Advertisement
Research Article

Identification of Genes Involved in Polysaccharide-Independent Staphylococcus aureus Biofilm Formation

  • Blaise R. Boles,

    Affiliation: Department of Microbiology, Roy J. and Lucille A. Carver College of Medicine, University of Iowa, Iowa City, Iowa, United States of America

    X
  • Matthew Thoendel,

    Affiliation: Department of Microbiology, Roy J. and Lucille A. Carver College of Medicine, University of Iowa, Iowa City, Iowa, United States of America

    X
  • Aleeza J. Roth,

    Affiliation: Department of Microbiology, Roy J. and Lucille A. Carver College of Medicine, University of Iowa, Iowa City, Iowa, United States of America

    X
  • Alexander R. Horswill mail

    alex-horswill@uiowa.edu

    Affiliation: Department of Microbiology, Roy J. and Lucille A. Carver College of Medicine, University of Iowa, Iowa City, Iowa, United States of America

    X
  • Published: April 14, 2010
  • DOI: 10.1371/journal.pone.0010146

Abstract

Staphylococcus aureus is a potent biofilm former on host tissue and medical implants, and biofilm growth is a critical virulence determinant for chronic infections. Recent studies suggest that many clinical isolates form polysaccharide-independent biofilms. However, a systematic screen for defective mutants has not been performed to identify factors important for biofilm formation in these strains. We created a library of 14,880 mariner transposon mutants in a S. aureus strain that generates a proteinaceous and extracellular DNA based biofilm matrix. The library was screened for biofilm defects and 31 transposon mutants conferred a reproducible phenotype. In the pool, 16 mutants overproduced extracellular proteases and the protease inhibitor α2-macroglobulin restored biofilm capacity to 13 of these mutants. The other 15 mutants in the pool displayed normal protease levels and had defects in genes involved in autolysis, osmoregulation, or uncharacterized membrane proteins. Two transposon mutants of interest in the GraRS two-component system and a putative inositol monophosphatase were confirmed in a flow cell biofilm model, genetically complemented, and further verified in a community-associated methicillin-resistant S. aureus (CA-MRSA) isolate. Collectively, our screen for biofilm defective mutants identified novel loci involved in S. aureus biofilm formation and underscored the importance of extracellular protease activity and autolysis in biofilm development.

Introduction

Staphylococcus aureus is a human commensal and the causative agent of diverse acute and chronic bacterial infections. The chronic infections persist and cause significant morbidity and mortality to the patient due to the development of a recalcitrant biofilm structure. Compared to the free-living (planktonic) state, S. aureus living in biofilms exhibit significant differences in gene expression and physiology [1], and the close proximity of organisms may also allow cooperative metabolic functions, promote horizontal gene transfer, and facilitate cell-to-cell communication [2], [3]. The most notorious biofilm characteristic is their extraordinary resistance to antimicrobial killing [4]. In a recent comparison, we observed a six-log difference in cell viability in the presence of antibiotics of an S. aureus biofilm versus planktonic cells [5].

Despite the important role of S. aureus biofilms in disease, our understanding of the molecular mechanisms contributing to biofilm formation is incomplete. Recent studies of S. aureus biofilm development suggest that the extracellular matrix consists of proteins, DNA, and/or polysaccharide (also called the polysaccharide intercellular adhesin or PIA). In support of this proposal, compounds capable of dissolving matrix components (proteases, DNAse, or glycoside hydrolases) can disrupt established biofilms or prevent the formation of a biofilm [5], [6], [7], [8]. Recently, it has become evident that emerging clinical S. aureus isolates are not reliant on PIA for biofilm formation [7], [9], [10]. Protein-mediated biofilm formation has emerged as a prominent alternative to PIA, and many surface adhesins, such as Bap [11], Spa [12], FnBPA and FnBPB [13], and SasG [14], [15], have been implicated in this divergent biofilm mechanism. Biofilms produced by these PIA-independent strains are unaffected by polysaccharide-degrading enzymes, such as dispersin B [6], or mutations in the ica gene locus that generates PIA [1], [5], [7], [13]. Therefore, we set out to uncover PIA-independent mechanisms of biofilm formation.

Here we report the generation of a mariner transposon mutant library of 14,880 mutants in a S. aureus strain that develops a biofilm by a PIA-independent mechanism. This library was screened for reduced biofilm formation in a microtiter assay and numerous novel loci were identified. This work expands our understanding of genetic factors controlling biofilm formation and may provide potential targets for therapeutic intervention.

Results

Identification of mariner transposon mutants defective in biofilm formation

To identify genes involved in PIA-independent biofilm formation, we mutagenized S. aureus strain SH1000 using the bursa aurealis (mariner) transposon mutagenesis system [16]. This strain was chosen for mutagenesis and screening because it forms PIA-independent biofilms and is readily amendable to genetic manipulation [5]. Preliminary testing of the mariner transposon system in strain SH1000 was shown to be successful [10]. Altogether, a transposon mutant library of 14,880 mutants was created and banked for further analysis.

Initial screening for biofilm formation in microtiter plates yielded 91 mutants with a defect in attachment. Mutants with severe growth defects were eliminated from further analysis and the remaining potential biofilm mutants were reexamined for reproducibility in the biofilm assay. Thirty-one mutants displayed reproducible biofilm formation defects and arbitrary PCR and sequencing was used to map the insertion location (Table 1). Transposon insertions resulting in a biofilm phenotype were mapped to a variety of genetic loci. Some of the loci, such as altA, fmtA, graS, rsbU and rsbV have previously been shown to be important in S. aureus biofilm formation [10], [17], [18], [19]. The remaining mutants had insertions in genes not previously identified to be involved in biofilm formation.

thumbnail

Table 1. Biofilm defective mutants.

doi:10.1371/journal.pone.0010146.t001

Extracellular protease activity of biofilm mutants

Recent studies have demonstrated that protease activity can have antibiofilm effects [5], [7], [20], [21]. To determine if any of the biofilm defective mutants produced increased levels of extracellular protease activity, we assayed protease levels in culture supernatants of the biofilm mutants (Fig. 1). We found that 16 of the 31 transposon mutants displayed an increase in protease activity in cell free supernatants. We hypothesized that the increase in extracellular protease production could be the cause of the biofilm defect in these mutants. To test this hypothesis, the general protease inhibitor α2-macroglobulin was added to mutant strains from the beginning of biofilm growth [15]. The addition of this protease inhibitor restored biofilm formation in 13 of the 16 protease overproducing mutants (blue bars, Fig. 2b). Recovery of the rsbU and rsbV insertions with α2-macroglobulin supports our previous report where the biofilm defect of a sigB deletion was recovered with the same inhibitor [10]. The three protease overproducing mutants that did not form a biofilm in the presence of α2-macroglobulin had insertions in a two-component system (graS, mutant 37 C9) or in a probable inositol monophosphate phosphatase (hereafter the gene is called “imp”, mutants 60 G7 & 64 G10). In mutants that displayed a wild-type level of extracellular protease activity, the addition of α2-macroglobulin had no effect. Collectively, these results indicate that extracellular protease activity is an important contributor to the biofilm defect in 13 of the biofilm mutants.

thumbnail

Figure 1. Extracellular protease activity of biofilm mutants.

Protease activity in cell-free supernatants from cultures grown in TSB for 12 hours was measured with Azocoll reagent as described in Materials and Methods. Supernatant protease activity of the wild-type strain (SH1000) was set to 1 as a reference. The graph shows the mean of three samples; error bars show standard deviation. Blue bars indicate mutants that show consistently higher levels of protease activity.

doi:10.1371/journal.pone.0010146.g001
thumbnail

Figure 2. Assessment of biofilm formation in transposon mutants.

Microtiter biofilm assays were performed in the absence (A) or presence (B) of the protease inhibitor α2-macroglobulin in triplicate, and the percentages of biofilm formation for each mutant relative to that of the wild type are shown. Error bars show standard deviation. Color coding is as follows: black bars indicate mutants with normal extracellular protease activity, blue bars indicate high protease activity and biofilm recovery with α2-macroglobulin, and red bars indicate the graS (37 C9) and imp (60 G7, 64 G10) mutations that did not recover with α2-macroglobulin.

doi:10.1371/journal.pone.0010146.g002

Extracellular nuclease activity of biofilm mutants

Evidence in many different bacterial species, including S. aureus and CA-MRSA, indicates that extracellular DNA (eDNA) is an important component of the biofilm matrix [6], [8], [9], [22],[23],[24],[25],[26]. Consistent with the key role of eDNA, the expression and extracellular activity of the S. aureus thermostable nuclease has profound effects on biofilm maturation [6], [8]. Based on these results, we hypothesized that some mutants may be unable to form biofilms due to increased nuclease expression. To address this hypothesis, a phenotypic plate assay was employed to assess the levels of extracellular nuclease activity in biofilm defective mutants. After testing all 31 mutants, four mutants in the pool, 3 C5 (rsbU), 37 G12 (rsbV), 60 G7 (imp) and 64 G10 (imp), had increased levels of extracellular nuclease activity (Fig. 3). These four mutants were also tested using a quantitative nuclease assay, and the results confirmed the plate assay phenotypes (Fig. 3). The increased nuclease activity of the rsbU and rsbV mutants is consistent with microarray profiling of Sigma B defective strains [27].

thumbnail

Figure 3. Extracellular nuclease activity of selected biofilm defective mutants.

Nuclease activity was measured as described in Materials and Methods and plotted relative to SH1000 levels. For the imp mutant, only the results of transposon mutant 60 G7 are shown. Results with imp mutant 64 G10 were indistinguishable (data not shown). Underneath the plotted nuclease activity results are representative images of colonies grown on methyl green DNase agar plates. Clearing zones around the colonies is indicative of increased nuclease activity. Error bars show standard deviation.

doi:10.1371/journal.pone.0010146.g003

Autolysis levels of biofilm mutants

S. aureus biofilm matrix is composed in part by eDNA that has been released by autolysis [8], [23]. Therefore if lysis is altered, the change could reduce the ability of S. aureus to effectively form a biofilm. To test for this phenotype, we utilized an assay that measures autolysis as a function of β-galactosidase release into culture supernatants [23]. We focused on the 18 transposon mutants in the pool of 31 unable to form a biofilm in the presence of α2-macroglobulin (black and red bars, Fig. 2). Due to some genes with multiple insertions (Table 1), this pool was reduced to 12 insertions in unique loci and each of these mutants was transformed with plasmid pAJ22, which constitutively expresses the lacZ gene. Cell free culture supernatants were assayed for β-galactosidase activity at indicated time points. During a time course, the autolysis profile of five mutants mirrored wild type (data not shown), while seven of the 12 mutants showed significant changes in β-galactosidase activity (Fig. 4). Four of these seven mutants, 42 F6 (purA), 54 C2 (opuD), 123 D2 (hypothetical membrane protein), and 132 G7 (atlA), all demonstrated reduced autolysis compared to their isogenic parent. Conversely, three mutants 51G5 (fmtA), 37 C9 (graS), and 60 G7 (imp), displayed an increase in autolysis. Of these, the fmtA mutant showed high levels of autolysis early in the time course (12–36 hrs, Fig. 4), while lysis in the graS and imp mutants was more pronounced later in the time course (36–72 hrs, Fig. 4). The altered ability of these mutants to precisely control autolysis (and thus release of eDNA) may contribute to their inability to effectively form biofilms.

thumbnail

Figure 4. Time course of autolysis in selected biofilm mutants.

Planktonic cultures of seven transposon mutants harboring plasmid pAJ22, which expresses cytoplasmic β-galactosidase, were grown for 72 hrs. Every 12 hr during the time course samples were removed from cultures and β-galactosidase activity in cell free supernatants was measured (reported in Miller units). SH1000 with pAJ22 was included as a control (shown as black squares). Results shown were the average of two independent experiments done in triplicate and error bars show standard deviation.

doi:10.1371/journal.pone.0010146.g004

graS and imp mutants are biofilm defective in a CA-MRSA strain

Mutations in the graS and imp genes were chosen for further study because of their unique combination of autolysis, nuclease, and protease phenotypes (Figs. 2, 3, 4). To assess the biofilm maturation phenotypes in a flowing environment, the graS and imp transposon mutants were grown in a flow cell biofilm model. As shown in Figure 5A, both the graS mutant (37 C9) and the imp mutant (60 G7) displayed profound defects in biofilm maturation in the flow cell. Importantly, the biofilm phenotype could be complemented by expressing the wild-type gene from a plasmid.

thumbnail

Figure 5. Flow cell biofilm formation of graS and imp mutants in different strain backgrounds.

S. aureus strains SH1000 (A) and LAC* (B), and graS and imp mutations in each strain, were grown in a flow cell apparatus for two days. A z series of images was obtained with CLSM, reconstructed with Volocity software, and each side of a grid square is 20 µm in the image reconstruction. The addition of a complementing plasmid containing either the graRS or imp genes is shown in the last column.

doi:10.1371/journal.pone.0010146.g005

To address potential issues of strain-to-strain variation, the graS and imp transposon insertions were transduced into a CA-MRSA isolate called LAC* (erythromycin sensitive variant of LAC, see Materials and Methods). The LAC* strain is a member of the USA300 lineage [28], and previous studies have demonstrated that the strain is a robust biofilm former on diverse surfaces [9], [10]. The graS and imp insertions were transduced into the LAC* strain and growth in a flow cell biofilm model was compared to wild type (Fig. 5B). Similar to the SH1000 genetic background, the LAC* graS and imp mutants were defective in biofilm maturation, and again the biofilm phenotype could be complemented through plasmid expression. These results demonstrate that the graS and imp mutant biofilm phenotypes are consistent across multiple in vitro models of biofilm maturation and the phenotype is conserved in a clinical isolate.

Discussion

The ability of S. aureus to form biofilms is an important virulence factor in many persistent infections [3], [29]. Recently, it has been shown that some S. aureus clinical isolates do not require polysaccharide production to form a biofilm [1], [7], [9], [10]. To the best of our knowledge, this type of polysaccharide-independent biofilm (termed PIA-independent) has not been systematically investigated through transposon mutagenesis. We created and screened a mariner transposon mutant library in a PIA-independent strain and identified 31 insertions that displayed reproducible biofilm defects. Our screen was large but not saturating, as some loci known to be biofilm deficient in the SH1000 background, such as sarA and dltA, were not identified (data not shown).

To understand the 31 identified biofilm mutants in more detail, various aspects of biofilm matrix production and breakdown were investigated. With the known importance of proteinaceous material in the matrix [5], [6], [7], we examined the contribution of secreted proteases to the biofilm phenotype. Almost half of the mutant pool displayed an increased level of protease activity in culture supernatants (Fig. 1), and the biofilm phenotype of this subset could be mostly restored with the general inhibitor α2-macroglobulin (Fig. 2). This finding suggests a critical and perhaps underappreciated role of the extracellular proteases in biofilm maturation. In recent reports, high levels of protease activity have been linked to biofilm phenotypes in sigB and sarA mutants [10], [20], [21], and this activity has an additional role in biofilm dispersal [5]. Numerous potential targets for the proteases have been investigated, including surface adhesins BAP [21], [30], Spa [12], SasG [14], [15], FnBPA, and FnBPB [13], and the murein hydrolyases have also been suggested as a target [10].

Along with proteins in the S. aureus biofilm matrix, growing evidence indicates eDNA is an important matrix material [8], [9], [23]. Microarray data has indicated that the nuc gene is down-regulated during biofilm formation as compared to planktonic cultures [1], suggesting a disregulation of nuclease could lead to defects in biofilm formation. Transposon insertions in rsbU, rsbV, and imp genes resulted in increased nuclease activity in culture supernatants (Fig. 3). Insertions in rsbU and rsbV eliminate SigB activity [10], and sigB mutants are known to have increased nuc gene expression [27]. However, the significance of this phenotype is not clear as higher levels of protease activity have been linked to the biofilm phenotype [10], which is supported by the recovery of the rsbU and rsbV mutants with α2-macroglobulin (Fig. 2). Increased nuclease activity may be a factor in the imp mutant biofilm phenotype, but further analysis will be necessary to demonstrate a connection.

In order to release eDNA into the environment, S. aureus cells lyse and are able to incorporate the eDNA into the biofilm matrix [8], [23]. This autolysis event is a complex and tightly controlled process that involves regulation of holins, antiholins and murein hydrolase activity [31]. In the pool of biofilm-defective mutants, seven displayed altered autolysis levels compared to the isogenic parent. Of this subset, four displayed a reduction in autolysis activity, suggesting they failed to release adequate amounts of eDNA as biofilm matrix material. As anticipated, mutations in the major murein hydrolase, atlA, possessed low levels of autolytic activity. Mutants in atlA in S. aureus and Staphylococcus epidermidis (called atlE) have previously been shown to have defects in biofilm formation [17], [32], and the expression of atlA is known to increase during biofilm growth [33]. In S. epidermidis, the reduction in biofilm formation by atlE mutants has been attributed to the ability of this protein to bind vitronectin, an abundant glycoprotein found in serum [32]. Considering that no serum was present in our biofilm growth conditions, we speculate that the biofilm defect in S. aureus atlA mutants is due to decreased autolysis and DNA release.

Three other transposon insertions in an osmoprotectant transporter (OpuD homolog), purA, and a hypothetical membrane protein (mutant 123 D2) also displayed decreased autolysis. The OpuD-like protein has sequence similarity to a glycine-betaine osmoprotectant transporter that is necessary for biofilm formation in Vibrio cholerae [34]. The purA gene encodes for a putative adenylosuccinate synthetase that is upregulated during biofilm growth [1], and the purA knockout displayed the lowest level of autolysis of tested mutants (Fig. 4). Studies in Bacillus cereus revealed that a purA mutant is unable to effectively form biofilms or release eDNA, and the expression of purA is upregulated in a biofilm versus planktonically grown cells [35].

In contrast, transposon insertions in the genes fmtA, graS, and imp displayed an overall increase in autolysis (Fig. 4). FmtA is an autolysis and methicillin-resistance related protein that was identified in screens for increased oxacillin sensitivity in the presence of detergent [36]. Biochemical analysis demonstrated that FmtA is a penicillin-binding protein that is resistant to β-lactam inactivation [37], and the protein is known to localize to the membrane and affect cell wall structure [38]. A previous transposon screen for biofilm defective mutants in a PIA-dependent strain identified the fmtA gene three different times [18], suggesting that the FmtA protein is important across both PIA-dependent and independent mechanisms of biofilm formation. The observation that both mutants that decrease autolysis (altA, opuD, purA, 123 D2) and increase autolysis (fmtA, graS, imp) have biofilm defects suggests that the timing of autolysis and the accumulation of eDNA in the biofilm matrix may be critical in biofilm development.

A transposon insertion in graS of the graRS (glycopeptide resistance-associated) two-component regulatory system also displayed an increase in autolysis (Fig. 4) and a pronounced biofilm defect in both laboratory and CA-MRSA strains (Fig. 5). Mutations in graRS are known to make S. aureus hyper-susceptible to vancomycin [39], cationic antimicrobial peptides [40], [41], and cell lysis inducing agents [19], [39], findings which correlate with our observed increase in graS mutant autolysis. Genes encoding proteins for D-alanylation of teichoic acids (dlt operon) and atlA are induced by the GraRS system, and graRS mutants are reported to have a microtiter-based biofilm defect [19]. The increase in graS mutant autolysis over wild-type levels did not occur until late in the time course (>24 hrs, Fig. 4), with the most significant increase after 36 hrs. In the flow cell biofilms (Fig. 5), most S. aureus attachment and preliminary biofilm formation is occurring in the first 24 hr, suggesting that the reduced dlt and atlA expression are the major contributors to the graS mutant biofilm phenotype.

The final mutant that displayed increased autolysis was a transposon insertion in the imp gene, which is predicted to encode for an inositol monophosphatase, an enzyme capable of dephosphorylating inositol phosphate to inositol. Mutations in imp displayed nuclease overproduction (Fig. 3) and a pronounced biofilm defect (Fig. 5) that was conserved in a CA-MRSA strain. Inositol is an important signaling molecule in eukaryotes, but its role in bacteria is not well understood [42]. The altered nuclease and autolysis levels suggest a potential regulatory role for the imp gene in S. aureus. Interestingly, an inositol monophosphatase mutant (suhB) was found in a search for biofilm defective mutants in Burkholderia cepacia [43], suggesting this gene may play an important role in biofilm formation in diverse bacterial species. Further analysis will be necessary to define the role of the imp gene in biofilm maturation and determine the significance of the observed nuclease and autolysis phenotypes.

Five remaining mutants did not fall into the categories of displaying increased protease or nuclease activity, or having an altered autolysis phenotype. The inactivated genes encode two potential membrane proteins (mutants 12 D3 and 46 H7), a glutamate transporter (gltT), a glutamate-1-semialdehyde-2,1-aminomutase​,and a glucose group IIA phosphotransferase protein. Microarray studies have demonstrated an upregulation of expression in gltT during PIA-dependent biofilm growth, potential evidence of a link between GltT and biofilms [44]. At this time the roles for these five genes and their encoded proteins in biofilm formation is unknown.

Overall, the work presented here confirms published reports and provides new insight into genetic loci required for PIA-independent biofilm formation. Over half of the biofilm defective mutants expressed high levels of extracellular protease activity, and a significant portion of the mutant pool either overproduced nuclease or had altered cell lysis phenotypes, indicating a major biofilm role for proteins and eDNA in the absence of exopolysaccharide. Moving forward, it will be important to assess how these various identified factors collaborate during the biofilm maturation mechanism.

Materials and Methods

Strains and growth conditions

The bacterial strains used in this study are described in Tables 1 and 2. Strains of Escherichia coli were grown in Luria-Bertani broth or Luria agar plates, and growth medium was supplemented with ampicillin (100 µg/ml) or chloramphenicol (10 µg/ml) as needed for maintenance of plasmids. Strains of S. aureus were grown in tryptic soy broth (TSB) or tryptic soy agar (TSA). For selection of chromosomal markers or maintenance of plasmids, S. aureus antibiotic concentrations were (in µg/ml) the following: chloramphenicol (Cam), 10; erythromycin (Erm), 10; and tetracycline (Tet), 5. All reagents were purchased from Fisher Scientific (Pittsburg, PA) and Sigma (St. Louis, MO) unless otherwise indicated.

thumbnail

Table 2. Strains and plasmids.

doi:10.1371/journal.pone.0010146.t002

Strain LAC was made Erm sensitive by serial passage in TSB in order to cure the strain of the native plasmid pUSA03 that confers Erm resistance [45]. A single colony was picked and saved as Erm sensitive strain AH1263, and hereafter this strain will be referred to as LAC*.

Recombinant DNA and genetic techniques

Restriction and modification enzymes were purchased from New England Biolabs (Beverly, MA). All DNA manipulations were performed in E. coli strain BW25141 [46]. Oligonucleotides were synthesized at Integrated DNA Technologies (Coralville, IA). Nonradioactive sequencing was performed at the DNA sequencing facility at the University of Iowa. Plasmids were transformed into S. aureus RN4220 by electroporation and moved to other strains using transduction by bacteriophage 80α as described previously [47], [48]. Chromosomal markers were moved between S. aureus strains using bacteriophage 80α or 11 transduction.

Generation and mapping of transposon mutants

SH1000 was transformed with plasmids pFA545 and pBursa, and mutagenesis was performed as described previously [10]. Transposon mutants with secondary agr defects were removed from the pool by testing for AIP-I production as described previously [49]. Mutants were banked in deep-well microtiter titer plates in TSB with 10% glycerol and stored at –80°C. Transposon insertion sites were mapped using arbitrary PCR [10].

Biofilm assays

Microtiter plate biofilms and flow cell biofilms were grown as described previously [5]. For culture media, microtiter biofilms were grown in 66% TSB supplemented with 0.2% glucose, and flow cell biofilms were grown in 2% TSB supplemented with 0.2% glucose. For protease inhibition in microtiter biofilms, cells were added to the plate with α2-macroglobulin (final concentration, 0.25 units/ml; Roche). Confocal scanning laser microscopy (CSLM) and image analysis was performed as described previously [5]. Biofilms were treated with 330 nM Syto9 (LIVE/DEAD BacLight Bacterial Viability Kit; Invitrogen, Carlsbad, CA) 15 min prior to visualization.

Protease and nuclease assays

Quantitative protease activity measurements were determined using Azocoll (Calbiochem, San Diego, CA) reagent as described previously [50]. Difco DNase test agar with methyl green (BD, Franklin Lakes, NJ) was used to screen biofilm mutants for altered nuclease production. Nuclease activity in culture supernatants was measured as described by Heins et. al [51].

Autolysis assay

To determine autolysis activity, overnight cultures of each strain harboring plasmid pAJ22 [52], were diluted to an OD at 600 nm of 0.1 in TSB (no antibiotic) and grown at 37°C shaking at 200 rpm. At various time points, supernatants from each culture were harvested by centrifugation. β-galactosidase activity in the supernatants was determined as described [53] using o-nitrophenyl-beta-d-galactopyranoside as the substrate and reported in Miller units [54].

Plasmid construction

pCM1.

Plasmid pCM1 was created to serve as a new chloramphenicol resistant S. aureus expression vector. This plasmid was constructed by moving the chloramphenicol acetyltransferase gene into plasmid pAH15 [55] and eliminating erythromycin resistance. The chloramphenicol acetyltransferase gene was amplified using oligonucleotides CLM329: GTTGTTGCTCAGGTAAAGGAGGCATATCAAATGAAC and CLM330: GTTGTTTGATCATTATAAAAGCCAGTCATTAGGCCTATC and plasmid pAH5 [55] as template. The PCR product was digested with BclI and Bpu10I and ligated to pAH15 digested with the same enzymes to create pCM1.

pCM1-imp.

Plasmid pCM1-imp was created by cloning a 1081 base pair PCR product containing the imp gene and promoter region into pCM1 that had been restriction digested with HindIII and EcoRI. The oligonucleotides used to generate the imp PCR product were: inositolREVecoRI (5′-GAGGAATTCACTGGTTTTATATTGGCGCGTG-3′) and inositiolFORhindIII (5′-GAGAAGCTTTAGfAGTACCTCCTGTATAGTGT-3′). The resulting pCM1-imp plasmid has the imp gene with its native promoter controlling expression.

pCM1-graRS.

Plasmid pCM1-graRS was created by cloning a 1751 base pair PCR product containing the graRS genes without their native promoter into pCM1 that had been restriction digested with KpnI and EcoRI. The oligonucleotides used to generate the graRS PCR product were: graSkpn (5′-AAAAAAGGTACCGTTTAAAATGACAAATTTGTC-3′) and graRecoR1 (5′-AAAGAATTCTGATATTGGGTGATATGGATGC-3′). The resulting pCM1-graRS plasmid has the graRS genes with their expression driven by the sarA promoter located on pCM1.

Acknowledgments

We thank D. Missiakas for providing the mariner transposon plasmids and K. Bayles for providing plasmid pAJ22.

Author Contributions

Conceived and designed the experiments: BRB ARH. Performed the experiments: BRB MT AJR. Analyzed the data: BRB MT ARH. Contributed reagents/materials/analysis tools: BRB MT. Wrote the paper: BRB ARH.

References

  1. 1. Beenken KE, Dunman PM, McAleese F, Macapagal D, Murphy E, et al. (2004) Global gene expression in Staphylococcus aureus biofilms. J Bacteriol 186: 4665–4684.
  2. 2. Parsek MR, Greenberg EP (2005) Sociomicrobiology: the connections between quorum sensing and biofilms. Trends Microbiol 13: 27–33.
  3. 3. Parsek MR, Singh PK (2003) Bacterial biofilms: an emerging link to disease pathogenesis. Annu Rev Microbiol 57: 677–701.
  4. 4. del Pozo JL, Patel R (2007) The challenge of treating biofilm-associated bacterial infections. Clin Pharmacol Ther 82: 204–209.
  5. 5. Boles BR, Horswill AR (2008) agr-mediated dispersal of Staphylococcus aureus biofilms. PLoS Pathogens 4: e1000053.
  6. 6. Izano EA, Amarante MA, Kher WB, Kaplan JB (2008) Differential roles of poly-N-acetylglucosamine surface polysaccharide and extracellular DNA in Staphylococcus aureus and Staphylococcus epidermidis biofilms. Appl Environ Microbiol 74: 470–476.
  7. 7. O'Neill E, Pozzi C, Houston P, Smyth D, Humphreys H, et al. (2007) Association between methicillin susceptibility and biofilm regulation in Staphylococcus aureus isolates from device-related infections. J Clin Microbiol 45: 1379–1388.
  8. 8. Mann EE, Rice KC, Boles BR, Endres JL, Ranjit D, et al. (2009) Modulation of eDNA release and degradation affects Staphylococcus aureus biofilm maturation. PLoS ONE 4: e5822.
  9. 9. Lauderdale KJ, Boles BR, Morcuende J, Horswill AR (2010) Biofilm dispersal of community-associated methicillin-resistant Staphylococcus aureus on orthopaedic implant material. Journal of Orthopedic Research 28: 55–61.
  10. 10. Lauderdale KJ, Boles BR, Cheung AL, Horswill AR (2009) Interconnections between Sigma B, agr, and proteolytic activity in Staphylococcus aureus biofilm maturation. Infect Immun 77: 1623–1635.
  11. 11. Cucarella C, Solano C, Valle J, Amorena B, Lasa I, et al. (2001) Bap, a Staphylococcus aureus surface protein involved in biofilm formation. J Bacteriol 183: 2888–2896.
  12. 12. Merino N, Toledo-Arana A, Vergara-Irigaray M, Valle J, Solano C, et al. (2009) Protein A-mediated multicellular behavior in Staphylococcus aureus. J Bacteriol 191: 832–843.
  13. 13. O'Neill E, Pozzi C, Houston P, Humphreys H, Robinson DA, et al. (2008) A novel Staphylococcus aureus biofilm phenotype mediated by the fibronectin-binding proteins, FnBPA and FnBPB. J Bacteriol 190: 3835–3850.
  14. 14. Conrady DG, Brescia CC, Horii K, Weiss AA, Hassett DJ, et al. (2008) A zinc-dependent adhesion module is responsible for intercellular adhesion in staphylococcal biofilms. Proc Natl Acad Sci U S A 105: 19456–19461.
  15. 15. Corrigan RM, Rigby D, Handley P, Foster TJ (2007) The role of Staphylococcus aureus surface protein SasG in adherence and biofilm formation. Microbiology 153: 2435–2446.
  16. 16. Bae T, Banger AK, Wallace A, Glass EM, Aslund F, et al. (2004) Staphylococcus aureus virulence genes identified by bursa aurealis mutagenesis and nematode killing. Proc Natl Acad Sci USA 101: 12312–12317.
  17. 17. Biswas R, Voggu L, Simon UK, Hentschel P, Thumm G, et al. (2006) Activity of the major staphylococcal autolysin Atl. FEMS Microbiol Lett 259: 260–268.
  18. 18. Tu Quoc PH, Genevaux P, Pajunen M, Savilahti H, Georgopoulos C, et al. (2007) Isolation and characterization of biofilm formation-defective mutants of Staphylococcus aureus. Infect Immun 75: 1079–1088.
  19. 19. Herbert S, Bera A, Nerz C, Kraus D, Peschel A, et al. (2007) Molecular basis of resistance to muramidase and cationic antimicrobial peptide activity of lysozyme in staphylococci. PLoS Pathog 3: e102.
  20. 20. Tsang LH, Cassat JE, Shaw LN, Beenken KE, Smeltzer MS (2008) Factors contributing to the biofilm-deficient phenotype of Staphylococcus aureus sarA mutants. PLoS ONE 3: e3361.
  21. 21. Marti M, Trotonda MP, Tormo-Mas MA, Vergara-Irigaray M, Cheung AL, et al. (2010) Extracellular proteases inhibit protein-dependent biofilm formation in Staphylococcus aureus. Microbes Infect 12: 55–64.
  22. 22. Thomas VC, Thurlow LR, Boyle D, Hancock LE (2008) Regulation of autolysis-dependent extracellular DNA release by Enterococcus faecalis extracellular proteases influences biofilm development. J Bacteriol 190: 5690–5698.
  23. 23. Rice KC, Mann EE, Endres JL, Weiss EC, Cassat JE, et al. (2007) The cidA murein hydrolase regulator contributes to DNA release and biofilm development in Staphylococcus aureus. Proc Natl Acad Sci U S A 104: 8113–8118.
  24. 24. Whitchurch CB, Tolker-Nielsen T, Ragas PC, Mattick JS (2002) Extracellular DNA required for bacterial biofilm formation. Science 295: 1487.
  25. 25. Guiton PS, Hung CS, Kline KA, Roth R, Kau AL, et al. (2009) Contribution of autolysin and Sortase a during Enterococcus faecalis DNA-dependent biofilm development. Infect Immun 77: 3626–3638.
  26. 26. Moscoso M, Garcia E, Lopez R (2006) Biofilm formation by Streptococcus pneumoniae: role of choline, extracellular DNA, and capsular polysaccharide in microbial accretion. J Bacteriol 188: 7785–7795.
  27. 27. Bischoff M, Dunman P, Kormanec J, Macapagal D, Murphy E, et al. (2004) Microarray-based analysis of the Staphylococcus aureus sigmaB regulon. J Bacteriol 186: 4085–4099.
  28. 28. Voyich JM, Braughton KR, Sturdevant DE, Whitney AR, Said-Salim B, et al. (2005) Insights into mechanisms used by Staphylococcus aureus to avoid destruction by human neutrophils. J Immunol 175: 3907–3919.
  29. 29. Costerton JW (2005) Biofilm theory can guide the treatment of device-related orthopaedic infections. Clin Orthop Relat Res. pp. 7–11.
  30. 30. Trotonda MP, Manna AC, Cheung AL, Lasa I, Penades JR (2005) SarA positively controls bap-dependent biofilm formation in Staphylococcus aureus. J Bacteriol 187: 5790–5798.
  31. 31. Rice KC, Bayles KW (2008) Molecular control of bacterial death and lysis. Microbiol Mol Biol Rev 72: 85–109.
  32. 32. Heilmann C, Hussain M, Peters G, Gotz F (1997) Evidence for autolysin-mediated primary attachment of Staphylococcus epidermidis to a polystyrene surface. Mol Microbiol 24: 1013–1024.
  33. 33. Brady RA, Leid JG, Camper AK, Costerton JW, Shirtliff ME (2006) Identification of Staphylococcus aureus proteins recognized by the antibody-mediated immune response to a biofilm infection. Infect Immun 74: 3415–3426.
  34. 34. Kapfhammer D, Karatan E, Pflughoeft KJ, Watnick PI (2005) Role for glycine betaine transport in Vibrio cholerae osmoadaptation and biofilm formation within microbial communities. Appl Environ Microbiol 71: 3840–3847.
  35. 35. Vilain S, Pretorius JM, Theron J, Brozel VS (2009) DNA as an adhesin: Bacillus cereus requires extracellular DNA to form biofilms. Appl Environ Microbiol 75: 2861–2868.
  36. 36. Komatsuzawa H, Sugai M, Ohta K, Fujiwara T, Nakashima S, et al. (1997) Cloning and characterization of the fmt gene which affects the methicillin resistance level and autolysis in the presence of triton X-100 in methicillin-resistant Staphylococcus aureus. Antimicrob Agents Chemother 41: 2355–2361.
  37. 37. Fan X, Liu Y, Smith D, Konermann L, Siu KW, et al. (2007) Diversity of penicillin-binding proteins. Resistance factor FmtA of Staphylococcus aureus. J Biol Chem 282: 35143–35152.
  38. 38. Komatsuzawa H, Ohta K, Labischinski H, Sugai M, Suginaka H (1999) Characterization of fmtA, a gene that modulates the expression of methicillin resistance in Staphylococcus aureus. Antimicrob Agents Chemother 43: 2121–2125.
  39. 39. Meehl M, Herbert S, Gotz F, Cheung A (2007) Interaction of the GraRS two-component system with the VraFG ABC transporter to support vancomycin-intermediate resistance in Staphylococcus aureus. Antimicrob Agents Chemother 51: 2679–2689.
  40. 40. Kraus D, Herbert S, Kristian SA, Khosravi A, Nizet V, et al. (2008) The GraRS regulatory system controls Staphylococcus aureus susceptibility to antimicrobial host defenses. BMC Microbiol 8: 85.
  41. 41. Li M, Cha DJ, Lai Y, Villaruz AE, Sturdevant DE, et al. (2007) The antimicrobial peptide-sensing system aps of Staphylococcus aureus. Mol Microbiol 66: 1136–1147.
  42. 42. Roberts MF (2006) Inositol in bacteria and archaea. Subcell Biochem 39: 103–133.
  43. 43. Huber B, Riedel K, Kothe M, Givskov M, Molin S, et al. (2002) Genetic analysis of functions involved in the late stages of biofilm development in Burkholderia cepacia H111. Mol Microbiol 46: 411–426.
  44. 44. Resch A, Rosenstein R, Nerz C, Gotz F (2005) Differential gene expression profiling of Staphylococcus aureus cultivated under biofilm and planktonic conditions. Appl Environ Microbiol 71: 2663–2676.
  45. 45. 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.
  46. 46. Datsenko KA, Wanner BL (2000) One-step inactivation of chromosomal genes in Escherichia coli K-12 using PCR products. Proc Natl Acad Sci U S A 97: 6640–6645.
  47. 47. Novick RP (1991) Genetic systems in staphylococci. Methods Enzymol 204: 587–636.
  48. 48. Schenk S, Laddaga RA (1992) Improved method for electroporation of Staphylococcus aureus. FEMS Microbiol Lett 73: 133–138.
  49. 49. Malone CL, Boles BR, Horswill AR (2007) Biosynthesis of Staphylococcus aureus autoinducing peptides by using the Synechocystis DnaB mini-intein. Appl Environ Microbiol 73: 6036–6044.
  50. 50. Fournier B, Hooper DC (2000) A new two-component regulatory system involved in adhesion, autolysis, and extracellular proteolytic activity of Staphylococcus aureus. J Bacteriol 182: 3955–3964.
  51. 51. Heins JN, Suriano JR, Taniuchi H, Anfinsen CB (1967) Characterization of a nuclease produced by Staphylococcus aureus. J Biol Chem 242: 1016–1020.
  52. 52. O'Neill AJ, Miller K, Oliva B, Chopra I (2004) Comparison of assays for detection of agents causing membrane damage in Staphylococcus aureus. J Antimicrob Chemother 54: 1127–1129.
  53. 53. Steinmoen H, Knutsen E, Havarstein LS (2002) Induction of natural competence in Streptococcus pneumoniae triggers lysis and DNA release from a subfraction of the cell population. Proc Natl Acad Sci U S A 99: 7681–7686.
  54. 54. Miller JH (1972) Experiments in Molecular Genetics. Cold Spring Harbor, NY: Cold Spring Harbor Laboratory Press.
  55. 55. Malone CL, Boles BR, Lauderdale KJ, Thoendel M, Kavanaugh JS, et al. (2009) Fluorescent reporters for Staphylococcus aureus. J Microbiol Methods 77: 251–260.
  56. 56. Horsburgh MJ, Aish JL, White IJ, Shaw L, Lithgow JK, et al. (2002) sigmaB modulates virulence determinant expression and stress resistance: characterization of a functional rsbU strain derived from Staphylococcus aureus 8325-4. J Bacteriol 184: 5457–5467.