. In E. coli, MCPs directly transfer phosphate to the TCSTS SK CheA that then transfers the phosphate to one of two RRs, CheY or CheB. Phosphorylated CheY interacts directly with the flagella motor and causes a directional change, whereas phosphorylated CheB acts a methylesterase on the signalling MCP and modulates the amount of signal [41]. The MCP Tar sensors induce bacterial cells to move towards aspartate/maltose and away from nickel/cobalt [42]. Bioinformatic analysis did not provide any information on the type of sensor the bpsl1829 gene encodes, but we predict that dysregulation of the expression of either MCP is likely to have an effect on motility. Although no studies have been conducted on chemotaxis mutants in any Burkholderia species, a study in a close relative, Ralstonia solanacearum, showed that a cheA mutant displayed significantly reduced virulence [43].

The genes bprP and bprQ, involved in the BsaN virulence regulon, both displayed increased expression when the BprRS TCSTS was perturbed. A recent transcriptomic study of a B. pseudomallei bsaN deletion mutant elucidated components of the BsaN virulence-associated regulatory system [32]. It is proposed that BprP directly activates the Ara-C like regulatory protein BsaN that, together with the T3SS3 chaperone BicA, act as a dual-function regulatory complex that controls the expression of the T6SS-1 (via activation of the VirAG TCSTS) and the T3SS3 effectors (bopA, bopC and bopE). In addition, in the bsaN mutant the TTSS3 genes showed increased expression, while the genes involved in malleilactone (bpss0303-0311) and flagella biosynthesis (bpsl0281, bpsl3319, bpsl3320, bpsl3321) showed decreased expression [32]. In our study, we observed an increase in expression of bprP and bprQ, but not the gene encoding the chaperone BicA. We also observed an increase in expression of malleilactone-associated and flagella-associated genes, but no significant change in expression of genes associated with the T3SS3 and T6SS-1. Nevertheless, it is possible that an imbalance in the expression of the proteins that initiate the transcription of bsaN (BprP/BicA) may have an effect on the expression of some genes within the BsaN regulon.

Perturbation of the BprRS TCSTS reduced the in vivo fitness of B. pseudomallei and this may, or may not have been directly associated with the loss of motility. An initial report demonstrated that a non-flagellated fliC mutant constructed in B. pseudomallei strain 1026b was not attenuated for virulence in BALB/c mice, diabetic rats or Syrian hamsters [44, 45]. In contrast, a fliC mutant of a more virulent strain of B. pseudomallei (KHW) was attenuated for virulence in BALB/c mice [46].

Conclusions

Phenotypic and transcriptomic analyses of a newly identified TCSTS BprRS, revealed that perturbation of the system via inactivation of the SK BprS or the RR BprR led to a reduction in virulence and reduced motility, as well as a wide range of gene expression changes. Our results support the concept that B. pseudomallei TCSTS regulatory networks can interact and show that selective perturbation of these systems can lead to attenuation of B. pseudomallei. Together our results highlight the need for further systematic studies of B. pseudomallei TCSTS regulation and show that targeting a single TCSTS component can attenuate virulence.

Methods

Bacterial strains, plasmids and culture conditions

The B. pseudomallei strain K96243 is a human clinical isolate obtained from Thailand [15]. B. pseudomallei directed mutants were generated by double cross-over insertional mutagenesis using recombinant derivatives of the λ pir-dependent plasmid pDM4 [47]. All pDM4 derivatives were maintained in E. coli SM10 λ pir (thi thr leu tonA lacY supE recA RP4-2-Tc::Mu::Km pir), or E. coli S17-1 λ pir (thi pro hsdR hsdM1 recA RP4-2-Tc::Mu-Km::Tn7 pir). For some clonings, pBlueScriptSK- (Stratagene) was used as an intermediate vector prior to transfer of the insert into pDM4. The pBlueScript derivatives were grown in E. coli DH5α cells (F− endA1 hsdR17 (rk −mk −) glnV44 thi-1 λ− recA1 gyrA96 relA1 ∆(argF- lacZYA)U196 ϕ80dlacZ ∆M15). The tetracycline resistance gene tetA(C) was used for selection of B. pseudomallei mutants and was isolated from either pUTminiTn5Tc (Biomedal S. L., Spain) or pWH1266 [48]. For complementation, the BprRS operon was cloned into the plasmid pBHR1, a derivative of the mobilizable broad-host-range plasmid pBBR1 [49]. All E. coli strains were routinely grown on lysogeny broth (LB) medium with or without selection. B. pseudomallei K96243 and derivatives were grown using either LB, yeast-tryptone medium (2YT), minimal medium (M9), or Ashdown’s medium (containing 64 μg/ml gentamicin). All strains were grown at 37 °C (liquid cultures with 200 rpm agitation).

Construction and screening of B. pseudomallei signature-tagged mutagenesis library

A B. pseudomallei signature-tagged mutagenesis library was constructed using a modified miniTn5 transposon (Biomedal S.L., Spain). Briefly, 42 unique DNA-tags were amplified from the STM-adapted Tn916 transposons generated by Harper et al. [50] and cloned into the unique NotI site of pUTminiTn5Tc. The 42 uniquely-tagged transposons were then separately introduced into B. pseudomallei by conjugation and pools of 42 mutants collected. Each STM pool was then screened for reduced in vivo growth in BALB/c mice [51]. An input pool inoculum of approximately 2 × 108 CFU was used to inoculate two 8–10 week old, female BALB/c mice by the i.n. route. DNA recovered from pooled input colonies and pooled output colonies (harvested from spleen), was used to generate digoxygenin-labelled (Roche) DNA probes representing tags present in each sample. Labelled probes were then used in dot blot hybridizations to determine the presence/absence of each mutant in input and output pools as described previously [50].

Generation of bprS, bprR and bprRS double cross-over mutants

The bprS, bprR and bprRS mutants were constructed by double cross-over insertional mutagenesis using the λ pir-dependent vector pDM4 [47] which carries a chloramphenicol resistance gene for selection and the counter-selectable sacB gene. To generate the bprS mutagenesis construct, an internal fragment of bprS was disrupted by cloning of the miniTn5 tetA(C) gene into the bprS BglII site. Insertion of the tetA(C) gene at this BglII site results in the termination of BprS translation at the second transmembrane region (Fig. 1). Briefly, the primers BAP4787 (5′ TTCGTGCTGCAGGATTATCTCGAACGCCATCC 3′) containing a PstI site, and BAP4788 (5′ CGAATCTCTAGAGTGGAACGGCTCGAACAC 3′) containing an XbaI site, were used to amplify a 981 bp PCR product from within the B. pseudomallei K96243 bprS gene. This PCR fragment, containing an internal BglII site, was digested with PstI and XbaI and ligated into similarly digested pDM4. Primers BAP3325 (5′ CGGCTTAGATCTAGGTCGAGGTGGCC 3′) and BAP4629 (5′ TCCACCAGATCTATTTGCCGACTACCTTGGTG 3′), both containing a BglII site, were used to amplify the miniTn5 tetA(C) gene. This PCR product and pDM4 containing the bprS internal fragment were digested with BglII and ligated to generate the plasmid pAL603 which was then introduced by transformation into E. coli SM10 λ pir.

For generation of the bprR mutagenesis construct, pBluescriptSK- was used as an intermediate plasmid prior to cloning into pDM4. Primers BAP6698 (5′ GAACACCCCGGGCGCGAGATCGACATGCCCGGACACGCC 3′) containing an XmaI site, and BAP6699 (5′ CGTCGTACTAGTACATGAAGCCGAAGCCCTCGTTGCCG 3′) containing an SpeI site, were used to amplify a 1648 bp PCR product from B. pseudomallei K96243 encompassing the entire bprR gene, 687 bp of upstream and 241 bp of downstream DNA. This PCR product, containing an internal AatII site within bprR (Fig. 1a) was digested with XmaI and SpeI and ligated into similarly digested pBluescriptSK-. Primers BAP6700 (5′ AAAACAGACGTCTTGCTAACGCAGT 3′) and BAP6701 (5′ AAAAATGACGTCAGTGGTGAATCC 3′), both containing an AatII site, were used to amplify the tetA(C) gene from pWH1266. This product and the pBluescriptSK- derivative containing the bprR fragment were digested with AatII and ligated to generate the plasmid pBluescriptSK::bprR-tet which was then introduced into E. coli DH5α by transformation. This insertion of the tetracycline resistance gene at the internal AatII site causes a truncation of bprR within the initial receiver domain (Fig. 1a). The fragment containing the disrupted bprR was released from pBluescriptSK::bprR-tet by digestion with XmaI and SpeI and ligated into pDM4, generating the plasmid pAL1067 which was then introduced into E. coli SM10 λ pir cells.

To generate the bprRS double mutant, up- and down-stream regions encompassing the 5′ and 3′ ends of bprR and bprS respectively were cloned into pBluescriptSK-, with the tetA(C) gene from miniTn5 gene inserted between the two fragments. Insertion of this construct into the genome leads to deletion of a 3′ segment of bprR (encoding part of the receiver domain and all of the effector domain) as well as deletion of a 5′ segment of bprS (encoding both transmembrane regions and the HAMP and HisKA domains) (Fig. 1b). Briefly, primers BAP6704 (5′ TCGACGCCCGGGTCACCGAGCTGCTGACGATCGGC 3′) containing an XmaI site, and BAP6705 (5′ CGGCGCACTAGTTATCAGACCGACTACGCGCC 3′), containing a SpeI site, were used to amplify a 973 bp PCR fragment including the 3′ end of bprS and down-stream flanking DNA. This product was digested with appropriate enzymes and ligated into pBluescriptSK- digested with XmaI and SpeI and introduced into DH5α cells. Primers BAP6685 (5′ AAAACAGAATTCTTGCTAACGCAGT 3′) and BAP6686 (5′ AAAAATGAATTCAGTGGTGAATCC 3′), both containing an EcoRI site, were used to amplify the tetA(C) gene from pWH1266. This product and pBluescriptSK- containing the DNA fragment containing bprS and flanking region were digested with EcoRI, ligated and introduced into E. coli DH5α. Primers BAP6702 (5′ AGCGGCGGGCCCCCGCATGCACCGAGCCC 3′) containing an ApaI site, and BAP6703 (5′ GAGGCCATCGATTTGATCGTAGACGTCCG 3′) containing a ClaI site, were used to amplify a 1021 bp PCR product encompassing the 5′ end of bprR and up-stream flanking DNA. This product was digested with ApaI and ClaI and ligated into the similarly digested pBluescriptSK- containing bprS plus flanking region and the tetA(C) gene, and then introduced into E. coli DH5α cells, generating the plasmid pAL1062. This plasmid was digested with ApaI and SpeI and the fragment containing bprR-tet-bprS was ligated into pDM4. The resulting plasmid, designated pAL1066, was then introduced into E. coli SM10 λ pir cells.

Each of the recombinant plasmids pAL603, pAL1067 and pAL1066 was mobilised from E. coli SM10 λ pir into B. pseudomallei K96243 by conjugation and putative double cross-over mutants were selected on LB agar containing gentamicin (8 μg/mL) and tetracycline (25 μg/mL). All mutations were confirmed by PCR and sequence analysis (data not shown).

Complementation of the bprS mutant

The bprS mutant was complemented by cloning an intact copy of the bprRS operon into the multicopy plasmid pBHR1. Primers BAP7136 (5′ CGGCGCTTTAAAGGCTCGATACTGACTGCTGCCGGC 3′) containing a DraI site, and BAP7137 (5′ CGCGCGCCATGGATCGTCTGACGGCCGAAACC 3′) containing an NcoI site, were used to amplify a 2483 bp PCR product from B. pseudomallei K96243. This fragment encoded bprS and bprR as well as 353 bp of the upstream region predicted to contain the bprRS promoter. The PCR product was digested with DraI and NcoI and ligated into similarly digested pBHR1, disrupting the cat gene and generating the plasmid pBHR1::bprRS. This plasmid was then introduced into E. coli S-17 λ pir and kanamycin resistant, chloramphenicol sensitive clones selected. The pBHR1::bprRS plasmid and empty pBHR1 (negative control) were separately mobilised from E. coli S-17 into the bprS mutant by conjugation. Recombinants containing the pBHR1::bprRS plasmid were selected on LB agar containing kanamycin (1000 μg/mL) and tetracycline (25 μg/mL) while those containing the empty pBHR1 plasmid were selected on LB agar containing kanamycin (1000 μg/mL), tetracycline (25 μg/mL) and chloramphenicol (40 μg/mL). Strains containing the correct plasmids were identified by PCR and nucleotide sequence analysis (data not shown). Neither bprR nor bprS alone could be cloned into the pBHR1 plasmid despite numerous attempts.

Competitive in vivo growth assays

Overnight cultures of B. pseudomallei wild-type parent strain K96243 and the bprS mutant were grown in LB to an optical density at 600 nm (OD600) of 0.2. Equal volumes of K96243 and bprS mutant culture were combined and 20 μl (containing approximately 4 × 105 CFU) of an appropriate dilution was used to infect three 6–8 week-old female BALB/c mice by the i.n. route. After 24 h, mice were euthanized in accordance with animal ethics requirements. Spleens were harvested, homogenised in phosphate-buffered saline pH = 7.2 (PBS) and plated onto LB agar. After growth at 37 °C for 24 h, 100 colonies from these in vivo growth plates and 100 colonies representing the input culture were patched onto LB agar with or without tetracycline (25 μg/ml) to determine the proportion of bprS mutant to K96243 wild-type bacteria. The competitive index was calculated as the proportion of mutant to wild-type bacteria recovered from the mouse spleens divided by the proportion of mutant to wild-type bacteria present in the input inoculum.

Virulence assays

Overnight cultures of the parent strain K96243 and the bprS, bprR and bprRS mutants were subcultured in fresh medium with appropriate antibiotics and grown to mid-log phase to an OD600 of 0.8 (equivalent to ~5.0 × 108 CFU/ml). For the ID50 assays, groups of five 8–10 week-old BALB/c mice were either inoculated i.n (1.0 × 106 CFU in 20 μl volume) or injected i.p (1.0 × 103 CFU in 200 μl volume) with LB containing mid-exponential phase bacteria. For the direct virulence assays, groups of nine 6–8 week-old, female BALB/c mice were infected i.n. with 20 μl doses containing approximately 5.0 × 104 CFU. Mice were monitored for 10 days for signs of disease and euthanized at the end of the experiment or when moribund, in accordance with animal ethics requirements. The ID50 for the parent strain K96243 and mutant strain was determined using the calculation described by Reed and Muench [52] based on cumulative moribund infections. For direct virulence assays, differences in survival were calculated using Fisher’s exact test and differences in time to death determined using the log-rank Mantel-Cox test. Spleens from three mice in each group were harvested, homogenised in PBS and plated onto LB agar. The stability of the mutants was assessed by patching the recovered colonies onto agar plates with or without tetracycline (25 μg/ml). All of the mutations were stable over the time course of the experiment. The virulence of the complementation strain bprS(bprRS) could not be assessed as the complementation plasmid was highly unstable in the absence of antibiotic selection (>90 % plasmid loss over 16 h).

RNA purification

B. pseudomallei parent strain K96243 and the directed bprS, bprR and bprRS mutants were grown overnight at 37 °C in LB with appropriate antibiotics (K96243 in gentamicin 64 μg/ml; mutants in gentamicin 64 μg/ml and tetracycline 25 μg/ml). Strains were subcultured 1/50 into fresh antibiotic-free medium and grown at 37 °C with shaking (200 rpm) to an OD600 of 0.5. The cells were harvested by centrifugation, and RNA purified using Trizol reagent (Gibco/BRL) as specified by the manufacturer. RNA was DNase treated using the TURBO DNA-free kit (Ambion), followed by processing with a QIAGEN RNeasy kit clean-up with on-column DNase digestion as per the manufacturer’s instructions.

High-throughput RNA sequencing

Double-stranded cDNA synthesis and high-throughput RNA-seq were performed as described previously [53]. For each strain three biological replicates were sequenced. Trimmed sequence reads were aligned to the B. pseudomallei K96423 genome sequence using SHRiMP [54] and normalised read counts were compared using voom and limma as described previously [53]. For each replicate sample, between 6.4 million and 14.0 million sequence reads were mapped uniquely to the K96423 genome sequence. The RNA-seq data is available at the NCBI Gene Expression Omnibus; accession number GSE77970. Differentially expressed genes were identified as those with a greater than 2-fold change in expression (1.0 log2) across all replicates at a false discovery rate (FDR) of <0.01.

Swarming motility assays

Swarming agar plates were prepared fresh on the day of the assay using the modified protocol of Tunpiboonsak et al. [55]. Briefly, plates were prepared using 0.5 % w/v agar-agar (Merck), 8 g/L nutrient broth No.2 (Oxoid) and 5 g/L D(+)- glucose (dextrose) (May and Baker) and dried carefully to give constant moisture content. Overnight cultures of B. pseudomallei parent strain K96243 and mutant strains were subcultured 1/50 into fresh medium with appropriate antibiotics (no selection for parent strain, 25 μg/ml tetracycline for all mutants and complemented mutants) and grown at 37 °C with shaking (200 rpm) to late exponential phase (OD600 of ~2.5). A 5 μl volume of each culture was spotted onto the centre of a swarming agar plate which was then incubated at 37 °C for 18 h in the dark. The diameter of the swarming population was then measured. Statistical analysis of swarming distance was determined by Student’s t-test with a P-value of <0.05 considered significant.

Ethics approval and consent to participate

All animal experiments were carried out in accordance with the provisions of the “Prevention of Cruelty to Animal Act, 1986”, the “Australian Code of Practice for the Care and Use of Animals for Scientific Purposes 7th edition, 2004” and the Monash University Animal Welfare Committee Guidelines and Policies. The protocol was approved by the Monash Animal Research Platform (MARP)-2 Animal Ethics Committee (AEC) of Monash University (AEC number MARP/2011/067).

Consent for publication

Not applicable.

Availability of data and materials

The RNA-seq data is available at the NCBI Gene Expression Omnibus; accession number GSE77970.

Abbreviations

2YT:

yeast-tryptone medium

AEC:

Animal Ethics Committee

FDR:

false discovery rate

HAMP:

Histidine kinases, Adenyl cyclases, Methyl-accepting proteins and Phosphatases

HATPase_c:

Histidine kinase-like ATPase, C-terminal domain

HisKA:

histidine kinase A domain

i.n.:

intranasal

i.p.:

intraperitoneal

LB:

lysogeny broth

MARP:

Monash Animal Research Platform

MCPs:

methyl-accepting chemotaxis proteins

OD600 :

optical density at 600 nm

PBS:

phosphate-buffered saline pH = 7.2

RNA-seq:

RNA sequencing

RND:

resistance-nodulation-division

RR:

response regulator

SK:

sensor kinase

T6SS-1:

type VI secretion system cluster 1

T6SS-2:

type 6 secretion system cluster 2

TCSTS:

two-component signal transduction system

TTSS3:

type III secretion system locus 3

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Acknowledgements

We thank Carla Osinski for excellent technical assistance and Alicia Shu-Chin Lai for her considerable help with animal experiments.

Funding

This work was funded by the Australian Research Council (Australia), Australian Research Council Centre of Excellence in Structural and Functional Microbial Genomics Grant number CE0562063 and the National Health and Medical Research Council (Australia), Project Grant numbers 545855 and 1043667.

Author information

Author notes

  1. Natalie R. Lazar Adler

    Present address: Core Biotechnology Services, University of Leicester, Leicester, LE1 9HN, UK

  2. Puthayalai Treerat

    Present address: Department of Molecular Microbiology, Washington University School of Medicine, St. Louis, MO, USA

  3. Priyangi Alwis

    Present address: Faculty of Dentistry, National University of Singapore, Singapore, Singapore

Authors and Affiliations

  1. Department of Microbiology, Monash University, 19 Innovation Walk, Clayton, Victoria, 3800, Australia

    Natalie R. Lazar Adler, Elizabeth M. Allwood, Deanna Deveson Lucas, Stephen Watts, Puthayalai Treerat, Priyangi Alwis, Ben Adler, Marina Harper & John D. Boyce

  2. Infection and Immunity Program, Monash Biomedicine Discovery Institute, Monash University, Victoria, Australia

    Deanna Deveson Lucas, Alexandra Dimitropoulos, Rodney J. Devenish, Mark Prescott, Ben Adler, Marina Harper & John D. Boyce

  3. Victorian Bioinformatics Platform, Monash University, Victoria, Australia

    Paul Harrison

  4. Department of Biochemistry and Molecular Biology, Monash University, Victoria, Australia

    Alexandra Dimitropoulos, Rodney J. Devenish & Mark Prescott

  5. Department of Microbiology and Immunology, James Cook University, Townsville, Queensland, Australia

    Brenda Govan

Authors
  1. Natalie R. Lazar Adler
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  2. Elizabeth M. Allwood
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  12. Ben Adler
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Corresponding author

Correspondence to John D. Boyce.

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Competing interests

The authors declare that they have no competing interests.

Authors’ contributions

NLA, EA, DDL, SW, AD, BA, PT and PA performed the experiments. PH, DDL, EA, NLA, MH, JB performed statistical and bioinformatic analysis on the RNA-seq transcriptomic data. EA, NLA, BA, RD, MH and JB wrote and edited the manuscript. NLA, EA, BG, RD, MP, BA, MH and JB supervised the study. All authors read and approved the final manuscript

Joint senior authors: Marina Harper and John D. Boyce

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Lazar Adler, N.R., Allwood, E.M., Deveson Lucas, D. et al. Perturbation of the two-component signal transduction system, BprRS, results in attenuated virulence and motility defects in Burkholderia pseudomallei . BMC Genomics 17, 331 (2016). https://doi.org/10.1186/s12864-016-2668-4

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Keywords

BMC Genomics

ISSN: 1471-2164

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