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Antimicrobial Agents and Chemotherapy, October 2004, p. 3743-3748, Vol. 48, No. 10
0066-4804/04/$08.00+0     DOI: 10.1128/AAC.48.10.3743-3748.2004
Copyright © 2004, American Society for Microbiology. All Rights Reserved.

Acquired Bacitracin Resistance in Enterococcus faecalis Is Mediated by an ABC Transporter and a Novel Regulatory Protein, BcrR

Janet M. Manson, Stefanie Keis, John M. B. Smith, and Gregory M. Cook*

Department of Microbiology and Immunology, Otago School of Medical Sciences, University of Otago, Dunedin, New Zealand

Received 26 January 2004/ Returned for modification 19 April 2004/ Accepted 24 May 2004


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ABSTRACT
 
Bacitracin resistance (bacitracin MIC, ≥256 µg ml–1) has been reported in Enterococcus faecalis, and in the present study we report on the genetic basis for this resistance. Mutagenesis was carried out with transposon Tn917 to select for E. faecalis mutants with decreased resistance to bacitracin. Two bacitracin-sensitive mutants (MICs, 32 µg ml–1) were obtained and Tn917 insertions were mapped to genes designated bcrA and bcrB. The amino acid sequences of BcrA (ATP-binding domain) and BrcB (membrane-spanning domain) are predicted to constitute a homodimeric ATP-binding cassette (ABC) transporter, the function of which is essential for bacitracin resistance in E. faecalis. The bcrA and bcrB genes were organized in an operon with a third gene, bcrD, that had homology to undecaprenol kinases. Northern analysis demonstrated that bcrA, bcrB, and bcrD were transcribed as a polycistronic message that was induced by increasing concentrations of bacitracin but not by other cell wall-active antimicrobials (e.g., vancomycin). Upstream of the bcrABD operon was a putative regulatory gene, bcrR. The bcrR gene was expressed constitutively, and deletion of bcrR resulted in a bacitracin-sensitive phenotype. No bcrABD expression was observed in a bcrR mutant, suggesting that BcrR is an activator of genes essential for bacitracin resistance (i.e., bcrABD). The bacitracin resistance genes were found to be located on a plasmid that transferred at a high frequency to E. faecalis strain JH2-2. This report represents the first description of genes that are essential for acquired bacitracin resistance in E. faecalis.


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INTRODUCTION
 
Bacitracin is an antimicrobial that comprises a mixture of high-molecular-weight polypeptides produced by the organism Bacillus licheniformis. Bacitracin works by binding to and sequestering the undecaprenol pyrophosphate (UPP) carrier in the bacterial cytoplasmic membrane (32). During the synthesis and transport of peptidoglycan monomer units, undecaprenol monophosphate (UP) is phosphorylated to UPP. The UPP must be converted back to UP by the membrane-bound pyrophosphatase to enable transport of further subunits (10). Binding of bacitracin prevents the recycling of UPP and therefore causes disruption of cell wall synthesis (31, 32, 33). Bacitracin is used widely in topical applications in human medicine, and its oral use for the control of vancomycin-resistant enterococci has been suggested (25). Bacitracin is also used extensively for prophylaxis and therapy in food animals, particularly in broiler chicken production.

A number of mechanisms of bacitracin resistance have been reported in bacteria (2, 4, 5, 24, 26, 28, 34). In the bacitracin-producing organism B. licheniformis, resistance is encoded by the bcrABC genes, which encode a putative heterodimeric ATP-binding cassette (ABC) transporter that has been proposed to mediate the active efflux of bacitracin (24, 28). Homologues of this transporter have been identified in Bacillus subtilis (26) and Streptococcus mutans (34). A second recognized mechanism of bacitracin resistance is the overproduction of undecaprenol kinase (4). This enzyme converts undecaprenol to UP, increasing the amount of lipid carrier present in the cell. It is proposed that up-regulation of this enzyme increases the levels of UP, thus overcoming the sequestration of UPP by bacitracin and increasing the resistance of the organism to bacitracin. Other reported mechanisms of bacitracin resistance are proposed to be mediated by a membrane-associated phospholipid phosphatase in B. subtilis (2, 5, 27). In S. mutans, it has been shown that inactivation of the rgpA gene, which is involved in glucose-rhamnose polysaccharide formation in the cell wall, results in increased bacitracin sensitivity (34).

In many bacterial genera, bacitracin resistance has been detected phenotypically (1, 8, 19, 21; J. M. Manson, S. Keis, J. M. B. Smith, and G. M. Cook, Abstr. 43rd Intersci. Conf. Antimicrob. Agents Chemother., abstr. C2-1490, 2003); however, the mechanism(s) of resistance remains unclear. With enterococci, for example, studies on bacitracin susceptibility and resistance are limited, and no set parameters have been defined to determine the breakpoint for resistant and susceptible isolates. Zinc bacitracin is the most widely used antimicrobial in poultry in New Zealand, and a survey of 382 New Zealand poultry enterococcal isolates found that bacitracin MICs were ≥256 µg ml–1 for 98% of the isolates (Manson et al., 43rd ICAAC). Despite the high percentage of resistance to bacitracin in some enterococcal isolates, the genes responsible for resistance in enterococci are unknown.

In this communication, we report on the isolation and characterization of acquired genes encoding high-level bacitracin resistance in Enterococcus faecalis AR01/DGVS. We propose that bacitracin resistance in this strain is mediated by a homodimeric ABC transporter that actively pumps bacitracin from the cell. The expression of this transporter is under the control of a novel regulatory protein, BcrR.


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MATERIALS AND METHODS
 
Bacterial strains, plasmids, and cultivation conditions. The bacterial strains and plasmids used in this study are listed in Table 1. Escherichia coli DH10B was routinely grown in Luria-Bertani (LB) broth or LB agar (1.4% [wt/vol]) at 37°C or, when harboring pTV1-OK, at 28°C. Enterococcus strains were grown without agitation in brain heart infusion (BHI) broth or BHI agar (1.4% [wt/vol]). All E. faecalis strains with the exception of strains carrying pTV1-OK were incubated at 37°C; strains carrying pTV1-OK were grown at 28°C. Antibiotics supplemented in the media included ampicillin (50 µg ml–1), kanamycin (50 µg ml–1 for E. coli and 500 µg ml–1 for Enterococcus), erythromycin (10 µg ml–1 for Enterococcus), chloramphenicol (50 µg ml–1 for E. coli and 20 µg ml–1 for Enterococcus), and tetracycline (10 µg ml–1).


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  		TABLE 1. Bacterial strains and plasmids used in this study

Antibiotic sensitivity tests and plasmid curing. Isolates were assayed for resistance to bacitracin (50,000 IU g–1; Aldrich Chemical Co.) in Mueller-Hinton broth by the broth microdilution technique, according to NCCLS guidelines (23). The MICs were the highest concentrations showing complete inhibition of growth. Sensitivities to tetraphenylphosphonium ion, rhodamine 123, zinc sulfate, nisin, valinomycin, and ethidium bromide were also determined by the broth microdilution method. Curing of plasmid pJM01 was carried out by subculturing an overnight culture of E. faecalis AR01/DG grown in BHI broth at 37°C for 5 days to obtain E. faecalis AR01/DG45.

Tn917 mutagenesis with pTV1-OK. Independent pools of Tn917 insertions in the host genomic DNA were generated by using a temperature switch from 28 to 44°C. An overnight culture of AR01/DGVS containing pTV1-OK was grown in BHI broth plus kanamycin (500 µg ml–1) at 28°C. This culture was subcultured into fresh prewarmed BHI broth containing erythromycin (0.04 µg ml–1) at 44°C and incubated overnight. Tn917 mutants were isolated by plating the overnight cultures onto BHI agar plates containing 10 µg of erythromycin ml–1. Colonies that were erythromycin resistant and kanamycin sensitive were screened for bacitracin sensitivity on BHI agar containing 100 µg of bacitracin ml–1. The presence of Tn917 in the bacitracin-sensitive mutants was confirmed by probing HindIII-digested genomic DNA with radioactively labeled pTV1-OK DNA.

Mapping of transposon inserts. To map the site of the Tn917 insertion in mutants DGM2 and DGM4, an inverse PCR with Tn917-derived primers ErmP2 (5'-TACAAATTCCTCGTAGGC-3') and Sau3A1F (5'-TCCGTTCCTTTTTCATAGTTCC-3') (11) was performed. Total DNA from the Tn917 mutants was digested with Sau3A1 and self-ligated. Self-ligated DGM4 DNA was subjected to inverse PCR with 0.5 U of Taq DNA polymerase (Roche), 1.25 µl of dimethyl sulfoxide, and the PCR program described previously (14). Inverse PCR of DGM2 DNA was performed by use of an Expand Long Template PCR system (Roche) and the conditions recommended by the manufacturer. Amplification consisted of one cycle at 94°C for 2 min and 10 cycles at 94°C for 10 s, 60°C for 30 s, and 68°C for 4 min. This was followed by 20 cycles at 94°C for 10 s, 60°C for 30 s, and 68°C for 4 min (with the elongation time increased by 10 s per cycle) and a final cycle at 68°C for 7 min. A 2.5-kb PCR product was obtained from the Sau3A1-digested DGM4 DNA, while the PCR product amplified from DGM2 DNA was 3.5 kb. The PCR products were sequenced with Tn917-specific primers ErmP2 and Sau3A1F (11).

Genomic DNA extraction, transformation, and genetic techniques. E. faecalis chromosomal DNA was obtained by a previously described method (21). Transformation of E. faecalis cells grown in the presence of glycine was performed as described by Shepard and Gilmore (30). Transformants of AR01/DGVS containing pTV1-OK were selected on SR agar (30) containing 500 µg of kanamycin ml–1 at 28°C. Other DNA manipulations were carried out by standard procedures (29). Purified plasmid DNA was prepared with a QIAprep spin miniprep kit (Qiagen) for high-copy-number plasmid extraction or a plasmid midi kit (Qiagen) for low-copy-number vectors. Gel-extracted DNA was prepared by use of a Qiaex II gel extraction kit (Qiagen). Restriction endonucleases, ligases, and polymerases were used according to the instructions of the manufacturer. PCRs were performed in accordance with the instructions of the manufacturer by using the PCR program described previously (14). The primer sequences and specificities used in this study are as follows: primers bcrBF (5'-AAAGAAACCGACTGCTGATA-3') and bcrBR (5'-GCTTACTTGTATAGCAGAGA-3') for bcrB, primers bcrDF (5'-AGGATTCGGCCGAATGGCACTTGATTTTAT-3') and bcrDR 5'-GTTTCTTCGCGAAATTGCCGTTATAAGTAA-3' for bcrD, and primers bcrRF (5'-AACAAACAGGGAGCGGCCGCATGGAATTTA-3') and bcrRR (5'-TGATGTTCGCGATTTCATTCCCATCTGCTT-3') for bcrR. Radiolabeled PCR products and plasmids were prepared by incorporation of [{alpha}-32P]dCTP-labeled deoxynucleotides (Amersham) by using Ready-To-Go DNA labeling beads (Amersham). Southern transfer and hybridization were performed as described previously (21).

Nucleotide sequencing and sequence analysis. PCR products and plasmids were sequenced directly. Sequencing reactions were carried out with a PRISM ready reaction DyeDeoxy terminator cycle sequencing kit (Applied Biosystems Inc., Warrington, United Kingdom) and a model ABI377 automated DNA sequencer (Applied Biosystems). The nucleotide sequences were assembled by using the Seqman program (DNASTAR, Inc.). Sequence analyses were carried out with Editseq software (DNASTAR, Inc.) for Apple Macintosh computers and the programs BLASTN, BLASTP, and BLASTX (National Center for Biotechnology Information, Los Alamos, N. Mex.), available via the Internet. The GeneMark and GeneMark.hmm software programs were used to predict the locations of gene boundaries (3, 18).

Cloning of bcr genes and plasmid construction. The bcr genes of E. faecalis AR01/DGVS were cloned as a 4.7-kb EcoRI fragment into pUC8, creating plasmid p2H7. The resulting insert in p2H7 was sequenced. To enable complementation, plasmid pAMBcr1 was constructed by ligating the 4.7-kb EcoRI fragment from p2H7 into the shuttle vector pAM401. To determine the role of bcrR, plasmid pAMBcr2 was constructed by digesting p2H7 with SspI and EcoRV (Fig. 1) and ligating the resulting 3.6-kb fragment with a truncated bcrR gene into pAM401. To examine the importance of bcrD in bacitracin resistance, plasmid pAMBcr3 was created by digesting p2H7 with EcoRI and NdeI, thereby excising the majority of the bcrD gene. This 3.2-kb fragment was ligated into pAM401. To express the bcrD gene separately from the other bacitracin resistance genes, the entire coding sequence of bcrD was amplified by PCR with primers bcrDF and bcrDR (see above). The amplified fragment was digested with EagI and NruI and inserted between the corresponding sites of the pMGS100 plasmid to obtain pMGSBcr4.



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  		FIG. 1. Organization and restriction map of the bcr region in E. faecalis AR01/DGVS. Open arrows indicate the positions of ORFs. The restriction sites and fragments used to generate further constructs are shown. PCR products and probes are indicated by thick black lines, and transcriptional terminators are indicated by circles on stems. The Tn917 insertion sites in bacitracin-sensitive mutants DGM2 and DGM4 are represented by triangles.

Isolation of RNA and Northern hybridization. Total RNA was isolated from cells grown to an optical density at 600 nm (OD600) of 0.6 in BHI broth, with or without antibiotics, following the instructions of the manufacturer of the RNeasy kit (Qiagen). To analyze the effect of BcrR on bcrABD expression in JH2-2 cells containing either pAMBcr1 (bcrR and bcrABD) or pAMBcr2 (bcrABD), cells were grown to an OD600 of 0.6 in BHI broth containing 20 µg of chloramphenicol ml–1 and total RNA was extracted (under noninducing conditions). Cells were also grown in BHI broth containing 20 µg of chloramphenicol ml–1 to an OD600 of 0.6 and then challenged by the addition of 256 µg of bacitracin ml–1 with further incubation at 37°C for 1 h. For experiments involving ZnSO4, cells (strain AR01/DGVS) were grown in medium containing 6 mM ZnSO4 to an OD600 of 0.6 and total RNA was extracted. For vancomycin, cells were also grown in the absence of antimicrobials to an OD600 of 0.6, harvested, resuspended in broth containing either no vancomycin or 256 µg of vancomycin ml–1, and incubated at 37°C for 1 h before RNA extraction. Purified RNA samples were either used immediately or frozen at –80°C. The RNA was quantified with a NanoDrop spectrophotometer. Northern blot analysis was carried out as described by Keis et al. (15). A 0.24- to 9.5-kb RNA ladder (Gibco BRL) was used as a standard.

Transfer experiments and PFGE. Transfer experiments were performed in broth, as described by Christie et al. (7), with E. faecalis JH2-2 (13) as the recipient strain and E. faecalis AR01/DGVS as the donor strain. Transconjugants were selected on BHI agar containing bacitracin (100 µg ml–1), rifampin (50 µg ml–1), and fusidic acid (25 µg ml–1). Genomic DNA embedded in agarose was prepared and digested with I-CeuI and SmaI, as described previously (21). Pulsed-field gel electrophoresis (PFGE) was performed by contour-clamped homogeneous electric field electrophoresis with a CHEF-DRIII system (Bio-Rad Laboratories). Gels were run at 6 V/cm and 14°C at an included angle of 120° on a 1.2% agarose gel (Amersham), with pulse times of 5 to 25 s for 22 h.

Nucleotide sequence accession number. The DNA sequence of the 4,702-bp EcoRI fragment encoding the bacitracin resistance genes bcrA, bcrB, bcrD, and bcrR has been deposited in GenBank under accession number AY496968.


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RESULTS AND DISCUSSION
 
Identification and characterization of bacitracin resistance genes in E. faecalis. In order to elucidate the genetic basis for bacitracin resistance in enterococci, we chose to study a previously described bacitracin-resistant (MIC, ≥256 µg ml–1) E. faecalis isolate, AR01/DG (20). To enable the use of pTV1-OK (which carries an erythromycin resistance gene) as a mutagenesis vector, strain AR01/DG was subcultured in the absence of antibiotics to cure the strain of plasmid pJM02 (20). This endogenous plasmid contains the vanA and ermB genes, responsible for vancomycin and erythromycin resistance, respectively, in this isolate (20). Importantly, curing of plasmid pJM02 did not affect the bacitracin MIC for this strain. The resulting strain, designated AR01/DGVS (bacitracin MIC, ≥256 µg ml–1), was transformed with pTV1-OK, and transposon mutagenesis was carried out to identify Tn917 insertional mutants with a bacitracin-sensitive phenotype. For the purpose of this communication, bacitracin sensitivity is defined as an MIC ≤32 µg ml–1.

In total, 8,000 Tn917 insertion mutants of strain AR01/DGVS were screened for their ability to grow on BHI agar containing 100 µg of bacitracin ml–1. This concentration of bacitracin was chosen as it was approximately threefold greater than the intrinsic bacitracin MIC of 32 µg ml–1 noted for JH2-2. Two bacitracin-sensitive mutants (MICs, 32 µg ml–1) were isolated and designated DGM2 and DGM4, and Southern hybridization confirmed that the Tn917 insertions were at different genetic loci (data not shown). Inverse PCR was used to determine the sequence flanking the left variable arm of Tn917, and the DNA sequence obtained from DGM2 was found to have homology to BcrB from B. licheniformis, which encodes a membrane-bound permease which is proposed to be involved in the efflux of bacitracin from the cell (28). Translated DNA from the PCR product amplified from DGM4 was found to have homology to BcrA from B. licheniformis, which encodes the bacitracin efflux ABC transporter BcrABC (28).

To further characterize the bacitracin-sensitive mutants and examine the specificity of the ABC transporter, the profiles of their susceptibilities to several cationic inhibitors were tested. No differences in susceptibilities to tetraphenylphosphonium ion, zinc sulfate, rhodamine 123, valinomycin, nisin, or ethidium bromide were observed between bacitracin-resistant parent strain AR01/DGVS and bacitracin-sensitive mutants DGM2 and DGM4 (data not shown).

Southern hybridization analysis of EcoRI-digested DNA of AR01/DGVS showed that bcrA is present on a 4.7-kb EcoRI fragment. This DNA fragment was cloned into pUC8 to create plasmid p2H7 and was sequenced by using synthetic oligonucleotide primers. By using GeneMark software, it was found that the 4,702-bp insert in p2H7 had four identifiable open reading frames (ORFs) (Fig. 1). The four ORFs were oriented in the same direction and were designated bcrR (615 bp), bcrA (927 bp), bcrB (750 bp), and bcrD (831 bp). Tn917 insertions were mapped to position 2049 within bcrB in mutant DGM2 and position 3038 within bcrA in mutant DGM4 (Fig. 1). The bcrR gene was located 166 bp upstream from the bcrA gene, while the intergenic regions between bcrA and bcrB and between bcrB and bcrD were –7 and 0 bp, respectively, and appear to comprise an operon (Fig. 1).

The complete amino acid sequences of BcrA (ATP-binding domain) and BrcB (membrane-spanning domain) are predicted to constitute a homodimeric ABC transporter. ABC transporters have previously been reported to be responsible for bacitracin resistance in B. licheniformis, B. subtilis, and S. mutans (26, 28, 34). In these three systems it has been proposed that bacitracin is pumped from the cell via an efflux mechanism, but this has yet to be proven experimentally. BcrD was found to have 62% identity and 81% similarity to a putative undecaprenol kinase in Clostridium thermocellum. Undecaprenol kinases have previously been postulated to be involved in bacitracin resistance (4, 6, 16).

The BcrR protein exhibited homology to the xenobiotic response element (XRE) family of transcriptional regulators, with a conserved domain spanning positions 5 to 61. This family of regulatory proteins is poorly characterized, with only a hypothetical function assigned to most members. However, some regulators of this family have been found to regulate stress responses in bacteria (17). In addition to the helix-turn-helix N-terminal domain of BcrR, analysis of the secondary structure of BcrR revealed four probable transmembrane helices (positions 82 to 104, 127 to 149, 155 to 177, and 180 to 202) in the C-terminal domain of the protein, which could indicate that BcrR is anchored in the cytoplasmic membrane. These data suggest that BcrR may act as a sensor and a transducer of bacitracin availability. A precedent for such a mechanism has been documented for other membrane-localized activators, like ToxR, that bind to DNA and activate transcription (22). In contrast to ToxR, BcrR is predicted to be anchored in the membrane by four membrane-spanning helices, whereas ToxR has a single transmembrane domain (22). No sequence for an apparent sensor type of protein was present upstream or downstream of the bcrR gene, and no regulatory protein-binding signatures were discernible (data not shown). In all other bacitracin efflux ABC transporters characterized to date, regulation of the transporter is controlled by a two-component regulatory system comprising a sensor kinase and a response regulator (24, 26, 34).

Complementation of bacitracin-sensitive mutants. The 4,702-bp EcoRI fragment containing bcrR, bcrA, bcrB, and bcrD was cloned into the E. coli-E. faecalis shuttle vector pAM401 for complementation studies. The resulting plasmid, pAMBcr1 (Fig. 1), was electroporated into DGM2 (bcrB::Tn917) and DGM4 (bcrA::Tn917), and in both the transformants, the wild-type bacitracin-resistant phenotype was restored (MIC, ≥256 µg ml–1). To determine if pAMBcr1 contained all the genes necessary for bacitracin resistance, pAMBcr1 was electroporated into JH2-2 (bacitracin MIC, 32 µg ml–1). The bacitracin MIC for the resulting strain (JH2-2/pAMBcr1) was ≥256 µg ml–1, suggesting that only bcrR, bcrA, bcrB, and bcrD are necessary to convey bacitracin resistance to a susceptible host. To examine the function of bcrR and its putative role in regulation, a plasmid construct that contained a deletion of the 5' end of the bcrR gene (pAMBcr2) was made (Fig. 1). Plasmid p2H7 was digested with SspI and EcoRV, and the resulting 3,578-bp fragment was ligated into pAM401. Electroporation of this construct into JH2-2 resulted in a bacitracin MIC of 32 µg ml–1, indicating that bcrR is essential for the bacitracin resistance phenotype. To examine the role of the putative undecaprenol kinase (bcrD) in bacitracin resistance, two constructs were made. First, p2H7 was digested with EcoRI and NdeI, and the resulting 3.2-kb fragment was blunt ended and ligated into pAM401. This plasmid (pAMBcr3; Fig. 1) contained bcrR, bcrA, bcrB, and truncated bcrD. The effect of truncation of bcrD on bacitracin resistance was tested by transformation of pAMBcr3 into JH2-2. The bacitracin MIC for strain JH2-2/pAMBcr3 was ≥256 µg ml–1, suggesting that bcrD is not required for high-level bacitracin resistance, but we cannot rule out the possibility that a chromosomal copy or homologue of bcrD may exist in JH2-2 and may rescue the phenotype. Interestingly, the genome sequence of E. faecalis V583 reveals a homologue of this enzyme on the chromosome, and this may explain the low level of intrinsic resistance (MIC, 32 µg ml–1) seen in JH2-2 if indeed an undecaprenol kinase is present on the chromosome of this bacterium. To further examine the role of bcrD, the gene was amplified by PCR and ligated in frame into the expression vector pMGS100. This plasmid, pMGSBcr4, was electroporated into JH2-2, and the bacitracin MIC was found to be 32 µg ml–1, demonstrating that bcrD alone has no significant effect on bacitracin resistance levels in JH2-2.

Transcriptional analysis of the bcr genes. From the DNA sequence analysis, it appeared that bcrA, bcrB, and bcrD comprise an operon. Northern blot analysis was performed to determine whether these genes are cotranscribed. The results obtained by using RNA isolated from AR01/DGVS cells grown in the presence of various concentrations (10 to 256 µg ml–1) of bacitracin revealed a 2.7-kb hybridizing band with probes specific for bcrA and bcrD (Fig. 2A and B), indicating that bcrABD is transcribed as a polycistronic message. The levels of the bcrA and bcrD transcripts increased significantly as the concentration of bacitracin in which the cells were grown increased, suggesting that bcrABD is inducible (Fig. 2A and B). Northern analysis with a probe specific for bcrR revealed a 0.7-kb transcript which was expressed constitutively in either the presence or the absence of bacitracin (Fig. 2C). No bcrABD transcript was detected in bacitracin-sensitive mutants DGM2 and DGM4; however, the bcrR transcript was present in the two strains at the same levels as in the wild-type strain, demonstrating that mutation in either bcrA or bcrB has no effect on bcrR transcription (data not shown). To determine the effect of BcrR on bcrABD expression, strain JH2-2 containing either pAMBcr1 (bcrR and bcrABD) or pAMBcr2 (bcrABD) was grown to mid-log phase and then challenged with 256 µg of bacitracin ml–1. The 2.7-kb bcrABD transcript was observed only in JH2-2 containing bcrR, demonstrating that BcrR is required for activation of bcrABD transcription (Fig. 2D).



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  		FIG. 2. Northern blot analysis of total RNA from JH2-2 and AR01/DGVS probed with bcrA (A), bcrD (B), and bcrR (C). Lanes 1, JH2-2 (negative control); lanes 2, AR01/DGVS; lanes 3 to 6, AR01/DGVS grown with bacitracin at 10, 50, 100, and 256 µg ml–1, respectively; lanes M, molecular size standard (in kilobases; Gibco BRL). Arrowheads indicate the major transcript for each gene, sized at 2.7 kb for bcrA and bcrD and 0.7 kb for bcrR. Fainter nonspecific hybridization to 16S rRNA can be observed in panels A and B. (D) Northern analysis of total RNA from JH2-2 probed with bcrD. Lane 1, JH2-2 (negative control); lane 2, JH2-2/pAMBcr1; lane 3, JH2-2/pAMBcr2; lane 4, JH2-2/pAMBcr1 after 1 h of exposure to 256 µg of bacitracin ml–1; lane 5, JH2-2/pAMBcr2 after 1 h of exposure to 256 µg of bacitracin ml–1. Isolation of total RNA and Northern hybridization were carried out as described in Materials and Methods, with 10 µg of RNA loaded per lane.

To determine whether induction of the bcr genes was due to the presence of bacitracin or to another downstream effect of bacitracin activity (e.g., the buildup of cell wall precursors), we tested the effect of vancomycin on bcrABD expression. No induction of the bcrABD operon was seen by Northern blot analysis (data not shown), suggesting that the buildup of cell wall precursors is not involved in the induction of bcrABD expression. As bacitracin is present as a zinc salt, the possible role of zinc in the induction of the bcr genes was investigated. Again, no induction of the bcrB or bcrD gene was noted (data not shown).

Bacitracin resistance is transferable and plasmid borne in E. faecalis. To examine if bacitracin resistance was transferable, broth matings were carried out with strain JH2-2 as the recipient (MIC, 32 µg ml–1). High-level bacitracin resistance (MIC, ≥256 µg ml–1) was found to be transferred at a frequency of conjugation of 7.28 x 10–3. Transfer of the resistance genes from the donor strain to the transconjugants was confirmed by PFGE and hybridization with a bcrB gene probe. The bcrB probe hybridized to a SmaI fragment of approximately 72 kb in both the donor and the transconjugant, illustrating the presence of the bcr operon (Fig. 3A, lanes 2 and 3). I-CeuI digestion of total genomic DNA was used to further investigate the location of the bcrB gene (Fig. 3B). I-CeuI is a restriction enzyme that recognizes a specific site in the 23S rRNA operon and thus cleaves only chromosomal DNA. Hybridization of I-CeuI-digested and nondigested DNA can therefore determine whether a gene is present on the chromosome or is plasmid borne. The bcrB probe hybridized to a band of approximately 72 kb in both I-CeuI-digested and nondigested DNA from AR01/DGVS, demonstrating that the bcr operon is plasmid borne in this isolate (Fig. 3B). In other bacterial genera, bacitracin resistance genes are chromosomally encoded (26, 28, 34).



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  		FIG. 3. Southern blot analysis of strains involved in conjugative transfer of bacitracin resistance. (A) SmaI-digested genomic DNA from donor, recipient, and transconjugant strains was probed with a bcrB gene probe. Lane 1, bacteriophage lambda DNA ladder standard; lane 2, donor strain AR01/DGVS; lane 3, transconjugant strain JH2-Bcr; lane 4, recipient strain JH2-2. (B) Hybridization with a bcrB gene probe to I-CeuI-digested genomic DNA. Two lanes of genomic DNA from each isolate are shown. The first DNA in each pair was not digested with I-CeuI, while the second DNA was incubated with the enzyme. Lanes 1 and 2, AR01/DGVS; lanes 3 and 4, JH2-Bcr; lanes 5 and 6, JH2-2; lane 7, bacteriophage lambda DNA ladder standard. Sizes (in kilobases) are indicated on the left and right.

Zinc bacitracin is used in New Zealand poultry production at very high levels, and the use of this compound has selected for enterococcal strains harboring bacitracin resistance genes. The fact that transferable bacitracin resistance has been detected in a vancomycin-resistant E. faecalis isolate potentially negates the use of bacitracin to eliminate colonization with vancomycin-resistant enterococci, as has been suggested previously (25). Further investigation is needed to determine how widespread these genes are in enterococcal strains and species from different environments.


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ACKNOWLEDGMENTS
 
This work was funded by an Otago Medical Research Foundation grant.

We thank Paula Crowley for supplying pTV1-OK and Shuhei Fujimoto for supplying vectors pAM401 and pMGS100.


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FOOTNOTES
 
* Corresponding author. Mailing address: Department of Microbiology and Immunology, Otago School of Medical Sciences, University of Otago, P.O. Box 56, Dunedin, New Zealand. Phone: 64 3 479 7722. Fax: 64 3 479 8540. E-mail: greg.cook{at}stonebow.otago.ac.nz. Back


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REFERENCES
 
    1
  1. Aarestrup, F. M., F. Bager, N. E. Jensen, M. Madsen, A. Meyling, and H. C. Wegener. 1998. Resistance to antimicrobial agents used for animal therapy in pathogenic-, zoonotic- and indicator bacteria isolated from different food animals in Denmark: a baseline study for the Danish Integrated Antimicrobial Resistance Monitoring Programme (DANMAP). APMIS 106:745-770.[Medline]
    2. 2
  2. Bernard, R., J. Pascale, G. Annick, M. Chippaux, and F. Denizot. 2003. YtsCD and YwoA, two independent systems that confer bacitracin resistance to Bacillus subtilis. FEMS Microbiol. Lett. 228:93-97.[CrossRef][Medline]
    3. 3
  3. Borodovsky, M., and J. McIninch. 1993. GeneMark: parallel gene recognition for both DNA strands. Comput. Chem. 17:123-133.
    4. 4
  4. Cain, B. D., P. J. Norton, W. Eubanks, H. S. Nick, and C. M. Allen. 1993. Amplification of the bacA gene confers bacitracin resistance to Escherichia coli. J. Bacteriol. 175:3784-3789.[Abstract/Free Full Text]
    5. 5
  5. Cao, M., and J. D. Helmann. 2002. Regulation of the Bacillus subtilis bcrC bacitracin resistance gene by two extracytoplasmic function sigma factors. J. Bacteriol. 184:6123-6129.[Abstract/Free Full Text]
    6. 6
  6. Chalker, A. F., K. A. Ingraham, R. D. Lunsford, A. P. Bryant, J. Bryant, N. G. Wallis, J. P. Broskey, S. C. Pearson, and D. J. Holmes. 2000. The bacA gene, which determines bacitracin susceptibility in Streptococcus pneumoniae and Staphylococcus aureus, is also required for virulence. Microbiology 146:1547-1553.[Abstract/Free Full Text]
    7. 7
  7. Christie, P. J., R. Z. Korman, S. A. Zahler, J. C. Adsit, and G. M. Dunny. 1987. Two conjugation systems associated with Streptococcus faecalis plasmid pCF10: identification of a conjugative transposon that transfers between S. faecalis and Bacillus subtilis. J. Bacteriol. 169:2529-2536.[Abstract/Free Full Text]
    8. 8
  8. Devriese, L. A., G. Daube, J. Hommez, and F. Haesebrouck. 1993. In vitro susceptibility of Clostridium perfringens isolated from farm animals to growth-enhancing antibiotics. J. Appl. Bacteriol. 75:55-57.[Medline]
    9. 9
  9. Fujimoto, S., and Y. Ike. 2001. pAM401-based shuttle vectors that enable overexpression of promoterless genes and one-step purification of tag fusion proteins directly from Enterococcus faecalis. Appl. Environ. Microbiol. 67:1262-1267.[Abstract/Free Full Text]
    10. 10
  10. Goldman, R., and J. L. Strominger. 1972. Purification and properties of C55-isoprenylpyrophosphate phosphatase from Micrococcus lysodeikticus. J. Biol. Chem. 247:5116-5122.[Abstract/Free Full Text]
    11. 11
  11. Gutierrez, J. A., P. J. Crowley, D. P. Brown, J. D. Hillman, P. Youngman, and A. S. Bleiweis. 1996. Insertional mutagenesis and recovery of interrupted genes of Streptococcus mutans by using transposon Tn917: preliminary characterization of mutants displaying acid sensitivity and nutritional requirements. J. Bacteriol. 178:4166-4175.[Abstract/Free Full Text]
    12. 12
  12. Hanahan, D., J. Jessee, and F. R. Bloom. 1991. Plasmid transformation of Escherichia coli and other bacteria. Methods Enzymol. 204:63-113.[Medline]
    13. 13
  13. Jacob, A. E., and S. J. Hobbs. 1974. Conjugal transfer of plasmid-borne multiple antibiotic resistance in Streptococcus faecalis var. zymogenes. J. Bacteriol. 117:360-372.[Abstract/Free Full Text]
    14. 14
  14. Keis, S., C. F. Bennett, V. K. Ward, and D. T. Jones. 1995. Taxonomy and phylogeny of industrial solvent-producing clostridia. Int. J. Syst. Bacteriol. 45:693-705.[Abstract/Free Full Text]
    15. 15
  15. Keis, S., G. Kaim, P. Dimroth, and G. M. Cook. 2004. Cloning and molecular characterization of the atp operon encoding for the F1F0-ATP synthase from a thermoalkaliphilic Bacillus sp. strain TA2.A1. Biochim. Biophys. Acta 1676:112-117.[Medline]
    16. 16
  16. Lis, M., and H. K. Kuramitsu. 2003. The stress-responsive dgk gene from Streptococcus mutans encodes a putative undecaprenol kinase activity. Infect. Immun. 71:1938-1943.[Abstract/Free Full Text]
    17. 17
  17. Liu, Y., J. Zhou, M. V. Omelchenko, A. S. Beliaev, A. Venkateswaran, J. Stair, L. Wu, D. K. Thompson, D. Xu, I. B. Rogozin, E. K. Gaidamakova, M. Zhai, K. S. Makarova, E. V. Koonin, and M. J. Daly. 2003. Transcriptome dynamics of Deinococcus radiodurans recovering from ionizing radiation. Proc. Natl. Acad. Sci. USA 100:4191-4196.[Abstract/Free Full Text]
    18. 18
  18. Lukashin, A. V., and M. Borodovsky. 1998. GeneMark.hmm: new solutions for gene finding. Nucleic Acids Res. 26:1107-1115.[Abstract/Free Full Text]
    19. 19
  19. Malhotra-Kumar, S., S. Wang, C. Lammens, S. Chapelle, and H. Goossens. 2003. Bacitracin-resistant clone of Streptococcus pyogenes isolated from pharyngitis patients in Belgium. J. Clin. Microbiol. 41:5282-5284.[Abstract/Free Full Text]
    20. 20
  20. Manson, J. M., S. Keis, J. M. B. Smith, and G. M. Cook. 2003. Characterization of a vancomycin-resistant Enterococcus faecalis (VREF) isolate from a dog with mastitis: further evidence of a clonal lineage of VREF in New Zealand. J. Clin. Microbiol. 41:3331-3333.[Abstract/Free Full Text]
    21. 21
  21. Manson, J. M., S. Keis, J. M. B. Smith, and G. M. Cook. 2003. A clonal lineage of VanA-type Enterococcus faecalis predominates in vancomycin-resistant enterococci isolated in New Zealand. Antimicrob. Agents Chemother. 47:204-210.[Abstract/Free Full Text]
    22. 22
  22. Miller, V. L., R. K. Taylor, and J. J. Mekalanos. 1987. Cholera toxin transcriptional activator toxR is a transmembrane DNA binding protein. Cell 48:271-279.[CrossRef][Medline]
    23. 23
  23. National Committee for Clinical Laboratory Standards. 2001. Performance standards for antimicrobial susceptibility testing; eleventh informational supplement. NCCLS document M100-S11. National Committee for Clinical Laboratory Standards, Wayne, Pa.
    24. 24
  24. Neumüller, A. M., D. Konz, and M. A. Marahiel. 2001. The two-component regulatory system BacRS is associated with bacitracin ‘self-resistance’ of Bacillus licheniformis ATCC 10716. Eur. J. Biochem. 268:3180-3189.[Medline]
    25. 25
  25. O'Donovan, C. A., P. Fan-Harvard, F. T. Tecson-Tumang, S. M. Smith, and R. H. K. Eng. 1994. Enteric eradication of vancomycin-resistant Enterococcus faecium with oral bacitracin. Diagn. Microbiol. Infect. Dis. 18:105-109.[CrossRef][Medline]
    26. 26
  26. Ohki, R., Giyanto, K. Tateno, W. Masuyama, S. Moriya, K. Kobayashi, and N. Ogasawara. 2003. The BceRS two-component regulatory system induces expression of the bacitracin transporter, BceAB, in Bacillus subtilis. Mol. Microbiol. 49:1135-1144.[CrossRef][Medline]
    27. 27
  27. Ohki, R., K. Tateno, Y. Okada, H. Okajima, K. Asai, Y. Sadaie, M. Murata, and T. Aiso. 2003. A bacitracin-resistant Bacillus subtilis gene encodes a homologue of the membrane-spanning subunit of the Bacillus licheniformis ABC transporter. J. Bacteriol. 185:51-59.[Abstract/Free Full Text]
    28. 28
  28. Podelsek, Z., A. Comino, B. Herzog-Velikonja, D. Zgur-Bertok, R. Komel, and M. Grabnar. 1995. Bacillus licheniformis bacitracin resistance ABC transporter: relationship to mammalian multidrug resistance. Mol. Microbiol. 16:969-976.[CrossRef][Medline]
    29. 29
  29. Sambrook, J., E. F. Fritsch, and T. Maniatis. 1989. Molecular cloning: a laboratory manual, 2nd ed. Cold Spring Harbor Laboratory Press, Cold Spring Harbor, N.Y.
    30. 30
  30. Shepard, B. D., and M. S. Gilmore. 1995. Electroporation and efficient transformation of Enterococcus faecalis grown in high concentrations of glycine. Methods Mol. Biol. 47:217-226.[Medline]
    31. 31
  31. Stone, K. J., and J. L. Strominger. 1972. Inhibition of sterol biosynthesis by bacitracin. Proc. Natl. Acad. Sci. USA 69:1287-1289.[Abstract/Free Full Text]
    32. 32
  32. Stone, K. J., and J. L. Strominger. 1971. Mechansim of action of bacitracin: complexation with metal ion and C55-isoprenyl pyrophosphate. Proc. Natl. Acad. Sci. USA 68:3223-3227.[Abstract/Free Full Text]
    33. 33
  33. Storm, D. R., and J. L. Strominger. 1973. Complex formation between bacitracin peptides and isoprenyl pyrophosphates. J. Biol. Chem. 248:3940-3945.[Abstract/Free Full Text]
    34. 34
  34. Tsuda, H., Y. Yamashita, Y. Shibata, Y. Nakano, and T. Koga. 2002. Genes involved in bacitracin resistance in Streptococcus mutans. Antimicrob. Agents Chemother. 46:3756-3764.[Abstract/Free Full Text]
    35. 35
  35. Wirth, R., F. Y. An, and D. B. Clewell. 1986. Highly efficient protoplast transformation system for Streptococcus faecalis and a new Escherichia coli-S. faecalis shuttle vector. J. Bacteriol. 165:831-836.[Abstract/Free Full Text]
    36. 36
  36. Yanisch-Perron, C., J. Vieira, and J. Messing. 1985. Improved M13 phage cloning vectors and host strains: nucleotide sequences of the M13mp18 and pUC19 vectors. Gene 33:103-119.[CrossRef][Medline]

Antimicrobial Agents and Chemotherapy, October 2004, p. 3743-3748, Vol. 48, No. 10
0066-4804/04/$08.00+0     DOI: 10.1128/AAC.48.10.3743-3748.2004
Copyright © 2004, American Society for Microbiology. All Rights Reserved.



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