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  • Research article
  • Open Access

Identification of the Streptococcus mutans LytST two-component regulon reveals its contribution to oxidative stress tolerance

  • 1,
  • 2,
  • 2,
  • 1 and
  • 2Email author
BMC Microbiology201212:187

  • Received: 29 May 2012
  • Accepted: 21 August 2012
  • Published:



The S. mutans LrgA/B holin-like proteins have been shown to affect biofilm formation and oxidative stress tolerance, and are regulated by oxygenation, glucose levels, and by the LytST two-component system. In this study, we sought to determine if LytST was involved in regulating lrgAB expression in response to glucose and oxygenation in S. mutans.


Real-time PCR revealed that growth phase-dependent regulation of lrgAB expression in response to glucose metabolism is mediated by LytST under low-oxygen conditions. However, the effect of LytST on lrgAB expression was less pronounced when cells were grown with aeration. RNA expression profiles in the wild-type and lytS mutant strains were compared using microarrays in early exponential and late exponential phase cells. The expression of 40 and 136 genes in early-exponential and late exponential phase, respectively, was altered in the lytS mutant. Although expression of comYB, encoding a DNA binding-uptake protein, was substantially increased in the lytS mutant, this did not translate to an effect on competence. However, a lrgA mutant displayed a substantial decrease in transformation efficiency, suggestive of a previously-unknown link between LrgA and S. mutans competence development. Finally, increased expression of genes encoding antioxidant and DNA recombination/repair enzymes was observed in the lytS mutant, suggesting that the mutant may be subjected to increased oxidative stress during normal growth. Although the intracellular levels of reaction oxygen species (ROS) appeared similar between wild-type and lytS mutant strains after overnight growth, challenge of these strains with hydrogen peroxide (H2O2) resulted in increased intracellular ROS in the lytS mutant.


Overall, these results: (1) Reinforce the importance of LytST in governing lrgAB expression in response to glucose and oxygen, (2) Define a new role for LytST in global gene regulation and resistance to H2O2, and (3) Uncover a potential link between LrgAB and competence development in S. mutans.


  • Stress
  • Oxygen
  • Competence
  • Cid/Lrg system
  • Streptococcus mutans


Streptococcus mutans is considered the primary causative agent of dental caries, and when transiently introduced into the bloodstream following daily dental hygienic practices such as toothbrushing and flossing, this bacterium can also cause potentially lethal infective endocarditis (IE) [14]. In both infectious scenarios, the virulence of S. mutans depends upon its ability to form biofilms and to withstand extreme changes in environmental conditions, including fluctuations in oxygenation, shear stress, as well as nutrient source and availability. For example, in the oral cavity, S. mutans must be able to rapidly alter its expression of transporters and metabolic enzymes to catabolize a variety of host-derived dietary carbohydrates. Internalized carbohydrates are metabolized through the glycolytic pathway, resulting in the accumulation of acidic end-products in the environment, which favors the growth of S. mutans and other acid-tolerant cariogenic species. Repeated cycles of acidification can lead to a net demineralization of tooth enamel and the development of caries. Sucrose, a common dietary sweetener, can also be utilized by S. mutans for the production of extracellular polysaccharides [58] that facilitate bacterial adhesion and biofilm formation. Aeration has also been found to have a profound effect on carbohydrate metabolism and biofilm formation by S. mutans[911]. It is therefore not surprising that there is overlap in the genetic regulatory circuits responsive to carbohydrate metabolism, aeration/oxidative stress resistance and control of biofilm formation in S. mutans, which include CcpA [1214], Rex [15], and Frp [16].

More recently, an emerging trend in the study of bacterial biofilms has been a focus on the contribution of bacterial cell death and autolysis to biofilm adherence, maturation, and dispersal. It has been demonstrated in a wide variety of bacteria that death and lysis of a subpopulation of cells can facilitate biofilm formation due to the release of DNA into the extracellular environment (eDNA) [1722]. Likewise, cell death and lysis have been implicated in dispersal of cells from a mature biofilm [2325]. In Staphylococcus aureus, the Cid/Lrg system has been shown to be involved in the regulation of cell death, autolysis, and biofilm formation [17, 21, 2628]. Characterization of S. aureus cid and lrg mutants has revealed that these operons have opposing effects on cell death and murein hydrolase activity [27, 29]. These observations, combined with the fact that LrgA and CidA share structural features with the bacteriophage lambda family of holin proteins [29], have led to the hypothesis that CidA and LrgA control cell death and lysis in a manner analogous to effector and inhibitor holins, respectively [26, 30]. Bacteriophage holins are small membrane proteins that oligomerize in the cell membrane, acting as “molecular clocks” that regulate the timing and lysis of the host cell during lytic infection [31]. For example, the lambda S holin regulates cell death and lysis by the formation of large lipid-excluding “rafts” that promote cytosolic leakage as well as access of the phage-encoded endolysin (murein hydrolase) to the cell wall [3234]. S. aureus CidA and LrgA have recently been shown to oligomerize into high-molecular-mass complexes in a cysteine disulfide bond-dependent manner, a biochemical feature also shared with holin proteins [35]. Although the molecular details of how Cid and Lrg function to control cell death and lysis have not yet been completely elucidated, the fact that cid and lrg homologues have been identified in a wide variety of bacterial and archeal genomes supports a fundamental and conserved role for this system in cell physiology [30, 36].

In previous work it was determined that expression of potential cidAB and lrgAB homologues in S. mutans is highly responsive to carbohydrate availability [12, 37] and oxygenation [11]. Given the potential importance of these genes to biofilm development in S. mutans, we previously characterized a panel of S. mutans cid and lrg isogenic mutants and found that a subset of these genes did indeed influence biofilm formation, production of glucosyltransferases (enzymes that synthesize extracellular glucan polymers that contribute to biofilm adhesion), and oxidative stress tolerance [37]. In this study it was also found that, as demonstrated previously in S. aureus[38, 39], the S. mutans LytST two-component system was required for activation of lrgAB expression, but not cidAB expression [37]. Genes homologous to lytST appear to be present in most Gram-positive organisms that contain lrgAB[30] and these genes are often linked to one another, inferring an important role for this two-component system in fine-tuning lrgAB expression in response to external environmental signals. Therefore in this study, we sought to determine if LytST is involved in regulation of lrgAB expression in response to glucose and oxygenation in S. mutans, and to elaborate on the contribution of LytST to cellular homeostasis and global control of gene expression.


Effects of oxygenation and glucose metabolism on S. mutans lrg and cid expression

The LytST two-component regulatory system has been shown to positively regulate lrgAB expression in a wide variety of bacteria, including various staphylococcal [3840] and Bacillus species [41, 42], as well as in S. mutans[37]. The conserved nature of this regulation in Gram-positive bacteria, combined with the known effects of LytST and LrgAB on cell death/lysis [29, 38, 39, 43], biofilm development [21, 37, 38], and oxidative stress resistance [37], suggests that LytST and LrgAB are central regulators of physiologic homeostasis. However, little is known about the environmental and/or cellular cues to which LytS responds. In S. aureus and B. anthracis, it has been shown that lrgAB expression is responsive to disruption of cell membrane potential in a LytST-dependent manner [41, 44]. However, we were unable to determine whether this regulation also occurs in S. mutans, as treatment with membrane-potential disrupting agents (gramicidin, carbonyl cyanide m-chlorophenylhydrazone) did not have a measurable effect on membrane potential, as assessed by staining with DIOC2 (3) (data not shown).

In previous studies, it was shown that oxygen and glucose metabolism have a pronounced effect on lrg and cid expression in S. mutans, but the specific role of LytS, if any, in this regulation was not addressed [11, 37]. Therefore, S. mutans UA159 and its isogenic lytS mutant were grown under aerobic and low-oxygen conditions to exponential (EP) and stationary (SP) growth phases in media containing 11 mM or 45 mM glucose. Quantitative real-time reverse transcriptase PCR (qRT-PCR) was performed on RNA isolated from cultures at each time point to assess changes in lrg expression (Figure 1). In UA159, stationary phase lrgAB expression was upregulated 365-fold relative to exponential phase when grown under 11 mM glucose and low-oxygen conditions (Figure 1A). Although mutation of lytS resulted in a severe loss of stationary phase lrgAB induction in cells grown in 11 mM glucose, lrgAB expression was not completely abolished. When grown under aerobic conditions and 11 mM glucose, stationary phase lrgAB expression was upregulated 2500-fold relative to exponential phase in the wild-type strain (Figure 1A), confirming previously-published observations that aerobic growth promotes lrgAB expression [11]. However, stationary-phase lrgAB expression was still induced 216-fold in the lytS mutant during aerobic growth, suggesting that (1) other as-yet-unknown regulators also contribute to the positive control of lrgAB expression during aerated growth, and (2) LytST is a predominant regulator of lrgAB expression during low oxygen growth, compared to aerobic growth. Under low-oxygen and aerated cultures, stationary phase induction of lrgAB expression was dramatically reduced when grown in 45 mM glucose, and similar levels of expression were observed in the wild-type and lytS mutant (Figure 1B), suggesting that growth in high levels of glucose abrogates oxygen-dependent regulation of lrgAB by LytST. Consistent with previously-published data [37], LytS did not appear to have a measurable effect on cidAB expression under any of the growth conditions tested here (data not shown). In summary, LytST-dependent regulation of lrgAB expression is much more pronounced during low-oxygen growth and at low glucose levels.
Figure 1
Figure 1

LytS-dependent expression of lrgAB in S . mutans . Overnight cultures were diluted in THYE, containing either 11 mM (A) or 45 mM glucose (B) to an OD600 = 0.02 and grown at 37°C as static cultures at 5% CO2 (“low-O2”) or as aerobic shaking cultures at 250 RPM (“aerobic”). RNA was harvested at exponential (EP) and stationary phase (SP). Reverse-transcription, real-time PCR reactions, and determination of copy number were performed as described previously using lrgA and 16S-specific primers [37, 77]. Fold-change expression of lrgAB and 16S under each growth condition was calculated by dividing the gene copy number of each test sample by the average gene copy number of UA159 EP. Data was then normalized by dividing each lrgAB fold-change value by its corresponding 16S fold-change expression value. Data represent the average of 3 biological replicates. Dark grey bars represent UA159 and light grey bars represent lytS mutant. Error Bars represent the standard error (SEM).

Microarray analysis of the LytS regulon

Based on the transcriptional data presented above, the effects of LytST regulation on lrgAB expression are most evident while S. mutans is growing under conditions of low-oxygen (5% CO2) with a lower concentration of glucose. To begin to explore how LytST impacts critical phenotypes of S. mutans, RNA expression profiles in UA159 and the lytS mutant were compared using an RNA microarray approach. RNA was isolated from early exponential and late exponential growth phases from static planktonic cultures grown in BHI (containing 11 mM total glucose) at 37°C in a 5% CO2 atmosphere (Additional file 1: Table S1 and Additional file 2: Table S2). At early exponential growth phase, loss of LytS affected the expression of 40 genes (12 upregulated and 28 downregulated; P < 0.005; Additional file 1: Table S1). Most of the upregulated genes in early exponential phase displayed only a modest increase in expression and included genes involved in DNA repair, purine/pyrimidine metabolism, competence, and a number of unassigned and hypothetical ORFs. RNA transcripts that were strongly down-regulated greater than 10-fold in cells lacking LytS during early exponential growth included those annotated as bacitracin/surfactin/gramicidin synthesis proteins, transport and binding proteins, and LrgAB. In contrast, loss of LytS affected the expression of a much larger number of genes in late exponential phase (136 genes total), with 79 upregulated transcripts and 57 downregulated transcripts (P < 0.001; Additional file 2: Table S2). Aside from dramatically decreased lrgAB expression, affected genes included those involved in amino acid and co-factor biosynthesis, carbohydrate and fatty acid metabolism, stress adaptation, toxin production, DNA repair/recombination, protein synthesis, transcriptional regulation, and competence, as well as multiple hypothetical and/or unassigned ORFs (Additional file 2: Table S2 and Figure 2). A subset of genes was differentially expressed as a function of the loss of LytS in both early exponential and late exponential growth phases (Additional file 1: Table S1 and Additional file 2: Table S2). These included many genes encoded by the S. mutans genomic island TnSMu2 [45] (SMU.1335c, 1339-1342, 1344c-1346, 1354c, 1360c, 1363c, 1366c), ssbA, comYB, and lrgAB. Given that these genes were regulated by LytS in both growth phases examined, it is possible that they are under the direct control of LytST. To validate the microarray data, qRT-PCR was performed on late exponential phase wild-type and lytS mutant RNA to assess expression of 14 of the affected genes. As shown in Table 1, the expression ratios (lytS mutant/wild-type) for each gene obtained by real-time PCR were similar to the microarray results. Interestingly, expression ratios of these genes were all close to 1.0 when comparing expression between the wild-type strain and a lrgAB mutant (Table 1), indicating that the differential expression patterns observed in the lytS mutant were not a consequence of down-regulated lrgAB expression.
Figure 2
Figure 2

Distribution of functions of genes affected by loss of LytS at late exponential phase. Statistical analysis was carried out with BRB array tools ( with a cutoff P value of 0.001. The 136 genes differentially expressed at P ≤0.001 are grouped by functional classification according to the Los Alamos S. mutans genome database (

Table 1

Real-time PCR validation of RNA microarray results



Real-time pcr


lytS mutant

lytS mutant

lrgAB mutant



comYA (comYB)












vicR (vicX)







































































Results are expressed in fold-change (mutant/wild-type).

Investigation of the effect of LytST and LrgAB on competence

In analyzing the microarray data in Additional file 1: Table S1 and Additional file 2: Table S2, it appeared that the gene most highly upregulated in response to loss of LytS in both phases of growth was comYB (SMU.1985), a homologue of the B. subtilis comGB gene that encodes part of an ABC transporter essential for DNA binding-uptake during competence in S. mutans[46]. Interestingly, a comYB mutant of S. mutans was shown to be unaffected in competence signaling, but showed reduced biofilm formation, which was thought to be a function of its inability to bind biofilm matrix eDNA [47]. Since the lytS mutant displayed an increase in comYB expression (Additional file 1: Table S1 and Additional file 2: Table S2), we hypothesized that this strain may display alterations in its ability to form biofilm and/or its transformability during genetic competence. However, the lytS mutant did not display any appreciable difference in its ability to form static biofilm in the presence of glucose or sucrose (data not shown), and likewise, did not display a difference in its ability to uptake plasmid DNA in a quantitative competence assay, relative to the wild-type strain (Figure 3). Since lrgAB expression is so strongly regulated by LytST, the ability of isogenic lrgA, lrgB, and lrgAB mutants to uptake plasmid DNA via competence was also assessed (Figure 3). Of all the mutants tested, the lrgA mutant was the most severely impaired in its ability to uptake plasmid DNA relative to the parental strain, displaying a 26- and 24-fold decrease in transformation efficiency in the presence and absence of competence-stimulating peptide (CSP), respectively (Figure 3), suggesting that LrgA is somehow involved in genetic transformation in a CSP-independent manner. This finding has particular significance considering that LrgAB has been linked to regulation of cell death and lysis in S. aureus[21, 29] and S. mutans[37], and these physiological processes are also extremely important during natural competence. It is interesting to note that, similar to the competence results described here, the lrgA mutant was previously shown to display decreased glucose-dependent biofilm formation and decreased glucosyltransferase production, whereas the lrgB and lrgAB mutants behaved in a manner similar to the parental strain [37]. These phenotypic patterns suggest that the presence of LrgB alone, rather than the lack of LrgA, may be responsible for the biofilm and competence phenotypes observed in the lrgA mutant.
Figure 3
Figure 3

Transformation efficiencies of UA159 and isogenic lytS and lrg mutants. To compare the ability of UA159 and its isogenic lytS, lrgA, lrgB, and lrgAB mutants to take up exogenously-added plasmid DNA, a quantitative competence assay was performed on n = 4-6 biological replicates of each strain as described in Methods [83]. Plasmid pAT28 [encoding spectinomycin resistance; [84] was used to assess transformation efficiency in UA159, lytS, lrgB, and lrgAB mutants. Because the lrgA mutant was generated with a spectinomycin-resistance cassette [37], plasmid pORi23 [encoding erythromycin resistance; [85]] was used to assess transformation efficiency in UA159 and lrgA mutant. Transformation efficiencies (Y axis) in the presence (grey bars) and absence (white bars) of CSP are expressed as the percentage of transformants (CFU/ml on BHI + selective antibiotic) among total viable cells (CFU/ml on BHI). Error bars represent SEM. Brackets with P values denote statistically-significant differences between two samples (Mann–Whitney Rank Sum Test).

Effect of LytST on oxidative stress tolerance

Previously, our investigations disclosed a strong link between oxidative stress tolerance and the Cid/Lrg system [37], a role for these genes that had not been described in other organisms. Specifically, we found that lrgAB, lrgB, cidAB, and cidB mutants exhibited reduced growth in the presence of paraquat, and growth of lrgAB, cidAB, and cidB mutants on BHI agar plates in aerobic conditions was almost completely inhibited [37]. It is therefore interesting to note that in the lytS microarray results (Additional file 2: Table S2), genes encoding antioxidant and DNA repair/recombination enzymes were significantly upregulated in the lytS mutant in late exponential phase. These included yghU and tpx, encoding the putative anti-oxidant enzymes glutathione S-transferase and thiol peroxidase, respectively, as well as recJ, which encodes a single-stranded DNA exonuclease protein that facilitates DNA repair in response to oxidative stress [4851]. To further investigate the effect of lytS and lrgAB on oxidative stress tolerance, wild-type, lytS, and lrgAB mutants were grown as planktonic static BHI cultures in aerobic atmosphere and in the presence and absence of H2O2 (Figure 4). When challenged with H2O2, UA159 experienced an increased lag phase of growth, and the overall OD of the culture was 10-25% less than the untreated culture until 20 h growth. Under these assay conditions, the lrgAB mutant displayed a dramatic growth defect in both the presence and absence of H2O2. It is interesting to note that this aerobic growth defect was also previously observed when the lrgAB mutant was grown in aerobic atmosphere on BHI agar plates [37]. The lytS mutant displayed an increased lag in growth relative to UA159 when cultured in the presence of H2O2, but OD values were comparable to the wild-type strain by 16 h growth. These results suggest that the LytST regulon impacts the ability of cells to grow under conditions of oxidative stress.
Figure 4
Figure 4

H 2 O 2 challenge assay of UA159, lytS and lrgAB mutants. Cultures of UA159, lytS, and lrgAB mutants (n = 6 biological replicates per strain) were grown in the presence (open symbols) and absence (filled symbols) of 1.0 mM H2O2 for 20 h at 37°C (aerobic atmosphere) in a Biotek microplate reader. OD600 measurements of each well were recorded at 2 h intervals. Black circles represent UA159, red triangles represent lytS mutant, blue squares represent lrgAB mutant. Error bars represent SEM.

The cell-permeable fluorescent dye CM-H2DCFDA (Invitrogen Molecular Probes) was also used to assess intracellular ROS in UA159 and the lytS mutant (Figure 5). This fluorescent compound is oxidized in the presence of H2O2 and other reactive oxygen species (ROS) and is considered a general indicator of intracellular oxidative stress [52, 53]. This analysis revealed that stationary-phase cultures of the wild-type and lytS mutant strains had similar “endogenous” intracellular levels of ROS (Figure 5, light grey bars). When stationary-phase cells from each strain were loaded with CM-H2DCFDA and then challenged with 5 mM H2O2 (Figure 5, dark grey bars), a greater increase in fluorescence was observed in the lytS mutant relative to UA159 (P = 0.009, Mann–Whitney Rank Sum Test), suggesting that loss of LytS has an impact on the ability of the cells to detoxify H2O2 and/or other intracellular ROS.
Figure 5
Figure 5

Measurement of intracellular ROS in UA159 and lytS mutant by CM-H 2 DCFDA staining. Cells were harvested from 20 h BHI cultures of UA159 and isogenic lytS mutant grown at 37°C 5% CO2 (n = 3-6 biological replicates each), resuspended in HBSS containing 5 μM CM-H2DCFDA, and incubated at 37°C to load the cells with stain. After 60 min incubation, cell suspensions were centrifuged, washed once in HBSS buffer, and then resuspended in HBSS buffer alone (light grey bars) or in HBSS containing 5 mM H2O2 (dark grey bars). Each suspension was transferred to wells of an optically-clear 96 well plate, and incubated at 37°C in a microplate reader. Cell fluorescence (as measured by relative fluorescence units; RFU) and the OD600 of each well was recorded after 30 min incubation. RFU measurements are expressed per OD600 of each well to account for any subtle variations in cell density. Error bars represent SEM. Brackets with P values denote statistically-significant differences between two samples (Mann–Whitney Rank Sum Test).


The transcriptome analyses presented in this study have revealed that the LytST two-component system has a widespread effect on gene expression in S. mutans. A much higher number of transcripts were affected by the lytS mutation in late exponential phase and the magnitude of changes in expression was greater (n = 136 genes, Additional file 2: Table S2) relative to early-exponential phase (n = 40 genes, Additional file 1: Table S1), where most genes exhibited only a modest (1-2 fold) change in expression. These differences in gene expression patterns are unlikely to be an indirect function of altered lrgAB expression in the lytS mutant, as expression of lytS-regulated genes was unaltered in an lrgAB mutant relative to the wild-type strain (Table 1). Taken together, these observations suggest that LytST exerts control over its transcriptome in a growth-phase dependent manner, and to our knowledge, this is the first study that has compared the scope of LytST regulation at different phases of growth. Interestingly, RNA microarray studies of lyt mutants have also been performed in S. aureus[38], S. epidermidis[40], and B. subtilis[42]. As we have observed here in S. mutans, a global effect of LytST on gene expression was also noted in S. aureus and S. epidermidis[38, 40]. In S. aureus, LytST appeared to exert primarily positive effects on gene expression in exponential phase when aerobic cultures were grown in media containing excess (35 mM) glucose, as only 7 genes were found to be upregulated in the lytS mutant [38]. In S. epidermidis, a large number of genes were up- or down-regulated as a function of the presence of LytST during exponential phase during aerobic growth in medium containing 12 mM glucose [40]. In contrast, mutation of lytS only appeared to affect the expression of lytST itself and genes encoding lrgAB and cidAB homologues in B. subtilis[42]. However, due to the differences in growth conditions used (glucose levels and/or culture aeration) and the differing metabolic pathways present in these organisms, it is difficult to establish direct correlations between these studies and the S. mutans microarray results presented here.

As demonstrated previously [37], expression of lrgAB was also shown to be tightly controlled by the LytST two-component system in S. mutans in this study. Specifically, we have found that LytST-dependent expression of lrgAB is regulated in part by glucose metabolism and oxygen in S. mutans (Figure 1). Furthermore, control of lrgAB expression by LytST appears to be highly growth-phase dependent: lrgAB expression in the lytS mutant exhibited only a modest decrease in expression in early exponential phase (0.49 relative to UA159, Additional file 1: Table S1), whereas lrgAB expression was down-regulated some 200-fold in the lytS mutant at late exponential phase (Additional file 2: Table S2). Alternatively, it is possible that control of lrgAB expression by LytST is related to higher glucose availability during early exponential phase. Although detailed mechanistic studies have not yet been performed, there is mounting evidence that these proteins are critical for oxidative stress resistance in S. mutans: (1) lrgAB expression is highly regulated by oxygen ([11] and this study); (2) a lrgAB mutant was defective in aerobic growth on BHI agar plates [37]; (3) a lrgAB mutant displayed a decreased growth rate in the presence of paraquat (a superoxide-generating agent) relative to the wild-type strain [37]; and (4) a lrgAB mutant displayed a strong growth defect during static planktonic aerobic growth in BHI in the presence and absence of H2O2 challenge (this study). Interestingly, a link between LrgAB and oxidative stress was also demonstrated in S. aureus, where lytSR and lrgAB expression were upregulated 2-5 fold in response to azurophilic granule proteins, H2O2, and hypochlorite [54].

In agreement with a role for LrgAB in oxidative stress resistance, several LytST-regulated genes identified in this study have also been implicated in bacterial oxidative stress responses. Upregulated potential oxidative stress genes include yghU, a putative anti-oxidant enzyme [50], tpx, a predicted thiol peroxidase [55], and recJ, a single-stranded DNA exonuclease protein that facilitates DNA repair in response to oxidative stress [51]. Conversely, several genes belonging to the TnSMu2 gene cluster (SMU.1334c – SMU.1359) were downregulated in the lytS mutant. These genes are annotated as encoding a series of gene products involved in bacitracin and gramicidin synthesis [56], but more recently have been shown to be responsible for nonribosomal peptide and polyketide (NRP/PK) biosynthesis of a pigment that enhances aerobic growth and tolerance to H2O2 challenge in S. mutans UA159 [45]. The altered expression of one or more of these genes may explain, in part, the increased ROS accumulation that was observed in the lytS mutant when challenged with H2O2 (Figure 5). Furthermore, it was previously found that a two-component system responsible for positive regulation of the NRP/PK genes was located on the TnSMu2 genomic island of UA140 but not in UA159 [45]. This observation, combined with the microarray results performed here (Additional file 1: Table S1 and Additional file 2: Table S2) suggest that LytST may have taken over some of the regulatory functions of this non-core-genome two-component system that is missing in UA159.

Interestingly, H2O2 has also been shown to be a potent stimulator of competence and eDNA release in S. sanguinis[57], S. gordonii[57, 58], and S. pneumoniae[59]. Although the effects of H2O2 on S. mutans competence, cell lysis, and eDNA release have not been directly measured, it has been shown that growth under aerobic conditions promotes competence in S. mutans[47], and that expression of competence-related genes is upregulated during aerobic growth [11]. The results presented here have demonstrated that expression of comYB, a gene encoding a component of the DNA-binding uptake system in S. mutans[47] was upregulated 2-fold in early exponential phase and 22-fold in late exponential phase in the lytS mutant (Additional file 1: Table S1 and Additional file 2: Table S2). The significance of high-level comYB expression in the lytS mutant at late exponential phase is unclear, given that maximal S. mutans competence develops in actively-growing populations [60, 61]. Accordingly, upregulation of comYB expression did not correlate with increased transformability of the lytS mutant under the conditions tested in this study (Figure 3). However, it was found that the lrgA mutant displayed a significant reduction in competence. It has been recently reported that only a subpopulation of S. mutans culture lyses in response to CSP, and this lysis event is controlled in part by the CipB bacteriocin and the CipI immunity protein [62]. Subsequent microarray analysis of a cipI (immunity protein) mutant showed that both lytST and lrgAB expression were highly upregulated in the cipI mutant [63]. These results, combined with the fact that LrgA/B has been shown to be involved in regulating cell lysis and eDNA release in S. aureus[21, 29], lends strong support to the idea that LrgA plays an important role during competence, possibly by altering membrane permeability or by modulating murein hydrolase activity.

The S. mutans comY operon consists of nine co-transcribed genes, of which the first eight genes are either essential to or significantly affect competence [46]. The ninth gene of this operon is predicted to encode acetate kinase (AckA), an enzyme that catalyzes the inter-conversion of acetyl-phosphate and acetate [46, 64]. For micro-organisms with an inefficient or incomplete TCA cycle such as S. mutans, AckA-mediated conversion of acetyl-phosphate to acetate is thought to be a critical mechanism of generating ATP [reviewed in [65]]. Since ackA (comYI) was previously found to be upregulated in S. mutans during aerated growth [11], it is possible that LytST is involved in the regulation of energy generation through the phosphate acetyltransferase (Pta)-AckA pathway during aerobic growth and/or during oxidative stress. In this respect, it has recently been reported that an S. mutans pta mutant was more susceptible to both acid and oxidative stresses [66].

The ability of S. mutans to combat H2O2 stress is critical for its survival in the oral cavity, yet H2O2 detoxifying mechanisms and their regulation have not been extensively-characterized in this organism, limited primarily to the ScnRK and VicRK two-component systems [67, 68], ropA[69], brpA[70], luxS[71] and genomic island TnSMu2 [45]. H2O2 has been shown to have potent antibacterial effects on S. mutans[72], and it is thought that H2O2 produced by other oral streptococcal species serves as an antagonist against S. mutans. For example, S. sanguinis and S. gordonii have been shown to produce H2O2 via pyruvate oxidase under aerobic growth conditions, and this H2O2 production allows them to compete effectively against S. mutans when co-cultured under aerobic growth conditions [57]. It is therefore possible that the S. mutans LytST regulon mediates a pleiotropic protective response against these H2O2-producing niche competitors. On-going and future studies by our group will focus on experimental testing of this hypothesis.


In summary, the LytST two-component system has been shown to have a pleiotropic effect on gene expression in S. mutans. This is congruent with microarray analyses of lytS mutants in S. aureus[38] and S. epidermidis[40]. However, unlike in other organisms, we have been able to identify a pattern of LytS-mediated gene expression that suggests a role for this regulon in responding to oxidative/H2O2 stress. Although we have not yet been able to identify the external signal to which LytS responds, it is likely linked to an oxidative stress-sensing mechanism, such as H2O2-mediated membrane damage (ie. lipid peroxidation) via its large number of transmembrane domains, or oxygen/ROS interactions with its predicted cytoplasmic GAF domain, a ubiquitous signaling domain that has been shown to detect changes in the redox state of bound iron or oxygen in Mycobacterium tuberculosis[7375]. Establishing mechanistic links between the LytST regulon, H2O2 resistance, and competence regulation will provide valuable new insights into S. mutans survival and virulence in the oral cavity.


Bacterial strains, media, and growth conditions

For all experiments, frozen glycerol stocks of S. mutans UA159 and its isogenic lytS (SAB111; ΔlytS::NPKmr), lrgA (SAB113; ΔlrgA::NPSpr), lrgB (SAB119; ΔlrgB::NPEmr), and lrgAB (SAB115; ΔlrgAB::ΩKmr) mutants [created previously in [37] were freshly streaked for isolation on either Todd Hewitt Yeast Extract (THYE) or Brain Heart Infusion (BHI), containing selective antibiotic as appropriate: kanamycin (Km) – 1000 μg/ml, erythromycin (Em) – 10 μg/ml, spectinomycin (Sp) - 1000 μg/ml). With the exception of SAB115 (lrgAB mutant), all mutants were created using non-polar (NP) antibiotic-resistance markers [37]. Unless otherwise indicated, all S. mutans cultures were grown as static cultures in BHI or THYE broth at 37°C and 5% CO2.

Analysis of lrgAB expression

To measure the effects of oxygen and glucose on lrg expression, overnight THYE cultures of UA159 and the lytS mutant (n = 3 biological replicates each, grown at 0 RPM, 37°C and 5% CO2) were each inoculated to an OD600 = 0.02 into THYE containing either 11 mM or 45 mM glucose. For “low O2” cultures, 2 L culture flasks each containing 400 ml media were grown at 0 RPM, 37°C, and 5% CO2. For aerobic cultures, 500 ml culture flasks each containing 100 ml media were grown at 37°C and 250 RPM. Total RNA was isolated from all cultures sampled at exponential (EP; OD600 = 0.2 – 0.4) and stationary (SP; OD600 = 1.4 – 1.7) growth phase, with an RNeasy Mini kit (Qiagen) and FASTPREP (MP Biomedicals) using previously-described methods [76]. Real-time reverse-transcriptase PCR and data analysis using lrgA and 16S primers was performed using previously described primers [37] and methods [77]. Fold-change expression of lrgA and 16S under each growth condition (11 mM low-O2, 11 mM aerobic, 45 mM low-O2, 45 mM aerobic) was calculated by dividing the gene copy number of each test sample by the average gene copy number of UA159 EP. Data was then normalized by dividing each lrgA fold-change expression value by its corresponding 16S fold-change expression value.

RNA microarray analysis of UA159 and lytS mutant

To assess the effect of LytS on global gene expression, overnight BHI cultures of UA159 and lytS mutant (n = 3 biological replicates per strain) were diluted to an OD600 = 0.02 in BHI, and grown as static cultures at 37°C and 5% CO2. Total RNA was isolated from each culture at early-exponential (OD600 = 0.15) and late exponential phase (OD600 = 0.9), using previously-published methods [77]. RNA microarray analysis was performed using S. mutans UA159 microarrays provided by The Institute for Genomic Research, and previously-described methods and data analysis [11, 70, 78]. In brief, 2 μg total bacterial RNA was used in each reverse-transcription and cDNA labeling reaction (performed as described in [70, 78]), and a single preparation from each culture was hybridized per microarray slide in a Maui hybridization chamber (BioMicro Systems, Salt Lake City, UT). The resulting microarray slides were scanned, analyzed, and normalized using TIGR Spotfinder software (, and in-slide replicate analysis was performed with the TIGR microarray data analysis system (MIDAS; Statistical analysis was carried out with BRB array tools ( with a cutoff P value < 0.005 for the early exponential-phase data and P < 0.001 for the late exponential phase data. To validate the microarray results, real-time quantitative RT-PCR was performed on a subset of the differentially-expressed genes, as described previously [77, 79]. All real-time PCR primers were designed with Beacon Designer 4.0 software (Premier Biosoft International, Palo Alto, CA), and standard curves for each gene were prepared as published elsewhere [80]. The microarray data obtained from these studies have been deposited to NCBI’s gene expression omnibus (GEO) [81] (GEO Accession #GSE39470) and comply with MIAME guidelines [82].

Quantitative competence assays

To compare the ability of UA159 and its isogenic lytS, lrgA, lrgB, and lrgAB mutants to take up exogenously-added plasmid DNA, a quantitative competence assay was performed on n = 4-6 biological replicates of each strain using a previously-published protocol [83] with the following modifications: Overnight cultures of each strain were diluted to an OD600 = 0.02 in BHI, and grown in a 96-well plate to an OD600 = 0.15 prior to addition of 500 ng plasmid DNA with and without 100 ng CSP. Plasmid pAT28 (encoding spectinomycin resistance; [84]) was used to assess transformation efficiency in UA159, lytS, lrgB, and lrgAB mutants. Because the lrgA mutant was generated with a spectinomycin-resistance cassette [37], plasmid pORi23 [encoding erythromycin resistance; [85]] was used to assess transformation efficiency in UA159 and lrgA mutant. After 2.5 h incubation in the presence of plasmid DNA +/- CSP, cultures were serially diluted and plated on BHI agar with and without selective antibiotic. CFU/ml of each culture were enumerated after 48 h growth at 37°C and 5% CO2, and transformation efficiencies were calculated as the percentage of transformants (CFU/ml on BHI + selective antibiotic) among total viable cells (CFU/ml on BHI).

H2O2 assays

To assess of the ability of UA159, lytS, and lrgAB mutants to grow in the presence of H2O2, overnight cultures of each strain (n = 6 biological replicates) were each diluted 40-fold into BHI. 1 ml aliquots of each diluted culture were either untreated or challenged with 1 mM H2O2. Aliquots of each (500 μl per well, 2 wells total) were then immediately transferred to an optically-clear 48-well tissue culture plate (Costar 3548), which was incubated for 20 h at 37°C (aerobic atmosphere) in a Biotek Synergy microplate reader. OD600 measurements of each well were recorded at 2 h intervals.

Oxidative stress measurements

To assess intracellular oxidative stress in UA159 and lytS mutant, single isolated colonies of each strain (n = 3-6 biological replicates per strain) were inoculated into culture tubes containing 4 ml BHI, and grown in “low-O2” conditions (37°C, 0 RPM, 5% CO2). After 20 h growth, 2 × 1 ml aliquots of each culture were harvested by centrifugation in a microcentrifuge (3 min at 13,000 RPM). The culture supernatants were discarded, and cell pellets were each resuspended in 1 ml Hanks Buffer (HBSS) containing 5 μM chloromethyl 2′,7′-dichlorofluorescein diaceate (CM-H2DCFDA; Invitrogen Molecular Probes), a cell-permeable fluorescent compound that is oxidized in the presence of H2O2 and other reactive oxygen species (ROS) and is considered a general indicator of cellular oxidative stress [52, 53]. Cell suspensions were incubated at 37°C for 60 min to “load” the cells with CM-H2DCFDA, followed by centrifugation (3 min at 13,000 RPM). Supernatants were discarded, and cell pellets were washed once with HBSS prior to resuspension in 1 ml HBSS or in 1 ml HBSS containing 5 mM H2O2. Each cell suspension was transferred into triplicate wells (200 μl per well) of an optically-clear 96 well plate (Costar 3614), and the plate was transferred to a Biotek Synergy microplate reader. Fluorescence in relative fluorescence units (RFU; using 492-495 nm excitation and 517-527 nm emission) and OD600 readings of each well were recorded after 30 min incubation at 37°C.

Statistical analysis

All statistical analyses, unless otherwise indicated, were performed using Sigmaplot for Windows 11.0 software (Build, Systat Software, Inc.).



This work was supported by a University of Florida HHMI-Science for Life Undergraduate Research Award to M. D. Q., NIH-NIDCR grants R03 DE019179 (KCR) and R01 DE13239 (RAB). We thank Christopher Browngardt for technical assistance in editing microarray data.

Authors’ Affiliations

Department of Oral Biology, College of Dentistry, University of Florida, Gainesville, FL 32611, USA
Department of Microbiology and Cell Science, College of Agricultural and Life Sciences, University of Florida, Gainesville, FL 32611, USA


  1. Deonarine B, Lazar J, Gill MV, Cunha BA: Quadri-valvular endocarditis caused by Streptococcus mutans. Clin Microbiol Infect. 1997, 3 (1): 139-141. 10.1111/j.1469-0691.1997.tb00267.x.PubMedView ArticleGoogle Scholar
  2. Biswas S, Bowler IC, Bunch C, Prendergast B, Webster DP: Streptococcus mutans infective endocarditis complicated by vertebral discitis following dental treatment without antibiotic prophylaxis. J Med Microbiol. 2010, 59 (Pt 10): 1257-1259.PubMedView ArticleGoogle Scholar
  3. Ullman RF, Miller SJ, Strampfer MJ, Cunha BA: Streptococcus mutans endocarditis: report of three cases and review of the literature. Heart Lung. 1988, 17 (2): 209-212.PubMedGoogle Scholar
  4. Vose JM, Smith PW, Henry M, Colan D: Recurrent Streptococcus mutans endocarditis. Am J Med. 1987, 82 (3 Spec No): 630-632.PubMedView ArticleGoogle Scholar
  5. Yamashita Y, Bowen WH, Burne RA, Kuramitsu HK: Role of the Streptococcus mutans gtf genes in caries induction in the specific-pathogen-free rat model. Infect Immun. 1993, 61 (9): 3811-3817.PubMedPubMed CentralGoogle Scholar
  6. Yamashita Y, Takehara T, Kuramitsu HK: Molecular characterization of a Streptococcus mutans mutant altered in environmental stress responses. J Bacteriol. 1993, 175 (19): 6220-6228.PubMedPubMed CentralGoogle Scholar
  7. Ooshima T, Matsumura M, Hoshino T, Kawabata S, Sobue S, Fujiwara T: Contributions of three glycosyltransferases to sucrose-dependent adherence of Streptococcus mutans. J Dent Res. 2001, 80 (7): 1672-1677. 10.1177/00220345010800071401.PubMedView ArticleGoogle Scholar
  8. Munro CL, Michalek SM, Macrina FL: Sucrose-derived exopolymers have site-dependent roles in Streptococcus mutans-promoted dental decay. FEMS Microbiol Lett. 1995, 128 (3): 327-332. 10.1111/j.1574-6968.1995.tb07544.x.PubMedView ArticleGoogle Scholar
  9. Ahn SJ, Browngardt CM, Burne RA: Changes in biochemical and phenotypic properties of Streptococcus mutans during growth with aeration. Appl Environ Microbiol. 2009, 75 (8): 2517-2527. 10.1128/AEM.02367-08.PubMedPubMed CentralView ArticleGoogle Scholar
  10. Ahn SJ, Burne RA: Effects of oxygen on biofilm formation and the AtlA autolysin of Streptococcus mutans. J Bacteriol. 2007, 189 (17): 6293-6302. 10.1128/JB.00546-07.PubMedPubMed CentralView ArticleGoogle Scholar
  11. Ahn SJ, Wen ZT, Burne RA: Effects of oxygen on virulence traits of Streptococcus mutans. J Bacteriol. 2007, 189 (23): 8519-8527. 10.1128/JB.01180-07.PubMedPubMed CentralView ArticleGoogle Scholar
  12. Abranches J, Nascimento MM, Zeng L, Browngardt CM, Wen ZT, Rivera MF, Burne RA: CcpA regulates central metabolism and virulence gene expression in Streptococcus mutans. J Bacteriol. 2008, 190 (7): 2340-2349. 10.1128/JB.01237-07.PubMedPubMed CentralView ArticleGoogle Scholar
  13. Browngardt CM, Wen ZT, Burne RA: RegM is required for optimal fructosyltransferase and glucosyltransferase gene expression in Streptococcus mutans. FEMS Microbiol Lett. 2004, 240 (1): 75-79. 10.1016/j.femsle.2004.09.012.PubMedView ArticleGoogle Scholar
  14. Wen ZT, Burne RA: Functional genomics approach to identifying genes required for biofilm development by Streptococcus mutans. Appl Environ Microbiol. 2002, 68 (3): 1196-1203. 10.1128/AEM.68.3.1196-1203.2002.PubMedPubMed CentralView ArticleGoogle Scholar
  15. Bitoun JP, Nguyen AH, Fan Y, Burne RA, Wen ZT: Transcriptional repressor Rex is involved in regulation of oxidative stress response and biofilm formation by Streptococcus mutans. FEMS Microbiol Lett. 2011, 320 (2): 110-117. 10.1111/j.1574-6968.2011.02293.x.PubMedPubMed CentralView ArticleGoogle Scholar
  16. Wang B, Kuramitsu HK: A pleiotropic regulator, Frp, affects exopolysaccharide synthesis, biofilm formation, and competence development in Streptococcus mutans. Infect Immun. 2006, 74 (8): 4581-4589. 10.1128/IAI.00001-06.PubMedPubMed CentralView ArticleGoogle Scholar
  17. Rice KC, Mann EE, Endres JL, Weiss EC, Cassat JE, Smeltzer MS, Bayles KW: The cidA murein hydrolase regulator contributes to DNA release and biofilm development in Staphylococcus aureus. Proc Natl Acad Sci U S A. 2007, 104 (19): 8113-8118. 10.1073/pnas.0610226104.PubMedPubMed CentralView ArticleGoogle Scholar
  18. Thomas VC, Hiromasa Y, Harms N, Thurlow L, Tomich J, Hancock LE: A fratricidal mechanism is responsible for eDNA release and contributes to biofilm development of Enterococcus faecalis. Mol Microbiol. 2009, 72 (4): 1022-1036. 10.1111/j.1365-2958.2009.06703.x.PubMedPubMed CentralView ArticleGoogle Scholar
  19. Harmsen M, Lappann M, Knochel S, Molin S: Role of extracellular DNA during biofilm formation by Listeria monocytogenes. Appl Environ Microbiol. 2010, 76 (7): 2271-2279. 10.1128/AEM.02361-09.PubMedPubMed CentralView ArticleGoogle Scholar
  20. Whitchurch CB, Tolker-Nielsen T, Ragas PC, Mattick JS: Extracellular DNA required for bacterial biofilm formation. Science. 2002, 295 (5559): 1487-10.1126/science.295.5559.1487.PubMedView ArticleGoogle Scholar
  21. Mann EE, Rice KC, Boles BR, Endres JL, Ranjit D, Chandramohan L, Tsang LH, Smeltzer MS, Horswill AR, Bayles KW: Modulation of eDNA release and degradation affects Staphylococcus aureus biofilm maturation. PLoS One. 2009, 4 (6): e5822-10.1371/journal.pone.0005822.PubMedPubMed CentralView ArticleGoogle Scholar
  22. Lappann M, Claus H, van Alen T, Harmsen M, Elias J, Molin S, Vogel U: A dual role of extracellular DNA during biofilm formation of Neisseria meningitidis. Mol Microbiol. 2010, 75 (6): 1355-1371. 10.1111/j.1365-2958.2010.07054.x.PubMedView ArticleGoogle Scholar
  23. Mai-Prochnow A, Evans F, Dalisay-Saludes D, Stelzer S, Egan S, James S, Webb JS, Kjelleberg S: Biofilm development and cell death in the marine bacterium Pseudoalteromonas tunicata. Appl Environ Microbiol. 2004, 70 (6): 3232-3238. 10.1128/AEM.70.6.3232-3238.2004.PubMedPubMed CentralView ArticleGoogle Scholar
  24. Webb JS, Thompson LS, James S, Charlton T, Tolker-Nielsen T, Koch B, Givskov M, Kjelleberg S: Cell death in Pseudomonas aeruginosa biofilm development. J Bacteriol. 2003, 185 (15): 4585-4592. 10.1128/JB.185.15.4585-4592.2003.PubMedPubMed CentralView ArticleGoogle Scholar
  25. Barraud N, Hassett DJ, Hwang SH, Rice SA, Kjelleberg S, Webb JS: Involvement of nitric oxide in biofilm dispersal of Pseudomonas aeruginosa. J Bacteriol. 2006, 188 (21): 7344-7353. 10.1128/JB.00779-06.PubMedPubMed CentralView ArticleGoogle Scholar
  26. Rice KC, Bayles KW: Molecular control of bacterial death and lysis. Microbiol Mol Biol Rev. 2008, 72 (1): 85-109. 10.1128/MMBR.00030-07. table of contentsPubMedPubMed CentralView ArticleGoogle Scholar
  27. Rice KC, Firek BA, Nelson JB, Yang SJ, Patton TG, Bayles KW: The Staphylococcus aureus cidAB operon: evaluation of its role in regulation of murein hydrolase activity and penicillin tolerance. J Bacteriol. 2003, 185 (8): 2635-2643. 10.1128/JB.185.8.2635-2643.2003.PubMedPubMed CentralView ArticleGoogle Scholar
  28. Rice KC, Nelson JB, Patton TG, Yang SJ, Bayles KW: Acetic acid induces expression of the Staphylococcus aureus cidABC and lrgAB murein hydrolase regulator operons. J Bacteriol. 2005, 187 (3): 813-821. 10.1128/JB.187.3.813-821.2005.PubMedPubMed CentralView ArticleGoogle Scholar
  29. Groicher KH, Firek BA, Fujimoto DF, Bayles KW: The Staphylococcus aureus lrgAB operon modulates murein hydrolase activity and penicillin tolerance. J Bacteriol. 2000, 182 (7): 1794-1801. 10.1128/JB.182.7.1794-1801.2000.PubMedPubMed CentralView ArticleGoogle Scholar
  30. Bayles KW: The biological role of death and lysis in biofilm development. Nat Rev Microbiol. 2007, 5 (9): 721-726. 10.1038/nrmicro1743.PubMedView ArticleGoogle Scholar
  31. Wang IN, Smith DL, Young R: Holins: the protein clocks of bacteriophage infections. Annu Rev Microbiol. 2000, 54: 799-825. 10.1146/annurev.micro.54.1.799.PubMedView ArticleGoogle Scholar
  32. Wang IN, Deaton J, Young R: Sizing the holin lesion with an endolysin-beta-galactosidase fusion. J Bacteriol. 2003, 185 (3): 779-787. 10.1128/JB.185.3.779-787.2003.PubMedPubMed CentralView ArticleGoogle Scholar
  33. Savva CG, Dewey JS, Deaton J, White RL, Struck DK, Holzenburg A, Young R: The holin of bacteriophage lambda forms rings with large diameter. Mol Microbiol. 2008, 69 (4): 784-793. 10.1111/j.1365-2958.2008.06298.x.PubMedView ArticleGoogle Scholar
  34. White R, Chiba S, Pang T, Dewey JS, Savva CG, Holzenburg A, Pogliano K, Young R: Holin triggering in real time. Proc Natl Acad Sci U S A. 2011, 108 (2): 798-803. 10.1073/pnas.1011921108.PubMedPubMed CentralView ArticleGoogle Scholar
  35. Ranjit DK, Endres JL, Bayles KW: Staphylococcus aureus CidA and LrgA proteins exhibit holin-like properties. J Bacteriol. 2011, 193 (10): 2468-2476. 10.1128/JB.01545-10.PubMedPubMed CentralView ArticleGoogle Scholar
  36. Bayles KW: Are the molecular strategies that control apoptosis conserved in bacteria?. Trends Microbiol. 2003, 11: 306-311. 10.1016/S0966-842X(03)00144-6.PubMedView ArticleGoogle Scholar
  37. Ahn SJ, Rice KC, Oleas J, Bayles KW, Burne RA: The Streptococcus mutans Cid and Lrg systems modulate virulence traits in response to multiple environmental signals. Microbiology. 2010, 156 (Pt 10): 3136-3147.PubMedPubMed CentralView ArticleGoogle Scholar
  38. Sharma-Kuinkel BK, Mann EE, Ahn JS, Kuechenmeister LJ, Dunman PM, Bayles KW: The Staphylococcus aureus LytSR two-component regulatory system affects biofilm formation. J Bacteriol. 2009, 191 (15): 4767-4775. 10.1128/JB.00348-09.PubMedPubMed CentralView ArticleGoogle Scholar
  39. Brunskill EW, Bayles KW: Identification of LytSR-regulated genes from Staphylococcus aureus. J Bacteriol. 1996, 178 (19): 5810-5812.PubMedPubMed CentralGoogle Scholar
  40. Zhu T, Lou Q, Wu Y, Hu J, Yu F, Qu D: Impact of the Staphylococcus epidermidis LytSR two-component regulatory system on murein hydrolase activity, pyruvate utilization and global transcriptional profile. BMC Microbiol. 2010, 10: 287-10.1186/1471-2180-10-287.PubMedPubMed CentralView ArticleGoogle Scholar
  41. Chandramohan L, Ahn JS, Weaver KE, Bayles KW: An overlap between the control of programmed cell death in Bacillus anthracis and sporulation. J Bacteriol. 2009, 191 (13): 4103-4110. 10.1128/JB.00314-09.PubMedPubMed CentralView ArticleGoogle Scholar
  42. Kobayashi K, Ogura M, Yamaguchi H, Yoshida K, Ogasawara N, Tanaka T, Fujita Y: Comprehensive DNA microarray analysis of Bacillus subtilis two-component regulatory systems. J Bacteriol. 2001, 183 (24): 7365-7370. 10.1128/JB.183.24.7365-7370.2001.PubMedPubMed CentralView ArticleGoogle Scholar
  43. Brunskill EW, Bayles KW: Identification and molecular characterization of a putative regulatory locus that affects autolysis in Staphylococcus aureus. J Bacteriol. 1996, 178 (3): 611-618.PubMedPubMed CentralGoogle Scholar
  44. Patton TG, Yang SJ, Bayles KW: The role of proton motive force in expression of the Staphylococcus aureus cid and lrg operons. Mol Microbiol. 2006, 59 (5): 1395-1404. 10.1111/j.1365-2958.2006.05034.x.PubMedView ArticleGoogle Scholar
  45. Wu C, Cichewicz R, Li Y, Liu J, Roe B, Ferretti J, Merritt J, Qi F: Genomic island TnSmu2 of Streptococcus mutans harbors a nonribosomal peptide synthetase-polyketide synthase gene cluster responsible for the biosynthesis of pigments involved in oxygen and H2O2 tolerance. Appl Environ Microbiol. 2010, 76 (17): 5815-5826. 10.1128/AEM.03079-09.PubMedPubMed CentralView ArticleGoogle Scholar
  46. Merritt J, Qi F, Shi W: A unique nine-gene comY operon in Streptococcus mutans. Microbiology. 2005, 151 (Pt 1): 157-166.PubMedView ArticleGoogle Scholar
  47. Petersen FC, Tao L, Scheie AA: DNA binding-uptake system: a link between cell-to-cell communication and biofilm formation. J Bacteriol. 2005, 187 (13): 4392-4400. 10.1128/JB.187.13.4392-4400.2005.PubMedPubMed CentralView ArticleGoogle Scholar
  48. Dubbs JM, Mongkolsuk S: Peroxiredoxins in bacterial antioxidant defense. Subcell Biochem. 2007, 44: 143-193. 10.1007/978-1-4020-6051-9_7.PubMedView ArticleGoogle Scholar
  49. Horst SA, Jaeger T, Denkel LA, Rouf SF, Rhen M, Bange FC: Thiol peroxidase protects Salmonella enterica from hydrogen peroxide stress in vitro and facilitates intracellular growth. J Bacteriol. 2010, 192 (11): 2929-2932. 10.1128/JB.01652-09.PubMedPubMed CentralView ArticleGoogle Scholar
  50. Stourman NV, Branch MC, Schaab MR, Harp JM, Ladner JE, Armstrong RN: Structure and function of YghU, a nu-class glutathione transferase related to YfcG from Escherichia coli. Biochem. 2011, 50 (7): 1274-1281. 10.1021/bi101861a.View ArticleGoogle Scholar
  51. Stohl EA, Seifert HS: Neisseria gonorrhoeae DNA recombination and repair enzymes protect against oxidative damage caused by hydrogen peroxide. J Bacteriol. 2006, 188 (21): 7645-7651. 10.1128/JB.00801-06.PubMedPubMed CentralView ArticleGoogle Scholar
  52. LeBel CP, Ischiropoulos H, Bondy SC: Evaluation of the probe 2',7'-dichlorofluorescin as an indicator of reactive oxygen species formation and oxidative stress. Chem Res Toxicol. 1992, 5 (2): 227-231. 10.1021/tx00026a012.PubMedView ArticleGoogle Scholar
  53. Jakubowski W, Bartosz G: 2,7-dichlorofluorescin oxidation and reactive oxygen species: what does it measure?. Cell Biol Int. 2000, 24 (10): 757-760. 10.1006/cbir.2000.0556.PubMedView ArticleGoogle Scholar
  54. Palazzolo-Ballance AM, Reniere ML, Braughton KR, Sturdevant DE, Otto M, Kreiswirth BN, Skaar EP, DeLeo FR: Neutrophil microbicides induce a pathogen survival response in community-associated methicillin-resistant Staphylococcus aureus. J Immunol. 2008, 180 (1): 500-509.PubMedView ArticleGoogle Scholar
  55. Cha MK, Kim HK, Kim IH: Mutation and Mutagenesis of thiol peroxidase of Escherichia coli and a new type of thiol peroxidase family. J Bacteriol. 1996, 178 (19): 5610-5614.PubMedPubMed CentralGoogle Scholar
  56. Ajdic D, McShan WM, McLaughlin RE, Savic G, Chang J, Carson MB, Primeaux C, Tian R, Kenton S, Jia H: Genome sequence of Streptococcus mutans UA159, a cariogenic dental pathogen. Proc Natl Acad Sci U S A. 2002, 99 (22): 14434-14439. 10.1073/pnas.172501299.PubMedPubMed CentralView ArticleGoogle Scholar
  57. Kreth J, Zhang Y, Herzberg MC: Streptococcal antagonism in oral biofilms: Streptococcus sanguinis and Streptococcus gordonii interference with Streptococcus mutans. J Bacteriol. 2008, 190 (13): 4632-4640. 10.1128/JB.00276-08.PubMedPubMed CentralView ArticleGoogle Scholar
  58. Itzek A, Zheng L, Chen Z, Merritt J, Kreth J: Hydrogen Peroxide-Dependent DNA Release and Transfer of Antibiotic Resistance Genes in Streptococcus gordonii. J Bacteriol. 2011, 193 (24): 6912-6922. 10.1128/JB.05791-11.PubMedPubMed CentralView ArticleGoogle Scholar
  59. Battig P, Muhlemann K: Influence of the spxB gene on competence in Streptococcus pneumoniae. J Bacteriol. 2008, 190 (4): 1184-1189. 10.1128/JB.01517-07.PubMedPubMed CentralView ArticleGoogle Scholar
  60. Li YH, Lau PC, Lee JH, Ellen RP, Cvitkovitch DG: Natural genetic transformation of Streptococcus mutans growing in biofilms. J Bacteriol. 2001, 183 (3): 897-908. 10.1128/JB.183.3.897-908.2001.PubMedPubMed CentralView ArticleGoogle Scholar
  61. Aspiras MB, Ellen RP, Cvitkovitch DG: ComX activity of Streptococcus mutans growing in biofilms. FEMS Microbiol Lett. 2004, 238 (1): 167-174.PubMedGoogle Scholar
  62. Perry JA, Jones MB, Peterson SN, Cvitkovitch DG, Levesque CM: Peptide alarmone signalling triggers an auto-active bacteriocin necessary for genetic competence. Mol Microbiol. 2009, 72 (4): 905-917. 10.1111/j.1365-2958.2009.06693.x.PubMedPubMed CentralView ArticleGoogle Scholar
  63. Dufour D, Cordova M, Cvitkovitch DG, Levesque CM: Regulation of the competence pathway as a novel role associated with a streptococcal bacteriocin. J Bacteriol. 2011, 193 (23): 6552-6559. 10.1128/JB.05968-11.PubMedPubMed CentralView ArticleGoogle Scholar
  64. Grundy FJ, Waters DA, Allen SH, Henkin TM: Regulation of the Bacillus subtilis acetate kinase gene by CcpA. J Bacteriol. 1993, 175 (22): 7348-7355.PubMedPubMed CentralGoogle Scholar
  65. Wolfe AJ: The acetate switch. Microbiol Mol Biol Rev. 2005, 69 (1): 12-50. 10.1128/MMBR.69.1.12-50.2005.PubMedPubMed CentralView ArticleGoogle Scholar
  66. Kim JN, Ahn SJ, Seaton K, Garrett S, Burne RA: Transcriptional Organization and Physiological Contributions of the relQ Operon of Streptococcus mutans. J Bacteriol. 2012, 194 (8): 1968-1978. 10.1128/JB.00037-12.PubMedPubMed CentralView ArticleGoogle Scholar
  67. Chen PM, Chen HC, Ho CT, Jung CJ, Lien HT, Chen JY, Chia JS: The two-component system ScnRK of Streptococcus mutans affects hydrogen peroxide resistance and murine macrophage killing. Microbes Infect. 2008, 10 (3): 293-301. 10.1016/j.micinf.2007.12.006.PubMedView ArticleGoogle Scholar
  68. Deng DM, Liu MJ, ten Cate JM, Crielaard W: The VicRK system of Streptococcus mutans responds to oxidative stress. J Dent Res. 2007, 86 (7): 606-610. 10.1177/154405910708600705.PubMedView ArticleGoogle Scholar
  69. Wen ZT, Suntharaligham P, Cvitkovitch DG, Burne RA: Trigger factor in Streptococcus mutans is involved in stress tolerance, competence development, and biofilm formation. Infect Immun. 2005, 73 (1): 219-225. 10.1128/IAI.73.1.219-225.2005.PubMedPubMed CentralView ArticleGoogle Scholar
  70. Wen ZT, Baker HV, Burne RA: Influence of BrpA on critical virulence attributes of Streptococcus mutans. J Bacteriol. 2006, 188 (8): 2983-2992. 10.1128/JB.188.8.2983-2992.2006.PubMedPubMed CentralView ArticleGoogle Scholar
  71. Wen ZT, Burne RA: LuxS-mediated signaling in Streptococcus mutans is involved in regulation of acid and oxidative stress tolerance and biofilm formation. J Bacteriol. 2004, 186 (9): 2682-2691. 10.1128/JB.186.9.2682-2691.2004.PubMedPubMed CentralView ArticleGoogle Scholar
  72. Baldeck JD, Marquis RE: Targets for hydrogen-peroxide-induced damage to suspension and biofilm cells of Streptococcus mutans. Can J Microbiol. 2008, 54 (10): 868-875. 10.1139/W08-078.PubMedView ArticleGoogle Scholar
  73. Cheung J, Hendrickson WA: Sensor domains of two-component regulatory systems. Curr Opin Microbiol. 2010, 13 (2): 116-123. 10.1016/j.mib.2010.01.016.PubMedPubMed CentralView ArticleGoogle Scholar
  74. Cho HY, Cho HJ, Kim YM, Oh JI, Kang BS: Structural insight into the heme-based redox sensing by DosS from Mycobacterium tuberculosis. J Biol Chem. 2009, 284 (19): 13057-13067. 10.1074/jbc.M808905200.PubMedPubMed CentralView ArticleGoogle Scholar
  75. Podust LM, Ioanoviciu A, de Montellano PR O: 2.3 A X-ray structure of the heme-bound GAF domain of sensory histidine kinase DosT of Mycobacterium tuberculosis. Biochem. 2008, 47 (47): 12523-12531. 10.1021/bi8012356.View ArticleGoogle Scholar
  76. Patton TG, Rice KC, Foster MK, Bayles KW: The Staphylococcus aureus cidC gene encodes a pyruvate oxidase that affects acetate metabolism and cell death in stationary phase. Mol Microbiol. 2005, 56 (6): 1664-1674. 10.1111/j.1365-2958.2005.04653.x.PubMedView ArticleGoogle Scholar
  77. Ahn SJ, Lemos JA, Burne RA: Role of HtrA in growth and competence of Streptococcus mutans UA159. J Bacteriol. 2005, 187 (9): 3028-3038. 10.1128/JB.187.9.3028-3038.2005.PubMedPubMed CentralView ArticleGoogle Scholar
  78. Abranches J, Candella MM, Wen ZT, Baker HV, Burne RA: Different roles of EIIABMan and EIIGlc in regulation of energy metabolism, biofilm development, and competence in Streptococcus mutans. J Bacteriol. 2006, 188 (11): 3748-3756. 10.1128/JB.00169-06.PubMedPubMed CentralView ArticleGoogle Scholar
  79. Ahn SJ, Wen ZT, Burne RA: Multilevel control of competence development and stress tolerance in Streptococcus mutans UA159. Infect Immun. 2006, 74 (3): 1631-1642. 10.1128/IAI.74.3.1631-1642.2006.PubMedPubMed CentralView ArticleGoogle Scholar
  80. Yin JL, Shackel NA, Zekry A, McGuinness PH, Richards C, Putten KV, McCaughan GW, Eris JM, Bishop GA: Real-time reverse transcriptase-polymerase chain reaction (RT-PCR) for measurement of cytokine and growth factor mRNA expression with fluorogenic probes or SYBR Green I. Immunol Cell Biol. 2001, 79 (3): 213-221. 10.1046/j.1440-1711.2001.01002.x.PubMedView ArticleGoogle Scholar
  81. Edgar R, Domrachev M, Lash AE: Gene Expression Omnibus: NCBI gene expression and hybridization array data repository. Nucleic Acids Res. 2002, 30 (1): 207-210. 10.1093/nar/30.1.207.PubMedPubMed CentralView ArticleGoogle Scholar
  82. Brazma A, Hingamp P, Quackenbush J, Sherlock G, Spellman P, Stoeckert C, Aach J, Ansorge W, Ball CA, Causton HC: Minimum information about a microarray experiment (MIAME)-toward standards for microarray data. Nat Genet. 2001, 29 (4): 365-371. 10.1038/ng1201-365.PubMedView ArticleGoogle Scholar
  83. Seaton K, Ahn SJ, Sagstetter AM, Burne RA: A transcriptional regulator and ABC transporters link stress tolerance, (p)ppGpp, and genetic competence in Streptococcus mutans. J Bacteriol. 2011, 193 (4): 862-874. 10.1128/JB.01257-10.PubMedPubMed CentralView ArticleGoogle Scholar
  84. Trieu-Cuot P, Carlier C, Poyart-Salmeron C, Courvalin P: A pair of mobilizable shuttle vectors conferring resistance to spectinomycin for molecular cloning in Escherichia coli and in gram-positive bacteria. Nucleic Acids Res. 1990, 18 (14): 4296-10.1093/nar/18.14.4296.PubMedPubMed CentralView ArticleGoogle Scholar
  85. Que YA, Haefliger JA, Francioli P, Moreillon P: Expression of Staphylococcus aureus clumping factor A in Lactococcus lactis subsp. cremoris using a new shuttle vector. Infect Immun. 2000, 68 (6): 3516-3522. 10.1128/IAI.68.6.3516-3522.2000.PubMedPubMed CentralView ArticleGoogle Scholar


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