- Research article
- Open Access
Role of AcsR in expression of the acetyl-CoA synthetase gene in Vibrio vulnificus
BMC Microbiology volume 15, Article number: 86 (2015)
VarS/VarA is one of the global factors regulating diverse aspects of the metabolism and virulence of bacteria including pathogenic Vibrio spp. An experiment to identify the VarS/VarA-regulon in V. vulnificus revealed that a putative LuxR-type transcriptional regulator was down-regulated in ΔvarA mutant. To investigate the roles of this regulatory cascade, the target gene regulated by a LuxR-regulator was identified and its expression was characterized.
Transcriptomic analysis of the mutant deficient in this LuxR-type regulator showed that the acsA gene encoding acetyl-CoA synthetase was down-regulated. Thus, this regulator was named AcsR for “regulator of acetyl-CoA synthetase”. A putative histidine kinase gene, acsS, was located five ORFs downstream of the acsR gene. Expression of an acsA::luxAB transcriptional fusion was decreased in both ΔacsR and ΔacsS mutants. Similar to a ΔacsA mutant, strains carrying deletions either in acsR or acsS grew slowly than wild type in a minimal medium with acetate as a sole carbon source. Growth defect of the ΔacsR strain in acetate-minimal medium was restored by complementation. To investigate if AcsR directly regulates acsA expression, in vitro-gel shift assays were performed using the recombinant AcsR and the regulatory region of the acsA gene, showing that AcsR specifically bound the upstream region of the acsA ORF.
This study indicates that the VarS/VarA system plays a role in V. vulnificus metabolism via regulating AcsR, which in turn controls acetate metabolism by activating the transcription of the acetyl-CoA synthetase gene.
Vibrio vulnificus is a halophilic marine microorganism that is frequently associated with gastroenteritis and septicemia in humans with risk factors such as uremia and liver diseases . The following microbial components of V. vulnificus have been determined as virulence factors: capsular polysaccharides , a cytolytic VvhA hemolysin , a contact-dependent RtxA toxin [4,5], an elastolytic VvpE protease , lipopolysaccharides , and a phospholipase A2 . In addition to these extracellular components, any microbial factor enhancing growth or survival of V. vulnificus under diverse environmental conditions, such as iron acquisition , motility [10,11], and fermentation efficiency , is critical for its pathogenicity.
VarA had initially been discovered as a response regulator of the two-component family modulating virulence of V. cholera . VarS was thought as a cognate histidine sensor kinase for VarA based on identification of BarA/UvrY, a VarS/VarA homologue of Escherichia coli . VarS/VarA homologous systems are also present in other Gram-negative bacteria, which are differently annotated as BarA/SirA (Salmonella), GacS/GacA (Pseudomonas) and LetS/LetA (Legionella pneumophila) [15-17]. This two-component regulatory system plays a pleiotropic role in the signaling cascades for bacterial survival as well as bacterial pathogenicity upon reception of appropriate signals . Well-characterized target genes of these VarS/VarA homologous systems include csrB- and csrC-encoding small RNAs (sRNA), the expression of which is positively regulated by VarS/VarA . These sRNAs then sequester a regulatory protein, CsrA that directly controls the expression of several genes at post-transcriptional level .
In V. cholerae, VarS/VarA system is known to control the expression of HapA, a hemagglutinin/protease along with CsrA/csrB/csrC/csrD . VarS/VarA also modulates expression of virulence proteins such as cholera toxin and toxin-coregulated pili by controlling ToxT expression . In addition, VarS/VarA-CsrA/csrB/csrC/csrD system regulates quorum sensing in V. cholerae by altering the expression level of HapR, a master regulator of quorum sensing [23,24].
Little is known about VarS/VarA and CsrA/csrB/csrC systems in V. vulnificus. Quantitative measurement of transcripts in the ΔvarA mutant V. vulnificus demonstrated that the amount of sRNAs, such as csrB1, csrB2, csrB3, and csrC was reduced in the mutant as well as mRNAs encoding flagellins, RpoS, RtxA1, and VvpE . Comparison of bacterial ability to form biofilm between csrA-positive and csrA-negative V. vulnificus strains clearly indicates that CsrA inhibits biofilm formation by V. vulnificus .
Based on the hypothesis that VarS/VarA could control other regulatory proteins in addition to the csrB and csrC sRNAs, we further searched VarS/VarA-target genes with special attention to any transcription factors. Among the down-expressed proteins in ΔvarA mutant, a putative transcription regulator with a LuxR-type DNA binding domain was selected and used to identify its regulon via comparative transcriptome analyses. Interestingly, expression of the acetyl-CoA synthetase gene (acsA) among others, was found to be reduced in a mutant defective in the LuxR-type regulator.
Production of acetyl-CoA occurs via two different catalytic reactions: i) Acetyl-CoA synthetase (Acs) forms acetyl-CoA from acetate through an acetyladenylate intermediate. ii) Alternatively, acetyl-CoA is formed via two enzymatic reactions catalyzed by acetate kinase (Ack) and phosphotransacetylase (Pta). In E. coli, Acs activity is induced by acetate and repressed by glucose. Thus, Acs functions as a high-affinity acetate uptake system scavenging extracellular acetate present at relatively low concentration . On the other hand, Ack and Pta primarily play a catabolic role showing a low affinity toward acetate. Although these two catalytic reactions appear to be present in V. vulnificus based upon genomic sequence analysis, which shows the presence of acsA (VVMO6_00187) and ack (VVMO6_01096)/pta (VVMO6_01095), little information regarding the functions and expressions of acetyl-CoA synthesizing enzymes is available in this species.
In the present study, the acsA gene was chosen from a series of comparative analyses of gene expression using DNA microarrays, and the regulatory mechanisms for acsA expression were examined.
Effect of the varA mutation on expression of various transcription factors, including a LuxR-type regulator
The VarS/VarA two-component systems are conserved among many γ-Proteobacteria. They modulate diverse biological activities relating to metabolism, motility, and protease activity, by which they eventually influence the extent of virulence, in the case of pathogens . This system positively controls the expression of small RNAs, which then bind to the RNA binding protein CsrA, in order to modulate translation of the target genes. In a previous study, the ΔvarA mutant V. vulnificus revealed a lower abundance of these small RNAs . The ΔvarA mutant constructed in this study also showed lower transcript levels of the small RNAs, csrB1, csrB2, csrB3, and csrC by Northern blot analysis and fusion assays, as expected (data not shown).
Microarray assays on transcriptomes of the ΔvarA mutant and wild-type V. vulnificus revealed 167 genes showing altered expression in the mutant (110 and 57 as down-regulated and up-regulated genes, respectively) when the normalized expression relative to wild type was confined to be <0.5 or >2 with a statistical significance (P-value <0.05) (Figure 1 and Additional file 1: Table S1). As expected, the transcript level of the varA gene in the ΔvarA mutant was not detected. Both down-regulated and up-regulated genes in the ΔvarA mutant were evaluated by Cluster of Orthologous Groups (COG) designation , and grouped into four functional categories, i.e., metabolism, cellular process, information process, and poorly characterized genes.
The largest group of both down- and up-regulated genes belonged to metabolism (42-43%), which covers various metabolic pathways for energy, carbon, nucleotide, lipid, amino acid, cofactor and secondary metabolites. One of the down-regulated genes was found to encode acetyl-CoA synthetase (Figure 1A). Interestingly, seven components involved in oligopeptide transport system (OppABCDF) and three subunits of the dipeptide transporter (Dpp) were concomitantly identified as down-regulated proteins in the ΔvarA mutant. A significant portion of the genes showing altered expression in the ΔvarA mutant (25-31%) encoded hypothetical proteins or putative proteins with biochemical activities. Another group of genes showing lower or higher expression in the ΔvarA mutant encodes proteins involved in cellular processes such as motility, signal transduction, resistance to oxidative stress and toxin secretion. Comparative transcriptome analysis also showed that several transcription factors were differentially expressed in the ΔvarA mutant compared to the wild type. Down-regulated genes in the ΔvarA mutant encode putative transcriptional regulators with conserved domains (annotated as a transcriptional regulator, a DNA-binding response regulator, a DNA-binding HTH domain-containing protein, and a LuxR family transcriptional regulator). One of the down-regulated genes encodes a negative regulator GcvR for the glycine cleavage system, a well-known metabolic pathway involved in glycine degradation . Up-regulated proteins in the ΔvarA mutant include RseC, a regulator of the extracytoplasmic stress response sigma factor, sigmaE [30,31]. Transcripts of two putative transcriptional factors containing the domains conserved in LytR/AlgR and LysR family proteins were found at a higher level in the ΔvarA mutant. Another up-regulated gene in the ΔvarA mutant encodes the LuxZ homologous protein involved in bioluminescence of Photobacterium . Lastly, higher expression of the rpiR gene was detected in the ΔvarA mutant, which encodes a regulatory protein with the binding domain for phosphosugar .
In this study, a putative LuxR-type transcription factor (VVMO6_00196) showing decreased expression in the ΔvarA mutant was chosen for further investigation. The transcript level of this LuxR-type regulator was measured in both wild type and ΔvarA mutant by quantitative real-time PCR. As expected from the microarray data, a relative transcript level of this gene in the ΔvarA mutant was 42 ± 9% of the wild-type level (Student t-test, P-value = 0.0008).
Identification of target gene(s) controlled by the putative LuxR-type transcription factor
In a subsequent experiment, we constructed a mutant V. vulnificus devoid of the LuxR-type regulator, the deletion of which was confirmed by PCR using specific primers annealed to upstream and downstream regions of this gene (Figure 2A and B). This mutant was also examined by western blot using polyclonal antibodies against the recombinant protein of the LuxR-type regulator (Figure 2C). As expected, the mutant did not show any immunoreactive band around 23 kDa, which was present in the extract of the wild type.
Comparative transcriptome analysis of this mutant was performed using a V. vulnificus DNA microarray (Table 1). As expected, the level of the luxR transcript was too low to be detected in the ΔluxR mutant transcriptome. Beside the luxR gene, twenty-three genes demonstrated altered expression in the ΔluxR mutant with statistical significances (11 down- and 12 up-regulated genes). Three genes showing decreased expression in the mutant encode metabolic enzymes such as acetyl-CoA synthetase, phosphoenolpyruvate carboxylase, and aspartate carbamoyltransferase. One of the down-regulated genes encodes the MarC protein, which had been thought as a multiple antibiotic resistance protein , but it was later found to be unrelated with the antibiotic resistance . It is most notable that the msh transcripts encoding five components of the mannose-sensitive hemagglutinin (MASH) pilus, were found at a lower level in the ΔluxR mutant. Another down-regulated gene encodes a homologous protein to E. coli DEAD-box protein A, an RNA helicase involved in structural rearrangement of ribosomal RNA .
Up-regulated genes in the ΔluxR mutant also encode three metabolic enzymes; a glycosyltransferase SypQ for poly-N-acetylglucosamine biosynthesis , an inosine-guanosine kinase for nucleotide metabolism, and an enzyme for siderophore biosynthesis. Another up-regulated gene in the ΔluxR mutant encodes a protein homologous to VgrG protein, a component comprising the type VI secretion system in gram-negative bacteria . Interestingly, the gene encoding CheW homologous protein was transcribed more in the ΔluxR mutant. CheW functions as a cytoplasmic adaptor protein to form the bacterial chemosensory array along with CheA protein . In addition, three genes encoding hypothetical proteins (VVMO6_01214, VVMO6_02404, and VVMO6_03566) showed increased expression in the ΔluxR mutant.
One of the down-regulated proteins in this mutant was acetyl-CoA synthetase [acetate:CoA ligase (AMP-forming) EC 188.8.131.52], which catalyzes a conversion of acetate to acetyl-CoA. The database of the V. vulnificus MO6-24/O genome showed that an ORF (VVMO6_00187) encoding acetyl-CoA synthetase is acsA gene. Down-expression of the acsA gene in the mutant defective in the LuxR-type regulator was confirmed by real-time PCR (Figure 2D). The acsA transcript level in this mutant was 38 ± 17% of the wild type, indicating that this LuxR-type protein is a positive regulator for expression of acetyl-CoA synthetase. Therefore, we named the ORF encoding this LuxR-type regulator acsR, a regulator of the acsA gene expression.
Regulation of acsA expression by AcsR
The effect of the acsR mutation on acsA gene expression was monitored using an acsA::luxAB transcriptional reporter fusion during the entire growth cycle of V. vulnificus (Figure 3A). The ΔacsR mutant strain carrying pHKacsA::luxAB showed basal levels of luciferase activity which were 50 ~ 100-folds lower than the wild-type strain carrying the same reporter, indicating that acsA gene expression is activated by AcsR.
To determine whether the effect of AcsR on acsA expression is mediated by direct binding to the regulatory region of the acsA gene, a gel-shift assay was performed using recombinant AcsR protein (rAcsR) and a 284-bp DNA fragment that included an upstream region of the acsA gene (Figure 3B, left panel). Addition of rAcsR resulted in retarded mobility of the DNA fragment due to the complex formation of rAcsR and probe DNA in an AcsR dose-dependent manner. Since AcsR is a putative response regulator of two-component signal transduction system, the phosphorylated form of rAcsR was prepared by pre-incubation with acetyl-phosphate, and then used for a gel-shift assay (Figure 3B, right panel). No apparent increase was observed in the binding to the acsA promoter DNA. Rather that, the degree of DNA binding seemed to be reduced in case of rAcsR treated with acetyl-phosphate. Thus, rAcsR was used for the subsequent gel-shift assays without acetyl-phosphate treatment. Binding of rAcsR to the DNA was found to be specific, because excess unlabeled probe DNA abolished the retarded bands (Figure 3C). On the other hand, inclusion of unlabeled gap DNA did not disrupt complex formation between rAcsR and the acsA promoter.
Role of AcsS, a putative sensor kinase in expression of the acsA gene
It has been proposed that in Shewanella oneidensis, a regulatory system composed of SO_2742 (sensor kinase) and SO_2648 (response regulator) controls acetate metabolism by positively regulating the expression of SO_2743 (acetyl-CoA synthetase) . Amino acid sequences of SO_2648 shows 56% identity to those of V. vulnificus AcsR (VVMO6_00196). In addition, we found that there is an ORF (VVMO6_00191) showing 46% identity with the amino acid sequences of the cognate sensor kinase, SO_2742. Therefore, we examined whether acsA expression of V. vulnificus is also regulated by this putative sensor kinase by constructing a ΔacsS mutant (Additional file 2: Figure S1A). Deletion of the acsS gene in the mutant V. vulnificus was confirmed by PCR analysis using a set of primers specific to upstream and downstream regions of the acsS gene, which showed different sizes of PCR products from the mutant and wild-type strains (Additional file 2: Figure S1B). Effect of the acsS mutation on acsA gene expression was examined using the acsA::luxAB transcription reporter fusion (Figure 4). The ΔacsS mutant carrying pHKacsA::luxAB showed significantly reduced luciferase activity similar to the ΔacsR mutant carrying the same reporter plasmid. Thus, it appears that AcsS also controls expression of the acsA gene.
Phylogenetic analysis of AcsR and AcsS proteins
Phylogeny reconstitution using Neighbor-Joining analysis revealed a cluster containing AcsR proteins of various Vibrio spp., including V. parahaemolyticus, V. alginolyticus, V. harveyi, V. vulnificus, V. splendidus, V. cholerae, and Vibrio fischeri (also known as Aliivibrio fischeri) (Figure 5A). Other AcsR proteins derived from Pseudomonas spp. and E. coli showed closer relationship with these Vibrio AcsR proteins than those of Gram-positive bacteria. In the same manner, AcsS proteins of Vibrio spp. also form a clade (Figure 5B); however, AcsS proteins of Pseudomonas spp. and E. coli are grouped with those derived from Brucella melitensis and Gram-positive bacteria, respectively.
Role of AcsA, AcsR, and AcsS in bacterial growth in acetate-minimal medium
A V. vulnificus strain lacking acetyl-CoA synthetase (VVMO6_00187) was constructed by deleting the acsA gene (Additional file 3: Figure S2A). Successful deletion of the internal region of the acsA gene in the chromosome of V. vulnificus was confirmed by PCR showing a smaller PCR product from the ΔacsA mutant than that from the wild type (Additional file 3: Figure S2B). To assess the physiological role of AcsA, growth of the ΔacsA mutant was compared with wild type in a medium containing glucose or acetate as the sole carbon source [Figure 6A, (a) and (b)]. While the ΔacsA mutant retained the ability to grow in glucose-minimal medium at ~80% of the wild type, it did not show any apparent ability to use acetate for its growth. Growth of the ΔacsA mutant in acetate-minimal medium returned to that of the wild type when the ΔacsA mutant strain was complemented by carriage of a copy of the original acsA gene [Figure 6A, (c)].
Mutant V. vulnificus strains devoid of either acsR [response regulator; Figure 6B, (a) and (b)] or acsS [sensor histidine kinase; Figure 6C, (a) and (b)] showed defective growth in acetate-minimal medium compared to wild-type V. vulnificus. When the ΔacsR mutant strain was complemented with the intact acsR gene, the mutant gained the ability to use acetate as a carbon source [Figure 6B, (c)]. In the same manner, a complemented ΔacsS mutant also exhibited the ability to grow in acetate-minimal medium at almost the same level as the wild-type growth [Figure 6C, (c)].
These results suggest that growth defect of ΔacsR and ΔacsS mutant in acetate-minimal medium is caused by attenuated production of acetyl-CoA synthetase. To examine this possibility, ΔacsR and ΔacsS mutant strains carrying a copy of the original acsA gene were constructed, and monitored for their growth in acetate-minimal medium (Figure 6D). However, growth of both the ΔacsR and ΔacsS mutant in acetate-minimal medium was not restored when these strains had the plasmid containing the acsA gene suggesting that control of acetate metabolism by AcsS/AcsR extends beyond regulation of acsA expression.
cAMP-independent catabolite repression of acsA expression
Acetyl-CoA synthetase is required for normal levels of V. vulnificus growth in media with acetate as the sole source, which was evidenced by the defective growth of the ΔacsA mutant in an acetate medium (Figure 6A). This mutant, however, did not show any defect in growth in a glucose-minimal medium. Thus, acsA expression may not be induced when cells are growing in the presence of other carbon sources such as glucose. This speculation implies the presence of another regulatory pathway for acsA expression in V. vulnificus. Therefore, expression of the acsA gene was monitored in wild type growing in a glycerol-minimal medium (Figure 7A). Addition of glucose to the glycerol-minimal medium reduced the expression of the acsA::luxAB fusion, indicating that acsA expression might be under the regulation of catabolite repression. In a subsequent experiment, we examined whether catabolite repression of acsA::luxAB activity is mediated by a well-known regulator, cAMP-CRP. The reporter plasmid of the acsA::luxAB fusion was transferred into a Δcya mutant, which was unable to synthesize cyclic AMP . There was no difference in acsA::luxAB expression in Δcya mutant and the wild type during the entire growth cycle of V. vulnificus including the phase at OD595 = 1.0 shown in Figure 7B. This result may indicate that repression of acsA expression by glucose is not mediated by cAMP-CRP in V. vulnificus. To investigate the mechanism underlying catabolite repression-like regulation of acsA expression, glucose was added to ΔacsR mutant growing with glycerol as a carbon source. Luciferase activities of acsA::luxAB were basal during the entire growth of the ΔacsR mutant in glycerol-minimal medium. Addition of glucose, however, did not cause any repressive effect on acsA expression (Figure 7C), which implies that the glucose effect on acsA expression might be mediated by AcsR.
The ability of a bacterium to use a specific carbon source is tightly controlled to assure the most efficient use of metabolic pathways under specific conditions, including those of characteristic of the host environment. Acetyl-CoA synthetase is an enzyme that converts acetate into acetyl-CoA, which is crucial in utilizing acetate as a carbon source . E. coli is able to grow by utilizing a wide range of acetate concentrations (2.5 to 50 mM), but an acsA-mutated E. coli grows poorly in media containing a relatively low concentration of acetate (<10 mM). In contrast, mutants deficient in the ack and pta genes encoding the second acetyl-CoA producing system grow poorly in a high concentration of acetate (>25 mM) . A metabolic phenomenon called “acetate switch” is a good example of how microorganisms such as E. coli modulate their metabolism under various growth conditions . During exponential growth, the bacteria consume carbon sources such as glucose via the Ack-Pta system in order to produce and excrete acetate. When these acetogenic sugars become exhausted, the cells then begin to import and utilize environmental acetate via the action of acetyl-CoA synthetase. The role of acetyl-CoA synthetase varies according to the metabolic versatility of the microorganism. A mutant P. aeruginosa unable to use ethanol had lost its acetyl-CoA synthetase activity . A study using an acsA::lacZ fusion indicated that transcription of the acsA gene is induced by acetate in an ErdR-dependent manner . Interestingly, the amino acid sequence of ErdR shows a 52% identity with that of AcsR of V. vulnificus. In the case of V. fischeri, a symbiotic microbe with an squid, the ainS mutant defective in production of octanoyl-homoserine lactone also lost the ability to perform an “acetate switch” because it had defects in the expression of the acsA gene . Their study demonstrated that acetate switch is controlled by quorum sensing and plays a role in light organ symbiosis by V. fischeri.
Experimental information regarding the metabolic versatility of V. vulnificus has not yet been available in the metabolic pathways utilizing acetate. When acetate was provided as a sole carbon source to V. vulnificus, the acsA gene product was essential for its growth (Figure 6A). AcsA is also used by the cell to recover catabolically produced acetate excreted during sugar metabolism. When the concentration of acetate was high (>20 mM), however, growth of wild-type V. vulnificus was affected (Kim, M-J. and Park, S-J., unpublished data). Therefore, V. vulnificus mutants devoid of ack and/or pta genes need to be characterized to fully understand acetate metabolism of V. vulnificus by comparing it to the growth of the ΔacsA mutant. These ΔacsA, ΔacsR, and ΔacsS mutant V. vulnificus strains should be examined to see whether they can perform the “acetate switch”, and this process is also regulated by quorum sensing in V. vulnifucus.
In E. coli, acsA expression is repressed by glucose, and this catabolite repression is mediated by CRP-cAMP . Although acsA expression was also repressed by the addition of glucose in V. vulnificus (Figure 7A), catabolite repression of acsA expression does not appear to be mediated by cAMP (Figure 7B). Interestingly, cAMP-independent catabolite repression of acsA expression was not observed in the acsR mutant (Figure 7C), which already had a greatly reduced expression. Thus, this study cannot rule out the possibility that AcsR might be involved in catabolite repression-like regulation of acsA expression. The regulatory mechanism underlying this catabolite repression needs to be elucidated in future studies. Transcription factors mediating catabolite repression via cAMP-CRP-independent manners have been reported in some microorganisms. AccR is known as a master regulator involved in carbon catabolite repression of the anaerobic catabolism of aromatic compounds in Azorcus sp. . In Pseudomonas, Crc, a translational repressor of multiple pathways linked to catabolite repression is known to be modulated by small RNAs, crcZ and crcY .
Expression of the acetyl-CoA synthetase gene is significantly reduced in V. vulnificus devoid of acsR or acsS using the luxAB-transcriptional reporter fused with the regulatory region of acsA (Figures 3A and 4). While the acsA mRNA level in the acsR mutant was decreased to 38% of wild type (Figure 2D), luciferase activity of the acsA::luxAB fusion was dramatically reduced in the mutant (Figure 3A). This discrepancy may be derived from the drawback of the acsA::luxAB fusion plasmid. Because this fusion plasmid is present in multiple copies, its expression level could be amplified or variable under certain conditions. Alternatively, in addition to direct transcriptional regulation, AcsS/AcsR might indirectly affect acsA expression at the post-transcriptional level.
Absence of the AcsR or AcsS protein resulted in a severe growth defect in the presence of acetate as a carbon source (Figure 6B and C). The subsequent experiment did not provide the evidence that the growth defect of the ΔacsR and ΔacsS mutants was caused from bacterial inability to express acetyl-CoA synthetase (Figure 6D). It is possible that the acsA gene in the complementation plasmid pRKacsA fails to express in the ΔacsR and ΔacsS mutants. Otherwise, Acs activity may be differentially affected in the ΔacsR and ΔacsS mutants from the wild type or ΔacsA mutant at a post-transcriptional level. In any cases, these data suggest that AcsR and AcsS are necessary for the acsA expression or Acs activity.
The positive effect of AcsR in acsA expression occurred through a direct interaction between this transcriptional factor and the regulatory region of acsA as shown in gel-shift assays (Figure 3B and C). It remains to be elucidated whether AcsR functions as a cognate response regulator of AscS in acsA transcription.
AcsR was found as a down-expressed protein in the ΔvarA mutant V. vulnificus along with 166 other genes showing the altered expression (Figure 1 and Additional file 1: Table S1). Both down- and up-regulated genes were found in the ΔvarA mutant as reported in the transcriptome profiling of the ΔuvrY mutant of Photorhabdus luminescens, a varA homologous gene of the insect pathogen . The comparative transcriptomic analysis between wild type and ΔuvrY indicated that UvrY negatively regulates flagella formation/motility, and iron acquisition, and positively regulates other processes, such as protease formation, resistance against oxidative stresses, and host colonization.
Initially AcsR was identified as a down-expressed clone in the ΔvarA mutant (Figure 1A and Additional file 1: Table S1), and the acsA gene was subsequently identified as a down-regulated gene in the ΔacsR mutant (Table 1 and Figure 2D). Luciferase activity of the acsA::luxAB fusion was also significantly reduced in the ΔvarA mutant V. vulnificus (Kim, M-J. and Park, S-J., unpublished data) indicating that the regulatory cascades for acsA expression are composed of the VarS/VarA system as an upstream component and the AcsR as a downstream component. It is not clear if VarA is directly involved in the expression of the acsR gene. It might be possible that acsR expression is controlled via csrB/csrC regulators, of which expressions are tightly regulated by VarA . Alternatively, VarA could directly modulate the expression of the acsR gene by binding to its upstream region.
In contrast to a large number of differentially expressed genes in the ΔvarA mutant, only two dozen genes were found at different levels between wild type and the ΔacsR mutant (Table 1), indicating that AcsR has a narrower spectrum of the target genes than VarA. However, it is likely that a portion of differentially expressed genes in the ΔvarA mutant are not directly regulated by VarS/VarA, rather that they are directly controlled via other regulatory systems such as CsrA/csrB/csrC system functioning at downstream of the VarS/VarA system.
Down-regulated genes in the ΔacsR mutant include the genes encoding MASH pilus. In V. cholerae, formation of MASH pilus was found specifically repressed in vivo, and thus it is considered as anti-colonization factor . The msh genes encoding MASH pilus were transcribed as two adjacent transcripts, i.e., the secretory genes and the structural genes . ToxT protein, a key regulator for V. cholerae virulence, represses transcription of these msh genes . In this study, mshMEG genes in the secretory operon and mshAF in the structural operon were found at a lower level in the ΔacsR mutant indicating that overall expression of msh genes was affected in this mutant. A possibility that AcsR activates transcription of these msh genes via direct binding to the two msh promoter regions will be examined, and if it is the case, the AcsR-mediated control of MASH in V. vulnficus should be evaluated for its physiological implication.
Transcriptome analysis of the ΔvarA mutant by comparison with wild-type V. vulnificus led us to identify a positive transcription factor, AcsR, for acetyl-CoA synthetase. Transcription of the acsA gene for acetyl-CoA synthetase by AcsR and AcsS is critical for bacterial growth when using acetate as a carbon source.
Bacterial strains and culture conditions
The bacterial strains and plasmids used in this study are listed in Table 2. E. coli strains used for manipulation of various plasmid DNAs were grown at 37°C in Luria-Bertani (LB) broth or on LB agar plate supplemented with the appropriate antibiotics. V. vulnificus strains were cultured at 30°C in LB medium supplemented with an additional 2% NaCl (LBS). Antibiotics were used at the following concentrations: ampicillin (100 μg/ml), chloramphenicol (25 μg/ml), kanamycin (50 μg/ml), and tetracycline (15 μg/ml) for E. coli, and ampicillin (500 μg/ml), chloramphenicol (2 μg/ml), kanamycin (100 μg/ml), and tetracycline (3 μg/ml) for V. vulnificus. To measure luciferase activities derived from a luxAB-transcription reporter fusion, the bacterial cells of V. vulnificus were grown in AB medium with 1% glycerol (300 mM NaCl, 50 mM MgSO4, 0.2% casamino acids, 1 mM L-arginine, and 10 mM potassium phosphate, pH 7.5).
To compare the growth pattern of V. vulnificus strains, each strain was grown in an NaCl-enriched M9 minimal medium (90 mM Na2HPO4, 22 mM KH2PO4, 18 mM NH4Cl, 2 mM MgSO4, 0.1 mM CaCl2, and 2.5% NaCl) with either 22 mM glucose or 10 mM sodium acetate as a carbon source, and bacterial growth was monitored by measuring the optical density at 595 nm (OD595). Overnight cultures of various V. vulnificus strains were prepared in LBS, washed with an NaCl-enriched M9 minimal medium without carbon source, and then used to inoculate into the fresh medium either with glucose or acetate at OD595 = 0.05.
A customized V. vulnificus DNA microarray (E-biogene) was used, which contained information of all 4,562 ORFs found in the genome of V. vulnificus MO6-24/O. Total RNAs were extracted from V. vulnificus strains grown to an OD595 of 1.0 using the RNeasy® Mini Kit (Qiagen). The integrity of bacterial total RNAs was checked by capillary electrophoresis with an Agilent 2100 bioanalyzer (Agilent Technologies) and further purified using the RNeasy Mini kit. cDNA probes were prepared by reverse transcription of total RNA (25 μg) in the presence of aminoallyl-dUTP and 6 μg of random primers (Invitrogen). Followed by coupling of Cy3-dye (for a reference) or Cy5-dye (for a test sample) (Amersham Pharmacia), Cy3- or Cy5-labeled cDNA probes were added for hybridizationon a microarray slide. Hybridization images on the slide were obtained using a GenePix 4000A scanner (Axon Instruments). The analysis of the microarray data was performed using GenePix Pro 6.0 (Axon Instruments). Fluorescent spots and local background intensities were quantified using Agilent GeneSpring 7.3.1 software package (Agilent Technologies) to obtain gene expression ratios (mutant versus the wild type). Agilent Feature Extraction Software (version 184.108.40.206) was used for background subtraction. Signals were calculated for both Cy3 and Cy5 channels by subtracting the median of background signals from the median of spot signal of each spot. Normalization was carried out using global loess algorithm  using Genowiz 4.0TM (Ocimum Biosolutions). The averages of the normalized ratios were calculated by dye-normalized signals of Cy3 and Cy5 channels. All samples were assayed in three different biological replicates. All measurements were performed on three technical replicates. An one-sample Student t-test was calculated to test whether the mean normalized ratio for the gene is statistically significant (P-value <0.05) using MultiExperiment Viewer (The Institute for Genome Research, http://www.tm4.org/mev.html) 4.8.1 version. A putative functional role of each gene was grouped by Cluster of Orthologous Groups (COG) of protein designation [28,61].
The microarray data have been deposited in the GEO database (http://www.ncbi.nlm.nih.gov/geo) under accession no. GSE67192.
Quantitative measurement of the transcripts of a putative LuxR-type regulator and acetyl-CoA synthetase
The cellular levels of the corresponding mRNAs were evaluated by real-time PCR. Total RNA was isolated from wild-type or mutant V. vulnificus strains using the RNeasy® Mini Kit and treated with the RNase-free DNase I (TaKaRa). cDNA was synthesized from 4 μg of RNA using the ImProm-IITM RT system (Promega) following the manufacturer’s directions. cDNA was then analyzed with the Light Cycler 480 II Real-Time PCR System (Roche Applied Science) using LightCycler 490 DNA SYBR Green I Master (Roche Applied Science). Real-time PCR was carried out in triplicate in a 96-well plate using the specific primers listed in Additional file 4: Table S2. The gap gene encoding NAD-dependent glyceraldehyde-3-phosphatase of V. vulnificus was used as an endogenous control for the reactions.
Data are presented as mean ± standard deviation from three independent experiments. Statistical analyses for pair-wise comparison were performed using Student t-test (SYSTAT, SigmaPlot version 11; Systat Software Inc.) to evaluate the statistical significance of the results. Differences were considered significant when P <0.05. Data with P <0.01 are indicated with two asterisks, whereas data with P-values between 0.01 and 0.05 are indicated with a single asterisk.
Construction of deletion mutants of V. vulnificus and complementation of the mutant strains
For construction of the ΔvarA mutant, the upstream region of the varA gene was amplified from the genomic DNA of V. vulnificus MO6-24/O with the primers, varAupF and varAupR (Additional file 4: Table S2). The resultant 501-bp DNA fragment was then digested with SalI and PstI and ligated into pBlueScript (II) SK (+) to produce pSKvarAU. The downstream region of the varA gene was amplified using the primers, varAdownF and varAdownR (Additional file 4: Table S2). The resultant DNA fragment of 520-bp was treated with PstI and XbaI and ligated into pSKvarAU to yield pSKvarAUD. The 1,021-bp SalI-XbaI DNA fragment of pSKvarAUD was transferred into a suicide vector pDM4 , resulting in formation of pDMΔvarA. The plasmid pDMΔvarA in SM10 λpir  was mobilized to V. vulnificus MO6-24/O, and the conjugants were selected by plating the conjugation mixture of E. coli and V. vulnificus on LBS plates supplemented with 2 μg/ml chloramphenicol. A colony with characteristics indicating a double homologous recombination event (resistance to 5% sucrose and sensitivity to chloramphenicol) was further confirmed by PCR using the primers, varAupF and varAdownR and then named MJ1.
ΔacsR mutant and complementation strains
For construction of the ΔacsR mutant, the upstream (410-bp) and downstream (424-bp) regions of the acsR gene were amplified using the primer set of luxRupF/luxRupR and luxRdownF/luxRdownR, respectively (Additional file 4: Table S2). The ApaI-SacI DNA fragment of pSKacsRUD was transferred into pDM4 to produce pDMΔacsR, which was then used to generate the ΔacsR mutant, as described above. For complementation of the mutant, a 951-bp DNA fragment was amplified using acsRcomF and acsRcomR (Additional file 4: Table S2), which contains a whole acsR ORF and a 315-bp upstream region of the acsR gene. This DNA fragment was then cloned into a broad-host-range vector, pRK415  to produce pRKacsR. This acsR +-containing plasmid was mobilized to the ΔacsR strain via conjugation. Wild type carrying pRK415 and the ΔacsR strain carrying pRK415 were also prepared in the same manner to serve as controls.
ΔacsS mutant and complementation strains
A plasmid (pSKacsSUD) was made to include the upstream (710-bp) and downstream (528-bp) regions of the acsS gene, which had been amplified by the following primer sets, acsSupF/acsSupR and acsSdownF/acsSdownR (Additional file 4: Table S2). The XhoI-XbaI DNA fragment of the resultant plasmid was ligated into pDM4 to produce pDMΔacsS, which was used to make the ΔacsS mutant, as described above. For complementation of the mutant, a 3,432-bp DNA fragment was amplified using acsScomF and acsScomR (Additional file 4: Table S2). This DNA fragment was then cloned into pRK415 to produce pRKacsS that was then mobilized to the ΔacsS strain.
ΔacsA mutant and complementation strains
To inactivate the acsA gene, the primer sets of acsAupF/acsAupR and acsAdownF/acsAdownR (Additional file 4: Table S2) were utilized to produce the 732-bp upstream and the 525-bp downstream regions of the acsA gene, respectively. A 1,953-bp DNA fragment of pSKacsAUD was cloned to pDM4 to make pDMΔacsA, which was used to generate an ΔacsA mutant. To complement the original acsA gene into the ΔacsA mutant, pRKacsA was constructed by cloning the 2,241-bp acsA DNA fragment into the HindIII/BamHI site of pRK415 and transferred into the ΔacsA strain as described above.
To delete the cya gene in V. vulnificus, pDMΔcya  was transferred to MO6-24/O via conjugation, and a V. vulnificus colony with characteristics indicating a double homologous recombination event was selected and named KJLΔcya.
Construction of a luxAB-transcription reporter fusion with the acsA promoter and measurement of its expression
The plasmid pHKacsA::luxAB was constructed by inserting a 284-bp DNA fragment including the regulatory region for acsA into the upstream region of the luxAB gene in pHK0011  by utilizing restriction sites for KpnI and BamHI. pHKacsA::luxAB in E. coli SM10λpir was conjugated to ΔacsR and wild-type strains. Aliquots of overnight-grown cultures were inoculated to fresh AB broth containing tetracycline (3 μg/ml) and incubated with shaking at 30°C.
Luciferase activity in the bacterial cells carrying these fusions was measured in the presence of 0.006% (v/v) n-decyl aldehyde using a luminometer (TD-20/20 Luminomter, Turners Designs). Specific bioluminescence was calculated by normalizing the relative light units (RLU) with respect to cell mass (OD595).
Preparation of polyclonal antibodies against recombinant AcsR and western blot analysis
A 636-bp DNA fragment encompassing the acsR ORF was amplified using two primers, racsRF and racsRR (Additional file 4: Table S2), and then cloned into an expression vector, pET28b (+) (Novagen). rAcsRwas overexpressed by adding isopropyl thio-β-D-galactoside at a concentration of 1 mM and purified using a TALON® affinity column (Clontech). Purified rAcsR was used to generate polyclonal antibodies by three immunizations of SPF/VAF outbred rats (200 μg AcsR per immunization) at 3-week intervals. Cellular extracts were prepared by sonicating harvested cells in TNT buffer [10 mM Tris-HCl (pH 8.0), 150 mM NaCl, and 0.05% (v/v) Tween 20]. Cell lysates were separated by SDS-PAGE and transferred to nitrocellulose membranes (Millipore). Membranes were blocked with 5% skim-milk in Tris-buffered saline with Tween 20 (TBST; 150 mM NaCl, 50 mM Tris-HCl, and 0.1% Tween 20) and then incubated overnight at 4°C with the anti-AcsR polyclonal antibodies (1:2,000 dilution). After incubation with alkaline phosphate-conjugated secondary antibodies, immunoreactive bands were visualized using nitro blue tetrazolium and 5-bromo-4-chloro-3-indolyl phosphate.
A 284-bp DNA fragment including the upstream region of the acsA gene was labeled with [γ-32P]ATP using T4 polynucleotide kinase. A labeled DNA probe (225 nM) was incubated with various concentrations of rAcsR (0.5 – 5 μM) for 30 min at 37°C. After the reactions were stopped, aliquots of the reaction mixtures were separated on a 6% non-denaturing polyacrylamide gel.
To prepare phosphorylated rAcsR used for gel shift assays, rAcsR (60 μg/ml) was incubated with for 1 h at 30°C in a buffer containing 100 mM Tris-HCl (pH 7.0), 10 mM MgCl2, 125 mM KCl, and 50 mM dilithium acetyl phosphate (Sigma) as described .
For competition analysis, the identical but unlabeled DNA probe was included in the reaction mixture at a concentration of 716 nM. As a nonspecific control, the gap DNA encoding glyceraldehyde 3 phosphate dehydrogenase was included in the binding reaction at 716 nM.
Phylogenetic analysis of AcsR and AcsS proteins
The evolutionary history was inferred using the Neighbor-Joining method . The percentages of replicate trees in which the associated taxa clustered together in the bootstrap test (1000 replicates) were shown next to the branches . The tree is drawn to scale, with branch lengths in the same units as those of the evolutionary distances used to infer the phylogenetic tree. The evolutionary distances, computed using the Poisson correction method , were in the units of the number of amino acid substitutions per site. Evolutionary analyses were conducted in MEGA6 . The scale bar indicates the number of amino acid substitutions per site.
Relative light unit
CLUSTER of orthologous groups
Strom MS, Paranjpye RN. Epidemiology and pathogenesis of Vibrio vulnificus. Microbes Infect. 2000;2:177–88.
Park NY, Lee JH, Kim MW, Jeong HG, Lee BC, Kim TS, et al. Identification of the Vibrio vulnificus wbpP gene and evaluation of its role in virulence. Infect Immun. 2006;74:721–8.
Wright AC, Morris Jr JG, Maneval Jr DR, Richardson K, Kaper JB. Cloning of the cytotoxin-hemolysin gene of Vibrio vulnificus. Infect Immun. 1985;50:922–4.
Kim YR, Lee SE, Kook H, Yeom JA, Na HS, Kim SY, et al. Vibrio vulnificus RTX toxin kills host cells only after contact of the bacteria with host cells. Cell Microbiol. 2008;10:848–62.
Lee JH, Kim MW, Kim BS, Kim SM, Lee BC, Kim TS, et al. Identification and characterization of the Vibrio vulnificus rtxA essential for cytotoxicity in vitro and virulence in mice. J Microbiol. 2007;45:146–52.
Miyoshi S, Shinoda S. Microbial metalloproteases and pathogenesis. Microbes Infect. 2000;2:91–8.
Bahrani K, Oliver JD. Studies on the lipopolysaccharide of virulent and avirulent strains of Vibrio vulnificus. Biochem Cell Biol. 1990;68:547–51.
Testa J, Daniel LW, Kreger AS. Extracellular phospholipase A2 and lysophospholipase produced by Vibrio vulnificus. Infect Immun. 1984;45:458–63.
Wright AC, Simpson LM, Oliver JD, Morris Jr JG. Role of iron in the pathogenesis of Vibrio vulnificus. Infect Immun. 1981;34:503–7.
Kim YR, Rhee JH. Flagellar basal body flg operon as a virulence determinant of Vibrio vulnificus. Biochem Biophys Res Commun. 2003;304:405–10.
Lee J, Rho JB, Park K, Kim CB, Han Y, Choi SH, et al. Role of flagellum and motility in pathogenesis of Vibrio vulnificus. Infect Immun. 2004;72:4905–10.
Lee KJ, Jeong CS, An YJ, Lee HJ, Park SJ, Seok YJ, et al. FrsA functions as a cofactor-independent decarboxylase to control metabolic flux. Nat Chem Biol. 2011;7:434–6.
Wong SM, Carroll PA, Rahme LG, Asubel FM, Calderwood SB. Modulation of expression of the ToxR regulon in Vibrio cholera by a member of the two component family of response regulators. Infect Immun. 1998;66:5854–61.
Pernestig AK, Melefors O, Georgellis D. Identification of UvrY as the cognate response regulator for the BarA sensor kinase in Escherichia coli. J Biol Chem. 2001;276:225–31.
Altier C, Suyemoto M, Ruiz AI, Burnham KD, Maurer R. Characterization of two novel regulatory genes affecting salmonella invasion gene expression. Mol Microbiol. 2000;35:635–46.
Heebs S, Haas D. Regulatory roles of the GacS/GacA two-component system in plant-associated and other gram-negative bacteria. Mol Plant Microbe Interact. 2001;14:1351–63.
Molofsky AB, Swanson MS. Differentiate to thrive: lessons from the Legionella pneumophila life cycle. Mol Microbiol. 2004;53:29–40.
Lapouge K, Schubert M, Allain FHT, Haas D. Gac/Rsm signal transduction pathway of γ-proteobacteria: from RNA recognition to regulation of social behavior. Mol Microbiol. 2008;67:241–53.
Seyell E, Melderen LV. The ribonucleoprotein Csr network. Int J Mol Sci. 2013;14:22117–31.
Timmermans J, Van Melderen L. Post-translational global regulator by CsrA in bacteria. Cell Mol Life Sci. 2010;67:2897–908.
Jang J, Jung KT, Yoo CK, Rhie GE. Regulation of hemagglutinin/protease expression by the VarS/VarA-CsrA/B/C/D system in Vibrio cholerae. Microb Pathog. 2010;48:245–50.
Jang J, Jung KT, Park J, Yoo CK, Rhie GE. The Vibrio cholerae VarS/VarA two-component system controls the expression of virulence proteins through ToxT regulation. Microbiology. 2011;157:1466–73.
Tsou AM, Liu Z, Cai T, Zhu J. The VarS/VarA two-component system modulates the activity of the Vibrio cholerae quorum-sensing transcriptional regulator HapR. Microbiology. 2011;157:1620–8.
Lenz DH, Miller MB, Zhu J, Kulkami RV, Bassler BL. CsrA and three redundant small RNAs regulate quorum sensing in Vibrio cholerae. Mol Microbiol. 2005;58:1186–202.
Gauthier JD, Jones MK, Thiaville P, Joseph JL, Swain RA, Krediet CJ, et al. Role of GacA in virulence of the Vibrio vulnificus. Microbiology. 2010;156:3722–33.
Jones MK, Warner EB, Oliver JD. csrA inhibits the formation of biofilms by Vibrio vulnificus. Appl Environ Microbiol. 2008;74:7064–6.
Brown TDK, Jones-Mortimer MC, Kornberg HL. The enzymatic interconversion of acetate and acetyl-coenzyme A in Escherichia coli. J Gen Microbiol. 1977;102:327–36.
Tatusov RL, Koonin EV, Lipman DJ. A genomic prospective on protein families. Science. 1997;278:631–7.
Okamura-Ikeda K, Ohmura Y, Fujiwara K, Motokawa Y. Cloning and nucleotide sequence of the gcv operon encoding the Escherichia coli glycine-cleavage system. Eur J Biochem. 1993;216:539–48.
Jitprasutwit S, Ong C, Juntawieng N, Ooi WF, Hemsley CM, Vattanaviboon P, et al. Transcriptional profiles of Burkholderia pseudomallei reveal the direct and indirect roles of sigma E under oxidative stress conditions. BMC Genomics. 2014;15:787.
Noor R, Murata M, Nagamitsu H, Klein G, Raina S, Yamada M. Dissection of sigma (E)-dependent cell lysis in Escherichia coli: roles of RpoE regulators RseA, RseB and periplasmic folding catalyst PpiD. Genes Cells. 2009;14:885–99.
Lin JW, Lu HC, Chen HY, Weng SF. The pkl gene encoding pyruvate kinase I links to the luxZ gene which enhances bioluminescence of the lux operon from Photobacterium leiognathi. Biochem Biophys Res Commun. 1997;239:228–34.
Daddaoua A, Krell T, Ramos JL. Regulation of glucose metabolism in Pseudomonas: the phosphorylative branch and entner-doudoroff enzymes are regulated by a repressor containing a sugar isomerase domain. J Biol Chem. 2009;284:21360–8.
Miller PF, Gambino LF, Sulavik MC, Gracheck SJ. Genetic relationship between soxRS and mar loci in promoting multiple antibiotic resistance in Escherichia coli. Antimicrob Agents Chemother. 1994;38:1773–9.
McDermott PF, McMurry LM, Podglajen I, Dzink-Fox JL, Schnieders T, Draper MP, et al. The marC gene of Escherichia coli is not involved in multiple antibiotic resistance. Antimicrob Agents Chemother. 2008;52:382–3.
Talavera MA, DeLa Cruz EM. Equilibrium and kinetic analysis of nucleotide binding to the DEAD-box RNA helicase DbpA. Biochemistry. 2005;44:959–70.
Ye L, Zheng X, Zheng H. Effect of sypQ gene on poly-N-acetylglucosamine biosynthesis in Vibrio parahaemolyticus and its role in infection process. Glycobiology. 2014;24:351–8.
Douzi B, Spinelli S, Blangy S, Roussel A, Durand E, Brunet YR, et al. Crystal structure and self-interaction of the type VI secretion tail-tube protein from enteroaggregative Escherichia coli. PLoS One. 2014;9, e86918.
Natale AM, Duplantis JL, Piasta KN, Falke JJ. Structure, function, and on-off switching of a core unit contact between CheA kinase and CheW adaptor protein in the bacterial chemosensory array: a disulfide mapping and mutagenesis study. Biochemistry. 2013;52:7753–65.
Deutschbauer A, Price MN, Wetmore KM, Shao W, Baumohl JK, Xu Z, et al. Evidence-based annotation of gene function in Shewanella oneidensis MR-1 using genome-wide fitness profiling across 121 conditions. PLoS Genet. 2011;7, e1002385.
Lee HJ, Park SJ, Choi SH, Lee KH. Vibrio vulnificus rpoS expression is repressed by direct binding of cAMP-cAMP receptor protein complex to its two promoter regions. J Biol Chem. 2008;283:30438–50.
Starai VJ, Escalante-Semerena JC. Acetyl-coenzyme A synthetase (AMP forming). Cell Mol Life Sci. 2004;61:2020–30.
Kumar S, Tishel R, Eisenbach M, Wolfe AJ. Cloning, characterization, and functional expression of acs, the gene which encodes acetyl coenzyme A synthetase in Escherichia coli. J Bacteriol. 1995;177:2878–86.
Wolfe AJ. The acetate switch. Microbiol Mol Biol Rev. 2005;69:12–50.
Kretzschmar U, Schobert M, Gorisch H. The Pseudomonas aeruginosa acsA gene, encoding an acetyl-CoA synthetase, is essential for growth on ethanol. Microbiology. 2001;147:2671–7.
Kretzschmar U, Khodaverdi, Adrian L. Transcriptional regulation of the acetyl-CoA synthetase gene acsA in Pseudomonas aeruginosa. Arch Microbiol. 2010;192:685–90.
Studer SV, Mandel MJ, Ruby EG. AinS quorum sensing regulates the Vibrio fischeri acetate switch. J Bacteriol. 2008;190:5915–23.
Castano-Cerezo S, Bernal V, Blanco-Catala J, Iborra JL, Canovas M. cAMP-CRP co-ordinates the expression of the protein acetylation pathway with central metabolism in Escherichia coli. Mol Microbiol. 2011;82:1110–28.
Valderrama JA, Shingler V, Carmona M, Diaz E. AccR is a master regulator involved in carbon catabolite repression of the anaerobic catabolism of aromatic compounds in Azoarcus sp. CIB J Biol Chem. 2014;289:1892–904.
Garcia-Maurino SM, Perez-Martinez I, Amardor CI, Canosa I, Santero E. Transcriptional activation of the CrcZ and CrcY regulatory RNAs by the CbrB response regulator in Pseudomonas putida. Mol Microbiol. 2013;89:189–205.
Krin E, Derzelle S, Bedard K, Adib-Conquy M, Turlin E, Lenormand P, et al. Regulatory role of UvrY in adaptation of Photorhabdus luminescens growth in inside the insect. Environ Microbiol. 2008;10:1118–34.
Hsiao A, Liu Z, Joelsson A, Zhu J. Vibrio cholerae virulence regulator-coordinated evasion of host immunity. Proc Natl Acad Sci U S A. 2006;103:14542–7.
Marsh JW, Taylor RK. Genetic and transcriptional analyses of the Vibrio cholerae mannose-sensitive hemagglutinin type 4 pilus gene locus. J Bacteriol. 1999;181:1110–7.
Hsiao A, Xu X, Kan B, Kukarni RV, Zhu J. Direct regulation by the Vibrio cholerae regulator ToxT modulate colonization and anticolonization pilus expression. Infect Immun. 2009;77:1383–8.
Simon R, Priefer U, Puhler A. A broad host range mobilization system for in vivo genetic engineering: transposon mutagenesis in gram negative bacteria. Biogeosciences. 1983;1:784–91.
Wright AC, Simpson LM, Oliver JD, Morris Jr JG. Phenotypic evaluation of acapsular transposon mutants of Vibrio vulnificus. Infect Immun. 1990;58:1769–73.
Milton DL, O'Toole R, Hörstedt P, Wolf WH. Flagellin A is essential for the virulence of Vibrio anguillarum. J Bacteriol. 1996;178:1310–9.
Jeong HS, Jeong KC, Choi HK, Park K, Lee KH, Rhee JH, et al. Differential expression of Vibrio vulnificus elastase gene in a growth phase-dependent manner by two different types of promoters. J Biol Chem. 2001;276:13875–80.
Keen NT, Tamaki S, Kobayashi D, Trollinger D. Improved broad-host-range plasmids for DNA cloning in gram-negative bacteria. Gene. 1988;70:191–7.
Smyth FK, Speed TP. Normalization of cDNA microarray data. Method. 2003;21:265–73.
Tatusov RL, Fedorova ND, Jackson JD, Jacobs AR, Kiryutin B, Koonin EV, et al. The COG database: an updated version includes eukaryotes. BMC Bioinform. 2003;4:41.
Lynch AS, Lin ECC. Transcriptional control mediated by the ArcA two component response regulator protein of Escherichia coli: characterization of DNA binding at target promoters. J Bacteriol. 1996;178:6235–49.
Saitou N, Nei M. The neighbor-joining method: A new method for reconstructing phylogenetic trees. Mo Biol Evol. 1987;4:406–25.
Felsenstein J. Confidence limits on phylogenies: an approach using the bootstrap. Evolution. 1985;39:783–91.
Zuckerkandl E, Pauling L. Evolutionary divergence and convergence in proteins. In: Bryson V, Vogel HJ, editors. Evolving Genes and Proteins. New York: Academic; 1965. p. 97–166.
Tamura K, Stecher G, Peterson D, Filipski A, Kumar S. MEGA6: molecular evolutionary genetics analysis version 6.0. Mol Biol Evol. 2013;30:2725–9.
Authors thank K.-J. Lee for constructing a Δcya mutant. Authors thank Dr. J-C Cho (Hankuk Univ. Foreign Studies), H-J Kim (HUFS), and J-A. Kim (Sogang Univ.) for analyzing the phylogenetic relationships of AcsR and AcsS. This work was supported by a grant from the National Research Foundation of Korea (NRF) (No. 2010-0029116) and a 2012 faculty research grant from Yonsei University College of Medicine (6-20120030). This study was also supported by the Mid-Career Researcher Program through a NRF grant funded by the Ministry of Education, Science and Technology, Korea (No. 2009-0092822 to K.-H.L.).
All authors declare that they have no competing interests.
MJK, JK, HYL and HJN performed experiments and analyzed data. KHL and SJP analyzed data and wrote the manuscript. All authors read and approved the final manuscript.
Genes showing altered expression in the ΔvarA mutant compared to wild-type V. vulnificus.
Construction of ΔacsS mutant V. vulnificus. A - Construction of V. vulnificus mutant defective in acsS by using two sets of primers (indicated by horizontal arrows with the primer names listed in Additional file 4: Table S2) to delete VVMO6_00191. A bar represents the length of DNA equivalent to 500 bp; B - Deletion of the corresponding gene was examined by PCR using a pair of primers, acsSupF and acsSdownR. SM indicates DNA size markers.
Construction of ΔacsA mutant V. vulnificus. A - Construction of V. vulnificus mutant defective in acsA by using two sets of primers (indicated by horizontal arrows with the primer names listed in Additional file 4: Table S2) to delete VVMO6_00187. A bar represents the length of DNA equivalent to 500 bp; B - Deletion of the corresponding gene was examined by PCR using a pair of primers, acsAupF and acsAdownR. SM indicates DNA size markers.
Oligonucleotide primers used in this study.
About this article
Cite this article
Kim, M.J., Kim, J., Lee, H.Y. et al. Role of AcsR in expression of the acetyl-CoA synthetase gene in Vibrio vulnificus . BMC Microbiol 15, 86 (2015). https://doi.org/10.1186/s12866-015-0418-4
- Vibrio vulnificus
- Acetate metabolism
- Acetyl-CoA synthetase