Community acquired-methicillin resistant Staphylococcus aureus (CA-MRSA) is a socially problematic pathogen that infects healthy individuals, causing severe disease. CA-MRSA is more virulent than hospital associated-MRSA (HA-MRSA). The underlying mechanism for the high virulence of CA-MRSA is not known. The transcription product of the psm-mec gene, located in the mobile genetic element SCCmec of HA-MRSA, but not CA-MRSA, suppresses the expression of phenol-soluble modulin α (PSMα), a cytolytic toxin of S. aureus. Here we report that psm-mec RNA inhibits translation of the agrA gene encoding a positive transcription factor for the PSMα gene via specific binding to agrA mRNA. Furthermore, 25% of 325 clinical MRSA isolates had a mutation in the psm-mec promoter that attenuated transcription, and 9% of the strains had no psm-mec. In most of these psm-mec-mutated or psm-mec-deleted HA-MRSAs, PSMα expression was increased compared with strains carrying intact psm-mec, and some mutated strains produced high amounts of PSMα comparable with that of CA-MRSA. Deletion of psm-mec from HA-MRSA strains carrying intact psm-mec increased the expression of AgrA protein and PSMα, and virulence in mice. Thus, psm-mec RNA suppresses MRSA virulence via inhibition of agrA translation and the absence of psm-mec function in CA-MRSA causes its high virulence property.
Methicillin-resistant Staphylococcus aureus (MRSA) is resistant to various antibiotics, including β-lactams, thus causing serious clinical problems. Hospital-associated (HA)-MRSA infects immunocompromised patients in hospitals. Community-acquired (CA)-MRSA causes serious diseases in healthy people who have not had contact with hospitals in the United States, Canada, or Europe. CA-MRSA produces higher amounts of extracellular toxins and has higher virulence than HA-MRSA, although the reason for this is unclear. SCCmec is a foreign DNA integrated into the MRSA chromosome that contains several genes including the mecA gene that confers resistance against methicillin. The SCCmec of CA-MRSA does not contain the psm-mec gene that exists in the HA-MRSA SCCmec. In the present study, we found that the transcription product of psm-mec inhibits translation of the agrA gene encoding a positive transcription factor for many extracellular toxins by direct binding to the agrA mRNA, resulting in decreased extracellular toxin production. Furthermore, some HA-MRSA strains carry mutated psm-mec or no psm-mec and produce higher amounts of extracellular toxins than HA-MRSA strains carrying intact psm-mec. These findings suggest that psm-mec RNA negatively regulates agrA and mutation or absence of psm-mec leads to a high virulence capacity of MRSA.
Citation: Kaito C, Saito Y, Ikuo M, Omae Y, Mao H, Nagano G, et al. (2013) Mobile Genetic Element SCCmec-encoded psm-mec RNA Suppresses Translation of agrA and Attenuates MRSA Virulence. PLoS Pathog 9(4): e1003269. doi:10.1371/journal.ppat.1003269
Editor: Andreas Peschel, University of Tubingen, Germany
Received: September 14, 2012; Accepted: February 8, 2013; Published: April 4, 2013
Copyright: © 2013 Kaito et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This study was supported by Grants-in-Aid for Scientific Research (23249009, 24590519). This study was supported in part by the Naito Foundation, the Program for Promotion of Fundamental Studies in Health Sciences of the National Institute of Biomedical Innovation (NIBIO), and the Genome Pharmaceutical Institute. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: We have received part of our funding from Genome Pharmaceutical Institute and have an agreement with them on taking patents. However, this does not alter our adherence to all PLoS Pathogens policies on sharing data and materials.
CA-MRSA, especially the USA300 clone, causes severe infectious diseases in many people in the United States and in European countries. CA-MRSA is generally considered more virulent than most HA-MRSA . Determining the molecular mechanism underlying the high virulence of CA-MRSA will be important toward establishing new therapeutic strategies against CA-MRSA infections. One reason for the high virulence of the CA-MRSA USA300 strains is suggested to be the high amounts of secreted toxins, including PSMα, α-hemolysin, δ-hemolysin (Hld), and the Panton-Valentine leukocidin (PVL) , , . The USA300 strains show increased expression of the agr locus, which upregulates the production of PSMα, α-hemolysin, and PVL, compared with HA-MRSA strains , , , . The agr locus is essential for the virulence of the USA300 strains against animals , . The agr locus encodes agrBDCA, which functions in quorum sensing . An extracellular quorum-sensing molecule made from AgrD activates the sensor protein AgrC. AgrC activates the transcription factor AgrA by phosphorylation. AgrA activates the transcription of agrBDCA, including agrA itself . Thus, quorum sensing is under positive feedback regulation. The agr locus also encodes RNAIII, which is an mRNA of Hld as well as a regulatory RNA that upregulates the expression of various toxins, including α-hemolysin, and downregulates the expression of various cell surface proteins . AgrA activates the transcription of RNAIII and other virulence genes, including the psmα operon, by direct binding to the promoter , . The mechanism that increases the expression of agr in the USA300 strains, however, is not known.
SCCmec is a mobile genetic element that confers methicillin resistance to MRSA strains. The structure of the SCCmec region differs between the CA-MRSA and HA-MRSA strains . We previously reported that the psm-mec gene that exists in type-II and type-III SCCmec, which is found in most HA-MRSA, regulates the virulence of S. aureus . The psm-mec gene is absent in type-IV SCCmec of the CA-MRSA USA300 strains . Introduction of psm-mec into FRP3757, a CA-MRSA USA300 strain, or Newman, a methicillin-sensitive S. aureus strain that carries neither SCCmec nor psm-mec, decreases the secreted amount of PSMα, suppresses colony-spreading ability, and promotes biofilm formation , . Furthermore, the psm-mec-transformed strains attenuate virulence in a mouse model of systemic infection , . The finding first revealed that a factor encoded by a mobile-genetic element negatively regulates bacterial virulence. Because the USA300 strains have no psm-mec, we proposed that the absence of psm-mec is a genetic determinant of the high virulence of USA300 . Suppression of colony-spreading and promotion of biofilm formation by the psm-mec gene are attributed to both the transcription product and the translation product of psm-mec . In contrast, suppression of the expression of PSMα is attributed to the transcription product of psm-mec, i.e., psm-mec RNA . An mRNA encoding protein rarely acts as a regulatory RNA. Such bifunctional RNA, other than psm-mec RNA, is found as S. aureus RNAIII  and Escherichia coli SgrS , and is important material for investigations of gene evolution. In this study, to clarify the molecular mechanisms underlying the inhibitory effect of psm-mec RNA on PSMα expression, we screened and identified a target molecule of psm-mec RNA. Additionally, we performed an epidemiologic study and a deletion analysis of psm-mec to verify whether psm-mec mutation confers a high virulence property to MRSA strains.
Results and Discussion
psm-mec RNA inhibits agrA translation
First, to identify the target molecule of psm-mec RNA, we compared the protein expression patterns of the CA-MRSA FRP3757 strain (USA300) and its transformant with psm-mec by two-dimensional gel electrophoresis. In the psm-mec (pF)-transformed FRP3757, the expression of HutU, protein A, and Ddh were increased (Fig. 1, Table S1). The increases in the amounts of the proteins were not diminished by the introduction of a stop-codon into the third codon of psm-mec open reading frame (ORF), but they were diminished by the introduction of synonymous codons into the psm-mec ORF, which altered the RNA nucleotide sequence but not the amino acid sequence (Fig. 1). The mutated psm-mec containing a stop-codon (pC1) expresses psm-mec RNA without the expression of PSM-mec protein . The mutated psm-mec harboring synonymous codon substitutions (pFP) expresses PSM-mec protein . Thus, we concluded that psm-mec RNA increased the expression of these proteins. Previous reports indicated that these three proteins are downregulated by the agr locus , , . We previously found that psmα promoter activity, which is enhanced by AgrA, was decreased in the Newman strain transformed with psm-mec, resulting in a decreased amount of PSMα, but no alteration of the amount of agrA mRNA . Based on these findings, we hypothesized that the introduction of psm-mec leads to the inhibition of the translation of agrA and decreases the amount of AgrA in the cells. To examine this possibility, we first established a method to determine the amount of AgrA protein in cells. Anti-AgrA immunoglobulin (IgG) was prepared from a rabbit immunized with His-tagged recombinant AgrA and Western blot analysis was performed. In cell extracts of the Newman strain, the 28-kDa band of AgrA was detected, which was consistent with the predicted molecular mass of AgrA, 27.9 kDa (Fig. 2A). In contrast, the band was not detected in cell extracts of the agr-null mutant (Fig. 2A). In addition, the band was not detected using IgG from a non-immunized rabbit (data not shown). Therefore, we concluded that the 28-kDa protein detected by anti-AgrA IgG was the AgrA protein. We then performed Western blot analysis of AgrA in psm-mec-transformed Newman strain. In the psm-mec (pF)-transformed Newman strain, the AgrA band intensity was decreased compared with the vector (pND50)-transformed Newman strain (Fig. 2B). Decreased intensity of the AgrA band was also observed in Newman transformed with psm-mec containing a stop-codon (pC1) (Fig. 2B), which expresses psm-mec RNA without the expression of PSM-mec protein . In contrast, the psm-mec gene, which has a -7T>C mutation in the promoter (pM1) and does not express psm-mec RNA , did not decrease the AgrA band intensity (Fig. 2B). These findings suggest that the transcription product of psm-mec acts to decrease the amount of AgrA in S. aureus cells. Furthermore, we examined whether psm-mec RNA also decreases the amount of AgrA in the CA-MRSA strains MW2 (USA400) and FRP3757 (USA300). In both CA-MRSA strains, the introduction of a plasmid carrying psm-mec (pF) led to a decrease in the amount of AgrA (Fig. 2C). We further analyzed whether a single copy of psm-mec is enough to decrease the amount of AgrA in respective S. aureus strains. We previously reported the construction of a Newman strain integrated with psm-mec into the chromosomal DNA . In this study, we constructed MW2 and FRP3757 strains into which psm-mec was integrated into the chromosomal regions near the mecA of SCCmec, where psm-mec is originally present in HA-MRSA strains (Fig. S1). In these three strains, integration of psm-mec into the chromosome decreased the amount of AgrA in the cells (Fig. 2C). These findings indicate that introduction of psm-mec into CA-MRSA strains decreases the amount of AgrA and that a single copy psm-mec is enough to exert the repression effect.
(A) The nucleotide sequence of the psm-mec ORF in pF, the stop-codon introduced sequence of psm-mec ORF in pC1, and the synonymous-codon substituted sequence of psm-mec ORF in pFP are shown. The substituted nucleotides are colored in red. The amino acid sequence of PSM-mec protein is shown below the respective nucleotide sequence. (B) Cell extract of FRP3757 strain that was transformed with empty vector (pND50), psm-mec (pF), mutated psm-mec harboring a stop codon (pC1), or mutated psm-mec harboring synonymous codon substitutions (pFP) was analyzed by two-dimensional electrophoresis. Proteins were stained with Coomassie Brilliant Blue. The protein spot was excised and identified by matrix-assisted laser desorption ionization time-of-flight mass spectrometry (Table S1).
(A) Cell extracts of overnight cultures of Newman strain (WT) and the agr-null mutant (Δagr) were electrophoresed in sodium dodecyl sulfate-polyacrylamide gels. One gel was stained with Coomassie Brilliant Blue (Left panel). Proteins in another gel were transferred to a membrane and used for Western blotting by anti-AgrA IgG (Right panel). (B) Cell extracts of 24 h-cultures of Newman strains transformed with empty vector (pND50), a plasmid carrying wild-type psm-mec (pF), a plasmid carrying psm-mec with a stop-codon (pC1), and a plasmid carrying psm-mec with the -7T>C promoter mutation (pM1) were subjected to Western blotting by anti-AgrA IgG. Each lane contains 3.5 µg proteins of cell extracts. (C) Cell extracts of 24 h-cultures of Newman, MW2 (USA400), and FRP3757 (USA300) strains that were transformed with pF carrying psm-mec (multi-copy), or integrated with psm-mec into the chromosome (single-copy) were subjected to Western blotting by anti-AgrA IgG (Upper panel). Each lane contains 3 µg proteins of cell extracts. Band intensities of AgrA were measured and are presented in the lower graph. The vertical axis represents the relative value against the AgrA band intensity of the parent strain in each Newman, MW2, and FRP3757 genetic background. Means ± standard deviations from four independent experiments are presented. Student t-test P-values between the parent strain and the psm-mec-introduced strain in each genetic background are presented. (D) The agr null mutant of Newman transformed with pMNS-agrBDCA carrying IPTG-inducible agrBDCA and pKE516 (empty vector), or pMNS-agrBDCA and pKE516-F carrying wild-type psm-mec was cultured in the presence or absence of IPTG. Cell extracts of 24-h cultures were subjected to Western blotting by anti-AgrA IgG. Each lane contains 6 µg proteins of cell extracts. (E) Schematic representation of luc-fusions of the recF promoter, agrA SD, the agrA ORF, and the luc ORF. Bold gray lines represent the plasmid construct. Horizontal dotted lines represent the regions deleted from the plasmids. Putative binding region means the region predicted to bind to the psm-mec RNA by in silico analysis. SD means Shine-Dalgarno sequence of agrA. (F) Luciferase activities of Newman strains that were transformed with the luc-fusion plasmids with psm-mec (+F) or without psm-mec (−F) were measured. The vertical axis represents the luciferase activity. Student t-test P-values between +F and −F are presented. NS, P>0.05. (G) Newman strain, which was integrated with psm-mec or without psm-mec, was transformed with the luc-fusion plasmids. Luciferase activities of the strains were measured. The vertical axis represents the relative luciferase activity of the psm-mec-integrated Newman [+F (single-copy)] against that of the Newman strain (−F). Student t-test P-values between +F and −F are presented. NS, P>0.05.
Next, we examined whether psm-mec represses the translation of agrA. AgrA functions in a positive feedback loop to activate the transcription of agrBDCA, including agrA itself. To exclude the effect on the transcription initiation of agrBDCA from its native promoter, we transformed the agr-null mutant of Newman with pMNS-agrBDCA, which expresses agrBDCA from an IPTG-inducible promoter. The amount of AgrA was increased by increasing the IPTG concentration in the strain transformed with pMNS-agrBDCA and empty vector (pKE516), whereas the introduction of a plasmid carrying psm-mec (pKE516-F) into the strain transformed with pMNS-agrBDCA diminished AgrA expression in the presence of IPTG (Fig. 2D). Thus, psm-mec inhibits AgrA expression without the transcriptional regulation of the agrBDCA promoter. To examine the effect of psm-mec on the agrA coding region, we constructed a reporter gene-fusion construct in which the Shine-Dalgarno sequence of agrA and agrA ORF was fused in frame with luc under the control of the recF promoter (Fig. 2E). The introduction of psm-mec did not decrease the luciferase activity of luc-fusion with the −20–+27 sequence of agrA (pGP-luc), although it decreased the luciferase activity of luc-fusion with the −20–+717 sequence of agrA (pGP-agrA-luc) (Fig. 2F). Decreased luciferase activity of pGP-agrA-luc was also observed in Newman integrated with a single copy of psm-mec (Fig. 2G). These findings indicate that psm-mec inhibits the translation of agrA.
psm-mec RNA specifically binds agrA mRNA
We next searched for mRNA interacting with psm-mec RNA using the in silico programs sRNATarget  and RNAhybrid , and identified agrA mRNA as a candidate (Fig. 3A). We hypothesized that the inhibition of agrA translation by psm-mec is caused by the direct binding of psm-mec RNA to agrA mRNA. Primer extension  and nuclease S1 protection analyses (Fig. S2) revealed that the size of psm-mec RNA was 157 bases. To examine the direct binding of psm-mec RNA to agrA mRNA, we performed a gel shift analysis using 157 bases of psm-mec RNA that was synthesized by in vitro transcription. The addition of the −20–+717 sequence of agrA mRNA retarded the mobility of the radiolabeled psm-mec RNA fragment in a dose-dependent manner (Fig. 3B). The retardation was cancelled by the addition of nonlabeled psm-mec RNA, although not by the addition of a 1000-fold amount of yeast tRNA (Fig. 3B). Thus, the binding of psm-mec RNA to agrA mRNA detected by gel shift assay was specific. Furthermore, to identify the region of agrA mRNA required for binding to psm-mec RNA, we examined whether the −20–+267 sequence of agrA mRNA (agrA1), which contains the binding regions predicted by in silico analysis; the +74-+267 sequence of agrA, and the −20–+198 sequence of agrA mRNA (agrA2), which partially disrupts the predicted binding region, bind psm-mec RNA. This finding demonstrated that agrA1 RNA binds psm-mec RNA, although agrA2 RNA does not bind psm-mec RNA (Fig. 3C). Thus, the +199-+267 sequence of agrA mRNA is required for binding to psm-mec RNA. To determine whether the binding of psm-mec RNA to agrA mRNA is required for the inhibition of agrA translation, we performed a reporter gene-fusion analysis with and without the +199-+267 region of agrA. We compared the luciferase activity of luc-fusions with agrA1 that can bind psm-mec RNA (pGP-agrA1-luc) and agrA2 that cannot bind psm-mec RNA (pGP-agrA2-luc) (Fig. 2E). The expression of agrA1-luc was suppressed by psm-mec in a similar manner as agrA-luc, although the expression of agrA2-luc was not suppressed by psm-mec (Fig. 2F). These findings suggest that the binding of psm-mec RNA to agrA mRNA leads to the inhibition of agrA translation.
(A) Hybridization between psm-mec RNA and agrA mRNA was predicted by an in silico program RNA hybrid. Black and gray lines represent strong and weak hydrogen bonds, respectively. (B) Binding between psm-mec RNA and agrA RNA (−20–717) was analyzed using a gel-retardation assay. Various amounts of nonlabeled agrA RNA were added to 32P-labeled psm-mec RNA (0.13 pmol), and electrophoresed in 6% native polyacrylamide gel. In the right six lanes, nonlabeled psm-mec RNA or yeast tRNA was added to compete with the binding between agrA RNA and 32P-labeled psm-mec RNA. (C) Binding experiment between psm-mec RNA and deletion mutants of agrA RNA. Various amounts of nonlabeled agrA1 RNA (−20–267) or agrA2 RNA (−20–198) were added to 32P-labeled psm-mec RNA (0.13 pmol). (D) Nucleotide sequences of psm-mec RNA, a deletion mutant of psm-mec RNA (psm-mec-D), and a nucleotide-substituted psm-mec RNA (psm-mec-M) are presented. Red dotted line in psm-mec-D indicates the deleted region. Red letters in psm-mec-M indicate the substituted nucleotides that are not complementary to agrA RNA. (E) Various amounts of nonlabeled psm-mec RNA, psm-mec-D RNA, or psm-mec-M RNA were added to 32P-labeled agrA1 RNA (−20–267), and electrophoresed in 6% native polyacrylamide gel. (F) Luciferase activities of Newman strains that were transformed with pGP-agrA-luc carrying no psm-mec (−F), psm-mec (+F), psm-mec-D, or psm-mec-M were measured. The vertical axis represents the relative luciferase activity against that of pGP-agrA-luc carrying no psm-mec. Means ± standard deviations from three independent experiments are presented. Student t-test P-values are presented. (G) Cell extracts (3 µg protein) of 24 h-cultures of Newman strains transformed with pND50 (empty vector), pF carrying psm-mec, p-psm-mec-D carrying psm-mec-D, or p-psm-mec-M carrying psm-mec-M were subjected to Western blotting by anti-AgrA IgG (Left panel). Band intensities of AgrA were measured (Right graph). Means ± standard deviations from three independent experiments are presented. Student t-test P-values are presented. (H) Amounts of PSMα3 in the supernatants of 24 h-cultures of Newman strains transformed with psm-mec, psm-mec-D, or psm-mec-M were measured. The vertical axis represents the relative amount of PSMα3 against that of Newman strain transformed with pND50 (empty vector). Student t-test P-values are presented.
To identify the region of psm-mec RNA that is required for binding agrA mRNA, we constructed a psm-mec-D disrupting 22–52 sequence that is a partial region of the in silico predicted binding region and a psm-mec-M carrying a mutated 21–39 sequence, which are not complementary to agrA mRNA (Fig. 3D). Wild-type psm-mec RNA retarded the migration of agrA1 RNA, whereas these mutated psm-mec RNA did not retard the migration of agrA1 RNA (Fig. 3E). Thus, the 21–52 sequence of psm-mec RNA is required for binding to agrA mRNA. To verify whether binding of psm-mec RNA to agrA mRNA is required to repress the translation of agrA and inhibit PSMα3 expression by psm-mec, we examined the effect of psm-mec-D and psm-mec-M on the activity of agrA-luc fusion, the amount of AgrA, and the expression of PSMα3. The luciferase activity of agrA-luc fusion was partially restored in the presence of psm-mec-D or psm-mec-M compared with wild-type psm-mec (Fig. 3F). The amount of AgrA was partially relieved in Newman transformed with psm-mec-D or psm-mec-M compared with that in Newman transformed with wild-type psm-mec (pF), which inhibited the expression of AgrA (Fig. 3G). The expression of PSMα3 was repressed by wild-type psm-mec, whereas the repression effect was attenuated in psm-mec-D or psm-mec-M (Fig. 3H). Therefore, binding of psm-mec RNA to agrA mRNA is required to repress the translation of agrA and to inhibit PSMα3 expression by psm-mec.
Translational inhibition of agrA by psm-mec might be due to the destabilization of agrA mRNA by psm-mec. We examined the stability of agrA mRNA in the presence or absence of psm-mec. In the vector (pND50)-transformed Newman strain, the half-life of agrA mRNA was 11 min, whereas in the psm-mec (pF)-transformed Newman strain, the half-life of agrA mRNA was 5 min (Fig. 4A). Thus, psm-mec slightly decreased the stability of agrA mRNA. RNase III is an endoribonuclease that catalyzes double-stranded RNA and contributes to repress gene expression by the regulatory RNA, RNAIII , , . We examined whether RNase III encoded by the rnc gene contributes to the alteration of the half-life of agrA mRNA by psm-mec. In the rnc-deleted mutant, introduction of psm-mec (pF) did not decrease the half-life of agrA mRNA compared with introduction of the vector (pND50) (Fig. 4B). Therefore, RNase III is required for the destabilization of agrA mRNA by psm-mec. We then examined the inhibitory effect of psm-mec on the translation of agrA under the rnc-deletion background, in which psm-mec did not decrease the stability of agrA mRNA. In the rnc-deleted mutant, introduction of psm-mec (pF) decreased the amount of AgrA (Fig. 4C). These results suggest that psm-mec represses the translation of agrA independently of the decrease in stability of agrA mRNA, although psm-mec acts to decrease the stability of agrA mRNA via RNase III. Next, we examined whether the stability of psm-mec RNA was affected by agrA. psm-mec RNA was expressed from an anhydrotetracycline-inducible promoter, because psm-mec transcription is positively regulated by AgrA . There was no difference in the half-life of psm-mec RNA between Newman strain and the agr-null mutant and the half-life was approximately 20 min (Fig. 4D). In this condition, psm-mec RNA slightly decreased the stability of agrA mRNA, which is consistent with the finding using psm-mec expressed from the native promoter (Fig. 4E). These results suggest that psm-mec RNA is stable and the stability is not affected by agrA mRNA.
(A) Northern blot analysis was performed to measure agrA mRNA stability in Newman strain transformed with an empty vector (pND50) or pF carrying psm-mec. Total RNA was extracted from cultures (A600 = 3) at the indicated time point after rifampicin treatment. agrA mRNA (RNAII) was detected by32P-labeled DNA probe. rRNA was stained with ethidium bromide. The amounts of agrA mRNA were normalized with the amount of 16S rRNA at each time-point and the amounts of agrA mRNA relative to the amount at 0 min are shown in graph. The half-life at which 50% of agrA mRNA remained was determined by exponential approximation. Data are representative from three independent experiments. (B) agrA mRNA stability was measured in the rnc-deleted mutant transformed with pND50 or pF. Total RNA was extracted from cultures (A600 = 3) at the indicated time point after rifampicin treatment. Data presentation and the calculation of the RNA half-life are the same as in (A). Data are representative from three independent experiments. (C) Cell extracts (4.2 µg protein) of 24-h cultures of Newman strains transformed with pND50 or pF and the rnc-deleted mutant transformed with pND50 or pF were subjected to Western blotting by anti-AgrA IgG (Left panel). Band intensities of AgrA were measured (Right graph). Means ± standard deviations from two independent experiments are presented. Student t-test P-values are presented. (D) psm-mec RNA stability was measured in Newman and the agr-null mutant, which were transformed with anhydrotetracycline-inducible psm-mec (pNDX1-F). S. aureus cells were grown to A600 = 2 in the presence of 0.4 µg/ml of anhydrotetracycline. Total RNA was extracted after rifampicin treatment and electrophoresed. Data presentation and the calculation of the RNA half-life are the same as in (A). Data are representative from two independent experiments. (E) agrA mRNA stability was measured in Newman transformed with empty vector (pNDX1) or anhydrotetracycline-inducible psm-mec (pNDX1-F). S. aureus cells were grown to A600 = 2 in the presence of 0.4 µg/ml of anhydrotetracycline. Total RNA was extracted after rifampicin treatment and electrophoresed. Data presentation and the calculation of the RNA half-life are the same as in (A). Data are representative from two independent experiments.
Mutation or absence of psm-mec correlates with high expression of extracellular PSMα in MRSA clinical isolates
Because psm-mec inhibits agrA translation, resulting in the repression of PSMα3 expression, we hypothesized that the psm-mec mutation was related to the high expression levels of PSMα3 in clinical MRSA isolates. We collected 325 clinical MRSA strains from three hospitals in the Kanto area in Japan, and sequenced their psm-mec genes. Eighty-one strains (25%) carried the -7T>C mutation in the psm-mec promoter and one strain carried an insertion of 2.2 kbp and the -4G>A mutation in the psm-mec promoter, both of which repressed the expression of psm-mec in the Newman strain (Table 1). Twenty-eight strains (9%) did not carry psm-mec (Table 1). As we reported previously , -7T>C-mutated psm-mec lacked the ability to inhibit PSMα3 expression and colony spreading, and to promote biofilm formation in the Newman strain (Fig. S3). The psm-mec carrying an insertion of 2.2 kbp and the -4G>A mutation also lacked these abilities (Fig. S3). In contrast, in other psm-mec mutations, such as D2, D4, and D5, which did not decrease the expression of psm-mec, the inhibitory abilities of PSMα3 expression and colony spreading, and the promotion of biofilm formation in the Newman strain were maintained (Fig. S3). We next examined whether 81 strains carrying -7T>C psm-mec and 28 strains without psm-mec had higher amounts of PSMα3 than the other 193 strains carrying intact psm-mec. The amount of PSMα3 in the culture supernatant of each strain was determined by high performance liquid chromatography analysis. The findings revealed that these strains carrying mutations in psm-mec expressed higher amounts of PSMα3 in the culture supernatant than the strains carrying intact psm-mec (Fig. 5). Some strains carrying the mutations produced higher amounts of PSMα3 than the CA-MRSA FRP3757 strain (USA300) (Fig. 5). These findings suggest that the psm-mec mutations increase the amount of PSMα3 in HA-MRSA isolates, and that there are some strains in the psm-mec-mutated isolates that produce even higher amounts of PSMα3 than produced by CA-MRSA.
Nucleotide sequences of psm-mec genes of 325 MRSA isolates were determined (Table 1). MRSA strains harboring intact psm-mec (Intact), -7T>C-mutated psm-mec (-7T>C), or no psm-mec (Absence) were cultured for 15 h. The amounts of PSMα3 in the culture supernatants were measured. The vertical axis represents the relative amount of PSMα3 against that of Newman strain. Closed circles represent the amounts of PSMα3 of each MRSA strains, which are the means from two independent experiments. Magenta lines represent the averaged amount of PSMα3 of each MRSA groups. Cyan dotted line represents the amount of PSMα3 of CA-MRSA strain FRP3757 (USA300). Student t-test P-values are presented. ND, not detected.
To investigate whether the genetic backgrounds of the clinical isolates carrying -7T>C psm-mec or no psm-mec differ from those carrying intact psm-mec, we determined the SCCmec types and spa types of all tested strains. One hundred and twenty-seven strains (65%) of the isolates carrying intact psm-mec had type II SCCmec (Table 2). Seventy-five of 81 strains (93%) carrying -7T>C psm-mec had type II SCCmec (Table 2). The results of SCCmec typing were in high agreement with the previously reported data that psm-mec is closely related to the class A mec gene complex carried by either types II, III, or VIII of the SCCmec element , , . Most of the strains carrying intact psm-mec or -7T>C psm-mec had type 2 spa: 122 (63%) of the isolates carrying intact psm-mec; 69 (85%) of the isolates carrying -7T>C psm-mec (Table 3). In contrast, all isolates not carrying psm-mec also did not carry class A mec and the majority of them carried either type I or IV SCCmec elements (Table 2). Sixteen strains (55%) of the isolates not carrying psm-mec had type 855 spa and three strains (10%) had type 2 spa (Table 3). These results indicate that most isolates carrying -7T>C psm-mec and intact psm-mec have closely related genetic backgrounds, whereas most isolates not carrying psm-mec have different genetic backgrounds compared to isolates carrying intact or -7T>C psm-mec. In addition, there are various spa types in the isolates carrying -7T>C psm-mec or no psm-mec, indicating that the isolates carrying the psm-mec mutation are polyclonal.
psm-mec is required for suppression of the virulence in MRSA clinical isolates
In our previous study, we transformed S. aureus strains carrying no psm-mec with psm-mec and investigated the function of psm-mec. Use of this method to evaluate gain of function cannot, however, establish the requirement of psm-mec to suppress HA-MRSA virulence. From 193 HA-MRSA strains carrying intact psm-mec, we selected 18 strains that produce the PSM-mec protein and are susceptible to antibiotics, from which psm-mec can be deleted by the antibiotics resistance gene. The psm-mec-deleted mutants of these 18 strains were constructed (Fig. S4), and were examined whether their PSMα production, AgrA expression, and colony spreading ability were increased, or biofilm formation was decreased. In 13 of 18 strains, each psm-mec-deleted mutant produced more PSMα3 than the respective parent strain (Fig. 6A). In 14 of 18 strains, each psm-mec-deleted mutant produced more PSMα1 and Hld than the respective parent strain (Fig. 6B). In 14 of 18 strains, each psm-mec-deleted mutant expressed more AgrA than the respective parent strain (Fig. 6C). In 15 of 18 strains, each psm-mec-deleted mutant had a greater colony spreading capacity than the respective parent strain (Fig. 6D). In contrast, in 8 of 18 strains, each psm-mec-deleted mutant formed less biofilm than the respective parent strain (Fig. 6E). Therefore, in most HA-MRSA strains, psm-mec is required for the suppression of PSMα production, AgrA expression, and colony spreading, as well as the promotion of biofilm formation.
(A, B) The amounts of PSMα3 (A) and Hld + PSMα1 (B) of 18 MRSA isolates and its psm-mec-deleted mutants were measured. White bar represents the clinical isolate used as the parent strain. Black bar represents the psm-mec-deleted mutant of the clinical isolate. The vertical axis represents the amount of PSMαs in arbitrary units based on A215. Means ± standard deviations from three independent experiments are shown. Student t-test P-values between the parent strain and the psm-mec-deleted mutant are presented. NS, P>0.05. (C) Cell extracts (3.7 µg protein) of 15 h-cultures of clinical MRSA isolates and the psm-mec-deleted mutants were subjected to Western blotting by anti-AgrA IgG (Upper panel). Band intensities of AgrA were measured and are presented as relative values against that of the parent strain (Lower graph). Means ± standard deviations from three independent experiments are presented. Student t-test P-values between the parent strain and the psm-mec-deleted mutant are presented. NS, P>0.05. (D) Colony spreading abilities of clinical MRSA isolates and the psm-mec-deleted mutants were evaluated. Overnight cultures were spotted onto soft agar plates and incubated for 24 h at 37°C. The vertical axis represents diameters of giant colonies. Means ± standard deviations from three independent experiments are shown. Student t-test P-values between parent strain and the psm-mec-deleted mutant are presented. NS, P>0.05. (E) Biofilm formation of clinical MRSA isolates and psm-mec-deleted mutants were evaluated. Bacterial strains were grown on polystyrene plates for 3 days and the biofilm amounts were measured. White bar represents the clinical isolate used as the parent strain. Black bar represents the psm-mec-deleted mutant of the clinical isolate. Means ± standard deviations from four independent experiments are shown. NS, P>0.05.
To further verify whether psm-mec is needed to suppress HA-MRSA virulence in animals, we examined the virulence of the psm-mec-deleted mutants of NI-13, SR-1, and NIR-34, which produced higher amounts of PSMα3 than their respective parent strain, using mouse models of skin infection and systemic infection. In the skin infection model, bacterial virulence was quantitatively evaluated by measuring the dermonecrosis area formed by the S. aureus injection . The psm-mec-deleted mutants of NI-13, SR-1, and NIR-34 formed a larger area of dermonecrosis than the respective parent strain (Fig. 7A). In the mouse systemic infection model, the psm-mec-deleted mutants of NI-13 and NIR-34 killed mice faster than the respective parent strain (Fig. 7B), although the psm-mec-deleted mutant of SR-1 killed mice in the same manner as the parent strain (data not shown). These results suggest that psm-mec suppresses the virulence of these HA-MRSA strains against animals.
(A) Mouse skin infection experiments using NI-13, SR-1, NIR-34, and the respective psm-mec-deleted mutants were performed. Mice (HR-1, n = 5) were subcutaneously injected with S. aureus cells and the dermonecrosis area was measured. Means ± standard deviations from the dermonecrosis areas of five mice are shown. Injected CFUs were as follows; NI-13 and its psm-mec-deleted mutant, 4×107 CFU; SR-1 and its psm-mec-deleted mutant, 8×106 CFU; NIR-34 and its psm-mec-deleted mutant, 2×107 CFU. Black stars indicate that Student's t-test P-values between the parent strain and the psm-mec-deleted mutant were less than 0.05. Upper right panel is a representative image of a mouse injected with NI-13 and the psm-mec-deleted mutant at 143 h after bacteria injection. (B) Mouse systemic infection experiments were performed. ICR mice (n = 10) were intravenously injected with S. aureus cells. Injected CFUs were as follows; NI-13 and its psm-mec-deleted mutant, 4×108 CFU; NIR-34 and its psm-mec-deleted mutant, 4×108 CFU. Log-rank test P-values between the parent strain and the psm-mec-deleted mutant in NI-13 and SR-1 are 0.0005 and <0.0001, respectively.
It was recently revealed that psm-mec is located between two regulatory loci, mecI and mecR2, which are transcribed in the opposite direction of psm-mec and regulate the expression of mecA . Expression of mecA encoding penicillin binding protein 2a interferes with the agr system, reduces toxin expression, and attenuates virulence in mice , . Deletion of psm-mec between mecI and mecR2 might alter the expression of mecR1-mecI-mecR2 mRNA, resulting in the altered expression of mecA. We examined whether psm-mec-deleted mutants of 18 HA-MRSA strains alter the expression of mecA. In 16 of 18 strains, each psm-mec-deleted mutant expressed an amount of mecA comparable with that of the respective parent strain (Fig. S5). In CR-11 and SR-1 strains, each psm-mec-deleted mutant expressed less mecA than the respective parent strain (Fig. S5). These results indicate that in most HA-MRSA strains, the effect of psm-mec-deletion on virulence phenotypes are not related to mecA expression, whereas in CR-11 and SR-1 strains, the reduced expression of mecA in the psm-mec-deleted mutants might contribute to the observed phenotype.
Here, we revealed that psm-mec RNA specifically binds agrA mRNA encoding an S. aureus virulence regulatory factor and inhibits its translation. We further demonstrated that the deletion of psm-mec from HA-MRSA strains carrying intact psm-mec led to increased expression of AgrA and PSMα. Furthermore, we demonstrated that one-third of HA-MRSA isolates from the Kanto area of Japan harbored -7T>C mutated psm-mec or did not carry psm-mec. These HA-MRSA strains produced high amounts of PSMα3. These findings support the notion that the mutation or absence of psm-mec in HA-MRSA strains leads to the high expression of AgrA, resulting in the high production of exotoxins and high virulence, whereas in almost two-thirds of HA-MRSA strains carrying intact psm-mec, the expression of AgrA is inhibited by psm-mec, resulting in attenuated virulence. In addition, we demonstrated that the integration of psm-mec into the chromosomes of the CA-MRSA strains, which do not carry psm-mec, led to a decrease in the expression of AgrA. Thus, we propose that the absence of psm-mec is a genetic determinant of the high virulence property of CA-MRSA, i.e., the high expression of agr locus. Identification of the psm-mec mutation could be a novel method for predicting the virulence properties of MRSA strains. We have revealed that HA-MRSA isolates carrying -7T>C psm-mec had closely related genetic backgrounds with isolates carrying intact psm-mec. Thus, the -7T>C mutation of psm-mec may frequently appear from intact psm-mec. In contrast, HA-MRSA isolates carrying no psm-mec have genetic backgrounds that differ from those carrying intact or -7T>C psm-mec, indicating that isolates not carrying psm-mec are evolutionarily distant from isolates carrying intact or -7T>C psm-mec. It will be interesting to see whether the ratio of these three MRSA groups in hospitals changes over time in relation to clinical outcome.
AgrA activates the transcription of psm-mec , . We also confirmed that the expression of psm-mec was diminished in the agr-null mutant and that psm-mec expression was restored by the introduction of agrBDCA. This study revealed that psm-mec RNA negatively regulates agrA translation. These results indicate that AgrA increases the amount of psm-mec RNA, psm-mec RNA inhibits agrA translation, and the decreased amount of AgrA leads to decreased expression of PSMαs as well as of psm-mec RNA itself. Thus, the expression of psm-mec RNA and AgrA is assumed to be maintained in a steady balance by this feedback loop, and the presence of psm-mec might moderately suppress AgrA expression.
Queck et al. revealed that psm-mec has a positive effect on virulence in mouse skin and systemic infection models of the HA-MRSA strain MSA890, in which the amount of PSM-mec, which has cytolytic activity against human neutrophils, was higher than that of PSMα peptides . Furthermore, the same group revealed that psm-mec had no effect on the virulence of HA-MRSA strains Sanger252, BK1406, and BK23684, in which the amount of PSM-mec was not higher than that of PSMα peptides , . In the present study, we constructed the psm-mec-deleted mutants from 18 clinical isolates of HA-MRSA and demonstrated that psm-mec represses the expression of PSMα and AgrA in most of these strains. In addition, we revealed that psm-mec suppresses virulence in mouse skin and systemic infection models of at least two HA-MRSA strains. To examine whether the discrepancy between our results and the results by Queck et al. was due to differences in the experimental procedure, we examined the virulence of MSA890, Sanger252, and their psm-mec-deleted mutants in a mouse systemic infection model. We found that the psm-mec-deleted mutant of the MSA890 strain showed decreased virulence compared with the parent strain, whereas the psm-mec-deleted mutant of Sanger252 did not show decreased virulence compared with the parent strain (Fig. S6), consistent with the reports by Queck et al. Therefore, the genetic backgrounds of the HA-MRSA strains, not differences in the assay system, might explain the discrepancy between our results and the results reported by Queck et al.
RNAIII was the first identified regulatory RNA in S. aureus  and regulates the expression of various genes . RNAIII inhibits the translation of spa encoding protein A , coa encoding staphylocoagulase , and rot encoding a transcription factor . RNAIII carries hairpin loops with a C-rich motif that binds the G-rich sequence of the SD region of target mRNA and inhibits its translation , . RNAIII forms an imperfect duplex with target mRNA, which is digested by RNase III, and decreases the stability of target mRNA , . RNAIII is stable with a half-life of over 20 min , . In the present study, we predicted that the C-rich motif (ACCC) of agrA mRNA binds the SD region (GGGU) of psm-mec RNA (Fig. 3A). We revealed that psm-mec RNA slightly destabilizes agrA mRNA in an RNase III-dependent manner (Fig. 4A). The psm-mec RNA was stable with a half-life of approximately 20 min (Fig. 4D). Therefore, the molecular mechanism underlying the interaction between psm-mec RNA and agrA mRNA is similar to that of RNAIII. Because the half-life of psm-mec RNA was not changed by the presence of agrA mRNA (Fig. 4D), it is possible that anhydrotetracycline induced excess amounts of psm-mec RNA relative to the amount of agrA mRNA, and thus digestion of the psm-mec RNA/agrA mRNA duplex structure did not affect the half-life of the psm-mec RNA. Furthermore, psm-mec inhibited the expression of AgrA in an RNase III-independent manner (Fig. 4C). These findings suggest that the destabilization of agrA mRNA by psm-mec RNA and RNase III occurs after the inhibition of agrA translation by psm-mec RNA. This is consistent with previous reports that translational repression by a small RNA does not require mRNA destabilization in E. coli and S. aureus , . Most small RNAs bind the SD sequence of target RNA, although recent reports indicate that some regulatory RNAs bind the coding region of target mRNA , . A unique feature of the interaction between psm-mec RNA and agrA mRNA is that both RNAs encode proteins and duplex formation involves the coding sequence of both RNAs, i.e., mRNA-mRNA interaction. Because psm-mec RNA binds the coding region of agrA mRNA, which is far from the ribosome binding site, it is possible that the conformational change of agrA mRNA by psm-mec RNA prevents ribosome recruitment or the RNA-RNA pairing inhibits translation elongation. Further studies are needed to clarify whether the interaction between psm-mec RNA and agrA mRNA leads to conformational alteration of the SD structure and to examine the effects of psm-mec RNA on the translation initiation and elongation of agrA mRNA. An mRNA-mRNA interaction might have a broad role in the regulation of gene expression and should be investigated further.
Materials and Methods
This study was performed in strict accordance with the recommendation of the Fundamental Guidelines for Proper Conduct of Animal Experiment and Related Activities in Academic Research Institutions under the jurisdiction of the Ministry of Education, Culture, Sports, Science, and Technology in Japan, 2006. All mouse protocols followed the Regulations for Animal Care and Use of the University of Tokyo and were approved by the Animal Use Committee at the Graduate School of Pharmaceutical Science at the University of Tokyo (approval number: 19–28). All clinical isolates of MRSA were obtained in accordance with the protocols approved by the ethics committee of Nippon Medical School Hospital (approval number: 18-03-49). All patients provided informed consent prior to donating S. aureus isolates. All clinical isolates of MRSA were anonymized because clinical data were not used.
We collected 325 clinical isolates of MRSA strains from Nippon Medical School Hospital (Bunkyo, Tokyo, Japan), Nippon Medical School Chiba Hokusoh Hospital (Inzei, Chiba, Japan), and Sekino Clinical Pharmacology Clinic (Toshima, Tokyo, Japan) from 2008-2010. These strains were streaked on mannitol sodium chloride plates (Eiken Chemical Inc., Tokyo, Japan) and their utilization of mannitol and high-salt resistance were confirmed. Their minimum inhibitory concentration values against oxacillin were examined and resistance to oxacillin was also confirmed. Bacterial strains used in this study are shown in Table 4.
To regulate the expression of AgrA protein under the control of IPTG, pMNS was constructed by fusing pMutinT3  and pTetON . pMNS contains the transcription terminators, Pspac promoter, lacZ, and lacI from pMutinT3 and pE194 ori, pUC ori, and the spectinomycin resistance gene from pTetON. pMNS is compatible with pKE516 . Plasmids used in this study are shown in Table 4.
Preparation of a polyclonal antibody against AgrA
A DNA fragment containing the agrA gene was amplified by polymerase chain reaction (PCR) using oligonucleotide primer pairs agrA-HisC-F and agrA-HisC-R and pW as a template . The amplified DNA fragment was phosphorylated by T4 polynucleotide kinase and self-ligated, resulting in pW-agrAHis. The DNA fragment was amplified by PCR using oligonucleotide primer pairs AgrA-F-NdeI and AgrA-R-BamHI and pW-agrAHis as a template. The amplified DNA fragment was inserted into pET-9a at the Nde I and BamH I sites, resulting in pET-9a-agrAHis. E. coli BL21 (DE3) carrying pLysS was transformed with pET-9a-agrAHis. Transformants were cultured in Terrific broth containing 1 M sorbitol and 10 mM betaine at 25°C according to Koenig RL et al. . Isopropyl β-D-1-thiogalactopyranoside (0.4 mM) was added to the culture at A600 = 0.3 and cultured further for 2.5 h. Cells were collected and lysed by freezing and thawing, and subsequent sonication in a lysis buffer (20 mM Tris-HCl [pH 7.9], 6 M guanidine hydrochloride, 0.5 M NaCl). His-tagged AgrA was purified using a Ni column (ProBond Resin, Life Technologies, Tokyo, Japan) according to the manufacturer's protocol. His-tagged AgrA (0.5 mg) was subcutaneously injected into a Japanese white rabbit 5 times at 2-week intervals. Blood was collected from the rabbit and used for IgG purification by protein G-Sepharose.
Western blotting for AgrA
S. aureus overnight culture was inoculated into a 100-fold amount of fresh tryptic soy broth (TSB) and cultured for 24 h or 15 h at 37°C. S. aureus cells were collected by centrifugation from 650 µl of culture and suspended in a lysis buffer (10 mM Tris-HCl [pH 8.0], 1 mM EDTA [pH 8.0], 25 µg/ml lysostaphin) and incubated at 37°C for 30 min. The sample was sonicated and centrifuged at 10,000 g for 10 min. The amount of protein in the supernatant was measured by the Bradford method and the protein concentration of different samples was equalized by adding a buffer. Proteins were electrophoresed in 15% sodium dodecyl sulfate (SDS)-polyacrylamide gel at 100 V for 3 h. Proteins were transferred from the gel to a membrane (Immobilon-P, Millipore) in buffer (10 mM CAPS, 20% methanol) at 150 mA for 3 h. The membrane was treated with a blocking buffer (Tris-buffered saline with Tween 20 [TBST] containing 5% Easy Blocker [GeneTex, Irvine, CA]) at room temperature for 1 h. The membrane was treated with a blocking buffer containing 1:1000 anti-AgrA IgG at room temperature for 1 h. After washing with TBST, the membrane was treated with a blocking buffer containing 1:2000 anti-rabbit IgG conjugated with alkaline phosphatase at room temperature for 1 h. After washing with TBST, the membrane was treated with a staining buffer (100 mM Tris-HCl [pH9.5], 100 mM NaCl, 50 mM MgCl2, 2% nitro-blue tetrazolium/5-bromo-4-chloro-3′-indolyphosphate)for 5 min. The band intensity was measured by densitometry scanning (Image J 1.45 s, NIH).
Gel shift assay
DNA fragments encoding psm-mec mRNA or agrA mRNA were amplified by PCR using the primers listed in Table S2 and pF and pGP-agrA-luc as a template, and used as templates for in vitro transcription. In vitro transcription was performed using the T7 RiboMAX Express Large Scale RNA Production System (Promega). The 5′ end-labeling of dephosphorylated RNA was performed with T4 polynucleotide kinase and [γ-32P]ATP. Gel shift assays were performed with 0.13 pmol of labeled RNA (final 19 nM) and various doses of nonlabeled RNA in 7 µl of binding buffer (10 mM Tris-HCl, pH8.0, 30 mM KCl) using our protocol modified from Kawamoto et al. and Antal et al. , . The samples were incubated at 95°C for 1 min and at 37°C for 90 min. Two microliters of 50% glycerol were added to the samples, which were then electrophoresed in a 6% polyacrylamide gel in 45 mM Tris-borate at 4°C. The gels were dried and RNA-RNA interactions were analyzed by phosphoimaging using Typhoon (GE) and Image Gauge v. 4.23 software (Fujifilm).
The mouse skin infection experiment was performed according to Bunce et al. . Female 6-week old Hos:HR-1 mice were purchased from Hoshino Laboratory Animals (Ibaraki, Japan). S. aureus overnight culture was inoculated into 100-fold amounts of fresh TSB and cultured to A600 = 0.5. Cells were centrifuged and suspended in phosphate-buffered saline (PBS). Colony forming units (CFU) were measured by spreading the suspended cells on TSB agar plates. Mice were anesthetized with pentobarbital and subcutaneously injected with the suspended bacterial cells containing 5% microbeads (Cytodex 1, GE Healthcare). The inflamed area around the injection site was measured daily (length [L] x width [W]). For mouse systemic infection, S. aureus overnight culture was inoculated into 100-fold amounts of fresh TSB and cultured for 20 h. S. aureus cultures were centrifuged and cells were suspended in PBS. Bacterial suspension (100 µl) was injected into the tail vein of 7-week-old female ICR mice. Survival after injection was monitored. All mice were killed after the experiment.
Protein separation by 2-DE
Overnight cultures of S. aureus strains were inoculated into 100-fold amounts of fresh TSB containing 12.5 µg chloramphenicol/ml and cultured for 14 h at 37°C. One milliliter of culture was centrifuged at 10,000 g for 5 min at 4°C and the pellet was frozen in liquid nitrogen. Pellets were resolved with 360 µl of PBS containing 4.8 U DNase, 9.6 µg RNase A, and 9.6 µg lysostaphin, and incubated for 60 min at room temperature. Cell lysates were centrifuged at 10,000 g for 5 min at 4°C. TCA was added to the samples (final 10%) and the samples were incubated for 60 min at 4°C. The lysates were centrifuged at 10,000 g for 60 min at 4°C, and the precipitates were washed with ethanol twice, and resolved with sample buffer (7 M urea, 2 M thiourea, 50 mM DTT, 4% CHAPS, 0.2% bio-lyte 3/10 ampholyte [Bio-rad], 0.001% BPB). The first isoelectric focusing was performed using 11 cm pH 4–7 IPG strips (Bio-rad) and the PROTEAN IEF system (Bio-rad). The samples (60 µg protein/200 µl sample buffer) were applied to an IPG strip rehydrated for 12 h, and isoelectrically focused at 250 V for 15 min, 8000 V for 6 h, and 500 V for 24 h. Each IPG gel strip was equilibrated in buffer (375 mM Tris-HCl (pH 8.8), 6 M urea, 20% glycerol, 2% SDS, 130 mM DTT) for 20 min and in 2.5% iodoacetamide for 10 min. The IPG gel strips were embedded onto 12.5%-SDS polyacrylamide gel (16 cm×16 cm) using 1% low-melting agarose. The second dimension electrophoresis was performed at a constant 200 V for 3 h at 4°C. Gels were subsequently stained with Coomassie Brilliant Blue.
Construction of the psm-mec integrated CA-MRSA strains
DNA fragments containing the kanamycin resistance gene, psm-mec, and upstream and downstream genomic regions of the desired integration site were spliced together by overlap extension PCR. The psm-mec-I-cassette was inserted into the Sma I site of pKOR3a, resulting in pKOR3a-psm-mec-I (Fig. S1A). MW2 and FRP3757 strains were transformed with the plasmid and the psm-mec-integrated mutants were obtained using the previous method . The desired integration by double recombination event was confirmed by Southern blot analysis (Fig. S1B). We confirmed that the 5′ and 3′ ends of psm-mec RNA transcribed from the genome-integrated psm-mec were the same as those transcribed from plasmid-encoded psm-mec (pF) by a circularized RACE experiment .
Determination of the 3′-terminus of psm-mec mRNA by S1 mapping
The DNA fragment containing psm-mec was amplified by PCR using primers S2 and F5, and pF as a template. The DNA fragment was digested with Nde I and its 3′-teminus was labeled with [α-32P]-dATP using a Klenow fragment. The labeled DNA fragment was electrophoresed in 5% native polyacrylamide gel in 0.5 x TBE. A single strand (242 bases) of the 32P-labeled DNA was cut out from the gel by UV-shadowing and purified. Maxam-Gilbert sequencing ladders were obtained from the end-labeled probe DNA . The end-labeled probe DNA and total RNA of Newman transformed with psm-mec were incubated at 75°C for 10 min and 37°C for 2 h in a buffer (20 mM HEPES-KOH [pH 6.5], 80% formamide, 400 mM NaCl). The polynucleotides in the sample were digested with S1 nuclease in a buffer (30 mM sodium acetate [pH 4.6], 0.3 M NaCl, 1 mM ZnSO4) at 37°C for 15 min. The reaction was terminated by adding PCI (phenol: chloroform: isoamylalcohol = 25:24:1). S1-reacted products and Maxam-Gilbert sequencing ladders were electrophoresed in 8 M urea-7.5% polyacrylamide gel. The gels were dried and DNA was analyzed by phosphoimaging using Typhoon (GE).
DNA fragments containing the recF promoter region and the agrA region (−20–717) were amplified by PCR and inserted into pluc , resulting in a pluc-recFP-agrA. The agrA ORF and luc ORF were fused by PCR using primers agrA-R and lucATG-F, resulting in pGP-agrA-luc. Deletion mutants of agrA region were constructed by PCR using pGP-agrA-luc as a template and primers listed in Table S2, resulting in pGP-luc, pGP-agrA1-luc, pGP-agrA2-luc. The DNA fragment containing psm-mec was inserted into these plasmids, resulting in +F constructs. Constructs of all plasmids were confirmed by sequencing. S. aureus RN4220 strain was transformed with the plasmids. The plasmids were transferred to Newman strain using phage 80α. Overnight cultures of the Newman strains transformed with the plasmids were inoculated into 100-fold amounts of fresh TSB, and cultured to A600 = 1. Cells were collected by centrifugation at 10,000 g for 1 min. Cells were lysed and luciferase activity was measured according to Hanada et al. .
Determination of RNA half-life
The half-life of mRNA was determined as previously described with slight modification . Overnight cultures of S. aureus were inoculated into 100-fold amounts of fresh TSB and cultured to A600 = 3. After treatment with rifampicin (300 µg/ml), samples were collected at the indicated time-points and immediately treated with RNAprotect Bacteria Reagent (Qiagen). Total RNA was extracted using an RNeasy mini kit (Qiagen) according to the manufacturer's protocol. RNA was electrophoresed onto a 1% agarose gel containing 6.6 M formaldehyde and transferred to a nylon membrane (GeneScreen Plus, Perkin Elmer). A DNA probe of the agrA gene or the psm-mec gene was labeled with [32P]-dCTP by random priming. Hybridization was performed at 42°C. Band intensity was measured by densitometry scanning (Image J 1.45 s, NIH). The amount of the detected RNA was normalized to the amount of 16S rRNA and the time-point at which the amount of RNA reached half that at time 0 min was calculated by exponential approximation.
Sequencing of psm-mec of clinical isolates
DNA fragments containing psm-mec were amplified by PCR using genomic DNAs of clinical isolates as a template and primer pairs of S2 and S3. The nucleotide sequence was determined using primers S2 and S3 (Table S2). DNA fragments containing intact psm-mec and mutated psm-mec were amplified by PCR using primer pairs of S2-XbaI and S3-SacI, and inserted into the Xba I and Sac I sites of pND50, resulting in pF, pM1, pD2, pD3, pD4, and pD5. The effects of these plasmids on the Newman strain were evaluated (Fig. S3).
Typing of the polymorphic region of the protein A gene (spa) was performed as described previously . Purified spa PCR products were sequenced, and short-sequence repeats were assigned using the spa database website (http://tools.egenomics.com./Public/Login.aspx).
Multiplex PCRs were performed to identify the SCCmec types according to the established method . Primer sets M-PCR1 and M-PCR2 were used. When DNA was not amplified by using one of the primer set, the stain was classified as non-typed.
Construction of the psm-mec-deleted MRSA strains and the rnc-deleted Newman strain
DNA fragments containing antibiotic-resistant gene and the upstream and downstream regions of psm-mec were spliced together by overlap extension PCR, resulting in a psm-mec-cassette. The psm-mec-cassette was inserted into the Sma I site of pKOR3a, resulting in pKOR3a-psm-mec. MRSA strains were transformed with the plasmid and the psm-mec-deleted mutants were obtained using the previously reported method . The desired deletion of psm-mec by double homologous recombination was confirmed by Southern blot analysis (Fig. S4). To disrupt rnc in the Newman strain, a single-cross over recombination method was used, as reported previously .
Measurement of PSMs
The amount of PSM was measured as previously described with slight modification . Overnight bacterial cultures (50 µl) were inoculated into 5 ml fresh tryptic soy broth and aerobically cultured at 37°C for 15 h without antibiotics. The cultures were centrifuged and the supernatants were evaporated using a centrifuge evaporator (CC-105, TOMY, Tokyo, Japan). The evaporated products were solved in 40% acetonitrile and centrifuged at 20,400 g for 5 min. The supernatants were evaporated using a centrifuge evaporator, and the evaporated products were dissolved in water, and analyzed by reversed phase-high performance liquid chromatography. Chromatography was performed using a SOURCE 5RPC ST 4.6/150 column (GE Healthcare, Tokyo, Japan) and 50% acetonitrile in 0.1% trifluoroacetic acid for 3 min and a water/acetonitrile gradient in 0.1% trifluoroacetic acid from 50 to 90% acetonitrile for 20 min at a flow rate of 1 ml/min (600E, Waters, Milford, MA). Absorbance at 215 nm was detected using a 2998 Photodiode Array Detector (Waters). The molecular mass in the respective peak was determined using liquid chromatography-electrospray ionization mass spectrometry (LC 1100 series, Agilent Technologies, Santa Clara, CA; ESI-MS, Bio-TOFQ, Bruker Daltonics, Billerica, MA) and the respective PSMs were identified as previously described . Hld and PSMα1 were not separated in this system.
Colony spreading assay
The colony spreading assay was basically performed according to our previous method . Two microliters of S. aureus overnight culture were spotted onto soft TSB agar plates containing 0.24% agar, and was incubated for 24 h at 37°C. The diameter of the giant colony was measured.
Biofilm formation assay
The biofilm formation assay was basically performed according to our previous method . S. aureus overnight culture was inoculated into a 200-fold amount of fresh TSB containing 0.25% glucose in 96-well polystyrene plates and cultured for 3 days at 37°C. Cells attached to the plate were stained with safranin and measured by A490.
Integration of psm-mec into chromosomes of CA-MRSA strains. (A) The genomic region that was integrated with psm-mec is schematically represented as the psm-mec-integrated CA-MRSA strain. Probe DNA regions, construct of targeting plasmid, genomic region of CA-MRSA (type-IV SCCmec) are presented above. Predicted lengths of DNA fragments that were digested with Sph I are presented. (B) Genomic DNAs of MW2, FRP3757, and their psm-mec-integrated mutants were digested with Sph I and subjected to Southern blot analysis using probes 1 and 2. P indicates the parent strain. A, B, and C means independently obtained psm-mec integrated mutants.
Determination of 3′-terminus of psm-mec RNA. The 3′-terminus of psm-mec RNA was determined by S1 mapping. S1-digested products and Maxam-Gilbert sequencing ladders were electrophoresed in 8 M urea-7.5% polyacrylamide gel. Lanes 1 and 2 represent products that were digested with 75 U and 450 U of S1 nuclease, respectively. Lanes AG, CT, and C represent Maxam-Gilbert sequencing ladders. The nucleotide sequences of psm-mec RNA and the antisense RNA are presented on the left side of the panel. Black stars represent the 3′-terminus of psm-mec RNA determined by the migration of the S1-digested product.
Effect of the mutated psm-mec sequences found in clinical MRSA isolates on S. aureus Newman strain. (A) The amount of PSM-mec in the culture supernatant of the Newman strain transformed with empty vector (pND50), intact psm-mec (pF), D1-mutated psm-mec (pM1), D2-mutated psm-mec (pD2), D3-mutated psm-mec (pD3), D4-mutated psm-mec (pD4), or D5-mutated psm-mec (pD5) was measured. The vertical axis represents the relative amount of PSM-mec against that of Newman transformed with pF. Means ± standard deviations from four independent experiments are shown. Student t-test P-values between pF-transformed Newman and other strains are presented. NS, P>0.05. ND, not detected. (B, C) The amount of PSMα3 (B) and PSMα1+Hld (C) of the psm-mec-transformed strains described above was measured. The vertical axis represents the relative amount of PSMα3 against that of Newman transformed with pND50. Means ± standard deviations from four independent experiments are shown. Student t-test P-values between pF-transformed Newman and other strains are presented. NS, P>0.05. (D) Colony spreading ability of the above psm-mec-transformed strains was evaluated. Two microliters of S. aureus overnight cultures was spotted onto soft agar plates and incubated at 37°C for 8 h. Diameter of the giant colony was measured. Means ± standard deviations from four independent experiments are shown. Student t-test P-values between pF-transformed Newman and other strains are presented. NS, P>0.05. (E) Biofilm formation of the above psm-mec-transformed strains was evaluated. S. aureus was cultured in polystyrene plates for 3 days and the biofilm was stained by safranin. Means ± standard deviations from six independent experiments are shown. Student t-test P-values between pF-transformed Newman and other strains are presented. NS, P>0.05.
Deletion of psm-mec from clinical MRSA isolates. (A) Schematic representation of the genomic region around psm-mec in type-II SCCmec. psm-mec was deleted by tetL in NI-13, NI-18, CR-11, CR-12, CR-18, CR-29, CR-38, SR-8, NIR-34, NIR-45, and NI-7 strains. psm-mec was deleted by the phleomycin resistance gene in NI-4, NI-22, NI-36, SR-1, NIR-121, NI-3, and NI-38 strains. DNA fragment lengths that were digested by Bgl II are presented. (B) Genomic DNAs of 18 clinical MRSA strains and their psm-mec-deleted mutants were digested with Bgl II and subjected to Southern blot analysis using the probes presented in (A). P indicates the parent clinical strain. A, B, and C indicate independently obtained psm-mec-deleted mutants.
Expression of mecA in the psm-mec-deleted mutants of clinical isolates. Northern blot analysis was performed to detect mecA mRNA in the psm-mec-deleted mutants and clinical isolates. Total RNA was extracted from cultures at the log phase (A600 = 0.5) and electrophoresed. rRNA stained with ethidium bromide is shown. Data are representative from three independent experiments.
Virulence of the psm-mec-deleted mutants of MSA890 and Sanger252 in a mouse systemic infection model. ICR mice (n = 10) were intravenously injected with S. aureus cells. Injected CFUs were as follows: MSA890 and its psm-mec-deleted mutant, 2×108 CFU; Sanger252 and its psm-mec-deleted mutant, 2×108 CFU. Log-rank test P-value between MSA890 and its psm-mec-deleted mutant is 0.0489.
Identification of proteins upregulated by psm-mec RNA in the FRP3757 strain.
Primers used in the study.
We thank M. Otto, B. Diep, H. F. Chambers, T. Naimi, and S. H. Leppla for kindly providing bacterial strains and plasmids. We appreciate the support from S. Naidich, J. R. Mediavilla, and B. N. Kreiswirth for assigning new spa types.
Conceived and designed the experiments: CK. Performed the experiments: CK YS MI YO HM GN TF SN XH. Analyzed the data: CK YS MI YO HM GN TF SN XH. Contributed reagents/materials/analysis tools: KO SH HY KI TI KH. Wrote the paper: CK KS.
- 1. Li M, Diep BA, Villaruz AE, Braughton KR, Jiang X, et al. (2009) Evolution of virulence in epidemic community-associated methicillin-resistant Staphylococcus aureus. Proc Natl Acad Sci U S A 106: 5883–5888. doi: 10.1073/pnas.0900743106
- 2. Wang R, Braughton KR, Kretschmer D, Bach TH, Queck SY, et al. (2007) Identification of novel cytolytic peptides as key virulence determinants for community-associated MRSA. Nat Med 13: 1510–1514. doi: 10.1038/nm1656
- 3. Montgomery CP, Boyle-Vavra S, Adem PV, Lee JC, Husain AN, et al. (2008) Comparison of virulence in community-associated methicillin-resistant Staphylococcus aureus pulsotypes USA300 and USA400 in a rat model of pneumonia. J Infect Dis 198: 561–570. doi: 10.1086/590157
- 4. Cheung GY, Wang R, Khan BA, Sturdevant DE, Otto M (2011) Role of the accessory gene regulator agr in community-associated methicillin-resistant Staphylococcus aureus pathogenesis. Infect Immun 79: 1927–1935. doi: 10.1128/iai.00046-11
- 5. Thurlow LR, Joshi GS, Richardson AR (2012) Virulence strategies of the dominant USA300 lineage of community-associated methicillin-resistant Staphylococcus aureus (CA-MRSA). FEMS Immunol Med Microbiol 65: 5–22. doi: 10.1111/j.1574-695x.2012.00937.x
- 6. Montgomery CP, Boyle-Vavra S, Daum RS (2010) Importance of the global regulators Agr and SaeRS in the pathogenesis of CA-MRSA USA300 infection. PLoS ONE 5: e15177. doi: 10.1371/journal.pone.0015177
- 7. Novick RP (2003) Autoinduction and signal transduction in the regulation of staphylococcal virulence. Mol Microbiol 48: 1429–1449. doi: 10.1046/j.1365-2958.2003.03792.x
- 8. Koenig RL, Ray JL, Maleki SJ, Smeltzer MS, Hurlburt BK (2004) Staphylococcus aureus AgrA binding to the RNAIII-agr regulatory region. J Bacteriol 186: 7549–7555. doi: 10.1128/jb.186.22.7549-7555.2004
- 9. Novick RP, Ross HF, Projan SJ, Kornblum J, Kreiswirth B, et al. (1993) Synthesis of staphylococcal virulence factors is controlled by a regulatory RNA molecule. EMBO J 12: 3967–3975.
- 10. Queck SY, Jameson-Lee M, Villaruz AE, Bach TH, Khan BA, et al. (2008) RNAIII-independent target gene control by the agr quorum-sensing system: insight into the evolution of virulence regulation in Staphylococcus aureus. Mol Cell 32: 150–158. doi: 10.1016/j.molcel.2008.08.005
- 11. Ma XX, Ito T, Tiensasitorn C, Jamklang M, Chongtrakool P, et al. (2002) Novel type of staphylococcal cassette chromosome mec identified in community-acquired methicillin-resistant Staphylococcus aureus strains. Antimicrob Agents Chemother 46: 1147–1152. doi: 10.1128/aac.46.4.1147-1152.2002
- 12. Kaito C, Saito Y, Nagano G, Ikuo M, Omae Y, et al. (2011) Transcription and translation products of the cytolysin gene psm-mec on the mobile genetic element SCCmec regulate Staphylococcus aureus virulence. PLoS pathogens 7: e1001267. doi: 10.1371/journal.ppat.1001267
- 13. Kaito C, Omae Y, Matsumoto Y, Nagata M, Yamaguchi H, et al. (2008) A novel gene, fudoh, in the SCCmec region suppresses the colony spreading ability and virulence of Staphylococcus aureus. PLoS ONE 3: e3921. doi: 10.1371/journal.pone.0003921
- 14. Vanderpool CK, Gottesman S (2004) Involvement of a novel transcriptional activator and small RNA in post-transcriptional regulation of the glucose phosphoenolpyruvate phosphotransferase system. Mol Microbiol 54: 1076–1089. doi: 10.1111/j.1365-2958.2004.04348.x
- 15. Peng HL, Novick RP, Kreiswirth B, Kornblum J, Schlievert P (1988) Cloning, characterization, and sequencing of an accessory gene regulator (agr) in Staphylococcus aureus. J Bacteriol 170: 4365–4372.
- 16. Dunman PM, Murphy E, Haney S, Palacios D, Tucker-Kellogg G, et al. (2001) Transcription profiling-based identification of Staphylococcus aureus genes regulated by the agr and/or sarA loci. J Bacteriol 183: 7341–7353. doi: 10.1128/jb.183.24.7341-7353.2001
- 17. Nagarajan V, Elasri MO (2007) SAMMD: Staphylococcus aureus microarray meta-database. BMC Genomics 8: 351. doi: 10.1186/1471-2164-8-351
- 18. Cao Y, Zhao Y, Cha L, Ying X, Wang L, et al. (2009) sRNATarget: a web server for prediction of bacterial sRNA targets. Bioinformation 3: 364–366. doi: 10.6026/97320630003364
- 19. Rehmsmeier M, Steffen P, Hochsmann M, Giegerich R (2004) Fast and effective prediction of microRNA/target duplexes. RNA 10: 1507–1517. doi: 10.1261/rna.5248604
- 20. Huntzinger E, Boisset S, Saveanu C, Benito Y, Geissmann T, et al. (2005) Staphylococcus aureus RNAIII and the endoribonuclease III coordinately regulate spa gene expression. Embo J 24: 824–835. doi: 10.1038/sj.emboj.7600572
- 21. Chevalier C, Boisset S, Romilly C, Masquida B, Fechter P, et al. (2010) Staphylococcus aureus RNAIII binds to two distant regions of coa mRNA to arrest translation and promote mRNA degradation. PLoS Pathog 6: e1000809. doi: 10.1371/journal.ppat.1000809
- 22. Boisset S, Geissmann T, Huntzinger E, Fechter P, Bendridi N, et al. (2007) Staphylococcus aureus RNAIII coordinately represses the synthesis of virulence factors and the transcription regulator Rot by an antisense mechanism. Genes Dev 21: 1353–1366. doi: 10.1101/gad.423507
- 23. Chatterjee SS, Chen L, Joo HS, Cheung GY, Kreiswirth BN, et al. (2011) Distribution and regulation of the mobile genetic element-encoded phenol-soluble modulin PSM-mec in methicillin-resistant Staphylococcus aureus. PLoS ONE 6: e28781. doi: 10.1371/journal.pone.0028781
- 24. Monecke S, Engelmann I, Archambault M, Coleman DC, Coombs GW, et al. (2012) Distribution of SCCmec-associated phenol-soluble modulin in staphylococci. Mol Cell Probes 26: 99–103. doi: 10.1016/j.mcp.2012.01.001
- 25. Bunce C, Wheeler L, Reed G, Musser J, Barg N (1992) Murine model of cutaneous infection with gram-positive cocci. Infect Immun 60: 2636–2640.
- 26. Arede P, Milheirico C, de Lencastre H, Oliveira DC (2012) The anti-repressor MecR2 promotes the proteolysis of the mecA repressor and enables optimal expression of beta-lactam resistance in MRSA. PLoS Pathog 8: e1002816. doi: 10.1371/journal.ppat.1002816
- 27. Rudkin JK, Edwards AM, Bowden MG, Brown EL, Pozzi C, et al. (2012) Methicillin resistance reduces the virulence of healthcare-associated methicillin-resistant Staphylococcus aureus by interfering with the agr quorum sensing system. J Infect Dis 205: 798–806. doi: 10.1093/infdis/jir845
- 28. Pozzi C, Waters EM, Rudkin JK, Schaeffer CR, Lohan AJ, et al. (2012) Methicillin resistance alters the biofilm phenotype and attenuates virulence in Staphylococcus aureus device-associated infections. PLoS Pathog 8: e1002626. doi: 10.1371/journal.ppat.1002626
- 29. Queck SY, Khan BA, Wang R, Bach TH, Kretschmer D, et al. (2009) Mobile genetic element-encoded cytolysin connects virulence to methicillin resistance in MRSA. PLoS Pathog 5: e1000533. doi: 10.1371/journal.ppat.1000533
- 30. Geisinger E, Adhikari RP, Jin R, Ross HF, Novick RP (2006) Inhibition of rot translation by RNAIII, a key feature of agr function. Mol Microbiol 61: 1038–1048. doi: 10.1111/j.1365-2958.2006.05292.x
- 31. Chevalier C, Geissmann T, Helfer AC, Romby P (2009) Probing mRNA structure and sRNA-mRNA interactions in bacteria using enzymes and lead(II). Methods Mol Biol 540: 215–232. doi: 10.1007/978-1-59745-558-9_16
- 32. Morita T, Mochizuki Y, Aiba H (2006) Translational repression is sufficient for gene silencing by bacterial small noncoding RNAs in the absence of mRNA destruction. Proc Natl Acad Sci U S A 103: 4858–4863. doi: 10.1073/pnas.0509638103
- 33. Chabelskaya S, Gaillot O, Felden B (2010) A Staphylococcus aureus small RNA is required for bacterial virulence and regulates the expression of an immune-evasion molecule. PLoS Pathog 6: e1000927. doi: 10.1371/journal.ppat.1000927
- 34. Bouvier M, Sharma CM, Mika F, Nierhaus KH, Vogel J (2008) Small RNA binding to 5′ mRNA coding region inhibits translational initiation. Mol Cell 32: 827–837. doi: 10.1016/j.molcel.2008.10.027
- 35. Pfeiffer V, Papenfort K, Lucchini S, Hinton JC, Vogel J (2009) Coding sequence targeting by MicC RNA reveals bacterial mRNA silencing downstream of translational initiation. Nat Struct Mol Biol 16: 840–846. doi: 10.1038/nsmb.1631
- 36. Moriya S, Tsujikawa E, Hassan AK, Asai K, Kodama T, et al. (1998) A Bacillus subtilis gene-encoding protein homologous to eukaryotic SMC motor protein is necessary for chromosome partition. Mol Microbiol 29: 179–187. doi: 10.1046/j.1365-2958.1998.00919.x
- 37. Sastalla I, Chim K, Cheung GY, Pomerantsev AP, Leppla SH (2009) Codon-optimized fluorescent proteins designed for expression in low-GC gram-positive bacteria. Appl Environ Microbiol 75: 2099–2110. doi: 10.1128/aem.02066-08
- 38. Matsuo M, Kurokawa K, Lee BL, Sekimizu K (2010) Shuttle vectors derived from pN315 for study of essential genes in Staphylococcus aureus. Biol Pharm Bull 33: 198–203. doi: 10.1248/bpb.33.198
- 39. Omae Y, Sekimizu K, Kaito C (2012) Inhibition of colony-spreading activity of Staphylococcus aureus by secretion of delta-hemolysin. J Biol Chem 287: 15570–15579. doi: 10.1074/jbc.m112.357848
- 40. Kawamoto H, Koide Y, Morita T, Aiba H (2006) Base-pairing requirement for RNA silencing by a bacterial small RNA and acceleration of duplex formation by Hfq. Mol Microbiol 61: 1013–1022. doi: 10.1111/j.1365-2958.2006.05288.x
- 41. Antal M, Bordeau V, Douchin V, Felden B (2005) A small bacterial RNA regulates a putative ABC transporter. J Biol Chem 280: 7901–7908. doi: 10.1074/jbc.m413071200
- 42. Britton RA, Wen T, Schaefer L, Pellegrini O, Uicker WC, et al. (2007) Maturation of the 5′ end of Bacillus subtilis 16S rRNA by the essential ribonuclease YkqC/RNase J1. Mol Microbiol 63: 127–138. doi: 10.1111/j.1365-2958.2006.05499.x
- 43. Sambrook J, Russell DW (2001) Molecular cloning : a laboratory manual. Cold Spring Harbor, N.Y.: Cold Spring Harbor Laboratory Press. 1 v. (various pagings) p.
- 44. Matsumoto Y, Kaito C, Morishita D, Kurokawa K, Sekimizu K (2007) Regulation of exoprotein gene expression by the Staphylococcus aureus cvfB gene. Infect Immun 75: 1964–1972. doi: 10.1128/iai.01552-06
- 45. Hanada Y, Sekimizu K, Kaito C (2011) Silkworm apolipophorin protein inhibits Staphylococcus aureus virulence. J Biol Chem 286: 39360–39369. doi: 10.1074/jbc.m111.278416
- 46. Lioliou E, Sharma CM, Caldelari I, Helfer AC, Fechter P, et al. (2012) Global regulatory functions of the Staphylococcus aureus endoribonuclease III in gene expression. PLoS Genet 8: e1002782. doi: 10.1371/journal.pgen.1002782
- 47. Shopsin B, Gomez M, Montgomery SO, Smith DH, Waddington M, et al. (1999) Evaluation of protein A gene polymorphic region DNA sequencing for typing of Staphylococcus aureus strains. J Clin Microbiol 37: 3556–3563.
- 48. Kondo Y, Ito T, Ma XX, Watanabe S, Kreiswirth BN, et al. (2007) Combination of multiplex PCRs for staphylococcal cassette chromosome mec type assignment: rapid identification system for mec, ccr, and major differences in junkyard regions. Antimicrob Agents Chemother 51: 264–274. doi: 10.1128/aac.00165-06
- 49. Kaito C, Kurokawa K, Matsumoto Y, Terao Y, Kawabata S, et al. (2005) Silkworm pathogenic bacteria infection model for identification of novel virulence genes. Mol Microbiol 56: 934–944. doi: 10.1111/j.1365-2958.2005.04596.x
- 50. Kaito C, Sekimizu K (2007) Colony spreading in Staphylococcus aureus. J Bacteriol 189: 2553–2557. doi: 10.1128/jb.01635-06
- 51. Duthie ES, Lorenz LL (1952) Staphylococcal coagulase; mode of action and antigenicity. J Gen Microbiol 6: 95–107. doi: 10.1099/00221287-6-1-2-95
- 52. Naimi TS, LeDell KH, Boxrud DJ, Groom AV, Steward CD, et al. (2001) Epidemiology and clonality of community-acquired methicillin-resistant Staphylococcus aureus in Minnesota, 1996–1998. Clin Infect Dis 33: 990–996. doi: 10.1086/322693
- 53. Diep BA, Gill SR, Chang RF, Phan TH, Chen JH, et al. (2006) Complete genome sequence of USA300, an epidemic clone of community-acquired meticillin-resistant Staphylococcus aureus. Lancet 367: 731–739. doi: 10.1016/s0140-6736(06)68231-7
- 54. Ueda T, Kaito C, Omae Y, Sekimizu K (2011) Sugar-responsive gene expression and the agr system are required for colony spreading in Staphylococcus aureus. Microb Pathog 51: 178–185. doi: 10.1016/j.micpath.2011.04.003
- 55. Kaito C, Hirano T, Omae Y, Sekimizu K (2011) Digestion of extracellular DNA is required for giant colony formation of Staphylococcus aureus. Microb Pathog 51: 142–148. doi: 10.1016/j.micpath.2011.04.007
- 56. Matsuo M, Kurokawa K, Nishida S, Li Y, Takimura H, et al. (2003) Isolation and mutation site determination of the temperature-sensitive murB mutants of Staphylococcus aureus. FEMS Microbiol Lett 222: 107–113. doi: 10.1016/s0378-1097(03)00260-x
- 57. Ichihashi N, Kurokawa K, Matsuo M, Kaito C, Sekimizu K (2003) Inhibitory effects of basic or neutral phospholipid on acidic phospholipid-mediated dissociation of adenine nucleotide bound to DnaA protein, the initiator of chromosomal DNA replication. J Biol Chem 278: 28778–28786. doi: 10.1074/jbc.m212202200
- 58. Oku Y, Kurokawa K, Matsuo M, Yamada S, Lee BL, et al. (2009) Pleiotropic roles of polyglycerolphosphate synthase of lipoteichoic acid in growth of Staphylococcus aureus cells. J Bacteriol 191: 141–151. doi: 10.1128/jb.01221-08