Skip to main content
Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

Response of Methicillin-Resistant Staphylococcus aureus to Amicoumacin A

  • Amrita Lama ,

    Contributed equally to this work with: Amrita Lama, Jan Pané-Farré

    Current address: Department of Molecular Microbiology & Immunology, Oregon Health & Science University, Beaverton, Oregon, United States of America

    Affiliation Division of Environmental and Biomolecular Systems, Institute of Environmental Health, Oregon Health & Science University, Beaverton, Oregon, United States of America

  • Jan Pané-Farré ,

    Contributed equally to this work with: Amrita Lama, Jan Pané-Farré

    Affiliation Institute for Microbiology, Ernst-Moritz-Arndt-University Greifswald, Greifswald, Germany

  • Tai Chon,

    Affiliation Division of Environmental and Biomolecular Systems, Institute of Environmental Health, Oregon Health & Science University, Beaverton, Oregon, United States of America

  • Anna M. Wiersma,

    Affiliation Department of Chemistry, University of Alberta, Edmonton, Alberta, Canada

  • Clarissa S. Sit,

    Affiliation Department of Chemistry, University of Alberta, Edmonton, Alberta, Canada

  • John C. Vederas,

    Affiliation Department of Chemistry, University of Alberta, Edmonton, Alberta, Canada

  • Michael Hecker,

    Affiliation Institute for Microbiology, Ernst-Moritz-Arndt-University Greifswald, Greifswald, Germany

  • Michiko M. Nakano

    Affiliation Division of Environmental and Biomolecular Systems, Institute of Environmental Health, Oregon Health & Science University, Beaverton, Oregon, United States of America


Amicoumacin A exhibits strong antimicrobial activity against methicillin-resistant Staphylococcus aureus (MRSA), hence we sought to uncover its mechanism of action. Genome-wide transcriptome analysis of S. aureus COL in response to amicoumacin A showed alteration in transcription of genes specifying several cellular processes including cell envelope turnover, cross-membrane transport, virulence, metabolism, and general stress response. The most highly induced gene was lrgA, encoding an antiholin-like product, which is induced in cells undergoing a collapse of Δψ. Consistent with the notion that LrgA modulates murein hydrolase activity, COL grown in the presence of amicoumacin A showed reduced autolysis, which was primarily caused by lower hydrolase activity. To gain further insight into the mechanism of action of amicoumacin A, a whole genome comparison of wild-type COL and amicoumacin A-resistant mutants isolated by a serial passage method was carried out. Single point mutations generating codon substitutions were uncovered in ksgA (encoding RNA dimethyltransferase), fusA (elongation factor G), dnaG (primase), lacD (tagatose 1,6-bisphosphate aldolase), and SACOL0611 (a putative glycosyl transferase). The codon substitutions in EF-G that cause amicoumacin A resistance and fusidic acid resistance reside in separate domains and do not bring about cross resistance. Taken together, these results suggest that amicoumacin A might cause perturbation of the cell membrane and lead to energy dissipation. Decreased rates of cellular metabolism including protein synthesis and DNA replication in resistant strains might allow cells to compensate for membrane dysfunction and thus increase cell survivability.


Staphylococcus aureus is the etiological agent for a large number of human infections, including pneumonia, meningitis, toxic shock syndrome, bacteremia, and endocarditis. S. aureus is notorious for developing rapid resistance to antibiotics, which is caused mainly by antibiotic selection and horizontal transfer of resistance genes [1]. Most notably, methicillin-resistant S. aureus (MRSA) has emerged quickly due to acquisition of the novel penicillin-binding protein 2A (PBP2A) encoded by mecA [2]. The mecA gene likely originated from Staphylococcus sciuri that is naturally sensitive to β-lactam [3] and mecA incorporated into a staphylococcal cassette chromosome (SCCmec) serves as a mobile genetic element, thus mediating transfer of the mecA gene into staphylococcal species [4]. Morbidity caused by MRSA infections per year in the U.S.A. was reported to be comparable to that caused by HIV/AIDS [5], which highlights the importance of this deadly pathogen. The glycopeptide vancomycin, the most commonly used antibiotic for the treatment of MRSA infections, is no longer effective enough because of the emergence of vancomycin-intermediate S. aureus (VISA) [6]. Therefore, there is an urgent need to find antibacterial agents with novel mechanisms of action and to understand how S. aureus acquires antibiotic resistance.

In this study, amicoumacin A, which possesses strong anti-MRSA activity, was investigated. Amicoumacin A, also known as AI-77-A, is one of numerous structurally related isocoumarin antibiotics [7], [8], [9], [10]. Other examples of this class of antibiotics include the xenocoumacins, the bacilosarcins, Sg17-1-4, PM-94128, and Y-05460 [11], [12], [13], [14], [15]. Figure 1 illustrates the structures of amicoumacin A and xenocoumacin 1. These isocoumarins exhibit a wide variety of biological effects, ranging from anti-bacterial to anti-tumor activity [11], [12], [13], [14], [15]. Amicoumacin A has anti-microbial, anti-inflammatory, and anti-ulcer properties [7], and anti-Helicobacter activity was later reported [16]. Despite the versatile activities, the mode of action remains unknown. Antibiotics currently used for MRSA infections either inhibit bacterial protein synthesis (linezolid) [17] or target the cell membrane (daptomycin) [18]. Amicoumacin A was reported to exhibit anti-MRSA activity [19]. This work has been aimed at elucidating the mechanism of action of amicoumacin A by examining genome-wide transcription induced by exposure of MRSA to amicoumacin A and identifying genetic changes that lead to reduced susceptibility to amicoumacin A.

Figure 1. The chemical structures of amicoumacin A and xenocoumacin 1.


Isolation and identification of Bacillus pumilus strain C9 with anti-MRSA activity

A collection of 60 bacterial strains isolated from the Columbia River Estuary was screened for their potential antimicrobial activity against S. aureus. Three isolates exhibited clear inhibitory zones and were identified as Pseudoalteromonas tunicata, Peudoalteromonas sp., and B. pumilus based on the analysis of 16S rRNA gene sequence. Among the three strains, B. pumilus (named the strain C9) had the strongest activity against methicillin-sensitive S. aureus (MSSA) and MRSA and was chosen for further investigation.

Purification and characterization of amicoumacin A

To identify its structure, the anti-MRSA substance was purified by methanol extraction, anion exchange column chromatography and RP-HPLC. The molecular mass of the compound was determined to be 424.2077 Da as determined by nanoESI FTICR mass spectrometry. FTICR analysis also revealed a plausible chemical formula (C20H30N3O7) for the substance. Through NMR analysis of the compound, chemical shifts and coupling constants were assigned for the protons in the molecule. Comparisons of the molecular mass, molecular formula and NMR data with the literature suggested that this substance is identical to amicoumacin A [7] (Figure 1).

Seven B. pumilus strains obtained from the Bacillus Genetic Stock Center were also checked for their anti-MRSA activity. No activity was detected from these strains except that 8A2 showed a weak anti-MRSA activity. However, the antibacterial spectrum of the compound from 8A2 significantly differed from that of the substance from C9 (data not shown). On the other hand, a similar anti-MRSA activity was detected in B. pumilus SAFR-032, a strain originally recovered from the Jet Propulsion Lab (Pasadena, CA) spacecraft assembly facility [20]. The results suggested that productivity of amicoumacin A was lost during domestication of B. pumilus strains and in fact, we have previously found a similar phenomenon for surfactin production in B. subtilis 168. In this case, introduction of sfp into domesticated B. subtilis strains restored surfactin production [21]. The sfp gene encodes 4′-phosphopantetheine transferase essential for nonribosomal peptides (NRP) and polyketides (PK) synthesis [22]. A recent study showed that PK and NRP synthesis genes are required for the production of xenocoumacin I [23], indicating that amicoumacin A is likely synthesized by a PK/NRP complex. It is conceivable that B. pumilus domesticated strains contain inactive sfp and hence are incapable of producing amicoumacin A. We designed primers using the sfp sequence of B. pumilus SAFR032 strain and used the primers to detect a PCR product with chromosomal DNA isolated from C9, 8A3, and 14A1. The PCR product with a high sequence homology to sfp from SAFR032 was detected in C9, but not in 8A3 and 14A1 (unpublished results), which is consistent with the notion that amicoumacin A is likely synthesized by a similar mechanism and the lack of an intact sfp is partially (if not solely) responsible for the loss of amicoumacin A production in domesticated B. pumilus strains.

Antimicrobial spectrum of amicoumacin A

In order to evaluate the antimicrobial effect of amicoumacin A, we examined the spectrum of amicoumacin A. Two gram-negative bacteria, E. coli and Pseudomonas aeruginosa were resistant as were three gram-positive bacteria, B. pumilus, Bacillus subtilis, and Listeria monocytogenes. Among the susceptible gram-positive bacteria, Bacillus anthracis, Bacillus cereus, and Bacillus thuringiensis showed a moderate sensitivity. These bacteria exhibited a fairly large zone of inhibition (∼2 cm in diameter) after 4–5 h of incubation with amicoumacin A; however, several resistant colonies appeared after overnight incubation and the inhibition zone became smaller (0.5 cm in diameter). In contrast, amicoumacin A showed highly potent activity (inhibition zone >2 cm in diameter after overnight incubation) against all MSSA and MRSA strains tested including hospital-acquired MRSA (HA-MRSA), community-acquired MRSA (CA-MRSA), and Mu50, a HA-MRSA/VISA strain. In addition, Staphylococcus carnosus and Streptococcus pyogenes are sensitive to amicoumacin A at a level similar to S. aureus strains. These results indicated that amicoumacin A is highly effective against gram-positive cocci including important pathogens.

Effect of amicoumacin A on the growth of S. aureus COL

The effect of amicoumacin A on the growth and survival of S. aureus COL was examined. As shown in Figure 2, the growth was inhibited after treatment with amicoumacin A and there was a significant ∼3-log10 decrease in the number of viable S. aureus cells. These effects on the growth and survival are similar to those by a bactericidal antibiotic vancomycin (Fig. 2), indicating that amicoumacin A is a bactericidal antibiotic as reported in H. pylori [16].

Figure 2. Effect of amicoumacin A (A and B) and vancomycin (C and D) on S. aureus COL.

(A) COL was grown in TSB and exponential growth phase cultures were divided into two flasks. Amicoumacin-A-treated (closed circles) and -untreated cultures (open circles) were further incubated and the optical density at 600 nm was measured at hourly intervals. Effect of inhibitory levels of amicoumacin A during longer cultivation is shown in the insert of Figure 2A. (B) The cultures in (A) were used to examine viable cell counts by plating diluted cells on TSB agar. (C) COL was treated with 10 µg/ml of vancomycin and growth was monitored as described in (A). (D) The cultures in (C) were used to examine viable cell counts. The data are the average of three independent experiments with standard deviations.

Changes in global transcription of S. aureus COL in response to amicoumacin A

Transcriptome analysis has been used to identify changes in gene expression in response to antibiotic treatment (reviewed in [24]). Samples were taken at 0, 10, and 40 min (t0, t10, and t40, respectively) after COL was treated with amicoumacin A and RNA was purified as described in Materials and Methods. Microarray experiments were carried out on three independent biological replicates. The results are included as supplemental information (Table S1, all genes with a minimum 2.5-fold up or down change) and Table 1 shows a list of selected genes that are upregulated more than 3-fold at 10 min after the treatment compared to unexposed control cells.

Table 1. Selected genes induced 3-fold or above by amicoumacin A.

In total, we identified 263 upregulated and 282 downregulated genes.

The overall transcriptome results indicated that genes involved in diverse biological processes are upregulated, which is similar to the transcriptome in response to unsaturated long chain free fatty acids [25]. Particularly intriguing is that 46 genes were co-upregulated and 27 co-downregulated by amicoumacin A and linoleic acid. Of the 46 co-upregulated genes, 30 belong to the S. aureus σB-regulon [26], [27]. σB is an alternative σ factor functioning in general stress response, the mechanism of which has been extensively studied in B. subtilis (reviewed in [28], [29]). A previous study suggested that σB of S. aureus functions in more basic cell physiology compared to the B. subtilis counterpart [27]. The σB-controlled genes upregulated by amicoumacin A were either transiently upregulated at t10 only or were upregulated at t10 and t40. We examined whether the sigB mutation leads to a higher susceptibility to amicoumacin A; however, the growth curve assay did not show any significant effect of the sigB mutation on amicoumacin A susceptibility (data not shown).

An annotation-based grouping of amicoumacin A regulated genes highlighted a particularly high number of induced genes with cell envelope and transport related processes. In total, 21 genes with cell envelope associated functions were upregulated including lrgA (SACOL0247) and lrgB (SACOL0248), which are among the most highly induced genes (Table 1). The lrgA gene and its homologous gene cidA are known to regulate murein hydrolase activity and affect sensitivity to penicillin [30], [31]. CidA is a holin-like protein that positively controls murein hydrolase activity and penicillin-induced killing, which is antagonized by LrgA, an anti-holin [30], [31]. Consistent with the notion, cidA transcription is regulated oppositely from lrgAB in response to amicoumacin A. The microarray result showed that cidA is downregulated 1.9-fold at 10 min, whereas expression of the downstream cidB and cidC gene is upregulated 2.8-fold and 4.2-fold, respectively, which was confirmed by Northern blot analysis (data not shown).

In addition, transcription of three peptidoglycan hydrolases (atl, lytM and sceD) was strongly upregulated in amicoumacin-A-treated cells. Transcription of atl encoding the major autolysin of S. aureus was about 4-fold induced at t10 and t40, while sceD encoding a lytic transglycosylase [32] was 2-fold induced at t10 and over 10-fold at t40. Similar to sceD, transcription of lytM, a Gly-Gly endopeptidase [33], was 4-fold induced at t40. Another group of upregulated genes encode proteins that function in cell wall and surface polysaccharides synthesis and turnover, which include a penicillin-binding protein (SACOL1490), MurG (SACOL1453), a predicted glycosyl-transferase (SACOL2578), and N-acetylmuramoyl-L-alanine amidase (SACOL1825) [34]. In addition, over 46 genes encoding proteins with functions in membrane transport were upregulated.

Validation of microarray results

Northern blot analysis was carried out with two independently isolated RNA samples to validate the microarray results. Five operons and one gene were randomly chosen and the results of two operons are shown in Figure 3. The operon of eight genes (SACOL0678 to SACOL0686) encodes a phage integrase family protein (SACOL0678) and monovalent cation/H+ antiporter subunits (SACOL0679 to 0686). A previous study showed that transcription of these genes is σB-dependent [27]. Based on the microarray result, all eight genes were induced at t10 and the increased level of transcription was sustained at similar levels at t40 (Table 1 and Table S1). In the Northern blot experiment, a low level of 6.8 kb transcript was detected in untreated cells and the transcript was highly elevated at t10 and t40 (Figure 3A). This result confirmed that the eight genes constitute an operon and that amicoumacin A upregulates the operon transcription as shown by the microarray hybridization result. Transcription of another operon starting from SACOL2176 was also upregulated at t10 in the microarray results but the transcription decreased to the untreated level at t40 (Table 1 and Table S1). SACOL2176 encodes an osmoprotectant transporter, SACOL2175 and SACOL2174 encode a protein of unknown function and a membrane protein, respectively, and SACOL2173 is asp23 that codes for alkaline shock protein 23 [35]. The Northern blot analysis detected three transcripts of 3.0 kb, 1.5 kb, and 0.6 kb, all of which increase at t10 but not at t40 (Figure 3B). The sizes of the transcripts correspond to the predicted transcripts initiated at the three σB-dependent promoters. In a similar way, we also validated the microarray result of SACOL0673-0672-0671, SACOL2596-2597, SACOL02554.1-2554-2553, and SACOL1062 (data not shown).

Figure 3. Northern blot analyses for SACOL0678 (A) and SACOL2176 (B) operon.

Total RNA was isolated from S. aureus COL at 0 (t0), 10 (t10), and 40 (t40) min after the addition of amicoumacin A. 10 µg of total RNA isolated from each culture was separated in a formaldehyde-agarose gel and the RNA-blotted membrane was hybridized with SACOL0678- or SACOL2173(asp23)-specific digoxigenin-labeled probes. The sizes of the transcripts were determined by comparison to an RNA ladder on the same gel. The corresponding stained gels are shown underneath each blot. Schematic views of the gene loci based on NCBI COL genome site are shown with predicted transcripts. σB indicates locations of σB-controlled promoters. Microarray results of each operon's genes are summarized in the right panel of the corresponding Northern blot gels. Closed squares and open squares show samples taken at t10 and t40, respectively. The average of triplicates and standard deviations are indicated.

Effect of amicoumacin A on autolysis

The transcriptome results showed that lrgA transcription is highly upregulated and cidA transcription is downregulated by amicoumacin A. It has been shown that the cidA mutation reduces murein hydrolase activity [31], whereas the lrgAB mutation increases activity [30]. This result implied that autolysis might be reduced in response to amicoumacin A. On the other hand, the major autolysin gene atl was upregulated by amicoumacin A treatment (Table 1), suggesting that amicoumacin A might cause increased autolysis. To determine which possibility is correct, we investigated whether and how amicoumacin A affects autolysis. Figure 4A showed that amicoumacin-A-treated cells are more resistant to Triton X-100-induced lysis than untreated cells. Therefore, increased transcription of atl did not result in higher autolysis, which is consistent with the model that LrgA/CidA system controls autolysin activity at the post-transcriptional level [36].

Figure 4. Effect of amicoumacin A on autolysis.

(A) Effect on whole cell autolysis. Cultures grown in the absence (open circles) and the presence (closed circles) of amicoumacin A were washed and suspended in autolysis buffer to an initial OD600 of around 1.0 and autolysis was monitored as decline in OD600. (B) Quantitative assay of murein hydrolase activity against cell wall. An equal amount (90 µg protein) of extracellular proteins were added to cell wall purified from amicoumacin-A-untreated cells and OD600 was monitored as described in Materials and Methods. Symbols: open circles, extracellular proteins from untreated cells; closed circles, extracellular proteins from amicoumacin-A-treated cells; open triangles, 10 mM Tris-HCl (pH 7.5). (C) Susceptibility assay of purified cell wall to murein hydrolase. Ninety µg of extracellular proteins from amicoumacin-A-untreated cells were added to cell wall purified from amicoumacin-A-treated and -untreated cells and OD600 was monitored. Symbols: open circles, cell wall from untreated cells with 10 mM Tris-HCl (pH 7.5); closed circles, cell wall from untreated cells with extracellular proteins; open triangles, cell wall from amicoumacin-A-treated cells with 10 mM Tris-HCl (pH 7.5); closed triangles, cell wall from amicoumacin-A-treated cells with extracellular proteins. (D) Zymographic analysis of murein hydrolase activity from amicoumacin-A-treated and -untreated cells against purified S. aureus COL cell wall. Autolytic extracts were prepared and assayed by electrophoresis on an SDS-polyacrylamide gel (10%) containing 1 mg/ml purified cell wall as described in Materials and Methods. Lanes: M, prestained molecular weight markers; 1, cell-wall-associated proteins from untreated cells; 2, cell-wall-associated proteins from amicoumacin-A-treated cells; 3, extracellular proteins from untreated cells; 4, extracellular proteins from amicoumacin-A-treated cells.

To distinguish whether the reduced autolysis is due to alterations of cell wall or to decreased activity of autolysin, purified cell wall and extracellular autolysin were prepared from cells grown in the presence and absence of amicoumacin A. Previous work showed that overexpression of lrgAB in S. aureus leads to decreased extracellular murein hydrolase activity [30]. We first conducted an experiment designed to determine if amicoumacin A inhibits autolysis by reducing extracellular autolysin activity. Purified cell wall from S. aureus COL was incubated with an equal amount of extracellular proteins from untreated or amicoumacin-A-treated cells (Figure 4B). No significant decrease in OD600 was detected in the sample of purified cell wall alone, confirming that it has no intrinsic autolysin activity. The addition of extracellular proteins from untreated cells hydrolyzed over 50% of cell wall after 7 h of incubation, whereas proteins from treated cells did not hydrolyze purified cell wall, indicating that amicoumacin A reduces murein hydrolase activity. In a reciprocal experiment, we demonstrated that cell wall purified from strain COL grown in the presence of amicoumacin A was susceptible to extracellular autolysin from amicoumacin-A-untreated cells, although the rate of hydrolysis was slightly slower than cell wall prepared from untreated cells (Figure 4C). These results clearly showed that reduced autolysis of S. aureus grown in the presence of amicoumacin A is due to the lower level and/or activity of autolysin.

We performed zymographic analysis to examine the autolysin profile (Figure 4D). Both cell-wall-associated and extracellular autolysin profiles were not significantly altered by amicoumacin A treatment, but overall activities were reduced by the treatment. Except for the 36 kDa protein identified as Aaa (autolysin/adhesion protein of S. aureus) [37], the other six bands likely represent differently processed forms of Atl [38], [39]. Among these Atl forms, the 113 kDa band, which corresponds to an intermediate generated from pro-Atl by cleavage of the pro-peptide, was particularly reduced in both cell wall and the extracellular fraction of cells treated by amicoumacin A.

Isolation of mutants with decreased susceptibility towards amicoumacin A

As amicoumacin A is highly effective against MRSA, we investigated whether resistant mutants are associated with antibiotic selection pressure. Identification of mutations that lead to the amicoumacin A resistance might also provide clues to its mechanism of action. We isolated strains with decreased susceptibility to amicoumacin A using a serial passage of COL in the presence of the compound. COL was able to grow in the presence of successively higher concentrations of amicoumacin A over time. The resistance increased 2-fold every two days. Although we were able to obtain an isolate with 16-fold higher resistance against amicoumacin A as compared to the wild-type strain, further incubation up to 15 days did not increase resistance (Figure 5).

Figure 5. Serial passage experiments with S. aureus COL selected for increasing resistance to amicoumacin A.

Each circle shows fold-resistance on each day.

Determination of the mutations associated with increased resistance to amicoumacin A

Whole-genome sequencing becomes a powerful tool for identifying genomic variation and was applied to track multidrug resistance in S. aureus recovered periodically from a patient undergoing chemotherapy with vancomycin [40]. We used the approach to identify genetic changes present in the amicoumacin A-resistant COL strains. Genome libraries were constructed from three resistant strains, namely SA-1, SA-3, and SA-6 that exhibit 2-fold, 8-fold, and 16-fold increase in resistance, respectively. The sequencing results uncovered a set of genes with varying numbers of single nucleotide polymorphisms (SNPs) in the resistant mutants (Table 2). The results revealed that more mutations were found in parallel with increasing levels of resistance. Among the mutations, SACOL0187 (in SA-1) and oppB (in SA-3) encode ABC-transporters. Both SA-3 and SA-6 contain missense mutations in fusA that encodes translation factor EF-G. Interestingly, the EF-G amino acid substitutions occur at adjacent glycine residues. The fusA gene has been known as the site of mutations that confer fusidic acid resistance in Salmonella enterica serovar Typhimurium [41] and S. aureus [42], [43]. Fusidic acid is a steroid-like antibiotic clinically used since the 1960s. Mutations that are responsible for fusidic acid resistance occur in domains I, III, and V of EF-G, as well as in domain II with less frequency, whereas the mutations found in the amicoumacin A-resistant isolates reside in domain IV. The ksgA mutation is the only nonsense mutation among the identified point mutations. The ksgA gene encodes the methyltransferase for two adjacent adenosines in 16 S rRNA. Kasugamycin resistance was shown to be associated with the loss of the methylation [44]. Other mutations were identified in dnaG encoding primase, lacD encoding tagatose 1,6-bisphosphate aldolase, and SACOL0611, a putative glycosyl transferase gene.

Table 2. Codon substitution mutations found in amicoumacin-A-resistant COL.

Construction of the ksgA knockout mutation and amicoumacin A resistance

To evaluate the role and impact of the ksgA mutation in amicoumacin A resistance, the same mutation was re-created in COL using plasmid pMAD with a temperature-sensitive replicon. The mutant allele (L260stp) of the ksgA gene that lacks the start codon was amplified by PCR and the product was cloned into pMAD. The PCR product was designed to position the mutation at the 3′-end of the insert DNA, thus maximizing the chance of homologous recombination at a region located the 5′ to the site of the mutation. A single crossover recombination of the resultant plasmid into COL chromosomal DNA thus results in the mutant ksgA gene expressed from the native promoter and inactivation of the wild-type ksgA gene due to the loss of its promoter and deletion of the 5′-end of the gene. The integration of the plasmid in the predicted manner was confirmed by PCR and sequence analysis of the ksgA region of the resultant strain, SA-8. The MIC of amicoumacin A increased 2-fold compared to the parent strain, confirming that the nonsense ksgA allele is responsible for a low level of resistance towards amicoumacin A. As expected, SA-8, like SA-6, exhibited increased kasugamycin resistance compared to the wild-type strain (data not shown).

Overexpression of fusA genes with mutant alleles in S. aureus COL

As described above, the fusA mutations found in two amicoumacin A-resistant strains locate in domain IV where no fusidic acid-resistant mutation has previously been isolated. We also found that the SA-3 and SA-6 fusA mutants are as sensitive to fusidic acid as the wild-type strain (MIC 0.08 µg/ml). In order to further characterize antibiotic-resistant phenotypes of fusA mutations, we isolated a fusidic acid-resistant mutant (SA-7) by the multiple passage method as described in Materials and Methods. The MIC of SA-7 for fusidic acid was 12.5 µg/ml, which is 156-fold higher than that of the wild-type strain, whereas SA-7 exhibited the same MIC as the wild-type COL towards amicoumacin A. Sequence analysis of fusA amplified from the SA-7 chromosomal DNA identified a point mutation of R464H in domain III, which is identical to the mutation identified in a fusidic acid-resistant S. aureus with the small-colony-variant phenotype [43].

We next checked whether SA-11, the wild-type COL strain carrying the mutant allele (R464H) of fusA on plasmid pDG148, confers resistance to fusidic acid. The MIC of this strain for fusidic acid was around 6.25 µg/ml irrespective of IPTG addition, probably because the control of the vector IPTG-inducible Pspac promoter is leaky. In contrast, the MIC of SA-11 for amicoumacin A was identical to that of the wild-type strain. SA-9 and SA-10 that express fusA(G530V) and fusA(G531S), respectively, on the multi-copy plasmid were sensitive to fusidic acid but exhibited 2-fold higher resistance to amicoumacin A as compared to the wild-type strain. These results confirmed that the fusA(G530V) and fusA(G531S) mutations cause amicoumacin A resistance and the fusA(R464H) mutation causes fusidic acid resistance, but not vice versa.


Amicoumacin A possesses strong bactericidal activity against MRSA. Xenocoumacin 1, another isocoumarin antibiotic, shares an identical dihydroisocoumarin moiety with amicoumacin A, but has a slightly different hydroxy amino acid side chain (Figure 1). Both compounds exhibit potent activity against gram-positive bacteria, but only xenocoumacin 1 exhibits activity against selected gram-negative bacteria, such as some E. coli strains [14]. Conversely, amicoumacin A can kill multi-resistant S. aureus, whereas xenocoumacin I has no effect on the organism [14]. This difference in spectra of activity might be due to the difference in the hydroxy amino acid side chains of the two molecules. In fact, it has been previously demonstrated that the amide at the terminal end of the side chain in amicoumacin A is essential for its activity against MRSA [19].

In this study, we aimed at elucidating the mechanism behind the strong bactericidal activity of amicoumacin A against MRSA. In hope of identifying the target of amicoumacin A, we isolated amicoumacin A resistant strains using the multiple passage method.

Two different alleles of fusA were found to cause amicoumacin A resistance, while other alleles lead to fusidic acid resistance as shown here and in previous work. Fusidic acid binds to an EF-G/ribosome complex and inhibits EF-G turnover. The crystal structure of Thermus thermophilus EF-G revealed that domains I and II are homologous to elongation factor Tu and domains III and V show structural similarities to ribosomal proteins [45]. Domain IV was shown to protrude from the main body of the protein. This could explain why no cross-resistance was observed between fusidic acid-resistant mutations found in all domains except domain IV and amicoumacin A-resistant mutations in domain IV. The high resistance to fusidic acid caused by a single mutation in fusA is attributed to the fact that EF-G is the direct target of fusidic acid [46]. On the contrary, amicoumacin A resistance caused by the fusA mutations or the ksgA mutation is only 2-fold. In addition, the resistance increased every 2-fold in parallel with increased numbers of mutations in such a way that 2-, 8-, and 16-fold increase in MIC was observed in the strains carrying 1, 3, and 4 point mutations. These results suggest that the direct target of amicoumacin A is neither EF-G nor proteins encoded by the other genes, the mutations of which were identified by genome-wide sequencing.

As described above, lrgAB transcription was most highly induced by amicoumacin A. The proton ionophore carbomyl cyanide m-chlorophenylhydrazone (CCCP) was known to induce lrgAB expression. Since valinomycin, which dissipates Δψ, but not nigericin that depletes ΔpH across the membrane, has a similar effect with CCCP on lrg expression, the authors concluded that lrgAB is upregulated in response to a collapse of Δψ [47]. As this induction of lrgAB transcription requires the LytSR two-component signal transduction system, the LytS kinase might respond to a collapse of Δψ [47]. Daptomycin induces genes including lrgAB that are induced by CCCP, hence it was proposed that a part of the mechanism of action of daptomycin is membrane depolarization [48], which is consistent with an earlier study on potassium release assays [18]. Given transcription of lrgAB is highly induced by amicoumacin A, it might be possible that membrane depolarization is at least a part of the mechanism of action.

In this study, we showed that autolysis is highly reduced in cells grown in the presence of amicoumacin A, which is mainly caused by decreased activity of murein hydrolase, very likely Atl. A similar inhibition of autolysis due to reduced murein hydrolase activity was recently reported in S. aureus treated with Magnolol (5, 5′-diallyl-2, 2′-dihydroxybiphenyl) [49]. In this case, transcription of atl and cidA was reduced and lrgAB transcription was highly induced after Magnolol treatment. In the case of amicoumacin A, atl transcription was upregulated and Atl activity was reduced. There is a precedent for this paradoxical observation. A teicoplanin-resistant MRSA isolate exhibited an autolysis-deficient phenotype, although expression of major autolytic genes (atl, lytM, and lytN) was not changed [50]. As the resistant strain displayed decreased extracellular murein hydrolase activity, the authors suggested post-transcriptional regulation of hydrolase activity, the same conclusion of our study. However, transcription analysis of cidABC and lrgAB in the teicoplanin-resistant strain ruled out the possibility of a role for CidA in post-transcriptional control of murein hydrolase activity. The major murein hydrolase Atl is involved in peptidoglycan turnover, daughter cell separation after cell division [51], biofilm formation [52], and penicillin-induced lysis [53]. Given the roles of Atl in diverse cellular function, its activity could be tightly controlled through multiple mechanisms. Future studies are needed to uncover whether amicoumacin A affects autolysin activity through the LytS-Lrg-Cid pathway.

Materials and Methods

Bacterial strains and media

All of the strains used in this study are listed in Table 3. Bacillus and Escherichia coli were cultured in 2×YT and methicillin-sensitive S. aureus (MSSA) and MRSA strains were routinely propagated in tryptic soy broth (TSB) (Cellgro, Manassas, VA). Half-diluted artificial seawater contains 13.75 g NaCl, 5.3 g MgCl2⋅6H2O, 1.95 g MgSO4⋅7H2O, 0.5 g KCl, 0.331 g CaCl2⋅2H2O, and 0.914 mg FeSO4⋅7H2O per liter. Antibiotic concentrations used are; ampicillin, 50 µg/ml; erythromycin, 10 µg/ml; kanamycin, 100 µg/ml (for RN4220) and 20 µg/ml (for COL).

Identification of Bacillus pumilus C9 that produces amicoumacin A

Water samples were collected from the estuary turbidity maximum of the North Channel in the Columbia River Estuary on June 14, 2007 (cruise data link No specific permissions were required for the described field studies. The water samples were incubated at 28°C for 8 days and plated on half-diluted artificial seawater containing 0.5% peptone, 0.1% yeast extract (SPY), and 1.5% agar. After incubation at 28°C for 3 to 4 days, each bacterium was purified by isolating a single colony. Isolated bacterium was grown on SPY agar for 2 to 3 days depending on growth and antimicrobial activity was determined by overlaying S. aureus RN6390 in 7 ml brain heart infusion (BHI) (Becton Dickinson, Franklin Lakes, NJ) with 0.7% soft agar. After incubation at 37°C overnight, antimicrobial activity was detected as a lysis zone of RN6390 around a colony of testing bacteria.

Overlay assay to determine anti-microbial spectrum of amicoumacin A

B. pumilus C9 was streaked onto a small piece (1×1 cm) of 0.22 µm Millipore filter placed on LB agar plate and incubated at 37°C overnight. The filters were removed and susceptibility to amicoumacin A was determined by overlaying cultures of testing strains in 7 ml of BHI or 2×YT with soft agar. The plates were incubated at 37°C for 5 h to overnight.

Isolation of the anti-MRSA substance and purification to homogeneity

A fresh colony of B. pumilus C9 was used to inoculate LB broth and was incubated by shaking (150 rpm) at 30°C for 24 h. The culture supernatant was passed through an Amicon® ultra filtration membrane (MW 3,000 cutoff, Millipore, Billerica, MA) and the filtrate was lyophilized. The lyophilized material was extracted with methanol and the dried methanol extract was dissolved in 20 mM Tris-HCl (pH 7.0) before applying to a Hi-Q column to remove impurities. The column was run with 20 mM Tris-HCl (pH 7.0) at a flow rate of 2 ml/min. The active fractions were pooled and lyophilized for further purification by reverse phase high performance liquid chromatography (RP-HPLC). A C18 semi-preparative column (Vydac 218TP510, 300 Å pore diameter, 250 mm×10 mm, 5 µm particle diameter) was developed with a gradient of 5% acetonitrile/0.1% trifluoroacetic acid (TFA) to 50% acetonitrile/0.1% TFA from 5 to 42 min using a 3 ml/min flow rate. The active peak was identified at 29.56 min, which corresponds to an acetonitrile concentration of 36%. This fraction was lyophilized prior to analysis by mass spectrometry and nuclear magnetic resonance (NMR) spectroscopy.

Mass spectrometry analysis

The purified anti-MRSA substance was analyzed by nano-electrospray ionization (nanoESI) Fourier transform ion cyclotron resonance (FTICR) mass spectrometry. The Bruker 9.4T Apex-Qe FTICR (Bruker Daltonics, Billerica, MA) was calibrated externally using polyethylene glycol. The sample was dissolved in 50% acetonitrile/0.1% formic acid for injection into the nanoESI.

NMR analysis

The purified anti-MRSA substance (200 µg) was dissolved in 300 µl of deuterium oxide (D2O, 99.96% D, Cambridge Isotopes Laboratories, Cambridge, MA) that also contained 100 µM 2,2-dimethyl-2-silapentane-5-sulfonate sodium salt (DSS). The sample was pipetted into a D2O-matched Shigemi NMR tube (Shigemi Co., Ltd., Tokyo, Japan) for NMR analysis. NMR experiments were performed on the sample using a Varian Inova 800-MHz spectrometer equipped with a triple resonance HCN probe and Z-axis pulsed field gradients.

Partial purification of amicoumacin A

For routine purposes such as MIC and growth inhibitory assay experiments, partially purified amicoumacin A was used. B. pumilus C9 culture supernatant was extracted with one-fourth volume of n-butanol and shaking for 2 h at 200 rpm. The mixture was then poured into a separatory funnel and allowed to stand for another 2 h. The organic layer was collected and evaporated at 55°C overnight. The dried sample was dissolved in 10 mM Tris-HCl (pH 7.0) and passed through an Amicon ultra filtration membrane (MW 3,000 cutoff) and the filtrate was re-extracted with butanol. The dried sample was resuspended with 10 mM Tris-HCl (pH 7.0) and then passed through LH-20 Sephadex column with 1 ml/min flow rate. The active fractions were pooled and extracted with butanol. The evaporated sample was dissolved in 10 mM Tris-HCl (pH 7.0) and aliquots were frozen at −80°C until use.

Growth profile and survival assay of S. aureus COL in the presence of amicoumacin A

A fresh colony of S. aureus was inoculated and cultured in TSB overnight at 37°C. Two hundred µl of the overnight culture was inoculated into a 250 ml flask containing 20 ml of TSB. The flask was incubated in a 37°C shaker until the OD600 reached 0.4–0.5. The culture was divided into two flasks, 50 µl of amicoumacin A or 10 mM Tris-HCl (pH 7.0) was added to each flask and incubation was continued at 37°C. The readings at OD600 were recorded at every 1 h. In order to determine the cell survival profile in response to amicoumacin A, the cells were withdrawn at 0 h and every 1 h after the drug treatment, serially diluted, and plated onto TSB agar. Numbers of colonies were counted after overnight incubation at 37°C.

MIC assays

MICs for S. aureus COL were determined by broth microdilution assays in 96 well microtiter plates. Fifty µl of 2-fold serial dilutions of amicoumacin A were mixed with an equal volume of 1∶100 diluted overnight COL cultures in TSB. Control wells without drug were also included. The microtiter plate was incubated at 37°C for 24 h.

Transcriptome analysis

A fresh colony of COL was used to inoculate 2 ml of BHI. The overnight culture (0.5 ml) was transferred to 50 ml BHI and incubated at 37°C until OD600≈0.5 (t0), when 20 ml of cultures were withdrawn into 10 ml of ice-cold killing buffer (20 mM sodium azide, 5 mM MgCl2, 20 mM Tris-HCl, pH 7.5). To the remaining cultures, amicoumacin A was added at the concentration leading to around 12% and 20% reduction of OD600 after 10 min and 40 min, respectively. At 10 min and 40 min (t10 and t40) after the addition of amicoumacin A, 10 to 15 ml of cultures were harvested by mixing a half volume of ice-cold killing buffer. Harvested cells were immediately centrifuged at 4°C for 5 min at 7,000× g and washed once with killing buffer before being frozen at −80°C. Each experiment was performed in biological triplicate. RNA was prepared from harvested cells using glass beads/phenol method as previously described [54] and DNA was removed using RNase-free RQ1 DNase (Promega, Madison, WI). The quality of RNA was checked by gel electrophoresis and an Agilent bioanalyzer.

The design and evaluation of the customized StaphChip oligoarray manufactured by Agilent Technologies (Palo Alto, CA, USA) used in this study has been described elsewhere [55]. Microarray analysis was employed as described previously [56]. In short, cDNA was synthesized from 10 µg of total RNA and labeled by incorporation of Cy5-dCTP or Cy3-dCTP (GE Healthcare, Little Chalfont, United Kingdom) by direct reverse-transcription using Superscript II (Invitrogen, Karlsruhe, Germany) and random hexamers (Promega Madison, WI) as primers. After denaturation of the RNA primer mix for 10 min at 70°C, cDNA synthesis was performed in a 50 µl reaction volume at 42°C for 60 min. The concentrations of enzyme and reagents in the reverse transcription reaction were as follows: Superscript II (400 units), Cy-dye (1.25 nmol), dATP, dGTP, dTTP (5 nmol each), dCTP (2.5 nmol), random hexamers (1.25 µg), DTT (0.01 M) and 1× first strand buffer. The Superscript II was heat-inactivated for 10 min at 70°C and template RNA degraded by incubation for 30 min at room temperature with E. coli RNase H (2 units) (Invitrogen, Karlsruhe, Germany). Labeled cDNA was purified with the CyScribe GFX Purification Kit following the instructions of the manufacturer (GE Healthcare, Little Chalfont, United Kingdom) and Cy-dye incorporation was analysed with a NanoDrop ND-1000 spectrophotometer (NanoDrop Technologies, Inc., Rockland, DE). Approximately 500 ng of each labelled cDNA corresponding to 3–6 pmol of incorporated dye were used in two-color pool-cDNA (Cy3) versus sample cDNA (Cy5) competitive hybridization experiments. For the pool-cDNA synthesis equal amounts of all RNA samples were mixed. The pool was used as common reference. For each time point (t0, t10, and t40), three biologically independent cDNAs were synthesized.

Hybridizations were done in a total sample volume of 40 µl for 17 h at 65°C at 10 rpm in a dedicated hybridization chamber (Agilent Technologies) and hybridization oven (Robbins Scientific, Sunnyvale, CA, USA). After hybridization, the slides were washed for 1 min at room temperature in wash buffer 1 followed by a 1-min washing step at 37°C with wash buffer 2. The slides were dried by submersion in acetonitrile for 30 sec. Blocking reagents, hybridization buffer (Gene Expression Hybridization Kit) and washing solutions (Gene Expression Wash Buffer Kit) were purchased from Agilent. Slides were scanned at a 5 µm resolution (Agilent Technologies Scanner) and fluorescence intensities were extracted and processed using the Feature Extraction™ software version (Agilent Technologies). Local background-subtracted signals of both fluorescence channels were normalized with the linear LOWESS function. To test whether genes were differentially expressed in response to amicoumacin A, a Welch's t-test (α of <0.05) with a Bejamini and Hochberg FDR correction for multiple testing was calculated in Genespring (Agilent Technologies). Genes that passed the significance test for at least one time point (t0 versus t10, t0 versus t40 or t10 versus t40) and with a mean 2.5-fold up or 2.5-fold down regulation were considered differentially expressed. Grouping of genes based on expression profiles was calculated with the hierarchical clustering algorithm implemented in the multiple experiment viewer MeV [57]. The complete microarray data set is available at the NIH Gene Expression Omnibus (GEO) database under record number GSE31342.

Northern blot analyses

Digoxigenin-labeled RNA probes were prepared by in vitro transcription with T7 RNA polymerase by using a PCR fragment (SACOL0678) or plasmid (asp23: pKSAP23 [58]) as template. The PCR fragment was generated from COL chromosomal DNA purified with a chromosomal DNA isolation kit (Promega, Madison, WI) and the respective oligonucleotides (SA0678_COL_F: 5′-ATGAATAA AGTAGAAGCGAT-3′ and SA0678_COL_RT7: 5′-CTAATACGACTCACTATAGGG AGACTATAATTGTA ATGAAATAT-3′). Northern blot analyses were carried out as previously described [59]. The digoxigenin-labeled RNA marker I (Roche, Indianapolis, IN) was used to calculate the sizes of the transcripts. The hybridization signals were detected using a Lumi-Imager (Roche Diagnostics, Mannheim, Germany) and analyzed using the software package Lumi-Analyst (Roche Diagnostics, Mannheim, Germany).

Autolysis assay

Cultures at OD600 of around 0.3 were either treated with amicoumacin A for 45 min or left untreated. Harvested cells from each culture were washed with cold water and suspended at OD600 of 1.0 in 50 mM Tris-HCl (pH 7.5) with 0.05% Triton X-100. Autolysis was measured during incubation at 37°C with shaking as a decrease in optical density at OD600.

Preparation of purified cell wall

Purified cell wall was prepared as described previously [60]. In short, cells harvested at OD600 of 0.6 were boiled for 30 min in 4% SDS and washed with water for 4 times. Cells were broken with glass beads on a Vortex mixer, followed by treatment with α-amylase (100 µg/ml), DNase (10 µg/ml), RNase (50 µg/ml), and trypsin (100 µg/ml). The enzymes were inactivated by boiling for 15 min in 1% SDS. Cell wall was collected by centrifugation and washed twice with water, once with 8 M LiCl, once with 100 mM EDTA, and twice with water. Acetone-washed pellet was resuspended in water and lyophilized.

Crude autolytic enzyme extracts

Cells untreated or treated with amicoumacin A for 45 min were harvested by centrifugation, washed twice with 50 mM Tris-HCl (pH 7.5). After centrifugation, pellet was suspended in 50 mM Tris-HCl-2% SDS (at the concentration of 200OD600/ml). After centrifugation, supernatant was saved as cell-wall-associated autolysin. As for a source of extracellular autolysins, culture media were filtered through Millipore filter (0.22 µm) and concentrated around 40-fold using Amicon Ultra 3 K. The concentrated culture media were adjusted by standardizing by OD600 harvested cells. Protein concentration of concentrated media was measured by BioRad assay and extracellular protein concentrations were at 0.6 µg/ml in thus concentrated cultured media from untreated and treated cells.

Cell wall hydrolysis in vitro

Purified cell wall isolated from S. aureus COL cultured in the absence and presence of amicoumacin A was suspended in 50 mM Tris-HCl (pH 7.5) to an OD600 of 0.7. Cell wall hydrolysis was initiated by addition of extracellular proteins (90 µg) prepared as described above. As a control, equal volume of 10 mM Tris-HCl (pH 7.5) was added. Activities of autolysins were monitored by a decline in OD600 during incubation at 37°C.

Detection of murein lytic activity was also carried out by zymographic analysis. Cell-wall-associated proteins prepared from 0.2 OD600 amicoumacin-A-treated or untreated cells (1 µl of 200OD600/ml cell wall extract) and 1.9 µg of extracellular proteins were separated in an SDS-10% polyacrylamide gel containing purified cell wall (1 mg/ml). After electrophoresis, the gel was rinsed with water and incubated overnight at 37°C in 25 mM Tris-HCl (pH 8.0) containing 1% Triton X-100. The gel was rinsed with water and stained with 0.1% methylene blue in 0.01% KOH.

Isolation of mutants with decreased susceptibility to amicoumacin A and fusidic acid

Mutants were isolated by multiple passage methods through progressively increasing concentration of amicoumacin A or fusidic acid. Bacterial cultures that grew at the highest concentrations of the drug were used as an inoculum for the subsequent culture. Three amicoumacin A-resistant strains (SA-1, SA-3, and SA-6) and one fusidic acid-resistant strain (SA-7) were used for further studies.

Genotypic characterization of amicoumacin A-resistant mutants

Comparative genome sequencing (CGS) was used to identify chromosomal mutations in amicoumacin A-resistant mutants of S. aureus COL, SA-1 (2-fold increase in MIC), SA-3 (8-fold), and SA-6 (16-fold). Genomic DNA was purified from the wild-type and mutant strains using Wizard® Genomic DNA Purification Kit (Promega, Madison, WI). DNA was sheared to the fragments of less than 800 bp using Nebulizer kit (Invitrogen, Carlsbad, CA). The fragments were blunt-ended using end-it DNA repair kit (Epicentre, Madison, WI) and “A-tailing” of the fragments was done using Klenow exo-minus and dATP. The adapters with different barcodes and an overhang-T were ligated to the A-tailed fragments using fast link kit (Epicentre, Madison, WI). The ligated products were loaded onto 2% agarose gels. A 400–450 bp range of DNA was cut from the gel to exclude the unligated adapters and eluted using gel extraction kit (Qiagen, Valencia, CA). PCR was carried out using primers DL139 (5′-AATGATACGGCGACCACCGAGATCTACACTCTTTCCCTACACGA-3′) and DL140 (5′-CAAGCAGAAGACGGCATACGAGATCGGTCTCGGCATTCCTGCTGA AC-3′) and PfuUltra™ II Fusion HS DNA polymerase (Stratagene, Santa Clara). The PCR fragments were cloned using TOPO blunt kit (Invitrogen, Carlsbad, CA) and 10 randomly chosen clones from each library were sequenced to check the quality of genomic DNA library. The library DNA was diluted to 20 nM and sent to the Genomics Core Facility at Tufts University School of Medicine for single-end sequencing in Illumina HiSeq 2000. The analysis was carried out using the wild-type COL genome as a control and later comparing with S. aureus COL genome available at NCBI (Accession no. NC_002951).

Construction of ksgA mutants

The ksgA gene carrying the mutation (L260stop) was amplified using primers, ksgAFEcoRI (5′-GCTCGAATTCGGATAATAAAGATA TTGCAACACC-3′, EcoRI site is underlined) and ksgARBamHI (5′-GATCGGATCCGCCTCCATTGGCTTTCAG TACAATAC-3′, BamHI site is underlined), and chromosomal DNA isolated from the SA-6 strain as a template. The PCR product digested with EcoRI and BamHI was cloned into pMAD vector [61] digested with the same enzymes to generate pALG26. pALG26 was introduced into RN4220 by electroporation with selection for erythromycin resistance (Ermr) at 30°C. Bacteriophage φ11-mediated transduction was used to introduce pALG26 from the RN4220 transformant into COL by selecting transductants on TSB agar plates containing erythromycin and X-gal at 30°C. A single clone of the transductants was grown in TSB containing erythromycin at 30°C for 3–4 h and at 42°C for 6 h before plating on TSB agar plates containing erythromycin and X-gal. After incubation at 42°C, light blue colonies were obtained, which resulted from a single crossover recombination between the plasmid-born and the chromosomal ksgA genes. The recombinant strain, SA-8, was checked for resistance against kasugamycin and amicoumacin A.

Overexpression of fusA carrying the mutant alleles in S. aureus COL

The wild-type and the fusA mutant (G530V, G531S, R464H) genes were amplified using primers fusASalIF (5′-GATCGTCGACATGGCTAGAGAATTTTCA-3′, SalI site is underlined) and fusASphIR (5′-GATCGCATGCTTATTCACCTTTATTTTT C-3′, SphI site is underlined) from chromosomal DNA isolated from SA-3, SA-6, and SA-7, respectively. Each PCR product was digested with SalI and SphI, and ligated with pDG148 [62] digested with the same enzymes to generate pALG43 (for G530V), pALG44 (for G531S), and pALG45 (for R464H). These plasmids were first transformed into RN4220, then introduced into COL by φ11-mediated transduction as described above. The resultant COL strains, SA-9 (G530V), SA-10 (G531S), and SA-11 (R464H), were examined for fusidic acid- and amicoumacin A-susceptibility by microdilution method.

Supporting Information

Table S1.

Changes in global transcription of S. aureus COL in response to amicoumacin A. Hierarchical clustering has been done to classify the regulated genes based on their expression profiles. Genes in clusters 1–4 were upregulated and those in clusters 5–8 were downregulated.



We are grateful to Bacillus Genetic Stock Center, Barry Hurlburt, Kasthuri Venkateswaran, and Ambrose Cheung for bacterial strains, Michel Débarbouillé for pMAD, and Kenneth Bayles for φ11 lysate and helpful discussion. We thank Peter Zuber for reading the manuscript. We thank Lydie Herfort for sampling of water from the Columbia River Estuary and Jacob Delepine for technical assistance. We would like to thank Randy Whittal (Mass Spectrometry Facility, Department of Chemistry, University of Alberta) for performing the FTICR analysis, as well as Ryan McKay at the Canadian National High Field NMR Centre (NANUC) for running the NMR experiments on amicoumacin A.

Author Contributions

Conceived and designed the experiments: JP JCV MMN. Performed the experiments: AL JP TC AMW CSS MMN. Analyzed the data: AL JP AMW CSS MMN. Contributed reagents/materials/analysis tools: JCV MH MMN. Wrote the paper: AL JP CSS MMN.


  1. 1. Chambers HF, DeLeo FR (2009) Waves of resistance: Staphylococcus aureus in the antibiotic era. Nat Rev Microbiol 7: 629–641.
  2. 2. Fuda C, Suvorov M, Vakulenko SB, Mobashery S (2004) The basis for resistance to beta-lactam antibiotics by penicillin-binding protein 2a of methicillin-resistant Staphylococcus aureus. J Biol Chem 279: 40802–40806.
  3. 3. Couto I, de Lencastre H, Severina E, Kloos W, Webster JA, et al. (1996) Ubiquitous presence of a mecA homologue in natural isolates of Staphylococcus sciuri. Microb Drug Resist 2: 377–391.
  4. 4. Ito T, Katayama Y, Hiramatsu K (1999) Cloning and nucleotide sequence determination of the entire mec DNA of pre-methicillin-resistant Staphylococcus aureus N315. Antimicrob Agents Chemother 43: 1449–1458.
  5. 5. Boucher HW, Corey GR (2008) Epidemiology of methicillin-resistant Staphylococcus aureus. Clin Infect Dis 46: S344–349.
  6. 6. Hiramatsu K, Aritaka N, Hanaki H, Kawasaki S, Hosoda Y, et al. (1997) Dissemination in Japanese hospitals of strains of Staphylococcus aureus heterogeneously resistant to vancomycin. Lancet 350: 1670–1873.
  7. 7. Itoh J, Omoto S, Shomura T, Nishizawa N, Miyado S, et al. (1981) Amicoumacin-A, a new antibiotic with strong antiinflammatory and antiulcer activity. J Antibiot (Tokyo) 34: 611–613.
  8. 8. Shimojima Y, Hayashi H, Ooka T, Shibukawa M (1982) Production, isolation and pharmacological studies of AI-77s. Agric Biol Chem 46: 1823–1829.
  9. 9. Shimojima Y, Hayashi H, Ooka T, Shibukawa M (1982) Studies on AI-77s, microbial products with pharmacological activity - Structures and the chemical nature of AI-77s. Tet Lett 23: 5435–5438.
  10. 10. Shimojima Y, Hayashi H, Ooka T, Shibukawa M (1984) Studies on AI-77s, microbial products with gastroprotective activity -Structures and the chemical nature of AI-77s. Tetrahedron 40: 2519–2527.
  11. 11. Azumi M, Ogawa K, Fujita T, Takeshita M, Yoshida R, et al. (2008) Bacilosarcins A and B, novel bioactive isocoumarins with unusual heterocyclic cores from the marine-derived bacterium Bacillus subtlis. Tetrahedron 64: 6420–6425.
  12. 12. Canedo LM, Fernandez Puentes JL, Perez Baz J, Acebal C, de la Calle F, et al. (1997) PM-94128, a new isocoumarin antitumor agent produced by a marine bacterium. J Antibiot 50: 175–176.
  13. 13. Huang YF, Li LH, Tian L, Qiao L, Hua HM, et al. (2006) Sg17-1-4, a novel isocoumarin from a marine fungus Alternaria tenuis Sg17-1. J Antibiot 59: 355–357.
  14. 14. McInerney BV, Taylor WC, Lacey MJ, Akhurst RJ, Gregson RP (1991) Biologically active metabolites from Xenorhabdus spp., Part 2. Benzopyran-1-one derivatives with gastroprotective activity. J Nat Prod 54: 785–795.
  15. 15. Sato T, Nagai K, Suzuki K, Morioka M, Saito T, et al. (1992) A new isocoumarin antibiotic, Y-05460M-A. J Antibiot 45: 1949–1952.
  16. 16. Pinchuk IV, Bressollier P, Verneuil B, Fenet B, Sorokulova IB, et al. (2001) In vitro anti-Helicobacter pylori activity of the probiotic strain Bacillus subtilis 3 is due to secretion of antibiotics. Antimicrob Agents Chemother 45: 3156–3161.
  17. 17. Shinabarger DL, Marotti KR, Murray RW, Lin AH, Melchior EP, et al. (1997) Mechanism of action of oxazolidinones: effects of linezolid and eperezolid on translation reactions. Antimicrob Agents Chemother 41: 2132–2136.
  18. 18. Silverman JA, Perlmutter NG, Shapiro HM (2003) Correlation of daptomycin bactericidal activity and membrane depolarization in Staphylococcus aureus. Antimicrob Agents Chemother 47: 2538–2544.
  19. 19. Hashimoto M, Taguchi T, Nishida S, Ueno K, Koizumi K, et al. (2007) Isolation of 8′-phosphate ester derivatives of amicoumacins: structure-activity relationship of hydroxy amino acid moiety. J Antibiot (Tokyo) 60: 752–756.
  20. 20. Gioia J, Yerrapragada S, Qin X, Jiang H, Igboeli OC, et al. (2007) Paradoxical DNA repair and peroxide resistance gene conservation in Bacillus pumilus SAFR-032. PLoS One 2: e928.
  21. 21. Nakano MM, Corbell N, Besson J, Zuber P (1992) Isolation and characterization of sfp - a gene that functions in the production of the lipopeptide biosurfactant, surfactin, in Bacillus subtilis. Mol Gen Genet 232: 313–321.
  22. 22. Lambalot RH, Gehring AM, Flugel RS, Zuber P, LaCelle M, et al. (1996) A new enzyme superfamily - The phosphopantetheinyl transferases. Chem Biol 3: 923–936.
  23. 23. Park D, Ciezki K, van der Hoeven R, Singh S, Reimer D, et al. (2009) Genetic analysis of xenocoumacin antibiotic production in the mutualistic bacterium Xenorhabdus nematophila. Mol Microbiol 73: 938–849.
  24. 24. Brazas MD, Hancock RE (2005) Using microarray gene signatures to elucidate mechanisms of antibiotic action and resistance. Drug Discov Today 10: 1245–1252.
  25. 25. Kenny JG, Ward D, Josefsson E, Jonsson IM, Hinds J, et al. (2009) The Staphylococcus aureus response to unsaturated long chain free fatty acids: survival mechanisms and virulence implications. PLoS One 4: e4344.
  26. 26. 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.
  27. 27. Pane-Farre J, Jonas B, Forstner K, Engelmann S, Hecker M (2006) The sigmaB regulon in Staphylococcus aureus and its regulation. Int J Med Microbiol 296: 237–258.
  28. 28. Hecker M, Pane-Farre J, Volker U (2007) SigB-dependent general stress response in Bacillus subtilis and related gram-positive bacteria. Annu Rev Microbiol 61: 215–236.
  29. 29. Price CW (2002) General stress response. In: Sonenshein AL, Hoch JA, Losick R, editors. Bacillus subtilis and its closest relatives. Washington, D. C.: ASM press. pp. 369–384.
  30. 30. Groicher KH, Firek BA, Fujimoto DF, Bayles KW (2000) The Staphylococcus aureus lrgAB operon modulates murein hydrolase activity and penicillin tolerance. J Bacteriol 182: 1794–1801.
  31. 31. Rice KC, Firek BA, Nelson JB, Yang SJ, Patton TG, et al. (2003) The Staphylococcus aureus cidAB operon: evaluation of its role in regulation of murein hydrolase activity and penicillin tolerance. J Bacteriol 185: 2635–2643.
  32. 32. Stapleton MR, Horsburgh MJ, Hayhurst EJ, Wright L, Jonsson IM, et al. (2007) Characterization of IsaA and SceD, two putative lytic transglycosylases of Staphylococcus aureus. J Bacteriol 189: 7316–7325.
  33. 33. Ramadurai L, Lockwood KJ, Nadakavukaren MJ, Jayaswal RK (1999) Characterization of a chromosomally encoded glycylglycine endopeptidase of Staphylococcus aureus. Microbiology 145: 801–808.
  34. 34. Oshida T, Sugai M, Komatsuzawa H, Hong YM, Suginaka H, et al. (1995) A Staphylococcus aureus autolysin that has an N-acetylmuramoyl-L-alanine amidase domain and an endo-beta-N-acetylglucosaminidase domain: cloning, sequence analysis, and characterization. Proc Natl Acad Sci USA 92: 285–289.
  35. 35. Kuroda M, Ohta T, Hayashi H (1995) Isolation and the gene cloning of an alkaline shock protein in methicillin resistant Staphylococcus aureus. Biochem Biophys Res Commun 207: 978–984.
  36. 36. Bayles KW (2007) The biological role of death and lysis in biofilm development. Nat Rev Microbiol 5: 721–726.
  37. 37. Heilmann C, Hartleib J, Hussain MS, Peters G (2005) The multifunctional Staphylococcus aureus autolysin aaa mediates adherence to immobilized fibrinogen and fibronectin. Infect Immun 73: 4793–4802.
  38. 38. Baba T, Schneewind O (1998) Targeting of muralytic enzymes to the cell division site of Gram-positive bacteria: repeat domains direct autolysin to the equatorial surface ring of Staphylococcus aureus. EMBO J 17: 4639–4646.
  39. 39. Schlag M, Biswas R, Krismer B, Kohler T, Zoll S, et al. (2010) Role of staphylococcal wall teichoic acid in targeting the major autolysin Atl. Mol Microbiol 75: 864–873.
  40. 40. Mwangi MM, Wu SW, Zhou Y, Sieradzki K, de Lencastre H, et al. (2007) Tracking the in vivo evolution of multidrug resistance in Staphylococcus aureus by whole-genome sequencing. Proc Natl Acad Sci USA 104: 9451–9456.
  41. 41. Johanson U, Hughes D (1994) Fusidic acid-resistant mutants define three regions in elongation factor G of Salmonella typhimurium. Gene 143: 55–59.
  42. 42. Chen HJ, Hung WC, Tseng SP, Tsai JC, Hsueh PR, et al. (2010) Fusidic acid resistance determinants in Staphylococcus aureus clinical isolates. Antimicrob Agents Chemother 54: 4985–4991.
  43. 43. Norstrom T, Lannergard J, Hughes D (2007) Genetic and phenotypic identification of fusidic acid-resistant mutants with the small-colony-variant phenotype in Staphylococcus aureus. Antimicrob Agents Chemother 51: 4438–4446.
  44. 44. Helser TL, Davies JE, Dahlberg JE (1971) Change in methylation of 16 S ribosomal RNA associated with mutation to kasugamycin resistance in Escherichia coli. Nat New Biol 233: 12–14.
  45. 45. AEvarsson A, Brazhnikov E, Garber M, Zheltonosova J, Chirgadze Y, et al. (1994) Three-dimensional structure of the ribosomal translocase: elongation factor G from Thermus thermophilus. EMBO J 13: 3669–3677.
  46. 46. Laurberg M, Kristensen O, Martemyanov K, Gudkov AT, Nagaev I, et al. (2000) Structure of a mutant EF-G reveals domain III and possibly the fusidic acid binding site. J Mol Biol 303: 593–603.
  47. 47. Patton TG, Yang SJ, Bayles KW (2006) The role of proton motive force in expression of the Staphylococcus aureus cid and lrg operons. Mol Microbiol 59: 1395–1404.
  48. 48. Muthaiyan A, Silverman JA, Jayaswal RK, Wilkinson BJ (2008) Transcriptional profiling reveals that daptomycin induces the Staphylococcus aureus cell wall stress stimulon and genes responsive to membrane depolarization. Antimicrob Agents Chemother 52: 980–990.
  49. 49. Wang D, Jin Q, Xiang H, Wang W, Guo N, et al. (2011) Transcriptional and functional analysis of the effects of magnolol: inhibition of autolysis and biofilms in Staphylococcus aureus. PLoS One 6: e26833.
  50. 50. Renzoni A, Barras C, Francois P, Charbonnier Y, Huggler E, et al. (2006) Transcriptomic and functional analysis of an autolysis-deficient, teicoplanin-resistant derivative of methicillin-resistant Staphylococcus aureus. Antimicrob Agents Chemother 50: 3048–3061.
  51. 51. Takahashi J, Komatsuzawa H, Yamada S, Nishida T, Labischinski H, et al. (2002) Molecular characterization of an atl null mutant of Staphylococcus aureus. Microbiol Immunol 46: 601–612.
  52. 52. Houston P, Rowe SE, Pozzi C, Waters EM, O'Gara JP (2010) Essential role for the major autolysin in the fibronectin-binding protein-mediated Staphylococcus aureus biofilm phenotype. Infect Immun 79: 1153–1165.
  53. 53. Sugai M, Yamada S, Nakashima S, Komatsuzawa H, Matsumoto A, et al. (1997) Localized perforation of the cell wall by a major autolysin: atl gene products and the onset of penicillin-induced lysis of Staphylococcus aureus. J Bacteriol 179: 2958–2962.
  54. 54. Igo MM, Losick R (1986) Regulation of a promoter that is utilized by minor forms of RNA polymerase holoenzyme in Bacillus subtilis. J Mol Biol 191: 615–624.
  55. 55. Charbonnier Y, Gettler B, Francois P, Bento M, Renzoni A, et al. (2005) A generic approach for the design of whole-genome oligoarrays, validated for genomotyping, deletion mapping and gene expression analysis on Staphylococcus aureus. BMC Genomics 6: 95.
  56. 56. Becher D, Hempel K, Sievers S, Zuhlke D, Pane-Farre J, et al. (2009) A proteomic view of an important human pathogen–towards the quantification of the entire Staphylococcus aureus proteome. PLoS One 4: e8176.
  57. 57. Saeed AI, Bhagabati NK, Braisted JC, Liang W, Sharov V, et al. (2006) TM4 microarray software suite. Methods Enzymol 411: 134–193.
  58. 58. Gertz S, Engelmann S, Schmid R, Ohlsen K, Hacker J, et al. (1999) Regulation of sigmaB-dependent transcription of sigB and asp23 in two different Staphylococcus aureus strains. Mol Gen Genet 261: 558–566.
  59. 59. Wetzstein M, Volker U, Dedio J, Lobau S, Zuber U, et al. (1992) Cloning, sequencing, and molecular analysis of the dnaK locus from Bacillus subtilis. J Bacteriol 174: 3300–3310.
  60. 60. de Jonge BL, Chang YS, Gage D, Tomasz A (1992) Peptidoglycan composition of a highly methicillin-resistant Staphylococcus aureus strain. The role of penicillin binding protein 2A. J Biol Chem 267: 11248–11254.
  61. 61. Arnaud M, Chastanet A, Debarbouille M (2004) New vector for efficient allelic replacement in naturally nontransformable, low-GC-content, gram-positive bacteria. Appl Environ Microbiol 70: 6887–6891.
  62. 62. Stragier P, Bonamy C, Karmazyn-Campelli C (1988) Processing of a sporulation factor in Bacillus subtilis: How morphological structure could control gene expression. Cell 52: 697–704.