Research Article

Activation of the SMU.1882 Transcription by CovR in Streptococcus mutans

  • Patrick Chong equal contributor,

    equal contributor Contributed equally to this work with: Patrick Chong, Partho Chattoraj

    Affiliation: Department of Microbiology, Molecular Genetics and Immunology, University of Kansas Medical Center, Kansas City, Kansas, United States of America

    Current address: Antimicrobial Resistance and Nosocomial Infections, National Microbiology Laboratory, Winnepeg, Canada

  • Partho Chattoraj equal contributor,

    equal contributor Contributed equally to this work with: Patrick Chong, Partho Chattoraj

    Affiliation: Department of Microbiology, Molecular Genetics and Immunology, University of Kansas Medical Center, Kansas City, Kansas, United States of America

  • Indranil Biswas mail

    Affiliation: Department of Microbiology, Molecular Genetics and Immunology, University of Kansas Medical Center, Kansas City, Kansas, United States of America

  • Published: November 22, 2010
  • DOI: 10.1371/journal.pone.0015528


In Streptococcus mutans, the global response regulator CovR plays an important role in biofilm formation, stress-tolerance response, and caries production. We have previously shown that CovR acts as a transcriptional repressor by binding to the upstream promoter regions of its target genes. Here, we report that in vivo, CovR activates the transcription of SMU.1882, which encodes a small peptide containing a double-glycine motif. We also show that SMU.1882 is transcriptionally linked to comA that encodes a putative ABC transporter protein. Several genes from man gene clusters that encode mannose phosphotranferase system flank SMU.1882 -comA genes. Genomic comparison with other streptococci indicates that SMU.1882 is uniquely present in S. mutans, while the man operon is conserved among all streptococci, suggesting that a genetic rearrangement might have taken place at this locus. With the use of a transcriptional reporter system and semi-quantitative RT-PCR, we demonstrated the transcriptional regulation of SMU.1882 by CovR. In vitro gel shift and DNase I foot-printing analyses with purified CovR suggest that CovR binds to a large region surrounding the -10 region of the P1882. Using this information and comparing with other CovR regulated promoters, we have developed a putative consensus binding sequence for CovR. Although CovR binds to P1882, in vitro experiments using purified S. mutans RpoD, E. coli RNA polymerase, and CovR did not activate transcription from this promoter. Thus, we speculate that in vivo, CovR may interfere with the binding of a repressor or requires a cofactor.


Streptococcus mutans, which is a part of the normal flora of the human oral cavity, is considered to be the primary etiological agent in the formation of dental caries [1], [2]. Dental caries is a global health problem that affects from 60–90% of school children, as well as many adults in industrialized countries [3], [4], [5]. Although not fatal, dental caries is a costly disease, leading to annual expenditure in billions of dollars in the U.S. alone. S. mutans is also a leading cause of bacterial endocarditis, with greater than 14% of viridians streptococcus-induced endocarditis triggered by infections of S. mutans [6]. For colonization in the oral cavity, S. mutans metabolizes the dietary carbohydrates ingested by its host to produce glucan and to anchor itself to the tooth surface, forming densely populated microbial biofilms known as dental plaque that includes hundreds of species of other oral bacteria [7]. The capacity of S. mutans to persist and to maintain a dominant presence in the oral cavity is due to its ability to adapt and respond to a variety of adverse growth-limiting conditions and production of antimicrobial peptides known as mutacins [8], [9].

Bacteria have evolved several strategies to adapt to unexpected changes in their extracellular environment, but the predominant mechanism is the so-called two-component signal transductions system (TCS) [10]. TCSs allow bacteria to coordinate a focused and appropriate physiological response to counter the effects of specific extracellular stimuli. A TCS typically consist of two main components: a membrane-bound sensor histidine kinase, which senses environmental cues, and a cytoplasmic response regulator, which upon activation by the cognate histidine kinase, elicits the appropriate cellular response, usually by binding to specific DNA target sequences, and acting as a transcriptional regulator to modulate the expression of various genes, depending on the growth condition [10].

The TCS CovRS has been extensively studied in streptococcal spp., particularly in group-A-streptococcus (GAS) [11], [12], [13], [14]. CovRS directly or indirectly regulates approximately 15% of the GAS genome, including many virulence genes. CovRS also mediates the growth of GAS during periods of iron starvation as well as growth in the bloodstream [14], [15], [16]. The vast majority of the CovR regulon is repressed by CovR [17]. CovS is thought to be the cognate sensor kinase for the phosphorylation or dephosphorylation of CovR, which typically functions as a transcriptional repressor [18]; environmental stimuli, particularly during periods of stress, are recognized by CovS, which regulates the activity of the global response regulator CovR [11]. Although CovR regulates the expression of common sets of genes in different GAS strains, there are also variations in the CovR regulon that arise between strains [19], [20]. CovRS is also associated with virulence in group-B-streptococcus (GBS) and in group-C-streptococcus (GCS) [17], [21], [22]. Approximately 6% of the genome of GBS is regulated by CovRS, including some virulence factors [22], [23]; as with GAS, the CovR regulon is mostly repressed by CovR.

S. mutans encodes 14 putative TCS in its genome [24], [25]; however, unlike other streptococcal spp., S. mutans does not encode covS, but does express CovR, also known as GcrR or TarC [26], [27], [28]. Therefore, CovR appears to be an orphan response regulator in S. mutans. As with other streptococcal spp., CovR is an important global response regulator in S. mutans, as it regulates the expression of various virulence genes that are essential for biofilm formation, such as the glucosyltransferases (gtfB/C), glucan-binding proteins C (gbpC), and also of its own expression [27], [29], [30].

In GAS, CovR typically functions as a transcriptional repressor [14], [17]. With respect to S. mutans, while CovR negatively regulates the expression of the afore-mentioned genes, our data indicates that CovR can also function as an activator of gene expression (Biswas, unpublished) one such example is an open reading frame encoded by SMU.1882. In order to gain further insight into the importance of CovR in the physiology of S. mutans, and the mechanism of gene regulation, we begin by having a look at the regulation of SMU.1882 by CovR. In this communication, we report that CovR, under in vivo conditions, activates the expression of SMU.1882. CovR directly binds to the putative promoter region of SMU.1882 and protects a region containing putative promoter elements against DNase I digestion. However, binding of CovR to the promoter of SMU.1882 did not stimulate transcription under in vitro conditions, suggesting other factors may be involved under in vivo conditions.


SMU.1882 is unique to S. mutans

Bioinformatics analysis of SMU.1882 gene (354-bp) reveals that it encodes a hypothetical protein of 117 amino acid residues in length containing three double-glycine (GG) motifs, one of which is at position 23. A recent in silico analysis suggests that the SMU.1882 peptide is a secretory molecule [31]; the GG motif at position 23 is thought to be the site at which the cleavage occurs. However, our analyses of the genome of S. mutans along with other streptococcal spp., including S. agalactiae, S. gordonii, S. mitis, S. pneumoniae, and S. pyogenes, S. thermophilus, using software at the Comprehensive Microbial Resource website (​HomePage.cgi), revealed that SMU.1882 is unique to S. mutans, as it is apparently not found in these streptococcal spp. (data not shown); however, several small GG containing peptides and homologs of the upstream SMU.1883 gene are present in some streptococci. While SMU.1882 and the adjacent comA homolog, SMU.1881, are unique to the S. mutans strains, the flanking genes, which encode mannose-phosphotransferase system (man-PTS) are very well conserved among streptococci and other Firmicutes [32].

Transcriptional organization of the SMU.1882 locus

A schematic diagram of the SMU.1882 locus and the genes in its vicinity are shown in Fig. 1A. Sequence analysis, confirmed using BPROM online software (Prediction of bacterial promoters, Softberry,, indicates the presence of putative -35 (GTGAGT) and -10 (TATAAT) box motifs 151- and 127-bp, respectively, upstream of the putative start codon with a putative ribosomal binding site (AGAGA) 11-bp upstream of the start codon. A putative rho-independent terminator sequence (GCCTGACTACATAGATGTCAGGC) was identified at position 402-bp downstream of SMU.1882 by TransTerm ( program.


Figure 1. Transcriptional analysis of SMU.1882 locus.

(A) Schematic diagram of SMU.1882 locus. Open reading frames (orf) are designated by block arrows, and their orientations indicate the direction of transcription. The sequence upstream of SMU.1882 orf is shown below the diagram. (B) Stability of SMU.1882 transcript. The stability of SMU.1882 transcript was measured using cultures at mid-exponential growth phase (70 KU). RNA was extracted from S. mutans wild type strain UA159 at the time (in minutes) indicated above the lanes following addition of rifampin to block de novo transcription. The mRNA decay curve was plotted as a function of time (in minutes). (C) Northern blotting was carried out using the SMU.1882 orf as a probe. A major band of 1.5 kb and two minor bands (3.0 kb and 6.0 kb) were obtained. (D) Transcriptional linkage analysis. Transcription linkage between SMU.1882/comA, and SMU.1884/SMU.1882 was analyzed using the primer pair 1+2 and 3+4, respectively. K-DNA denotes genomic DNA. (E) Amino acid sequence encoded by SMU.1882. The conserved GG-motif, the putative site for the signal peptide cleavage, is underlined.


Since the transcripts of many CovR regulated genes have relatively shorter half-life, we therefore evaluated the stability of SMU.1882 transcript. The results of the mRNA stability assay indicated that the chemical half-life of the SMU.1882 transcript was approximately 2–3 minutes (Fig. 1B). Northern blot analysis indicated that there was one major band of 1.5-kb (which was used for the stability determination) and two other minor bands of approximately 3.0- and 6.0-kb, which constituted less than 5% of the total signal (Fig. 1C), suggesting that other genes may be cotranscribed along with SMU.1882. To determine whether the downstream comA (SMU.1881) was transcriptionally linked to SMU.1882, PCR analysis was performed using cDNA, with chromosomal DNA and RNA as the positive and negative controls, respectively. As shown in Fig. 1D, SMU.1882 appears to be transcriptionally linked with comA, which would account for the presence of the 3-kb transcript seen in the northern blot. This product could be generated due to read-through transcription from the SMU.1882 promoter.

CovR upregulates transcription from P1882 in vivo

To gain insight into the link between CovR and expression of SMU.1882, sqRT-PCR was used to quantify the level of CovR-dependent expression of SMU.1882. Wild-type S. mutans UA159, and its isogenic ΔcovR derivative, IBS603, were grown to mid-exponential phase (KU70), followed by harvesting and extraction of RNA. The gyrA gene was included as control to ensure that equivalent amounts of RNA were being used for each reaction. Fig. 2A shows that higher levels of SMU.1882 transcript are being produced from the wild-type strain compared to the covR mutant strain, with approximately three-fold difference in expression of SMU.1882; complementation of the ΔcovR mutant strain with plasmid pIB30 (IBS603/pIB30), which carries the full length, wild-type covR gene in trans, restores expression of SMU.1882 to the wild type level. Since SMU.1883 gene appears to be divergently transcribed from the promoter upstream of the SMU.1882, we also measured the level of SMU.1883 transcript by sqRT-PCR. We found no significant difference between the wild type and the covR mutant strains. Thus, although SMU.1882 and SMU.1883 share the same intergenic region, CovR appears to only activate transcription of the SMU1882 gene. The results of the sqRT-PCR were further supported by real-time RT-PCR analysis. As shown in Fig. 2B, we found that the transcript level in the covR mutant strain was approximately 2.5-fold lower compared to the wild type strain.


Figure 2. CovR is required for SMU.1882 expression.

(A). Semi-quantitative RT-PCR analysis of SMU.1882, SMU.1883, and gyrA for the strains UA159, ΔcovR (IBS603) and ΔcovR complemented with pIB30 (IBS603/pIB30). The gyrA gene was included as an internal control to ensure that equal amounts of RNA were loaded per lane. Experiments were repeated at least twice with two independent RNA isolations. (B) Quantitative real-time PCR analysis of SMU.1882 transcript in wild type, ΔcovR (IBS603) and ΔcovR complemented with pIB30 (IBS603/pIB30). The expression of SMU.1882 was normalized to the expression level of gyrA as an internal reference. Relative fold changes in gene expression are represented as histograms with error bars. Each histogram is the mean of four biological replicates. (C) Reporter fusion assay. The putative promoter of SMU.1882 was fused to a promoter-less gusA reporter gene and inserted into the S. mutans UA159 chromosome. Expression driven from the promoters was evaluated by measuring Gus activity. Gus values were measured from at least three independent cultures; mean values with standard deviations are shown.


To confirm that CovR can regulate SMU.1882 promoter at a non-native locus, we used a transcriptional reporter fusion for analysis to avoid any cis-effect that may alter the gene expression. Transcriptional fusion reporter strains were constructed by cloning the putative promoter region of SMU.1882 into plasmid pIB107, which contains a promoterless gusA gene [29]. This construct was inserted at the SMU.1405 locus, which is well separated from the native SMU.1882 locus [29]. When the wild type, covR-deletion mutant (IBS606), and complemented covR-deletion mutant (IBS606/pIB30) strains, containing the P1882-gusA transcriptional fusion reporter, were assayed for Gus activity. As shown in Fig. 2B, GusA activity was significantly reduced in the mutant strain IBS606, indicating that CovR is required to activate transcription from P1882. However, GusA activity was restored to the parental level when the ΔcovR strain was complemented with covR in trans (IBS606/pIB30). Taken together, the results of the RT-PCR analyses and the reporter fusion assays indicate that expression of SMU.1882 is up regulated in the presence of CovR.

CovR directly binds to P1882 in vitro

Electrophoretic mobility shift assays (EMSA) and DNase I protection assays were used to demonstrate the specific binding of CovR to the putative promoter region of SMU.1882, P1882. As shown in Fig. 3A, incubation of the P1882 DNA fragment with increasing amounts of CovR leads to retardation in the mobility of the DNA fragment. Incubation of the 32P-labeled P1882 fragment with a 25-fold higher amount of non-labeled P1882 DNA fragment resulted in no shifting of the labeled band, while the addition of a 25-fold higher amount of a DNA fragment containing the promoter region for the nlmA gene (PnlmA), which encodes a peptide component of mutacin IV and is not regulated by CovR, did not inhibit shifting of the CovR-bound P1882 fragment (Fig. 3A). This demonstrates that CovR binds specifically to the promoter region of SMU.1882.


Figure 3. CovR binds to SMU.1882 promoter region.

(A) In vitro binding of CovR to the promoter of SMU.1882. EMSA was performed with His-tagged CovR as described in the text. Lanes: 1, no CovR; 2, 14.97 pmol CovR; 3, 29.94 pmol CovR; 4, 59.88 pmol CovR; 5, 89.82 pmol CovR; 6, 119.76 pmol CovR; 7 and 8, 29.94 pmol CovR. 0.5 pmol labelled P1882 was used in all the reactions. 25-fold molar excess of cold P1882 and PnlmA were used in lanes 7 and 8 respectively. B: bound DNA; F: free DNA. (B) DNase I protection assay of the putative SMU.1882 promoter. 0.5 pmol labelled P1882 was used in all the reactions. Lane: 1, no CovR; 2, 59.88 pmol CovR; 3, 89.82 pmol CovR; 4, 119.76 pmol CovR; 5, 187.125 pmol CovR. Footprints were run in an 8% sequencing gel next to sequencing ladders (G, A, T, and C). CovR binding regions are indicated by vertical lines at the side of the sequencing gels, while horizontal lines mark -10 and -35 regions of the promoter. All experiments were carried out at least thrice, and a representative gel is shown.


DNase I protection assays were performed to determine the portion of P1882 that binds to CovR, using the same P1882-CovR mixtures prepared for EMSA, as described above. Analysis of the gel indicates that CovR binds to the DNA fragment from position -200 to -1, relative to the start codon, and protects this region against digestion by DNase I (Fig. 3B). This region also includes the putative ribosomal binding site, AGAGA, which is found 13-bp upstream of the start codon, as well as the putative -35 and -10 box regions. Taken together, the results of the EMSA and DNase I analyses suggest that CovR activates the expression of SMU.1882 by specifically binding to P1882.

CovR regulation of SMU.1882 expression is not strain-specific

Bioinformatics analysis at the CMR website indicates that gene SMU.1882 is not found in streptococcal spp. outside of S. mutans strain UA159; however, it was not known whether SMU.1882 is conserved in other isolates of S. mutans. To determine whether SMU.1882 is present in other S. mutans strains, we used Southern hybridization to verify whether SMU.1882 was present in other isolates, from three different serotypes (c, e, and f) of S. mutans. A 32P-labeled DNA fragment containing a 267-bp internal SMU.1882 sequence derived from the genome of UA159 was used as a probe against the XmnI-digested chromosomal DNA from a number of S. mutans isolates. The results of the Southern hybridization analysis are shown in Figure 4A. Sequence analysis predicts that, a diagnostic 6-kb DNA fragment will be generated after XmnI-digestion UA159 genomic DNA. As shown in Fig. 4A, with the exception of strains T8, 109C, and UA130 that did not produce bands, the hybridization pattern observed for the majority of the isolates was identical with that of UA159 (6 kb); however, the observed band for strain OMZ175 was 4-kb. The overall results suggest that SMU.1882 is conserved in most, but not all, strains of S. mutans.


Figure 4. Presence of SMU.1882 locus in different strains of S. mutans.

(A) Southern hybridization blot of XmnI digested chromosomal DNA from different S. mutans strains belonging to three serotypes (c, e and f). A 267-bp internal SMU.1882 sequence was used as a probe against the digested DNA. Semi-quantitative RT-PCR analysis (B) and quantitative real-time PCR analysis (C) of S. mutans strain GS-5, its isogenic ΔcovR strain (IBS07) and the complementing strain (IBS07/pIB30). (D) Quantitative real-time PCR analysis of SMU.1882 transcript in NG-8, its isogenic ΔcovR strain (IBS06) and ΔcovR complemented with pIB30 (IBS06/pIB30). The expression of SMU.1882 was normalized to the expression level of gyrA as an internal reference for quantitative real-time PCR analyses.


GS-5 and NG-8 are two other S. mutans strains that have been characterized to some degree. To determine whether CovR-activation of SMU.1882 is unique to strain UA159, sQRT-PCR analysis was performed on S. mutans strain GS-5 and its isogenic covR mutant derivative, IBS07; the results indicate that CovR-dependent regulation of SMU.1882 is not limited to strain UA159. Fig. 4B shows that there is a 1.8 to 2.0-fold drop in expression of SMU.1882 in IBS07 relative to the wild-type GS-5. Complementation of the covR mutant with full-length covR (IBS07/pIB30), in trans, restores the expression of SMU.1882 slightly higher than the wild-type level. sQ-RT results were further confirmed by real-time RT-PCR that showed a similar reduction of SMU.1882 transcript in IBS07 as compared with GS-5 (Fig. 4C). Furthermore, inactivation of covR in S. mutans strain NG8 also indicates that CovR activates the expression of SMU.1882 in this strain (Fig. 4D). Taken together, the results suggest that CovR regulation of SMU.1882 expression is not limited to the UA159 strain alone and the degree of reduction of SMU.1882 transcript in different strains appears to be similar.

CovR does not activate expression of SMU.1882 in vitro

In vitro transcription assays were performed to demonstrate direct activation of expression from P1882. A 319-bp fragment, containing the first 82-bp of SMU.1882 as well as the putative promoter elements, was PCR-amplified from the S. mutans chromosome, and used as template for the in vitro transcription run-off assays, along with a 319-bp fragment containing Pami that was amplified from pIB163 which was used as a control. To perform the reaction, E. coli RNA polymerase core enzyme was reconstituted with purified his-tagged RpoD from S. mutans. As shown in Fig. 5, addition of reconstituted RNA polymerase holoenzyme, but not the core enzyme, generated expected size bands of 193-nt and 158-nt when P1882 and Pami, respectively, were used as template (lanes 2 and 7). However, the addition of CovR did not lead to any observable increase in transcription from P1882. The level of transcription in the reaction mixes containing purified CovR (lanes 4–6) did not appear to be any different than the lanes that did not contain CovR (Lane 3).


Figure 5. Effect of CovR on transcription from P1882.

In vitro transcription was carried out using P1882 and Pami template DNA according to the protocol as described in the text. Lanes 1–3: no CovR; lanes 4–6: increasing concentration of CovR (1, 4, and 10 pmole, respectively). The experiments were repeated at least twice and a representative gel is shown.



Many bacterial TCS activate gene expression, but CovR in GAS and GBS typically acts to repress gene expression; of the 271 genes regulated by CovR in GAS, only 26 are upregulated by CovR (during late exponential phase) [17]. Our own data suggest that CovR of S. mutans predominantly functions as a repressor [27], [29], [30]. However, CovR can also act as a transcriptional activator in streptococci, either directly or indirectly [17], [33]; and in the case of S. mutans, one such gene that appears to be activated by CovR is SMU.1882. The goal of this study was to elucidate the nature of the regulatory interaction between CovR and SMU.1882.

In GAS, binding of CovR to the promoter sequences of the has, covR, and dppA, under in vitro conditions, requires the presence of a consensus binding sequence (CB) ATTARA, or the near-CB ATTAAC [33], [34], [35]. However, the importance of this sequence in the promoter regions of S. mutans genes for CovR-binding is unclear, since the ATTARA sequence is not found in the intragenic sequences of some CovR-regulated genes of S. mutans [29], [30]. Given the high degree of similarity between CovR of GAS and S. mutans, it is surprising that the ATTARA sequence is not more prevalent in the promoter regions of S. mutans genes. A single ATTAAA sequence is found 67-bp upstream of the start codon; whether this sequence is a CB for P1882 remains to be studied. However, mutation of the ATTARA sites of PdppA in GAS did not inhibit transcription in vivo, although the ATTARA sequences appeared to be essential under in vitro conditions [33]. As such, it is possible that the lone ATTARA site in P1882 may not function as a CB under in vivo conditions.

In S. mutans, CovR has been shown to bind directly to five promoters, including P1882, to modulate gene expression [27], [29], [30]. However, a consensus DNA binding sequence (CBS) motif for CovR has not been developed. In an effort to create a CBS for CovR, we have used GLAM2 [36] program on the five promoter sequences that are regulated by CovR to develop an optimized position weight matrix for CovR binding. We obtained four different CBSs with overall weight score varied from 78.4 to 67.8. The CBS with the highest score and the location of the CBS on five promoter regions are shown in Fig. 6. Interestingly for one promoter, PgtfC, this CBS was present twice, one on the sense and another on the nonsense strands. However, the significance of this newly derived CBS in CovR binding needs to be verified experimentally.


Figure 6. Potential consensus sequence for CovR binding.

(A) WebLogo representation of the position weight matrices derived from five CovR regulated promoters using GLAM2 [36]. (B) The location of the consensus sequence in the promoter region of the corresponding genes.


The results of the sQRT-PCR and reporter expression analyses demonstrate that CovR is required for the increased expression of P1882 under in vivo conditions, while in vitro gel shift and DNase I protection assays show that CovR directly binds to a portion of the intragenic region upstream of SMU.1882. Taken together, the results suggested to us that CovR might play a direct role in the activation of expression of SMU.1882. However, the results of the in vitro transcription assays appear to indicate otherwise, since activation of SMU.1882 expression was not observed with the addition of purified CovR. Our results are similar to the observations made with the in vitro transcription reactions with PdppA of GAS, where CovR appeared to be required for in vivo activation of transcription of dppA, but could not activate transcription under in vitro conditions [33]. It is always possible that the in vitro transcription reaction conditions were much different than the in vivo conditions or the role of CovR may not be to directly activate transcription of SMU.1882, but to displace other proteins that may be inhibiting or silencing transcription of SMU.1882. It is possible that the RpoD (sigma factor) does not functionally interact with E. coli RNA core polymerase and thus CovR's effect is not seen in vitro. However, we believe this scenario is unlikely since several heterologous sigma factors are shown to functionally interact both in vivo and in vitro with E. coli RNA polymerase [37], [38], [39]. Thus, how CovR activates SMU.1882 expression in vivo needs to be elucidated.

There are several possibilities by which CovR can activate gene transcription. For example, CovR can acts as an anti-silencer of gene expression. Recently, in Salmonella, it has been shown that response regulator such as PhoP [40] or SsrB [41] can overcome H-NS (a nucleoid-binding protein) mediated gene silencing; however, the exact molecular mechanism by which these response regulators function as anti-silencers is not yet known. However, it is conceivable that HLP, an H-NS homolog, can also silence gene expression in S. mutans and the role of CovR is to overcome the silencing effect of HLP by replacing it from the promoter. We believe this scenario is very unlikely since the binding of HLP to P1882 is non-specific as opposed to the silenced promoters where HLP binding is specific (data not shown). Furthermore, if a repressor protein, such as HLP, binds to the intergenic region between SMU.1882 and SMU.1883, then the expression of SMU.1883 would also be affected in the covR deleted strain, which was not the case (Fig. 2A). The SMU.1883 gene encodes a component of the man-PTS system (ManO) and is highly conserved among various streptococci [32]. Because other genes of the man-PTS system are not regulated by CovR in other bacteria [17], we believe that this gene is not under the CovR regulatory pathway.

The other possibility is that CovR might work alongside other regulatory proteins in order to interactively regulate the expression of target genes, similar to RcsB response regulator of Salmonella. In this case, RcsB requires a co-activator, RcsA, for the expression of certain genes such as ugd [42]. On the other hand, a small molecule can bind to CovR and change its conformation/oligomerization state such that CovR can act as an activator. A well-know example of a transcriptional regulator that changes its conformation upon small molecule binding is TraR of Agrobacterium tumefaciens. In this case, when the cognate autoinducer ligand binds to TraR, it changes the conformation and the oligomerization of the TraR [43]. Further experiments are required to verify whether CovR interacts with other regulatory proteins or ligands as well as to understand the molecular mechanism by which CovR activates the transcription from the SMU.1882 promoter.

At the present time, the exact physiological role of SMU.1882 is unclear. This gene appears to be found only in S. mutans, but not in other streptococci. Based on the sequence and the presence of a GG motif at the N-terminal region coupled with the fact that SMU.1882 is topologically and transcriptionally associated with an ABC transporter (ComA) strongly suggest that SMU.1882 might encode a bacteriocin related peptide. Inactivation of SMU.1882 did not produce any noticeable phenotypes when tested against five streptococcal and one lactococcal species (data not shown). Analysis of the S. mutans UA159 genome by BAGEL [44] suggests that this strain encodes at least 26 putative bacteriocins. Since S. mutans resides in the dental plaque that contains over 700 different bacterial species [45], it is possible that for successful colonization and survival, S. mutans may need such a high number of bacteriocins. Although the target species remain to be identified, we believe that SMU.1882 is one of such bacteriocin that may provide a fitness advantage to S. mutans by controlling the growth of other competing species in the dental plaque.

Materials and Methods

Bacterial strains and growth conditions

Escherichia coli strain DH5α was grown in Luria-Bertani (LB) medium supplemented (when necessary) with ampicillin (50 or 100 µg/ml) or kanamycin (50 µg/ml). S. mutans strains UA159 and GS-5, and other mutans isolates, were typically grown in Todd-Hewitt medium (BBL, Becton Dickson) supplemented with 0.2% yeast extract (THY). Growth of the S. mutans cultures was monitored using a Klett-Summerson colorimeter with a red filter.

Extraction of RNA from S. mutans strain UA159

RNA, which was used for various experiments, was isolated from cultures of S. mutans strains UA159 (and its derivatives) and GS-5 (and its derivatives), grown to mid-exponential phase (Klett unit (KU) 70), under the growth conditions specified above. The cultures were harvested via centrifugation, re-suspended and incubated in RNA protect reagent (Qiagen) at room temperature for 30 min, and then re-centrifuged to form a pellet, which was either stored overnight at −20°C or processed immediately for RNA extraction. RNA extraction was performed as described by Biswas et al. [30].

Determination of the stability of the SMU.1882 transcript of S. mutans

The stability of SMU.1882 mRNA was determined using a protocol described by Biswas et al. [30]. Upon reaching the desired optical density (O.D.), the RNA polymerase inhibitor rifampin was immediately added to each culture to prevent the de novo synthesis of RNA. RNA was then collected from aliquots of S. mutans at 8 time points, during a total incubation period of 30 minutes at 37°C. At each time point, sodium azide (final concentration: 50 mM) was added to the culture to terminate cellular processes, and then immediately placed in dry ice. RNA (4 µg) from each time point was denatured, loaded onto a 1% agarose gel, and separated via electrophoresis for northern blot analysis. DNA probes were synthesized via PCR amplification using the primer pairs Smu1882 F3 and Smu1882 R3 (for a list of primers see Table 1), with chromosomal DNA of S. mutans UA159 as template. The probes were labeled using [α-32P] dATP, with a DECAprimeII kit (Ambion), and added to a hybridization tube containing the transfer membrane and ULTRAhyb buffer (Ambion), followed by overnight incubation. Following hybridization, the membrane was washed according to manufacturer's instructions, dried, and exposed to a phosphorimager plate and analyzed using a Typhoon phosphorimager (Molecular Dynamics).


Table 1. Primers used in the analysis.


Semiquantitative and real-time RT-PCR analyses

Semi-quantitative (sq) RT-PCR was used to quantify the level of expression of various genes in UA159 and GS-5, along with the respective covR mutant strains. The S. mutans cultures were grown to mid-exponential phase (KU70), followed by RNA extraction. sqRT-PCR was performed as previously described [30] using the Titan one-tube RT PCR system (Roche). The gyrA gene was included as control to ensure that equivalent amounts of RNA were being used for each reaction. For real-time RT-PCR, cDNA was prepared from samples as described above. cDNA levels were quantified in 7500 Fast real-time PCR machine (Applied Biosystems). The reactions were performed in 20 µl final volume, consisting of 1X Fast SYBR Green Master Mix (Applied Biosystems) and 0.5 µM of each sense and antisense primer pair. For every primer pair, four different cDNA concentrations were analysed in duplicate. Cycling conditions were as follows: 95°C for 1 min, followed by 40 cycles of 95°C for 15 s and 60°C for 1 min with fluorescent measurement at the end of each cycle and one dissociation step of 95°C for 15 s, 60°C for 30 s and 95°C for 15 s. gyrA housekeeping gene served as an internal control to normalize the expression levels between samples. No template controls were included in all real-time PCR reactions. Standard curves were plotted (GraphPad Prism) for all three samples using log input dilution series of K-DNA templates against cycle threshold values (Ct) of the performed qPCR. Slopes and R2 values were obtained and were used to calculate real time PCR reaction efficiencies [E = 10̂(−1/slope)]. The relative expression levels were calculated according to the method developed by Pfaffl [46]. GraphPad prism software was employed to analyze the experimental data. The data are presented as mean value +/− SD.

Construction of CovR deleted strains

To create a covR-deleted strain, we used pIB10 [29] that contains a 1.7-kb fragment containing the entire covR gene with flanking regions. A Km resistant cassette with flanking modified loxP sites, was amplified from pUC4ΩKm2 [47] using the primers lox71-Km-F and lox66-Km-R [48] and cloned into the BseRI -NruI digested and T4-DNA polymerase blunted sites to generate pIB-601. Plasmid pIB-601 was linearized with EcoRI and transformed into S. mutans UA159 as previously described [48]. Transformants were selected on THY plates containing Km; one such transformant was named IBS-601. To eliminate the loxP-Kmr cassette from the chromosome, IBS-601 was transformed with pCrePA [48], which expresses the cre recombinase gene from a temperature-sensitive replicon (pWV01). Subsequently, Emr and Kms colonies were selected; those colonies contain pCrePA and lost the Km resistance gene from the chromosome. Subsequently, pCrePA plasmid was cured as described previously to generate IBS-603, which contains a markerless covR deletion.

To generate covR deletion construct in GS-5 and NG-8, plasmid pIB26 [29] was used that contains a spectinomycin resistant gene inserted in the middle of the covR gene. This plasmid was linearized with NotI and used for S. mutans transformation.

Construction of P1882-gusA reporter strains and quantification of transcription from P1882

To quantify transcription from P1882 from S. mutans UA159, a reporter strain was constructed by cloning the putative promoter region of SMU.1882 into plasmid pIB107 [29], which contains a promoterless gusA gene. The putative P1882 region was amplified from S. mutans chromosomal DNA using primers Smu1882 F1 and Smu1882 R1, which contain BamHI and XhoI sites, respectively (Table 1). This fragment was digested using BamHI and XhoI, and cloned into BamHI-XhoI-digested pIB107 [29] to yield plasmid pIB602, which was then transformed into E. coli DH5α. Plasmid pIB602 was purified from overnight grown cultures of E. coli DH5α, linearized with BglI, and used for the transformation of S. mutans strains UA159 (wild-type), IBS603 (ΔcovR), and IBS603/pIB30 (ΔcovR, complemented with wild-type covR in trans) to generate the reporter strains IBS602, IBS606, and IBS606/pIB30, respectively. The reporter strains were grown to mid-exponential phase (KU70) in THY broth containing Em to maintain the complementing plasmid. The cells were harvested via centrifugation and lysed for β-glucuronidase (GusA) assays, as described by Biswas et al. [29].

Electrophoretic mobility shift assay (EMSA) and DNase I protection assay (DPA)

EMSA and DPA were used to demonstrate binding of CovR to P1882. Primer Smu1882 F1 was labeled with γ32-ATP and, along with Smu1882 R1, was used to PCR amplify a DNA fragment containing P1882, with a radiolabel at the 5′-end of the fragment. Each fragment was incubated with various concentrations of 6XHis-tagged CovR protein in binding buffer (final volume - 50 µl) as described by Biswas et al. [30]. Following 40–45 minutes incubation, at ambient room temperature, 10 µl of the nucleo-protein mix was loaded onto a 4% (29:1) native PAGE gel, buffered with 0.5X TBE buffer, pH 8.0. The loaded PAGE was then electrophoresed at room temperature, in the same buffer for 2 hours, 80 V. The gel was then dried and exposed to phosphorimager plate and developed using a Typhoon phosphorimager.

DPA was performed using the same P1882 fragment with or without CovR. Reactions were prepared similarly to EMSA and after 40 min incubation, the mixtures were treated with a dilute DNase I solution (Epicentre) for 5 minutes, as described previously [30]. The samples were denatured and loaded onto an 8% denaturing PAGE gel containing urea and buffered with 1X TBE for electrophoresis. The gel was then dried and exposed to a phosphorimager plate.

Purification of His-RpoD

To synthesize His-RpoD, an 1127-bp DNA fragment, containing the entire rpoD gene without its stop codon, was PCR amplified from chromosomal DNA of S. mutans UA159, using the primer pair Smu-Nco-RpoD-F and Smu-Xho-RpoD-R. The DNA fragment was digested with XhoI and NcoI, and cloned into XhoI/NcoI-digested pET23D (Novagen), generating pIB611. Plasmid pIB611 was then transformed into E. coli BL21 DE3 pLysS. His-RopD was purified on Ni NTA column (Qiagen) following manufacturer's protocol and the purified protein was dialyzed against buffer B.

In vitro transcription (IVT) assay

A DNA fragment containing P1882 was amplified from UA159 genomic DNA by PCR using the primer pair: smu1882-F2 and smu1882- R5. Similarly, the promoter Pami, which was originally isolated from a Streptococcus pneumoniae gene that encodes amidase, was amplified from pIB163 [49]using the primer pair: PJRS-F and PJRS-R. In vitro transcription assay was carried out with the desired templates in reaction buffer containing 50 mM Tris-Cl (pH 7.5), 150 mM NaCl, 2 mM MgCl2, 0.1 mM EDTA, and 0.1 mM DTT in 20 µl volume. CovR (1–10 pmol) was preincubated in the reaction buffer along with the template DNAs for 20 min at room temperature. After incubation, 500 µM each (final conc.) of ATP, CTP, GTP, and 50 µM UTP with 1.0 µCi of [α-32P] UTP [~9000 Ci/mmol] were added to the reaction mixture. To initiate transcription, 0.25 U E. coli core RNA polymerase (Epicentre), RpoD (1.0 µg), and RNase inhibitor (40 U, Promega). After the incubation at 37°C for 15 min, samples were resolved by electrophoresis in a 4% urea gel. Transcripts were quantitated by densitometry with the ImageQuant software (GE Healthcare) by exposing the dried gel on a phosphorimager plate.


We thank Saswati Biswas for some strain constructions.

Author Contributions

Conceived and designed the experiments: IB PCN PCT. Performed the experiments: PCN PCT IB. Analyzed the data: IB PCN PCT. Wrote the paper: IB PCN.


  1. 1. Loesche WJ (1986) Role of Streptococcus mutans in human dental decay. Microbiol Rev 50: 353–380.
  2. 2. Hamada S, Slade HD (1980) Biology, immunology, and cariogenicity of Streptococcus mutans. Microbiol Rev 44: 331–384.
  3. 3. Peterson P (2003) The World Oral Health Report 2003. Geneva.
  4. 4. Kaste LM, Selwitz RH, Oldakowski RJ, Brunelle JA, Winn DM, et al. (1996) Coronal caries in the primary and permanent dentition of children and adolescents 1-17 years of age: United States, 1988-1991. J Dent Res 75(Spec No): 631–641.
  5. 5. Pitts NB, Chestnutt IG, Evans D, White D, Chadwick B, et al. (2006) The dentinal caries experience of children in the United Kingdom, 2003. Br Dent J 200: 313–320.
  6. 6. Horaud T, Delbos F (1984) Viridans streptococci in infective endocarditis: species distribution and susceptibility to antibiotics. Eur Heart J 5: Suppl C39–44.
  7. 7. Tanzer JM, Livingston J, Thompson AM (2001) The microbiology of primary dental caries in humans. J Dent Educ 65: 1028–1037.
  8. 8. Nicolas GG, Lavoie MC, LaPointe G (2007) Molecular Genetics, Genomics and Biochemistry of Mutacins: Global Science Books. pp. 193–208.
  9. 9. Lemos JA, Burne RA (2008) A model of efficiency: stress tolerance by Streptococcus mutans. Microbiology 154: 3247–3255.
  10. 10. Stock AM, Robinson VL, Goudreau PN (2000) Two-component signal transduction. Annu Rev Biochem 69: 183–215.
  11. 11. Dalton TL, Scott JR (2004) CovS inactivates CovR and is required for growth under conditions of general stress in Streptococcus pyogenes. J Bacteriol 186: 3928–3937.
  12. 12. Engleberg NC, Heath A, Vardaman K, DiRita VJ (2004) Contribution of CsrR-regulated virulence factors to the progress and outcome of murine skin infections by Streptococcus pyogenes. Infect Immun 72: 623–628.
  13. 13. Ferretti JJ, McShan WM, Ajdic D, Savic DJ, Savic G, et al. (2001) Complete genome sequence of an M1 strain of Streptococcus pyogenes. Proceedings of the National Academy of Sciences of the United States of America 98: 4658–4663.
  14. 14. Federle MJ, McIver KS, Scott JR (1999) A response regulator that represses transcription of several virulence operons in the group A streptococcus. Journal of Bacteriology 181: 3649–3657.
  15. 15. Heath A, DiRita VJ, Barg NL, Engleberg NC (1999) A two-component regulatory system, CsrR-CsrS, represses expression of three Streptococcus pyogenes virulence factors, hyaluronic acid capsule, streptolysin S, and pyrogenic exotoxin B. Infection and Immunity 67: 5298–5305.
  16. 16. Levin JC, Wessels MR (1998) Identification of csrR/csrS, a genetic locus that regulates hyaluronic acid capsule synthesis in group A Streptococcus. Molecular Microbiology 30: 209–219.
  17. 17. Graham MR, Smoot LM, Migliaccio CA, Virtaneva K, Sturdevant DE, et al. (2002) Virulence control in group A Streptococcus by a two-component gene regulatory system: global expression profiling and in vivo infection modeling. Proc Natl Acad Sci U S A 99: 13855–13860.
  18. 18. Churchward G (2007) The two faces of Janus: virulence gene regulation by CovR/S in group A streptococci. Mol Microbiol 64: 34–41.
  19. 19. Dalton TL, Hobb RI, Scott JR (2006) Analysis of the role of CovR and CovS in the dissemination of Streptococcus pyogenes in invasive skin disease. Microb Pathog 40: 221–227.
  20. 20. Sumby P, Whitney AR, Graviss EA, DeLeo FR, Musser JM (2006) Genome-wide analysis of group a streptococci reveals a mutation that modulates global phenotype and disease specificity. PLoS Pathog 2: e5.
  21. 21. Steiner K, Malke H (2002) Dual control of streptokinase and streptolysin S production by the covRS and fasCAX two-component regulators in Streptococcus dysgalactiae subsp. equisimilis. Infect Immun 70: 3627–3636.
  22. 22. Lamy MC, Zouine M, Fert J, Vergassola M, Couve E, et al. (2004) CovS/CovR of group B streptococcus: a two-component global regulatory system involved in virulence. Mol Microbiol 54: 1250–1268.
  23. 23. Jiang SM, Cieslewicz MJ, Kasper DL, Wessels MR (2005) Regulation of virulence by a two-component system in group B streptococcus. J Bacteriol 187: 1105–1113.
  24. 24. Ajdic D, McShan WM, McLaughlin RE, Savic G, Chang J, et al. (2002) Genome sequence of Streptococcus mutans UA159, a cariogenic dental pathogen. Proc Natl Acad Sci U S A 99: 14434–14439.
  25. 25. Biswas I, Drake L, Erkina D, Biswas S (2008) Involvement of sensor kinases in the stress tolerance response of Streptococcus mutans. J Bacteriol 190: 68–77.
  26. 26. Sato Y, Yamamoto Y, Kizaki H (2000) Construction of region-specific partial duplication mutants (merodiploid mutants) to identify the regulatory gene for the glucan-binding protein C gene in vivo in Streptococcus mutans. FEMS Microbiol Lett 186: 187–191.
  27. 27. Chong P, Drake L, Biswas I (2008) Modulation of covR expression in Streptococcus mutans UA159. J Bacteriol 190: 4478–4488.
  28. 28. Idone V, Brendtro S, Gillespie R, Kocaj S, Peterson E, et al. (2003) Effect of an Orphan Response Regulator on Streptococcus mutans Sucrose-Dependent Adherence and Cariogenesis. Infect Immun 71: 4351–4360.
  29. 29. Biswas S, Biswas I (2006) Regulation of the glucosyltransferase (gtfBC) operon by CovR in Streptococcus mutans. J Bacteriol 188: 988–998.
  30. 30. Biswas I, Drake L, Biswas S (2007) Regulation of gbpC expression in Streptococcus mutans. J Bacteriol 189: 6521–6531.
  31. 31. Dirix G, Monsieurs P, Marchal K, Vanderleyden J, Michiels J (2004) Screening genomes of Gram-positive bacteria for double-glycine-motif-containing peptides. Microbiology 150: 1121–1126.
  32. 32. Abranches J, Chen YY, Burne RA (2003) Characterization of Streptococcus mutans strains deficient in EIIAB Man of the sugar phosphotransferase system. Appl Environ Microbiol 69: 4760–4769.
  33. 33. Gusa AA, Froehlich BJ, Desai D, Stringer V, Scott JR (2007) CovR activation of the dipeptide permease promoter (PdppA) in Group A Streptococcus. J Bacteriol 189: 1407–1416.
  34. 34. Federle MJ, Scott JR (2002) Identification of binding sites for the group A streptococcal global regulator CovR. Molecular Microbiology 43: 1161–1172.
  35. 35. Gusa AA, Scott JR (2005) The CovR response regulator of group A streptococcus (GAS) acts directly to repress its own promoter. Mol Microbiol 56: 1195–1207.
  36. 36. Frith MC, Saunders NF, Kobe B, Bailey TL (2008) Discovering sequence motifs with arbitrary insertions and deletions. PLoS Comput Biol 4: e1000071.
  37. 37. Surzycki SJ, Shellenbarger DL (1976) Purification and characterization of a putative sigma factor from Chalamydomonas reinhardi. Proc Natl Acad Sci U S A 73: 3961–3965.
  38. 38. Steffen P, Goyard S, Ullmann A (1997) The Bordetella pertussis sigma subunit of RNA polymerase confers enhanced expression of fha in Escherichia coli. Mol Microbiol 23: 945–954.
  39. 39. Malakooti J, Ely B (1995) Principal sigma subunit of the Caulobacter crescentus RNA polymerase. J Bacteriol 177: 6854–6860.
  40. 40. Perez JC, Latifi T, Groisman EA (2008) Overcoming H-NS-mediated transcriptional silencing of horizontally acquired genes by the PhoP and SlyA proteins in Salmonella enterica. J Biol Chem 283: 10773–10783.
  41. 41. Walthers D, Carroll RK, Navarre WW, Libby SJ, Fang FC, et al. (2007) The response regulator SsrB activates expression of diverse Salmonella pathogenicity island 2 promoters and counters silencing by the nucleoid-associated protein H-NS. Mol Microbiol 65: 477–493.
  42. 42. Mouslim C, Latifi T, Groisman EA (2003) Signal-dependent requirement for the co-activator protein RcsA in transcription of the RcsB-regulated ugd gene. J Biol Chem 278: 50588–50595.
  43. 43. Zhu J, Winans SC (2001) The quorum-sensing transcriptional regulator TraR requires its cognate signaling ligand for protein folding, protease resistance, and dimerization. Proc Natl Acad Sci U S A 98: 1507–1512.
  44. 44. de Jong A, van Heel AJ, Kok J, Kuipers OP (2010) BAGEL2: mining for bacteriocins in genomic data. Nucleic Acids Res 38: SupplW647–651.
  45. 45. Aas JA, Paster BJ, Stokes LN, Olsen I, Dewhirst FE (2005) Defining the normal bacterial flora of the oral cavity. J Clin Microbiol 43: 5721–5732.
  46. 46. Pfaffl MW (2001) A new mathematical model for relative quantification in real-time RT-PCR. Nucleic Acids Res 29: e45.
  47. 47. Perez-Casal J, Caparon MG, Scott JR (1991) Mry, a trans-acting positive regulator of the M protein gene of Streptococcus pyogenes with similarity to the receptor proteins of two-component regulatory systems. Journal of Bacteriology 173: 2617–2624.
  48. 48. Banerjee A, Biswas I (2008) Markerless multiple-gene-deletion system for Streptococcus mutans. Appl Environ Microbiol 74: 2037–2042.
  49. 49. Biswas I, Jha JK, Fromm N (2008) Shuttle expression plasmids for genetic studies in Streptococcus mutans. Microbiology 154: 2275–2282.