Construction and verification of the transcriptional regulatory response network of Streptococcus mutansupon treatment with the biofilm inhibitor carolacton
- Padhmanand Sudhakar†1,
- Michael Reck†2,
- Wei Wang1,
- Feng Q He3,
- Irene W Dobler2Email author and
- An-Ping Zeng1Email author
© Sudhakar et al.; licensee BioMed Central Ltd. 2014
Received: 27 November 2013
Accepted: 17 April 2014
Published: 12 May 2014
The Erratum to this article has been published in BMC Genomics 2014 15:739
Carolacton is a newly identified secondary metabolite causing altered cell morphology and death of Streptococcus mutans biofilm cells. To unravel key regulators mediating these effects, the transcriptional regulatory response network of S. mutans biofilms upon carolacton treatment was constructed and analyzed. A systems biological approach integrating time-resolved transcriptomic data, reverse engineering, transcription factor binding sites, and experimental validation was carried out.
The co-expression response network constructed from transcriptomic data using the reverse engineering algorithm called the Trend Correlation method consisted of 8284 gene pairs. The regulatory response network inferred by superimposing transcription factor binding site information into the co-expression network comprised 329 putative transcriptional regulatory interactions and could be classified into 27 sub-networks each co-regulated by a transcription factor. These sub-networks were significantly enriched with genes sharing common functions. The regulatory response network displayed global hierarchy and network motifs as observed in model organisms. The sub-networks modulated by the pyrimidine biosynthesis regulator PyrR, the glutamine synthetase repressor GlnR, the cysteine metabolism regulator CysR, global regulators CcpA and CodY and the two component system response regulators VicR and MbrC among others could putatively be related to the physiological effect of carolacton. The predicted interactions from the regulatory network between MbrC, known to be involved in cell envelope stress response, and the murMN-SMU_718c genes encoding peptidoglycan biosynthetic enzymes were experimentally confirmed using Electro Mobility Shift Assays. Furthermore, gene deletion mutants of five predicted key regulators from the response networks were constructed and their sensitivities towards carolacton were investigated. Deletion of cysR, the node having the highest connectivity among the regulators chosen from the regulatory network, resulted in a mutant which was insensitive to carolacton thus demonstrating not only the essentiality of cysR for the response of S. mutans biofilms to carolacton but also the relevance of the predicted network.
The network approach used in this study revealed important regulators and interactions as part of the response mechanisms of S. mutans biofilm cells to carolacton. It also opens a door for further studies into novel drug targets against streptococci.
KeywordsStreptococcus mutans Caries Biofilm inhibitor Carolacton Transcriptome Reverse engineering Transcriptional regulatory network Key regulators Network verification
Streptococcus mutans is an oral pathogen, which along with other closely related streptococci called the mutans streptococci, plays an important role in the formation of caries and tooth decay in humans. This is attributed to its ability to form biofilms which are generally difficult or impossible to eradicate by antibiotic therapy because biofilm cells are resistant to antibiotics [1, 2].
Recently, it was shown that carolacton, a secondary metabolite from the myxobacterial species Sorangium cellulosum has a high inhibitory activity against actively growing S. mutans biofilm cells resulting in changes in cell morphology, elongation of cell chains, membrane damage and death of a part of the population. Carolacton was also found to induce a dose-dependent damage of S. mutans biofilms over a wide concentration range resembling a sigmoid dose–response curve . Carolacton inhibits S. mutans biofilms even at nanomolecular concentrations  implying that it primarily targets molecular entities which are present only as a few copies per cell. In this regard, carolacton is very similar to compounds which target cellular signaling networks  rather than directly targeting particular enzymes in pathways associated with vital processes such as protein, DNA/RNA synthesis, cell division etc.
To decipher the genes whose expression is affected by carolacton, a time resolved transcriptome analysis of S. mutans biofilms after carolacton treatment was carried out by Reck et al. . Results from the study indicate that carolacton affects changes in the expression of genes related to biofilm formation, autolysis, pyrimidine and histidine metabolism, cell shape and cell division in addition to two component systems (TCSs). Among the TCSs, the vicRK system shows an immediate strong downregulation, while the comDE system controlling competence development through quorum sensing [6, 7] is upregulated. A deletion mutant for the histidine kinase encoding gene vicK which responds instantaneously to carolacton treatment together with all the vicR-coexpressed genes, was similarly tested for carolacton-sensitivity, but since the vicK mutant showed very poor biofilm growth, further inferences could not be made. VicR is an essential gene and cannot be deleted in S. mutans. Meanwhile, the S. mutans eukaryotic-like serine-threonine protein kinase pknB whose ortholog has been shown to be a master regulator of virulence in S. pneumoniae displayed no observable changes in transcription . However, when pknB is knocked out, it results in a carolacton-insensitive mutant . These data show that even though the physiological and genetic responses of carolacton-treated S. mutans biofilm cells are known, the underlying network which orchestrates the expression of affected genes in response to carolacton still remains a mystery. This calls for an effort to uncover the effect of carolacton at the network level. Although Reck et al.  have already measured the temporal progression of the S. mutans transcriptome in response to carolacton, their dataset is characterized by a small number of sampling points (five) and large time intervals, which does not allow for a reliable network inference. Hence, an extended time-series transcriptome is required encompassing a higher number of sampling points with relatively short intervals and was carried out in the current study.
Reverse engineering based network reconstruction methods have widely been used to infer genetic networks from gene expression data measured most commonly using cDNA microarrays. Excellent reviews about genetic network reconstruction from expression data have been published . In order to capture the network level events of biological systems upon exposure to various stimuli, reverse engineering methods have been developed to infer underlying networks from time series expression data in addition to static data . For instance, methods such as Time Series Network Identification (TSNI) were used for inferring co-expression networks and compound mode of action from time-series gene expression data following interventions . Although the inferred co-expression network using TSNI involved only nine genes of the E. coli DNA-damage response pathway, it is seen as one of the first attempts in network reconstruction for determining the compound mode of action from a time series transcriptome. Further tools and algorithms were also developed to deal with whole genome network inference [13, 14], but the gene-gene interactions in such inferred networks were either undirected (no assigned causality) or carry only a statistical probability of causality. Despite lacking directionality, undirected co-expression networks have nevertheless been used to infer critical genes and networks involved in T cell functions .
Meanwhile, whole genome directed networks were inferred by using combinatorial methodologies  incorporating gene-gene interactions from reverse engineering algorithms with biological information such as data on binding motifs and promoter elements , functional genomics , genome annotation  and transcription factor activities . Although non-exhaustive due to the lack of sufficient biological information, genome wide transcriptional regulatory networks have nevertheless been constructed from heterogeneous data for a few organisms such as Escherichia coli, Saccharomyces cerevisiae, Bacillus subtilis, Candida albicans, Streptomyces coelicolor, Halobacterium NRC-1, Pseudomonas aeruginosa and others. Despite the advances made in the field of genome-wide regulatory network reconstruction, most of these attempts have been carried out for model or standard organisms (for which ample biological information exists) such as E. coli, S. cerevisiae, B. subtilis, P. aeruginosa[17, 20, 23, 24]. Some progress has also been made in the case of human cells as shown by Basso et al. where human B cell gene regulatory interactions were inferred . Hence, one of the major current challenges in the field is the network inference for less-studied organisms which are either pathogens or are industrially important.
Even though genetic networks have been inferred under drug treatment conditions for some organisms, most of them have either been limited to compounds and molecules whose targets and mode of action were already known and/or limited to model organisms and certain human cell lines. To the best of our knowledge, reconstruction of a contextual genome-scale regulatory network for the human caries pathogen S. mutans has not yet been carried out although studies focusing on genome-wide transcriptome profiling have been reported [5, 26–29]. A workflow based on a combinatorial strategy was executed in an attempt to infer a genome-wide network for S. mutans biofilms under conditions of treatment with the biofilm inhibitor carolacton. The Trend Correlation method which has been used to construct co-expression networks of human T cells  was used for inferring the S. mutans co-expression network under carolacton treatment conditions using microarray data generated in this study. This was followed by the construction of a transcriptional regulatory response network (TRRN) by incorporating binding site information. From the TRRN, we detected sub-networks whose activation or repression could be related to the biological effect of carolacton. A key regulator was identified based on its connectivity in the regulatory network and when knocked out, rendered S. mutans biofilms insensitive to carolacton. Furthermore, tested interactions from the inferred regulatory response network were confirmed using in vitro interaction detection assays.
Results and discussion
Dynamic genome-wide transcriptome profiling
A high resolution transcriptomic time-course experiment with S. mutans biofilms (with 11 samples taken from 5 to 300 min post carolacton treatment) was performed to capture the temporal response over an extended period of time. Our time-series data included results from a sample taken at 5 min post carolacton treatment and is expected to identify genes whose expression patterns were immediately affected by carolacton. A total of 772 GTAAs (genes corresponding to transcripts with altered abundances) or differentially expressed genes were identified at a log-fold change > =0.8.
Enrichment analysis with respect to various categories such as biological functional classes and KEGG metabolic pathways was performed for the up- and downregulated GTAAs at every time point in order to gain an overview of the various categories of genes affected by carolacton (Additional file 1). The results from the enrichment analysis of upregulated GTAAs indicated that transcripts from the pyrimidine ribonucleotide biosynthesis (P-value < = 4.09E-18), nucleosides, purines and pyrimidines’ transport (P-value < = 2.45E-2), and metabolism of alanine, aspartate and glutamate (P-value < = 7.2E-4) were most significantly over-represented at both 5 min and 20 min but not at 40 min. These observations suggest a possible specific role of pyrimidine biosynthesis and metabolism in the initial response of S. mutans biofilms to carolacton. At later time points however, many more categories were found to be over-represented among the set of upregulated GTAAs due to probable cascade effects.
Enrichment analysis of the downregulated GTAAs at 20 min revealed categories such as glutamate biosynthesis, TCA cycle, anaerobic energy metabolism, glyoxylate and dicarboxylate metabolism, nitrogen metabolism as well the signal transduction related two component systems (TCSs). TCSs impart various virulence characteristics to S. mutans by sensing and responding to various signals related to stress, thus enabling it to survive and tolerate unfavourable conditions [30, 31]. The transcriptional downregulation of TCS genes could indicate a possible effect of carolacton having a repressive effect on the signaling mechanisms of S. mutans. In general, downregulated GTAAs in the early part of the response were enriched with categories corresponding to the processes of signaling, energy and amino acid metabolism. The set of downregulated GTAAs in the later phases after 20 min was also found to be enriched with many categories over the course of the experiment. Interestingly, the alanine, aspartate and glutamate metabolic pathways were found to be over-represented in both the up- and downregulated GTAA sets at the time point of 20 min after carolacton treatment suggesting a dual regulation of such pathway enzymes in the initial response to carolacton. The information from our transcriptome data largely agrees with those from a previous study by Reck et al.  where only five sampling points with large intervals were used.
Contextual co-expression network
Regulator-target gene binding site map of S. mutansUA159
The edges of the carolacton-context co-expression network derived from the dynamic transcriptome data are undirected. In other words, the mere presence of an edge between two genes does not necessarily represent a transcriptional regulatory relationship between them. Although time-lags between the co-expressed regulator and target gene(s) could possibly serve as a preliminary proof of direct/indirect transcriptional regulation , further evidence is required for at least assigning putative biological causality and for pursuing precise experimental validation of transcriptional regulatory relationships.
Among the more than 100 known or predicted transcriptional regulators in the S. mutans UA159 genome, only a few have been studied experimentally and characterized with respect to their DNA binding site(s). We compensated for the non-availability of experimentally verified transcriptional regulatory binding sites for the S. mutans transcriptional factors by applying comparative genomic approaches [33–35]. Binding site data for 44 transcriptional regulators were recovered from different sources such as experimental data from S. mutans itself or information from comparative genomic analysis. In cases where the collective number of binding sites inferred for a transcriptional regulator were fewer or equal to three, respective regulogic  sites from other species within the Streptococccus genus were retrieved. These were then used to construct PSSMs (Position Specific Scoring Matrices, see Methods) with improved predictive capacities. PSSMs were also constructed from regulogic sites available in the RegPrecise database  and from phylogenetic footprinting studies. An online Regulatory Sequence Analysis Tool (RSAT) termed matrix-quality was used to objectively determine the optimal P-value for every PSSM (see Additional file 3). The PSSMs were then used to predict binding sites (at the corresponding optimal P-values) in the upstream regulatory regions of all the genes in the S. mutans UA159 genome. A total of 1397 unique regulator-target gene relationships (corresponding to 2056 predicted binding sites) based on binding site data alone corresponding to 44 S. mutans UA159 transcriptional regulators were thus compiled (see Additional file 4). After integrating operon structure information, 2445 regulator-target gene relationships were found to comprise the final regulator-target gene binding site map. The global regulators CcpA (catabolite repressor protein) and CodY (global regulator of amino acid metabolism) together accounted for ~29.22% of the 2445 regulator-target gene relationships based on binding sites.
S. mutansTranscriptional Regulatory Response Network (TRRN) under carolacton treatment
The TRRN (Figure 2) represented a “waterfall-like” model with respect to its global topological structure and hierarchy [39, 40] with some regulators apart from modulating their own sub-networks also exerting indirect control over other sub-networks by putatively modulating the expression of the corresponding transcription factors. For example, it can be seen from the inferred TRRN (Figure 2) that the global regulator CodY putatively regulated the expression of two distinct genes encoding the TCS response regulators VicR and ComE, thus potentially exerting an indirect influence on their sub-networks as well. Although global hierarchical organization was observed in the inferred TRRN, it was nevertheless confined only to a double-layered hierarchy compared to multi-layered hierarchies reported in the regulatory networks of well-studied organisms [40, 41]. This could primarily be due to the lack of biological connectivity data, firstly as a result of the limited experimentally verified binding site information of S. mutans transcription factors. Secondly, the functional and/or evolutionary divergence of S. mutans transcription factors from their corresponding orthologs in standard organisms has a certain limiting influence on the comparative genomic based extrapolation of binding sites .
The overlap between co-regulated gene groups, which was previously observed in bacteria [42, 43], is also a characteristic of the inferred TRRN. 13% of the 307 TRRN genes were found to be under the putative control of more than one transcriptional regulator (implying an incoming degree > 1). From a local network structure point of view, the nodes putatively controlled by just one regulator resemble single input motifs (SIM) whereas the nodes co-regulated by several regulators form multiple input motifs (MIMs) . Besides MIMs, overlap between co-regulated gene groups could be the manifestations of more complicated network motifs such as the feed forward loop (FFL) in which a regulator encoding gene is modulated by another regulator, both of which control the expression of a common gene . If multiple genes are controlled by a single FFL, then it is termed as a multi-output FFL (MOFFL) . Additional file 6 lists the various types of significant motifs identified (P-value < = 0.01 after 10000 randomizations) in the carolacton context dependent TRRN among which were found FFLs including other motifs such as regulatory bi-fans  and their derivatives . Local network topologies such as the motifs found here were consistent with previous observations in other organisms [44–46, 48] and could be important for eliciting quick and flexible responses to stimuli . Although the exact biological mechanisms which give rise to such motifs remain to be understood, these observations demonstrate not only the relevance of the constructed network but can also be further used for detailed dynamic quantitative modeling of smaller sub-systems.
Biological context within co-regulated sub-networks in the TRRN
TRRN sub-networks co-regulated by global transcription factors
The sub-networks of the global transcriptional regulators affecting central metabolism namely CodY and CcpA [38, 51] were among the top three sub-networks in terms of the number of genes. CcpA is reported to modulate sugar uptake and metabolism, carbon catabolite repression and expression of virulence related genes in S. mutans. The treatment of S. mutans biofilms with carolacton caused an immediate downregulation of CcpA modulated genes (Additional file 8). The CcpA sub-network consisted of genes encoding components of two mannose specific phosphotransferase systems (ptnAC (manLM)-SMU_1879 and SMU_1960c-SMU_1961c) [52–54], as well as three ATP dependent transporter complexes (msmEFG, SMU_921-SMU_922 and SMU_1315c-SMU_1317c) among others. While msmEFG is reportedly involved in the energy dependent transport of multiple sugars , the substrate specificities of the other two clusters are unknown. Sub-networks of other sugar-specific transcription factors such as the repressors GalR and FruR of galactose and fructose metabolism respectively were also found to be downregulated. Sugars serve as substrates for the synthesis of glucans and associated by-products required for adherence to the tooth surface, biofilm formation as well as for the formation of organic acids which aid cariogenic disease progression [56–60]. The sub-network co-regulated by CodY (Additional file 8) meanwhile was found to be enriched with genes belonging to the metabolism and biosynthesis of amino acids, particularly the branched chain ones such as leucine, valine and isoleucine. The control of the metabolism of these amino acids by CodY has already been reported . Hence, from the preliminary analysis of the regulatory response network, it can be stated that carolacton has an inhibitory effect on the central metabolism of sugars and amino acids by downregulating genes co-regulated by the global transcriptional factors CcpA and CodY.
Immediate induction of the pyrimidine metabolism
Carolacton affects glutamine metabolism
Genes in the TRRN predicted to be co-regulated by the glutamine synthetase repressor GlnR along with glnR itself were associated with a sharp downregulation initially (Figure 5B). It is known that glutamine is an important source of nitrogen for S. mutans. Some of the GlnR-modulated genes in response to carolacton treatment included a glutamine transporter gene-cluster (SMU_1519-SMU_1522), the glutamine/glutamate biosynthesis operon (glnRA-gltAD), as well as an operon consisting of the putative ammonium transporter coding gene nrgA and the nitrogen regulatory protein coding gene glnB. Other glutamate and glutamine metabolism related genes such as citZH and idh, whose modulation was also reported to be mediated by GlnR , were downregulated initially until 20 min post carolacton addition. The protein products of the citZH and idh genes catalyze the steps leading to the formation of alpha-ketoglutarate from oxaloacetate (feeding the de-novo glutamine synthesis pathway) . The expression pattern of the genes predicted to be controlled by GlnR suggests an activational (positive) rather than an inverted (negative) relationship. But GlnR is known to function as a repressor protein. However, this does not seem to be a conflicting observation since GlnR orthologs have been known to have dual activator-repressor functions . Hence, the S. mutans GlnR could also be a dual regulator given that several transcriptional regulators with dual functions have been reported earlier in S. mutans[66–68].
Glutamate is known to play a role in the acid tolerance response (ATR) mechanism of S. mutans[69–71] which is crucial for the survival and adaptation of S. mutans. Carolacton has the maximum effect in terms of membrane damage and cell death in actively growing biofilm cultures at low pH. But the transcriptional changes (immediate downregulation until 20 min post treatment) of glnR and its target genes occurred at a neutral pH (data not shown) thus ruling out ATR as a cause for the intial modulation of GlnR mediated genes. At later time points which correspond to a low pH, the upregulation of the GlnR-modulated genes occurred although a downregulation should have been the expected trend to enhance the ATR. This suggests that carolacton directly or indirectly diminishes the ATR thereafter. Alternatively, the upregulation of the glutamine metabolism genes comprising the GlnR co-regulated gene group after the initial downregulation could possibly be explained as a means to provide precursors for peptidoglycan biosynthesis. Thus, it is plausible that the pyrimidine metabolism is induced to feed the peptidoglycan biosynthesis during the initial phase (until 20 min after carolacton treatment) followed by the upregulation of the glutamine metabolism related genes during the later phase.
TRRN genes co-regulated by the essential response regulator VicR
The microarray data show that vicKR, one of the earliest responding TCSs upon carolacton treatment, was downregulated. The vicKR TCS plays a major role in the biofilm formation, competence development, oxidative stress tolerance, acid tolerance, autolysin production, glucan and fructan metabolism of S. mutans[27, 72–77]. In addition, the response regulator vicR has also been identified as being essential for the survival of S. mutans, i.e. it is an essential gene which cannot be deleted . The gene group co-regulated by VicR (Figure 5C) in the TRRN consisted mostly of downregulated genes including those encoding surface structure and cell wall proteins such as glucosyltransferases (gtf) B and D, glucan binding protein B (gbpB), and the sortase-anchored cell wall protein wapE among others. This is consistent with the previous study  whereby all the genes including the ones described here and co-expressed with the downregulated vicR had reduced transcript abundances. The evidence put together suggests that carolacton could interfere with the signalling mechanisms related to the activity of this essential response regulator thereby exerting its biofilm inhibitory and membrane damaging effects. Some of the genes such as gtfB, gbpB and comC in the VicR co-regulated gene cluster were already known to be direct transcriptional regulatory targets [76, 79, 80] of the VicR protein thus contributing to an independent verification of our network prediction based on time-series microarray data and binding motif information.
Modulation of genes co-regulated by the cysteine metabolism controlling transcription factor CysR
Genes connected by edges to cysR (encoding a regulatory protein controlling the metabolism of sulfur containing amino acids ) in the co-expression network had both inverted and positive expression patterns compared to that of cysR (Additional file 2). After combining the CysR binding motif information , directionality was assigned to the edges after which all of the cysR co-regulated genes were having only positive expression patterns (Figure 5D) in relation to cysR. CysR was found to modulate 26 TRRN genes (Figure 5E) making it the transcriptional regulator with the second highest degree (number of modulated genes) in the carolacton context TRRN. Some of the genes transcriptionally modulated by CysR include SMU_609 encoding a putative-40 K cell wall protein precursor, SMU_246 encoding a putative glycosyltransferase-N-acetylglucosaminyltransferase and SMU_984 whose gene product has been predicted to be an uncharacterized autolysin among others. Besides, SMU_1509 whose gene product is a Rgg family  regulator protein was also observed to be among the CysR sub-network as were genes encoding putative Nif proteins related to nitrogen metabolism and those such as the SMU_1074-SMU_1077 operon involved in cysteine metabolism. Statistically significant enrichment for various functional categories was not observed within the CysR sub-network and this might be attributed to the low number of genes from any given category. Nevertheless, the functional relevance of the individual genes (such as SMU_609 which is one of the strongest modulated genes with > 2 log2-fold upregulation in response to carolacton treatment) within the CysR sub-network as well as its connectivity in the TRRN point out the importance of CysR in the response of S. mutans biofilms to carolacton.
Experimental verification of the predicted regulatory interactions between MbrC (BceR) and the murMN-SMU_718 operon
By combining gene expression and binding motif information, mbrC was predicted to regulate four so far unidentified target genes (the SMU_716-SMU_717-SMU_718c operon and SMU_610 encoding the cell surface antigen SpaP) in the carolacton treatment context TRRN. The autoregulatory response regulator MbrC -also known as BceR- is encoded within a four-gene operon (mbrABCD/bceABRS) and has been shown to regulate cell envelope stress response mechanisms in S. mutans. Ouyang et al. demonstrated that MbrC transcriptionally regulates the genes SMU_302, SMU_862, SMU_1006 and SMU_1856 by binding to their promoter elements via a conserved binding motif. The binding motif consensus consists of a conserved pair of inverted repeats separated by 2 variable nucleotides (TTACAAnnTTGTAA) .
To verify this predicted regulatory relationship, Electro Mobility Shift Assays (EMSA) were carried out. The promoter region of SMU_1006 served as a positive control as the binding of MbrC to it was reported previously . An unrelated DNA fragment (around 100–150 bp, lower DNA band in all the lanes) was added in all the samples to prove the specificity of the binding reaction. As shown in Figure 6C, the results confirmed the binding of MbrC to the SMU_1006 promoter as well as the necessity of the consensus motif for the binding of MbrC to its target. When an unrelated transcriptional regulator VicR was used instead of MbrC in the binding reaction as a control to test the specificity of the assay, no shifting of the DNA band was found while with increasing MbrC concentrations, a clear shift was observed (upper band around 350 bp). No significant shift was observed upon deleting the binding motif from the SMU_1006 promoter. Similarly, MbrC also bound to the promoter region of SMU_718c as indicated by a band shift at MbrC concentrations higher than or equal to 5pmol (Figure 6D). With increasing amounts of MbrC (5–20 pmol) present in the binding reaction mixture, a shift from 250 bp (upper DNA band) to around 1 kbp was observed. No shift was observed in the control lane corresponding to the reaction mixture containing an unrelated transcriptional regulator VicR (whose binding site was not present in the murMN-SMU_718 promoter) confirming the absence of non-specific binding. Furthermore, the deletion of the MbrC binding site from the murMN-SMU_718 promoter also abolished the binding of MbrC to its DNA target. Thus the observations from the EMSA studies have confirmed that the murMN-SMU_718 operon is a direct target of the MbrC response regulator as predicted from the regulatory response network. The two substitutions present in the MbrC binding site upstream of the murMN-SMU_718c operon could reflect a less stringent binding of MbrC. Accordingly, the shift of the SMU_718c target DNA occurred at a higher MbrC protein concentration (10 pmol) than that (5 pmol) observed for the corresponding SMU_1006 target DNA.
Our finding that MbrC directly controls the expression of two enzymes involved in a central step of cell wall synthesis further highlights the importance of this response regulator for the cell envelope stress response and for maintaining cell wall homeostasis. The reconstitution of the Gram positive bacterial cell wall during growth is intricately linked to the synthesis of peptidoglycan polymer chains . Both murM and murN encode alanine adding enzymes involved in the branched peptide peptidoglycan biosynthetic pathway and have also been reported to be primary determinants of the peptidoglycan stem peptide structure [83, 86] which in turn affects various virulence properties such as antibiotic resistance [88–90] and pathogenesis . Thus, although the transcriptional induction of the murMN-SMU_718 operon and the mbrC gene is relatively weak following carolacton treatment, it might still be significant since only a few copies of the enzymes might potentially be required to catalyze the peptidoglycan biosynthetic reactions. Post transcriptional regulation of enzymes involved in cell wall synthesis and cell division might also significantly contribute to a quick and efficient adaptation of the cell to maintain cell wall homeostasis. Thus small transcriptional changes might result in strong changes of enzyme activity. Induction of the MbrC regulon by carolacton is reminiscent of the previously observed  bacitracin induced cell envelope stress response mediated by this regulon in S. mutans. This finding further points out the influence of carolacton on cell wall synthesis as reported previously .
Deletion mutants of “key” transcriptional regulators
Based on the inferred TRRN and co-expression networks, single gene deletion mutants corresponding to five different transcriptional regulators (CysR, Rgg, GlnR, SpxA, and FabT) were constructed. We chose these potential key genes for experimental evaluation based on the following criteria. Next to that of CodY, CysR (SMU_852) was identified as the regulator with the highest connectivity in the regulatory response network. CodY is a well-known global master regulator  and its deletion has been shown to have obvious phenotypic effects such as the reduced capacity to form biofilms . Since biofilm growth is a pre-requisite for the inhibitory action and membrane damage caused by carolacton, codY was not chosen as a deletion candidate. rgg (SMU_1509) was identified as the only transcriptional regulator encoding gene among the CysR co-regulated genes and hence was chosen as a candidate for deletion. Alterations in the cell wall metabolism could play a critical role in the response of S. mutans biofilms to carolacton due to the observed membrane and cell wall damage [3, 5]. GlnR was chosen as a possible knock-out target due to its importance in peptidoglycan biosynthesis and cell wall metabolism via many of the glutamine-metabolism and transport genes which it modulates as observed in the TRRN. spxA (SMU_1142) and fabT (SMU_1745) were identified as the top two nodes purely based on connectivity in the co-expression network and hence chosen for further testing. The other genes from the co-expression network were not chosen in this work.
The role of cysR in the response of S. mutansbiofilms to carolacton
From our initial susceptibility studies of mutant biofilms under carolacton treatment, cysR could be identified as being essential for the sensitivity of growing S. mutans biofilms to carolacton treatment. The almost complete loss of sensitivity of the cysR mutant to carolacton treatment was independently confirmed by the determination of colony forming units of carolacton treated and untreated biofilms of the wild type and cysR gene deletion strains. While the wildtype showed a reduction of CFUs of approximately 75%, the carolacton treated and untreated mutant cells showed almost no difference in the amount of colony forming units (Figure 7B). Thus the experiment clearly confirms the essential role of cysR in the response of S. mutans biofilms to carolacton treatment, as predicted from the TRRN. The genome of S. mutans encodes 4 LysR-type transcriptional regulators, of which 3 (CysR, MetR, HomR) are phylogenetically linked and control the supply of sulfur amino acids [81, 93]. CysR is known to modulate the expression of genes involved in cysteine metabolism in S. mutans. Here, we provide data showing that apart from its role in cysteine metabolism, CysR is essential for the response of S. mutans biofilms to the biofilm inhibitor carolacton. This implies a potential role of CysR in cell wall maintenance, as this trait was shown to be impaired in carolacton treated biofilm cells and cell wall changes are most likely responsible for cell death caused under acidic conditions .
The inferred transcriptional regulatory targets of CysR, as identified after the integration of contextual coexpression correlation and binding motif information, indeed comprise genes involved in maintaining cell wall homeostasis. Genes SMU_984 and SMU_609 encode two autolysins which were not characterised so far. Interestingly, both genes were immediately (5 min after treatment) and constantly upregulated after carolacton treatment and belong to the strongest regulated genes of our time-resolved transcriptome study. SMU_609 encodes a 40 K cell wall protein which was shown to exhibit murein hydrolase activity using a peptidoglycan zymogram assay and is likely linked to the cell surface via the sortase system [78, 94]. As cell wall synthesis during growth depends on a balanced interplay between build-up and breakdown of the cell-wall, enhanced autolysin activity might promote cell lysis  and thus explain the influence of CysR on cell death. However, deletion of SMU_609 and SMU_984 did not cause a carolacton insensitive phenotype (data not shown). Another CysR regulated gene, rgpG (SMU_246), encodes a putative UDP-N-acetylglucosamine undecaprenyl-phosphate GlcNac 1-phosphate transferase. This enzyme catalyses the first membrane localized step of the biosynthesis of various polymers of the bacterial cell wall. The other potential target genes include the gene cluster SMU_1074-SMU_1077 which encode putative metabolic enzymes belonging to the pathways related to cysteine metabolism and is concurrent with the known role of cysR in cysteine metabolism .
It should also be noted that cysR and its paralog cpsY are located in close vicinity to the genes of the de novo pyrimidine biosynthesis pathway on the genome of S. mutans. The pyrimidine biosynthesis genes were shown to be the strongest upregulated genes 5 min post carolacton treatment. The functionality of pyrimidine metabolism, especially of the pyr gene clusters upregulated specifically under carolacton treatment, could possibly be linked to the availability and synthesis of cell wall precursors. In prokaryotes, genes encoding products involved in the same or related biological functions are often located in close neighbourhoods on the genome [96–98].
Moreover, for the S. iniae cysR ortholog cpsY, it was shown that this LysR type transcriptional regulator (LTTR) induced cell wall changes essential for the intracellular survival of this invasive pathogen in neutrophils . Interestingly, in the study of Allen et al., it was determined that deletion of cpsY alters the cell surface charge, muropeptide composition and susceptibility to lysozyme treatment. This is fully in accordance with the current understanding of the mode of action of carolacton . However further experiments are necessary to verify the targets of CysR experimentally (e.g. EMSA experiments with purified CysR protein) and to fully address the role of cysR in cell wall metabolism e.g. by knocking out the CysR regulated autolysins. Altogether, our data strongly suggest a so far unidentified role of the CysR transcriptional regulator in cell wall homeostasis.
A highly interesting aspect of the network prediction is the finding that CysR potentially regulates another transcriptional regulator (Rgg). As the carolacton specific regulatory response network contains albeit only two levels of hierarchy, CysR can thus be considered as a potential global regulator. Rgg transcriptional regulators associated with small hydrophobic peptides (SHP) were identified to represent a part of a novel quorum sensing mechanism in Streptococci [82, 100]. Rgg proteins have been identified and conserved in nearly all streptococci . This mechanism works independently of a TCS, but senses the signalling molecule inside the cell after its internalisation via an oligopeptide permease . But the Rgg knockout strain showed comparable susceptibility to carolacton treatment as the wildtype strain (Figure 7A) thus excluding the possibility of Rgg being a critical regulator mediating the observed effects of carolacton.
With respect to cysR however, its deletion mutant displayed a loss of sensitivity to carolacton as a result of a reduction in the inhibition of viability caused by carolacton. Nevertheless, CysR might not represent the primary target of carolacton as the treated biofilm cells of the cysR gene deletion mutant still exhibit an inhibition of about 10%. Moreover, phenotypic differences between carolacton treated and untreated cysR mutant biofilm cells were observed, indicating that carolacton can still bind to its target(s) and induce changes in the cellular morphology. Nevertheless, the lethal effects of carolacton treatment apparently rely to a large extent on the presence of an intact copy of the cysR gene. Another interesting question is the link of CysR to the PknB controlled regulon, as pknB was also shown to be essential for carolacton mediated cell death . With PknB being a global regulator of cell division  and virulence attributes , the regulons of PknB and CysR might converge at the level of the modulated autolysins. The CysR coregulated genes SMU_984 and SMU_609 were 2 of the 3 strongest modulated genes in the transcriptome analysis of an exponentially growing pknB deletion strain . However, as the deletion mutants of SMU_609 and SMU_984 are still susceptible to carolacton treatment, this potential overlap of the regulatory systems does not provide an explanation why both the pknB and cysR deletion mutant biofilms exhibited almost no sensitivity to carolacton treatment.
Since LTTRs show a high degree of sequence conservation, control important metabolic pathways of sulfur containing amino acids, and since sulfur is essential for the active sites of many enzymes, the transcriptional regulator CysR might also be an attractive drug target. Co-factor binding is required for its transcriptional activation, and the likely cofactor could be O-Acetylserine (OAS) . Thus, small molecule inhibitors could potentially be designed to compete with the co-effector molecule for the binding site on this LTTR and to finally block its biological function. To conclude, we have shown here strong evidence that the role of CysR may be much more diverse and important than previously expected. Traits essential for survival like cell wall metabolism and sulfur amino acid supply are controlled by this LTTR. Thus CysR might represent an attractive novel streptococcal drug target.
Linkage between the PknB and CysR regulons
Deletion of cysR almost completely prevents cell death in carolacton treated biofilms, a finding previously reported for the gene deletion strain of the Serine Threonine Protein Kinase (STPK) encoding gene pknB as well . This instantly raises the question whether the regulons of these two proteins overlap or if PknB is located upstream of CysR in the regulatory cascade and thus controls the latter’s activity. Both regulators putatively modulate the expression of the two carolacton responsive autolysins SMU_984 and SMU_609, which might explain the shared insensitive phenotype to carolacton of their mutant strains.
However, in this study, we focus only on the transcriptional network analysis, while PknB modulates its target genes via protein phosphorylation at the post-transcriptional level [9, 103, 104]. Thus the question whether and on which level the modulated networks of PknB and CysR converge and if they represent the essential pathway for the carolacton mediated cell death cannot be fully answered from the transcriptional regulatory network analysis. To quantitatively understand the effects of carolacton on cell metabolism and to determine the missing layers in the regulatory cascades of CysR and PknB, it is necessary to consider the regulatory effects of small non-coding RNAs  and other post-transcriptional and post-translational modifications [106, 107] including modulation by other signalling pathways . Transcriptional network analysis is generally lacking in information about these important regulatory mechanisms which have been shown to be essential for cellular metabolism and homeostasis [105, 106, 109]. Nevertheless, we have demonstrated here the high merit of transcriptional network prediction and analysis to identify a key regulator mediating cell death in S. mutans biofilms in response to the biofilm inhibitor carolacton.
We have used a combination of transcriptional network prediction and experimental verification to analyse the response of S. mutans biofilms upon treatment with the biofilm inhibitor carolacton. According to our knowledge, this is the first study inferring a genome-wide transcriptional regulatory response network for S. mutans using heterogeneous data including a time-series transcriptomic dataset and transcription factor binding site information. Based on the inferences from the regulatory network, we experimentally verified important predicted transcriptional regulatory interactions between the cell envelope stress modulating TCS response regulator MbrC and the operon harbouring the murMN genes encoding cell wall metabolism associated enzymes. CysR, a regulator known to modulate cysteine metabolism, was predicted and experimentally verified to be an essential key regulator for the mode of action of the biofilm inhibitor carolacton. Our data strongly suggest a role of cysR in cell wall metabolism, cell division and cell surface biogenesis, apart from its already known role in cysteine metabolism and sulfur supply in S. mutans, thus highlighting its potential as an attractive novel streptococcal drug target. We here also demonstrate the high predictive power of the network construction and analysis strategy used in this work.
Static biofilm cultures of S. mutans UA159 were grown in routine 24 well plates (Greiner Bio One, Frickenhausen, Germany) using 800 μl Todd Hewitt Broth (Becton Dickinson, Heidelberg, Germany) supplemented with 0.5% sucrose (Sigma, Taufkirchen, Germany) per well as media. Overnight cultures of planktonic cells in Todd Hewitt Broth were diluted in the biofilm medium to a starting OD of 0.05 and biofilms were grown for 3 hours under anaerobic conditions (80% N2, 10% CO2, 10% H2) in a chamber (Don Whitley Scientific, Shipley, England). Thereafter, the supernatants were completely removed and exchanged with fresh medium (control samples) or either fresh medium supplemented with 2.5 μg/ml carolacton (treated samples). For the control, an equivalent volume of methanol was added. Samples were taken after 0, 5, 20, 40, 60, 80, 100, 120, 160, 200, 240 and 300 minutes by removing the supernatant and adding 200 μl fresh medium and 400 μl of RNA protect (Qiagen, Hilden Germany). Biofilms representing one condition were scraped from at least 3 individual wells and pooled together. Cells were pelleted by centrifugation, washed with Molecular biology grade water (Sigma, Taufkirchen, Germany) and lysed with a combination of Lysozyme/mutanolysin treatment and mechanical disruption of cells with glass beads . Total RNA was extracted using the RNeasy Kit (Qiagen, Hilden Germany) as recommended by the manufacturer. The overall experiment was repeated once.
2 μg of total RNA from each sample was labeled with Cy3 and Cy5-ULS (Kreatech, Netherlands) according to the protocol of the company. Fragmentation of RNA and further processing was performed according to the Agilent hybridization kit procedure. Samples were hybridized in a dye swap design on 8x15K S. mutans custom arrays (Agilent, Böblingen, Germany) for 14 h at 65°C as previously described .
The array design is described in detail in . Slides were washed and scanned as recommended by Agilent. For feature extraction, the Agilent extraction software (V. 10.7) was used. The further data analysis was performed using the R package LIMMA. For dye specific within-array normalization, the LOWESS algorithm was applied. Quantile normalization was used for between array-normalization. Genes corresponding to rows with blanks were omitted. From the log transformed and background corrected median signal intensities, the fold change between treated and untreated samples was calculated for every gene at each time point. The log2 (treated/untreated) expression ratios were then subjected to a within-gene normalization. Genes with a log2-fold ratio greater than 0.8 were regarded as genes corresponding to transcripts with altered abundances (GTAAs).
Functional context enrichment analysis
Enrichment analysis was performed separately for the up- and downregulated GTAAs (at every measured time point) with respect to each of the known biological functional classes and KEGG metabolic pathways in order to gain an overview of the various functional categories affected by carolacton treatment. 15 main and 97 sub functional classes of S. mutans UA159 were compiled using the gene annotation information furnished in the Oralgen database (version 2011 and now re-named as The Bioinformatic Resource for Oral Pathogens). The gene membership information of S. mutans UA159 corresponding to 84 different pathways was retrieved from the KEGG database (version 2011). The hypergeometric test with Benjamini-Hochberg correction was used to quantify the significance of the overlap between the GTAAs and the functional categories. A corresponding significance score was also calculated as a negative logarithmic function of the corrected P value. The significance score is a user friendly measure of the relevance of the overlap between functional categories and the GTAAs. The higher the significance score, the more relevant is the overlap. Categories with significance score greater than 0 represented significant enrichment.
Inferring gene-gene correlation relationships from transcriptomic data using the Trend Correlation (TC) method
The TC method  allows the inference of gene-to-gene time-lagged positive or negative “associations” or pairs of genes based on extracting the main features of the change trend and the correlation of gene expression changes between consecutive time points . Time lagged co-expression relationships are those in which the expression patterns of two genes are better correlated when a time shift is introduced . In this work, we adapted the TC method by calculating the correlation coefficient from the change rates rather than change levels between consecutive time points since the time interval of the measurements was not constant (personal communication, Feng He). Potential co-expression relationships were checked for every possible regulator-gene pair given the minimum number of expression measurements in the chosen time window was four. The genetic response network consisted of optimal expression relationships which started either at 0, 5 or 20 min post carolacton treatment in order to capture the correlations mediating the initial response to carolacton. The significance of correlation of a gene-pair for every time-window is measured by the co-expression P-value by procedures described previously in the TC method by He et al. . The individual P-values of correlation for a gene pair within every considered time-window are compared among each other. Optimal correlation for a gene pair refers to the time window within which the correlation between the genes is most significant statistically. Parameters such as the correlation co-efficient, the trend score, and the P-value were calculated as described previously  to characterize the degree and randomness of correlation between the temporal expression patterns of genes. The association between two genes was considered to be statistically significant if the corresponding P-value of their co-expression was determined to be lower than the optimal P-value cutoff calculated using standard performance metrics as explained below.
Performance metrics for the determination of the optimal P-value threshold
The optimality of the P-value threshold was determined based on the F-score (Eq. 1) which in turn is a function of the equilibrium between the Recall (Eq. 2) and Precision (Eq. 3) functions which are defined below.
F-score: this is predictive of the balancing property or equilibrium between the Precision and Recall parameters. The F-score usually reaches a maximum peak at the P-value optimum.(1)
Recall (also termed as True Positive Rate or Sensitivity): defined as the fraction of true “associations” which are inferred as significant by the TC method(2)
Precision (also termed as Positive Predictive Value): defined as the fraction of inferred significant “associations” which are true(3)
Gene pairs within the same operon because of their virtue of coherent co-expression were used as the “gold standard” or true positives. False positives constitute the inferred significant “associations” between genes from different operons whereas false negatives represent the intraoperonic gene pairs which were considered as insignificant and which were seemingly missed out at the particular P-value threshold. The operon information was predicted by Pathway Tools . Differential edges [111, 112] in response to carolacton treatment were pooled together to form the final co-expression network.
Construction of Position Specific Scoring Matrices (PSSMs) representing transcription factor binding motifs
Experimentally verified DNA binding sites of S. mutans transcription factors were retrieved from literature when available. The comparitive genomics based approach using the concept of regulogic extrapolation as explained in  was carried out to retrieve orthologous regulatory relationships in S. mutans from experimentally verified relationships in B. subtilis. Validated binding sites of B. subtilis transcription factors were retrieved from the DBTBS database . OrthoMCL , which is a genome-scale algorithm for grouping matching protein sequences, was used to identify orthologous genes shared between S. mutans UA159 and other gram positive bacterial species including some representative species from the Streptococcus genus. The OrthoMCL results were verified by manually searching for the presence of commonly occurring domains in the protein sequences of the orthologous pairs of transcription factors. To increase the reliability of a particular predicted regulog in S. mutans, a check was performed to ascertain if the regulog was conserved in at least some species within the Streptococcus genus. Consensus motifs constructed from too few binding sites have a low predictive value . Hence the available binding sites were enriched with corresponding putative sites from regulogs identified from different species within the Streptococcus genus. In addition to the PSSMs constructed from manually identified regulogs, PSSMs were also compiled from already assembled regulogic sites retrieved from the RegPrecise database  and from phylogenetic footprinting studies. Each resulting set of binding sites was submitted to consensus, which is a tool for mining out conserved motifs. The tab-formatted PSSMs were then converted into TRANSFAC formatted PSSMs which enable an user-friendly organization of pattern matching results. Additional file 3 lists the transcription factors with their corresponding binding site information.
Prediction of putative binding sites by Pattern Matching
Since the predictive capacity of each PSSM (due to its varying information content) differs from case to case, a generic or common P-value could not be used to screen out “putative-target hits” (i.e. genes or operons harboring binding sites predicted by the corresponding PSSMs). The RSAT tool termed matrix-quality was used to objectively determine the optimal P-value for every PSSM. The TRANSFAC formatted PSSMs were then employed to search for putative sites using the tool matrix-scan (http://www.rsat.eu/) [115, 116] with the determined optimal P-values set as the cut-offs. Putative sites were searched for in the upstream regions (1000 bps upstream of the start codon with no overlap with the coding regions of the preceding ORF) of all genes in the S. mutans UA159 genome. A markov order of 0 and a background model comprising S. mutans specific upstream regions (no overlap with ORF coding regions) was used during the pattern matching scan. The resulting sites with a P-value smaller than the determined optimal P-value were considered as significant. In cases of PSSMs for which the optimal P-values could not be determined due to the inherent low complexity of the motifs , a whole genome string-based site identification was performed using the non-matrix based tool genome-scale dna pattern (http://www.rsat.eu/)  with an allowance for a maximum of 2 mismatches. Both the forward and reverse strands were subject to the pattern matching procedure.
Analysis of sub-networks
Even if the expression profiles of not all the genes in the same operon are well correlated with the expression of a certain regulator gene, we assume that all the genes in the same operon will be regulated by the regulator provided that the corresponding binding sites are found in the upstream regulatory regions of the operon. This is what we refer to as operon-oriented adjustment.
To obtain the TRRN, the co-expression network was superimposed onto the regulator-target gene binding site map. The genes in each co-regulated TRRN group or subnetwork after operon-oriented adjustment were analyzed to detect any significant over-representation of categories such as biological functional classes, KEGG metabolic pathways and gene ontology terms. The hypergeometric distribution was employed to determine over-represented categories with the network analysis tool compare-classes (http://www.rsat.eu/). Self and reciprocal comparisons were avoided. Enrichment events with significance scores > =0 were considered as statistically significant. Gene ontology information was retrieved from the Pathosystems Resource Integration Center (PATRIC) . All the network visualizations were performed using Cytoscape . Network motifs were analyzed using the tool MFINDER . The significance of the discovered motifs in the real network was determined in comparison to their occurrences after 10000 randomizations (at a P-value < =0.01). Heat map representation of metabolic pathways was generated using the Mayday visualization tool version 2.12.
Heterologous expression and purification of response regulator proteins
Coding sequences corresponding to the S. mutans response regulators MbrC (SMU_1008) and VicR (SMU_1517c) were PCR-amplified with Phusion-Polymerase (NEB) using primer pairs MbrCFor/MbrCRev and VicRFor/VicRRev respectively (see Additional file 9). Homologous flanks to the vector sequence of pET28c were implemented at the 5’ ends of the primer. The purified DNA was subsequently cloned in expression vector pET28c (Novagen) cut with NcoI/XhoI (Fermentas) using the CloneEZKit (Genescript). Resulting plasmids bearing the coding sequence for a N-terminal His-Tag were verified by sequencing and transformed in BL21Star. Cells were grown in 4 l shaking flaks, induced with 1 mM IPTG at an OD600 of 0.5 and harvested 4 hours after induction. The resulting cell pellet was re-suspended in lysis buffer (50 mM Tris, 150 mM NaCl, pH 7.4) supplemented with 4 mg/ml lysozyme (Sigma) and frozen at −20°C. After de-freezing the pellet, 100 μg DNAse I (Roche) and 5 mM MgSO4 (Sigma, final concentration) were added and 5 cycles of sonification for 60 seconds were applied to lyse cells (duty cycle 0.5 Sec, pause 1 sec, amplitude 60%). Finally 0.1% NP40 (Sigma, final concentration) and 10 mM imidazol (Sigma, final concentration) were added and cell debris was removed by centrifugation and filtration (0.45 μm). His-tagged proteins were purified on a HIS-Talon (Clontech) column using a Duo Flow FPLC (Biorad) at a flow rate of 0.5 ml/h. Resulting purified proteins were desalted using PD10 columns (Amersham), eluted in 1xPBS buffer and measured using a spectrophotometer (Nanodrop ND1000, Peqlab) to determine the protein concentration. The response regulator was over 99% pure as confirmed by SDS-PAGE (data not shown). Promoter regions containing the potential binding sites of MbrC were PCR amplified using Taq-polymerase. The primers used are listed in Additional file 9. PCR-products were purified using the PCR-Purification Kit (Qiagen) and used as targets for EMSA.
Deletion of potential binding sites
Potential binding sites of the response regulator MbrC were deleted using a PCR-driven overlap extension method . Motifs in the promoter regions of SMU_610, SMU_718, and SMU_1006 were deleted by two initial PCRs generating overlapping DNA sequences. Taq polymerase (Qiagen) was used for the amplification of regions flanking the potential binding sites. PCR-products were purified from an agarose gel using the Gel Extraction Kit (Qiagen) and used as template for a third PCR with Phusion polymerase using primers (Additional file 9) spanning the whole region. Purified PCR-products were cloned blunt-end in the EcoRV restriction site of vector pGEM5Zf(+) (Promega). Resulting plasmids were verified by sequencing and used as template for a PCR to finally generate the DNA-targets for EMSA.
The response regulator (MbrC and VicR) proteins were activated by acetylphosphate (Sigma). An aliqot of the protein was incubated for 2 h at RT (room temperature) in reaction buffer (25 mM acetylphosphate, 50 mM Tris–HCl, 50 mM KCl, 10 mM MgCl2, 4 mM dithiothreitol) as described previously. Excess of acetylphosphate was removed by filtration and the protein was serially diluted in binding buffer (10 mM Tris, 1 mM EDTA, 100 mM KCl, 100 μM DTT, 5% vol/vol glycerol, 10 μg/ml BSA, pH 7.5). 0.5 pmol of target and competitor DNA was added to each reaction and incubated for 1 h at RT. The unrelated response regulator VicR which has a similar MW and pI as the response regulator MbrC under study was used as a negative control to rule out unspecific DNA binding. Four μl of the reaction mixture was applied on a 5% acrylamide gel run in Tris-borate-EDTA (TBE) buffer at pH 7.4. Gels were stained using SybrGold and visualized in a transilluminator (Alpha DigiDoc, Biorad) at 254 nm.
Construction of gene deletion mutants and a cysRcomplementation strain
Upstream and downstream flanking regions of cysR were PCR-amplified using primers CysR P1/2 and CysR P3/4 (see Additional file 9 for the primers used to generate deletion mutants) and genomic DNA of S. mutans UA159 as template. The erythromycin resistance cassette was amplified from genomic DNA of a previously constructed mutant . Restriction sites of AscI and FseI were introduced via the 5’-termini of the primers. After restriction digestion of purified PCR-products with the appropriate restriction enzymes, the up and downstream flanks were ligated to the ERM cassette using T4 DNA Ligase and directly transformed in the S. mutans UA159 WT strain according to the procedure of Li et al. . Gene deletion strains were selected on THBY agar plates containing 10 μg/ml erythromycin. Genomic DNA of isolated clones was analysed with PCR and primers P1 and P4 spanning the entire gene deletion construct. Sequencing was used to further confirm the correct insertion of the gene deletion construct via double homologous recombination. For the generation of the four other gene deletion strains (glnR, fabT, rgg and spxA), a similar procedure was carried out.
RNA was isolated from the exponentially growing cysR gene deletion strain and was verified for the absence of cysR mRNA with RT-PCR using the 3 primer pairs Q-CYSR1-F/R, Q-CYSR2-F/R, and Q-CYSR3-F/R. Primers specific for the ComX (ComX F/R) and ComE (ComE F/R) encoding genes were used as positive controls for the RT-PCR reaction. Reactions in which the reverse transcriptase was replaced with water functioned as negative controls. For the complementation of the cysR gene deletion strain, the entire cysR gene including its promoter region were PCR-amplified with primers C-CYSR1-F and C-CYSR1-R and cloned blunt end via the SmaI restriction site in the replicative plasmid pDL278 . Resulting plasmids were verified by sequencing and transformed in the cysR gene deletion strain as described elsewhere .
Viability measurements of the carolacton treated cysRdeletion strain using Live/Dead viability staining and by Cfu determination
Viability measurements using live/dead viability staining of carolacton treated and untreated biofilms of the S. mutans UA159 wildtype, gene deletion and complementation strains were essentially performed as previously described . Biofilms of S. mutans UA159 WT were used as positive control. The experiment was repeated in two biological replicates. For the cfu determination, biofilms representing one condition were harvested and pooled from 5 individual wells. Chains and biofilm clumps were dispersed and destroyed using mild ultrasonification conditions as described before  and plated on THBY-agar plates (containing 10 μg/ml erythromycin for the mutant) in 3 technical replicates. Live dead staining before and after sonification verified that the sonification had no significant influence on cell viability. The overall experiment was repeated in 2 biological replicates.
Transcriptional regulatory response network
Electro mobility shift assay
Two component system
glucan binding protein B
Time series network identification
Genes corresponding to transcripts with altered abundances
Kyoto encyclopedia of genes and genomes
- TC Method:
Trend Correlation method
Open reading frame
Pathosystems resource integratrion center
Reverse transcriptase polymerase chain reaction
Sodium Do-decyl Sulfate Poly-Acrylamide Gel Electrophoresis
Position specific scoring matrix
Regulatory sequence analysis tools
Guanosine tri phosphate
Single input module
Multiple input module
Feed forward loop
Uridine di phosphate
Uridine tri phosphate
Uridine mono phosphate
Uridine Di-Phosphate N-Acetyl Glucosamine
Acid tolerance response
Colony forming units
LysR type transcriptional regulators
sigX inducing peptide
This study was done within the project “Development of biofilm inhibitors using a systems biology approach” (0315411) which is financed by the German Federal Ministry of Education and Research (BMBF) in the frame of the Research Program “Medical systems biology - MedSys”.
The time-series microarray data set generated as part of this study is available in the Gene Expression Omnibus (GEO) repository [accession id GSE53264].
- Stoodley P, Sauer K, Davies DG, Costerton JW: Biofilms as complex differentiated communities. Annu Rev Microbiol. 2002, 56: 187-209. 10.1146/annurev.micro.56.012302.160705.PubMedGoogle Scholar
- Dufour D, Leung V, Levesque CM: Bacterial biofilm: structure, function, and antimicrobial resistance. Endo Topics. 2012, 22 (1): 2-16.Google Scholar
- Kunze B, Reck M, Dötsch A, Lemme A, Schummer D, Irschik H, Steinmetz H, Wagner-Döbler I: Damage of Streptococcus mutans biofilms by carolacton, a secondary metabolite from the myxobacterium Sorangium cellulosum. BMC Microbiol. 2010, 10: 199-10.1186/1471-2180-10-199.PubMed CentralPubMedGoogle Scholar
- Roychoudhury S, Zielinski NA, Ninfa AJ, Allen NE, Jungheim LN, Nicas TI, Chakrabarty AM: Inhibitors of two-component signal transduction systems: inhibition of alginate gene activation in Pseudomonas aeruginosa. Proc Natl Acad Sci U S A. 1993, 90: 965-969. 10.1073/pnas.90.3.965.PubMed CentralPubMedGoogle Scholar
- Reck M, Rutz K, Kunze B, Tomasch J, Surapaneni SK, Schulz S, Wagner-Döbler I: The biofilm inhibitor carolacton disturbs membrane integrity and cell division of Streptococcus mutans through the serine/threonine protein kinase PknB. J Bacteriol. 2011, 193: 5692-5706. 10.1128/JB.05424-11.PubMed CentralPubMedGoogle Scholar
- Li Y, Tang N, Aspiras MB, Lau PCY, Lee JH, Ellen RP, Cvitkovitch DG: A quorum-sensing signaling system essential for genetic competence in Streptococcus mutans is involved in biofilm formation. J Bacteriol. 2002, 184: 2699-2708. 10.1128/JB.184.10.2699-2708.2002.PubMed CentralPubMedGoogle Scholar
- Qi F, Kreth J, Lévesque CM, Kay O, Mair RW, Shi W, Cvitkovitch DG, Goodman SD: Peptide pheromone induced cell death of Streptococcus mutans. FEMS Microbiol Lett. 2005, 251: 321-326. 10.1016/j.femsle.2005.08.018.PubMedGoogle Scholar
- Bhagwat SP, Nary J, Burne RA: Effects of mutating putative two-component systems on biofilm formation by Streptococcus mutans UA159. FEMS Microbiol Lett. 2001, 205: 225-230. 10.1111/j.1574-6968.2001.tb10952.x.PubMedGoogle Scholar
- Sasková L, Nováková L, Basler M, Branny P: Eukaryotic-type serine/threonine protein kinase StkP is a global regulator of gene expression in Streptococcus pneumoniae. J Bacteriol. 2007, 189: 4168-4179. 10.1128/JB.01616-06.PubMed CentralPubMedGoogle Scholar
- He F, Balling R, Zeng A: Reverse engineering and verification of gene networks:principles, assumptions, and limitations of present methods and future perspectives. J Biotechnol. 2009, 144: 190-203. 10.1016/j.jbiotec.2009.07.013.PubMedGoogle Scholar
- Cabusora L, Sutton E, Fulmer A, Forst CV: Differential network expression during drug and stress response. Bioinformatics. 2005, 21: 2898-2905. 10.1093/bioinformatics/bti440.PubMedGoogle Scholar
- Bansal M, Della Gatta G, Di Bernardo D: Inference of gene regulatory networks and compound mode of action from time course gene expression profiles. Bioinformatics. 2006, 22: 815-822. 10.1093/bioinformatics/btl003.PubMedGoogle Scholar
- Aluru M, Zola J, Nettleton D, Aluru S: Reverse engineering and analysis of large genome-scale gene networks. Nucleic Acids Res. 2013, 41: e24-10.1093/nar/gks904.PubMed CentralPubMedGoogle Scholar
- Faith JJ, Hayete B, Thaden JT, Mogno I, Wierzbowski J, Cottarel G, Kasif S, Collins JJ, Gardner TS: Large-scale mapping and validation of Escherichia coli transcriptional regulation from a compendium of expression profiles. PLoS Biol. 2007, 5: e8-10.1371/journal.pbio.0050008.PubMed CentralPubMedGoogle Scholar
- He F, Chen H, Probst-Kepper M, Geffers R, Eifes S, Del Sol A, Schughart K, Zeng A, Balling R: PLAU inferred from a correlation network is critical for suppressor function of regulatory T cells. Mol Syst Biol. 2012, 8: 624-PubMed CentralPubMedGoogle Scholar
- Faria JP, Overbeek R, Xia F, Rocha M, Rocha I, Henry CS: Genome-scale bacterial transcriptional regulatory networks: reconstruction and integrated analysis with metabolic models. Brief Bioinform. 2013, Epub ahead of print. doi: 10.1093/bib/bbs071Google Scholar
- Fadda A, Fierro AC, Lemmens K, Monsieurs P, Engelen K, Marchal K: Inferring the transcriptional network of Bacillus subtilis. Mol Biosyst. 2009, 5: 1840-1852. 10.1039/b907310h.PubMedGoogle Scholar
- Castro-Melchor M, Charaniya S, Karypis G, Takano E, Hu W: Genome-wide inference of regulatory networks in Streptomyces coelicolor. BMC Genomics. 2010, 11: 578-10.1186/1471-2164-11-578.PubMed CentralPubMedGoogle Scholar
- Bonneau R, Reiss DJ, Shannon P, Facciotti M, Hood L, Baliga NS, Thorsson V: The Inferelator: an algorithm for learning parsimonious regulatory networks from systems-biology data sets de novo. Genome Biol. 2006, 7: R36-10.1186/gb-2006-7-5-r36.PubMed CentralPubMedGoogle Scholar
- Fu Y, Jarboe LR, Dickerson JA: Reconstructing genome-wide regulatory network of E. coli using transcriptome data and predicted transcription factor activities. BMC Bioinformatics. 2011, 12: 233-10.1186/1471-2105-12-233.PubMed CentralPubMedGoogle Scholar
- Guelzim N, Bottani S, Bourgine P, Képès F: Topological and causal structure of the yeast transcriptional regulatory network. Nat Genet. 2002, 31: 60-63. 10.1038/ng873.PubMedGoogle Scholar
- Altwasser R, Linde J, Buyko E, Hahn U, Guthke R: Genome-Wide Scale-Free Network Inference for Candida albicans. Front Microbiol. 2012, 3: 51-PubMed CentralPubMedGoogle Scholar
- He FQ, Wang W, Zheng P, Sudhakar P, Sun J, Zeng AP: Essential O2-responsive genes of Pseudomonas aeruginosa and their network revealed by integrating dynamic data from inverted conditions. Integr Biol. 2014, 6: 215-223. 10.1039/c3ib40180d.Google Scholar
- Bailly-Bechet M, Braunstein A, Pagnani A, Weigt M, Zecchina R: Inference of sparse combinatorial-control networks from gene-expression data: a message passing approach. BMC Bioinformatics. 2010, 11: 355-10.1186/1471-2105-11-355.PubMed CentralPubMedGoogle Scholar
- Basso K, Margolin A, Stolovitzky G, Klein U, Dalla-Favera R, Califano A: Reverse engineering of regulatory networks in human B cells. Nat Genet. 2005, 37: 382-390. 10.1038/ng1532.PubMedGoogle Scholar
- O’Rourke KP, Shaw JD, Pesesky MW, Cook BT, Roberts SM, Bond JP, Spatafora GA: Genome-wide characterization of the SloR metalloregulome in Streptococcus mutans. J Bacteriol. 2010, 192: 1433-1443. 10.1128/JB.01161-09.PubMed CentralPubMedGoogle Scholar
- Ahn S, Wen ZT, Burne RA: Effects of oxygen on virulence traits of Streptococcus mutans. J Bacteriol. 2007, 189: 8519-8527. 10.1128/JB.01180-07.PubMed CentralPubMedGoogle Scholar
- Ajdić D, Pham VTT: Global transcriptional analysis of Streptococcus mutans sugar transporters using microarrays. J Bacteriol. 2007, 189: 5049-5059. 10.1128/JB.00338-07.PubMed CentralPubMedGoogle Scholar
- Liu J, Wu C, Huang I, Merritt J, Qi F: Differential response of Streptococcus mutans towards friend and foe in mixed-species cultures. Microbiology. 2011, 157: 2433-2444. 10.1099/mic.0.048314-0.PubMed CentralPubMedGoogle Scholar
- Lévesque CM, Mair RW, Perry JA, Lau PCY, Li Y, Cvitkovitch DG: Systemic inactivation and phenotypic characterization of two-component systems in expression of Streptococcus mutans virulence properties. Lett Appl Microbiol. 2007, 45: 398-404. 10.1111/j.1472-765X.2007.02203.x.PubMed CentralPubMedGoogle Scholar
- Perry JA, Lévesque CM, Suntharaligam P, Mair RW, Bu M, Cline RT, Peterson SN, Cvitkovitch DG: Involvement of Streptococcus mutans regulator RR11 in oxidative stress response during biofilm growth and in the development of genetic competence. Lett Appl Microbiol. 2008, 47: 439-444. 10.1111/j.1472-765X.2008.02455.x.PubMed CentralPubMedGoogle Scholar
- He F, Zeng A: In search of functional association from time-series microarray data based on the change trend and level of gene expression. BMC Bioinformatics. 2006, 7: 69-10.1186/1471-2105-7-69.PubMed CentralPubMedGoogle Scholar
- Rodionov DA: Comparative genomic reconstruction of transcriptional regulatory networks in bacteria. Chem Rev. 2007, 107: 3467-3497. 10.1021/cr068309+.PubMed CentralPubMedGoogle Scholar
- Leyn SA, Kazanov MD, Sernova NV, Ermakova EO, Novichkov PS, Rodionov DA: Genomic Reconstruction of Transcriptional Regulatory Network in Bacillus subtilis. J Bacteriol. 2013, 195: 2463-2473. 10.1128/JB.00140-13.PubMed CentralPubMedGoogle Scholar
- Cornish JP, Matthews F, Thomas JR, Erill I: Inference of self-regulated transcriptional networks by comparative genomics. Evol Bioinform Online. 2012, 8: 449-461.PubMed CentralPubMedGoogle Scholar
- Novichkov PS, Laikova ON, Novichkova ES, Gelfand MS, Arkin AP, Dubchak I, Rodionov DA: RegPrecise: a database of curated genomic inferences of transcriptional regulatory interactions in prokaryotes. Nucleic Acids Res. 2010, 38: D111-8. 10.1093/nar/gkp894.PubMed CentralPubMedGoogle Scholar
- Medina-Rivera A, Abreu-Goodger C, Thomas-Chollier M, Salgado H, Collado-Vides J, van Helden J: Theoretical and empirical quality assessment of transcription factor-binding motifs. Nucleic Acids Res. 2011, 39: 808-824. 10.1093/nar/gkq710.PubMed CentralPubMedGoogle Scholar
- Lemos JA, Nascimento MM, Lin VK, Abranches J, Burne RA: Global regulation by (p)ppGpp and CodY in Streptococcus mutans. J Bacteriol. 2008, 190: 5291-5299. 10.1128/JB.00288-08.PubMed CentralPubMedGoogle Scholar
- Isalan M, Lemerle C, Michalodimitrakis K, Horn C, Beltrao P, Raineri E, Garriga-Canut M, Serrano L: Evolvability and hierarchy in rewired bacterial gene networks. Nature. 2008, 452: 840-845. 10.1038/nature06847.PubMed CentralPubMedGoogle Scholar
- Ma H, Buer J, Zeng A: Hierarchical structure and modules in the Escherichia coli transcriptional regulatory network revealed by a new top-down approach. BMC Bioinformatics. 2004, 5: 199-10.1186/1471-2105-5-199.PubMed CentralPubMedGoogle Scholar
- Galán-Vásquez E, Luna B, Martínez-Antonio A: The Regulatory Network of Pseudomonas aeruginosa. Microb Inform Exp. 2011, 1: 3-10.1186/2042-5783-1-3.PubMed CentralPubMedGoogle Scholar
- Dufour YS, Kiley PJ, Donohue TJ: Reconstruction of the core and extended regulons of global transcription factors. PLoS Genet. 2010, 6: e1001027-10.1371/journal.pgen.1001027.PubMed CentralPubMedGoogle Scholar
- Chaturongakul S, Raengpradub S, Palmer ME, Bergholz TM, Orsi RH, Hu Y, Ollinger J, Wiedmann M, Boor KJ: Transcriptomic and phenotypic analyses identify coregulated, overlapping regulons among PrfA, CtsR, HrcA, and the alternative sigma factors sigmaB, sigmaC, sigmaH, and sigmaL in Listeria monocytogenes. Appl Environ Microbiol. 2011, 77: 187-200. 10.1128/AEM.00952-10.PubMed CentralPubMedGoogle Scholar
- Konagurthu AS, Lesk AM: Single and multiple input modules in regulatory networks. Proteins. 2008, 73: 320-324. 10.1002/prot.22053.PubMedGoogle Scholar
- Mangan S, Alon U: Structure and function of the feed-forward loop network motif. Proc Natl Acad. Sci. U.S.A. 2003, 100: 11980-11985. 10.1073/pnas.2133841100.PubMed CentralPubMedGoogle Scholar
- Kalir S, McClure J, Pabbaraju K, Southward C, Ronen M, Leibler S, Surette MG, Alon U: Ordering genes in a flagella pathway by analysis of expression kinetics from living bacteria. Science. 2001, 292: 2080-2083. 10.1126/science.1058758.PubMedGoogle Scholar
- Kashtan N, Itzkovitz S, Milo R, Alon U: Topological generalizations of network motifs. Phys Rev E Stat Nonlin Soft Matter Phys. 2004, 70: 31909-Google Scholar
- Ma H, Kumar B, Ditges U, Gunzer F, Buer J, Zeng A: An extended transcriptional regulatory network of Escherichia coli and analysis of its hierarchical structure and network motifs. Nucleic Acids Res. 2004, 32: 6643-6649. 10.1093/nar/gkh1009.PubMed CentralPubMedGoogle Scholar
- Chen P, Chen YM, Yu S, Sher S, Lai C, Chia J: Role of GlnR in acid-mediated repression of genes encoding proteins involved in glutamine and glutamate metabolism in Streptococcus mutans. Appl Environ Microbiol. 2010, 76: 2478-2486. 10.1128/AEM.02622-09.PubMed CentralPubMedGoogle Scholar
- Ouyang J, Tian X, Versey J, Wishart A, Li Y: The BceABRS four-component system regulates the bacitracin-induced cell envelope stress response in Streptococcus mutans. Antimicrob Agents Chemother. 2010, 54: 3895-3906. 10.1128/AAC.01802-09.PubMed CentralPubMedGoogle Scholar
- 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: 2340-2349. 10.1128/JB.01237-07.PubMed CentralPubMedGoogle Scholar
- Abranches J, Chen YM, Burne RA: Characterization of Streptococcus mutans strains deficient in EIIAB Man of the sugar phosphotransferase system. Appl Environ Microbiol. 2003, 69: 4760-4769. 10.1128/AEM.69.8.4760-4769.2003.PubMed CentralPubMedGoogle Scholar
- Zeng L, Wen ZT, Burne RA: A novel signal transduction system and feedback loop regulate fructan hydrolase gene expression in Streptococcus mutans. Mol Microbiol. 2006, 62: 187-200. 10.1111/j.1365-2958.2006.05359.x.PubMedGoogle Scholar
- Zeng L, Das S, Burne RA: Genetic analysis of the functions and interactions of components of the LevQRST signal transduction complex of Streptococcus mutans. PLoS One. 2011, 6: e17335-10.1371/journal.pone.0017335.PubMed CentralPubMedGoogle Scholar
- Webb AJ, Homer KA, Hosie AHF: Two closely related ABC transporters in Streptococcus mutans are involved in disaccharide and/or oligosaccharide uptake. J Bacteriol. 2008, 190: 168-178. 10.1128/JB.01509-07.PubMed CentralPubMedGoogle Scholar
- Loesche WJ: Role of Streptococcus mutans in human dental decay. Microbiol Rev. 1986, 50: 353-380.PubMed CentralPubMedGoogle Scholar
- Touger-Decker R, van Loveren C: Sugars and dental caries. Am J Clin Nutr. 2003, 78: 881S-892S.PubMedGoogle Scholar
- van Houte J, Upeslacis VN, Jordan HV, Skobe Z, Green DB: Role of sucrose in colonization of Streptococcus mutans in conventional Sprague–Dawley rats. J Dent Res. 1976, 55: 202-215. 10.1177/00220345760550020801.PubMedGoogle Scholar
- Cury JA, Francisco SB, Del Bel Cury AA, Tabchoury CP: In situ study of sucrose exposure, mutans streptococci in dental plaque and dental caries. Braz Dent J. 2001, 12: 101-104.PubMedGoogle Scholar
- Nobre dos Santos M, Melo dos Santos L, Francisco SB, Cury JA: Relationship among dental plaque composition, daily sugar exposure and caries in the primary dentition. Caries Res. 2002, 36: 347-352. 10.1159/000065959.PubMedGoogle Scholar
- Sadykov MR, Mattes TA, Luong TT, Zhu Y, Day SR, Sifri CD, Lee CY, Somerville GA: Tricarboxylic acid cycle-dependent synthesis of Staphylococcus aureus Type 5 and 8 capsular polysaccharides. J Bacteriol. 2010, 192: 1459-1462. 10.1128/JB.01377-09.PubMed CentralPubMedGoogle Scholar
- Howden BP, McEvoy CRE, Allen DL, Chua K, Gao W, Harrison PF, Bell J, Coombs G, Bennett-Wood V, Porter JL, Robins-Browne R, Davies JK, Seemann T, Stinear TP: Evolution of multidrug resistance during Staphylococcus aureus infection involves mutation of the essential two component regulator WalKR. PLoS Pathog. 2011, 7: e1002359-10.1371/journal.ppat.1002359.PubMed CentralPubMedGoogle Scholar
- Dashper SG, Riley PF, Reynolds EC: Characterization of glutamine transport in Streptococcus mutans. Oral Microbiol Immunol. 1995, 10: 183-187. 10.1111/j.1399-302X.1995.tb00140.x.PubMedGoogle Scholar
- Cvitkovitch DG, Gutierrez JA, Bleiweis AS: Role of the citrate pathway in glutamate biosynthesis by Streptococcus mutans. J Bacteriol. 1997, 179: 650-655.PubMed CentralPubMedGoogle Scholar
- Yu H, Yao Y, Liu Y, Jiao R, Jiang W, Zhao G: A complex role of Amycolatopsis mediterranei GlnR in nitrogen metabolism and related antibiotics production. Arch Microbiol. 2007, 188: 89-96. 10.1007/s00203-007-0228-7.PubMedGoogle Scholar
- Rolerson E, Swick A, Newlon L, Palmer C, Pan Y, Keeshan B, Spatafora G: The SloR/Dlg metalloregulator modulates Streptococcus mutans virulence gene expression. J Bacteriol. 2010, 192: 1433-1443. 10.1128/JB.01161-09.Google Scholar
- Chattoraj P, Mohapatra SS, Rao JLUM, Biswas I: Regulation of transcription by SMU.1349, a TetR family regulator, in Streptococcus mutans. J Bacteriol. 2011, 193: 6605-6613. 10.1128/JB.06122-11.PubMed CentralPubMedGoogle Scholar
- Kreth J, Hung DCI, Merritt J, Perry J, Zhu L, Goodman SD, Cvitkovitch DG, Shi W, Qi F: The response regulator ComE in Streptococcus mutans functions both as a transcription activator of mutacin production and repressor of CSP biosynthesis. Microbiology. 2007, 153: 1799-1807. 10.1099/mic.0.2007/005975-0.PubMed CentralPubMedGoogle Scholar
- Krastel K, Senadheera DB, Mair R, Downey JS, Goodman SD, Cvitkovitch DG: Characterization of a glutamate transporter operon, glnQHMP, in Streptococcus mutans and its role in acid tolerance. J Bacteriol. 2010, 192: 984-993. 10.1128/JB.01169-09.PubMed CentralPubMedGoogle Scholar
- Matsui R, Cvitkovitch D: Acid tolerance mechanisms utilized by Streptococcus mutans. Future Microbiol. 2010, 5: 403-417. 10.2217/fmb.09.129.PubMed CentralPubMedGoogle Scholar
- Svensäter G, Larsson UB, Greif EC, Cvitkovitch DG, Hamilton IR: Acid tolerance response and survival by oral bacteria. Oral Microbiol Immunol. 1997, 12: 266-273. 10.1111/j.1399-302X.1997.tb00390.x.PubMedGoogle Scholar
- Liu Y, Burne RA: Multiple two-component systems of Streptococcus mutans regulate agmatine deiminase gene expression and stress tolerance. J Bacteriol. 2009, 191: 7363-7366. 10.1128/JB.01054-09.PubMed CentralPubMedGoogle Scholar
- Lee SF, Delaney GD, Elkhateeb M: A two-component covRS regulatory system regulates expression of fructosyltransferase and a novel extracellular carbohydrate in Streptococcus mutans. Infect Immun. 2004, 72: 3968-3973. 10.1128/IAI.72.7.3968-3973.2004.PubMed CentralPubMedGoogle Scholar
- Deng DM, Liu MJ, Cate JM t, Crielaard W: The VicRK system of Streptococcus mutans responds to oxidative stress. J Dent Res. 2007, 86: 606-610. 10.1177/154405910708600705.PubMedGoogle Scholar
- Tremblay YDN, Lo H, Li Y, Halperin SA, Lee SF: Expression of the Streptococcus mutans essential two-component regulatory system VicRK is pH and growth-phase dependent and controlled by the LiaFSR three-component regulatory system. Microbiology. 2009, 155: 2856-2865. 10.1099/mic.0.028456-0.PubMedGoogle Scholar
- Senadheera MD, Guggenheim B, Spatafora GA, Huang YC, Choi J, Hung DCI, Treglown JS, Goodman SD, Ellen RP, Cvitkovitch DG: A VicRK signal transduction system in Streptococcus mutans affects gtfBCD, gbpB, and ftf expression, biofilm formation, and genetic competence development. J Bacteriol. 2005, 187: 4064-4076. 10.1128/JB.187.12.4064-4076.2005.PubMed CentralPubMedGoogle Scholar
- Senadheera D, Krastel K, Mair R, Persadmehr A, Abranches J, Burne RA, Cvitkovitch DG: Inactivation of VicK affects acid production and acid survival of Streptococcus mutans. J Bacteriol. 2009, 191: 6415-6424. 10.1128/JB.00793-09.PubMed CentralPubMedGoogle Scholar
- Lévesque CM, Voronejskaia E, Huang YC, Mair RW, Ellen RP, Cvitkovitch DG: Involvement of sortase anchoring of cell wall proteins in biofilm formation by Streptococcus mutans. Infect Immun. 2005, 73: 3773-3777. 10.1128/IAI.73.6.3773-3777.2005.PubMed CentralPubMedGoogle Scholar
- Duque C, Stipp RN, Wang B, Smith DJ, Höfling JF, Kuramitsu HK, Duncan MJ, Mattos-Graner RO: Downregulation of GbpB, a component of the VicRK regulon, affects biofilm formation and cell surface characteristics of Streptococcus mutans. Infect Immun. 2011, 79: 786-796. 10.1128/IAI.00725-10.PubMed CentralPubMedGoogle Scholar
- Senadheera DB, Cordova M, Ayala EA, LE de Chávez P, Singh K, Downey JS, Svensäter G, Goodman SD, Cvitkovitch DG: Regulation of bacteriocin production and cell death by the VicRK signaling system in Streptococcus mutans. J Bacteriol. 2012, 194: 1307-1316. 10.1128/JB.06071-11.PubMed CentralPubMedGoogle Scholar
- Sperandio B, Gautier C, Pons N, Ehrlich DS, Renault P, Guédon E: Three paralogous LysR-type transcriptional regulators control sulfur amino acid supply in Streptococcus mutans. J Bacteriol. 2010, 192: 3464-3473. 10.1128/JB.00119-10.PubMed CentralPubMedGoogle Scholar
- Fleuchot B, Gitton C, Guillot A, Vidic J, Nicolas P, Besset C, Fontaine L, Hols P, Leblond-Bourget N, Monnet V, Gardan R: Rgg proteins associated with internalized small hydrophobic peptides: a new quorum-sensing mechanism in streptococci. Mol Microbiol. 2011, 80: 1102-1119. 10.1111/j.1365-2958.2011.07633.x.PubMedGoogle Scholar
- Filipe SR, Severina E, Tomasz A: Functional analysis of Streptococcus pneumoniae MurM reveals the region responsible for its specificity in the synthesis of branched cell wall peptides. J Biol Chem. 2001, 276: 39618-39628. 10.1074/jbc.M106425200.PubMedGoogle Scholar
- Filipe SR, Severina E, Tomasz A: The role of murMN operon in penicillin resistance and antibiotic tolerance of Streptococcus pneumoniae. Microb Drug Resist. 2001, 7: 303-316. 10.1089/10766290152773310.PubMedGoogle Scholar
- Filipe SR, Severina E, Tomasz A: The murMN operon: a functional link between antibiotic resistance and antibiotic tolerance in Streptococcus pneumoniae. Proc Natl Acad Sci U S A. 2002, 99: 1550-1555. 10.1073/pnas.032671699.PubMed CentralPubMedGoogle Scholar
- Filipe SR, Tomasz A: Inhibition of the expression of penicillin resistance in Streptococcus pneumoniae by inactivation of cell wall muropeptide branching genes. Proc Natl Acad Sci U S A. 2000, 97: 4891-4896. 10.1073/pnas.080067697.PubMed CentralPubMedGoogle Scholar
- Typas A, Banzhaf M, Gross CA, Vollmer W: From the regulation of peptidoglycan synthesis to bacterial growth and morphology. Nat Rev Microbiol. 2012, 10: 123-136.Google Scholar
- de Jonge BLM, Gage D, Xu N: The carboxyl terminus of peptidoglycan stem peptides is a determinant for methicillin resistance in Staphylococcus aureus. Antimicrob Agents Chemother. 2002, 46: 3151-3155. 10.1128/AAC.46.10.3151-3155.2002.PubMed CentralPubMedGoogle Scholar
- Garcia-Bustos JF, Chait BT, Tomasz A: Altered peptidoglycan structure in a pneumococcal transformant resistant to penicillin. J Bacteriol. 1988, 170: 2143-2147.PubMed CentralPubMedGoogle Scholar
- Garcia-Bustos J, Tomasz A: A biological price of antibiotic resistance: major changes in the peptidoglycan structure of penicillin-resistant pneumococci. Proc Natl Acad Sci U S A. 1990, 87: 5415-5419. 10.1073/pnas.87.14.5415.PubMed CentralPubMedGoogle Scholar
- Simelyte E, Rimpiläinen M, Zhang X, Toivanen P: Role of peptidoglycan subtypes in the pathogenesis of bacterial cell wall arthritis. Ann Rheum Dis. 2003, 62: 976-982. 10.1136/ard.62.10.976.PubMed CentralPubMedGoogle Scholar
- Kajfasz JK, Rivera-Ramos I, Abranches J, Martinez AR, Rosalen PL, Derr AM, Quivey RG, Lemos JA: Two Spx proteins modulate stress tolerance, survival, and virulence in Streptococcus mutans. J Bacteriol. 2010, 192: 2546-2556. 10.1128/JB.00028-10.PubMed CentralPubMedGoogle Scholar
- Sperandio B, Gautier C, McGovern S, Ehrlich DS, Renault P, Martin-Verstraete I, Guédon E: Control of methionine synthesis and uptake by MetR and homocysteine in Streptococcus mutans. J Bacteriol. 2007, 189: 7032-7044. 10.1128/JB.00703-07.PubMed CentralPubMedGoogle Scholar
- Catt DM, Gregory RL: Streptococcus mutans murein hydrolase. J Bacteriol. 2005, 187: 7863-7865. 10.1128/JB.187.22.7863-7865.2005.PubMed CentralPubMedGoogle Scholar
- Dufour D, Lévesque CM: Cell death of Streptococcus mutans induced by a quorum-sensing peptide occurs via a conserved streptococcal autolysin. J Bacteriol. 2013, 195: 105-114. 10.1128/JB.00926-12.PubMed CentralPubMedGoogle Scholar
- Huynen M, Snel B, Lathe W, Bork P: Predicting protein function by genomic context: quantitative evaluation and qualitative inferences. Genome Res. 2000, 10: 1204-1210. 10.1101/gr.10.8.1204.PubMed CentralPubMedGoogle Scholar
- Wu H, Su Z, Mao F, Olman V, Xu Y: Prediction of functional modules based on comparative genome analysis and Gene Ontology application. Nucleic Acids Res. 2005, 33: 2822-2837. 10.1093/nar/gki573.PubMed CentralPubMedGoogle Scholar
- Mavromatis K, Chu K, Ivanova N, Hooper SD, Markowitz VM, Kyrpides NC: Gene context analysis in the Integrated Microbial Genomes (IMG) data management system. PLoS One. 2009, 4: e7979-10.1371/journal.pone.0007979.PubMed CentralPubMedGoogle Scholar
- Allen JP, Neely MN: CpsY influences Streptococcus iniae cell wall adaptations important for neutrophil intracellular survival. Infect Immun. 2012, 80: 1707-1715. 10.1128/IAI.00027-12.PubMed CentralPubMedGoogle Scholar
- Federle MJ, Morrison DA: One if by land, two if by sea: signalling to the ranks with CSP and XIP. Mol Microbiol. 2012, 86: 241-245. 10.1111/mmi.12029.PubMed CentralPubMedGoogle Scholar
- Mashburn-Warren L, Morrison DA, Federle MJ: A novel double-tryptophan peptide pheromone controls competence in Streptococcus spp. via an Rgg regulator. Mol Microbiol. 2010, 78: 589-606. 10.1111/j.1365-2958.2010.07361.x.PubMed CentralPubMedGoogle Scholar
- Beilharz K, Nováková L, Fadda D, Branny P, Massidda O, Veening J: Control of cell division in Streptococcus pneumoniae by the conserved Ser/Thr protein kinase StkP. Proc Natl Acad Sci U S A. 2012, 109: E905-13. 10.1073/pnas.1119172109.PubMed CentralPubMedGoogle Scholar
- Banu LD, Conrads G, Rehrauer H, Hussain H, Allan E, van der Ploeg JR: The Streptococcus mutans serine/threonine kinase, PknB, regulates competence development, bacteriocin production, and cell wall metabolism. Infect Immun. 2010, 78: 2209-2220. 10.1128/IAI.01167-09.PubMed CentralPubMedGoogle Scholar
- Hussain H, Branny P, Allan E: A eukaryotic-type serine/threonine protein kinase is required for biofilm formation, genetic competence, and acid resistance in Streptococcus mutans. J Bacteriol. 2006, 188: 1628-1632. 10.1128/JB.188.4.1628-1632.2006.PubMed CentralPubMedGoogle Scholar
- Güell M, Yus E, Lluch-Senar M, Serrano L: Bacterial transcriptomics: what is beyond the RNA horiz-ome?. Nat Rev Microbiol. 2011, 9: 658-669. 10.1038/nrmicro2620.PubMedGoogle Scholar
- Bhatt S, Romeo T, Kalman D: Honing the message: post-transcriptional and post-translational control in attaching and effacing pathogens. Trends Microbiol. 2011, 19: 217-224. 10.1016/j.tim.2011.01.004.PubMed CentralPubMedGoogle Scholar
- Koyanagi S, Lévesque CM: Characterization of a Streptococcus mutans intergenic region containing a small toxic peptide and its cis-encoded antisense small RNA antitoxin. PLoS One. 2013, 8: e54291-10.1371/journal.pone.0054291.PubMed CentralPubMedGoogle Scholar
- Hasona A, Crowley PJ, Levesque CM, Mair RW, Cvitkovitch DG, Bleiweis AS, Brady LJ: Streptococcal viability and diminished stress tolerance in mutants lacking the signal recognition particle pathway or YidC2. Proc Natl Acad Sci U S A. 2005, 102: 17466-17471. 10.1073/pnas.0508778102.PubMed CentralPubMedGoogle Scholar
- Hasona A, Zuobi-Hasona K, Crowley PJ, Abranches J, Ruelf MA, Bleiweis AS, Brady LJ: Membrane composition changes and physiological adaptation by Streptococcus mutans signal recognition particle pathway mutants. J Bacteriol. 2007, 189: 1219-1230. 10.1128/JB.01146-06.PubMed CentralPubMedGoogle Scholar
- Karp PD, Paley SM, Krummenacker M, Latendresse M, Dale JM, Lee TJ, Kaipa P, Gilham F, Spaulding A, Popescu L, Altman T, Paulsen I, Keseler IM, Caspi R: Pathway Tools version 13.0: integrated software for pathway/genome informatics and systems biology. Brief Bioinform. 2010, 11: 40-79. 10.1093/bib/bbp043.PubMed CentralPubMedGoogle Scholar
- Ideker T, Krogan NJ: Differential network biology. Mol Syst Biol. 2012, 8: 565-PubMed CentralPubMedGoogle Scholar
- Valcárcel B, Würtz P, al Seich Basatena N, Tukiainen T, Kangas AJ, Soininen P, Järvelin M, Ala-Korpela M, Ebbels TM, de Iorio M: A differential network approach to exploring differences between biological states: an application to prediabetes. PLoS One. 2011, 6: e24702-10.1371/journal.pone.0024702.PubMed CentralPubMedGoogle Scholar
- Sierro N, Makita Y, de Hoon M, Nakai K: DBTBS: a database of transcriptional regulation in Bacillus subtilis containing upstream intergenic conservation information. Nucleic Acids Res. 2008, 36: D93-96. 10.1093/nar/gkn421.PubMed CentralPubMedGoogle Scholar
- Li L, Stoeckert CJ, Roos DS: OrthoMCL: identification of ortholog groups for eukaryotic genomes. Genome Res. 2003, 13: 2178-2189. 10.1101/gr.1224503.PubMed CentralPubMedGoogle Scholar
- Thomas-Chollier M, Sand O, Turatsinze J, Janky R, Defrance M, Vervisch E, Brohée S, van Helden J: RSAT: regulatory sequence analysis tools. Nucleic Acids Res. 2008, 36: W119-27. 10.1093/nar/gkn304.PubMed CentralPubMedGoogle Scholar
- Turatsinze J, Thomas-Chollier M, Defrance M, van Helden J: Using RSAT to scan genome sequences for transcription factor binding sites and cis-regulatory modules. Nat Protoc. 2008, 3: 1578-1588. 10.1038/nprot.2008.97.PubMedGoogle Scholar
- Gillespie JJ, Wattam AR, Cammer SA, Gabbard JL, Shukla MP, Dalay O, Driscoll T, Hix D, Mane SP, Mao C, Nordberg EK, Scott M, Schulman JR, Snyder EE, Sullivan DE, Wang C, Warren A, Williams KP, Xue T, Yoo HS, Zhang C, Zhang Y, Will R, Kenyon RW, Sobral BW: PATRIC: the comprehensive bacterial bioinformatics resource with a focus on human pathogenic species. Infect Immun. 2011, 79: 4286-4298. 10.1128/IAI.00207-11.PubMed CentralPubMedGoogle Scholar
- Smoot ME, Ono K, Ruscheinski J, Wang P, Ideker T: Cytoscape 2.8: new features for data integration and network visualization. Bioinformatics. 2011, 27: 431-432. 10.1093/bioinformatics/btq675.PubMed CentralPubMedGoogle Scholar
- Kashtan N, Itzkovitz S, Milo R, Alon U: Efficient sampling algorithm for estimating subgraph concentrations and detecting network motifs. Bioinformatics. 2004, 20: 1746-1758. 10.1093/bioinformatics/bth163.PubMedGoogle Scholar
- Heckmann KL, Pease LR: Gene splicing and mutagenesis by PCR-driven overlap extension. Nat Protoc. 2007, 2: 924-932. 10.1038/nprot.2007.132.Google Scholar
- Li YH, Lau PC, Lee JH, Ellen RP, Cvitkovitch DG: Natural genetic transformation of Streptococcus mutans growing in biofilms. J Bacteriol. 2001, 183: 897-908. 10.1128/JB.183.3.897-908.2001.PubMed CentralPubMedGoogle Scholar
- Dunny GM, Lee LN, LeBlanc DJ: Improved electroporation and cloning vector system for gram-positive bacteria. Appl Environ Microbiol. 1991, 57: 1194-1201.PubMed CentralPubMedGoogle Scholar
- Lemme A, Gröbe L, Reck M, Tomasch J, Wagner-Döbler I: Subpopulation-specific transcriptome analysis of competence-stimulating-peptide-induced Streptococcus mutans. J Bacteriol. 2011, 193: 1863-1877. 10.1128/JB.01363-10.PubMed CentralPubMedGoogle Scholar
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