A LacI-Family Regulator Activates Maltodextrin Metabolism of Enterococcus faecium

Abstract

Enterococcus faecium is a gut commensal of humans and animals. In the intestinal tract, E. faecium will have access to a wide variety of carbohydrates, including maltodextrins and maltose, which are the sugars that result from the enzymatic digestion of starch by host-derived and microbial amylases. In this study, we identified the genetic determinants for maltodextrin utilization of E. faecium E1162. We generated a deletion mutant of the mdxABCD-pulA gene cluster that is homologous to maltodextrin uptake genes in other Gram-positive bacteria, and a deletion mutant of the mdxR gene, which is predicted to encode a LacI family regulator of mdxABCD-pulA. Both mutations impaired growth on maltodextrins but had no effect on the growth on maltose and glucose. Comparative transcriptome analysis showed that eight genes (including mdxABCD-pulA) were expressed at significantly lower levels in the isogenic ΔmdxR mutant strain compared to the parental strain when grown on maltose. Quantitative real-time RT-PCR confirmed the results of transcriptome analysis and showed that the transcription of a putative maltose utilization gene cluster is induced in a semi-defined medium supplemented with maltose but is not regulated by MdxR. Understanding the maltodextrin metabolism of E. faecium could yield novel insights into the underlying mechanisms that contribute to the gut commensal lifestyle of E. faecium.

About the Authors:

Xinglin Zhang

* E-mail: [email protected]

Affiliation: Department of Medical Microbiology, University Medical Center Utrecht, Utrecht, The Netherlands

Malbert Rogers

Affiliation: Department of Medical Microbiology, University Medical Center Utrecht, Utrecht, The Netherlands

Damien Bierschenk

Affiliation: Department of Medical Microbiology, University Medical Center Utrecht, Utrecht, The Netherlands

Marc J. M. Bonten

Affiliation: Department of Medical Microbiology, University Medical Center Utrecht, Utrecht, The Netherlands

Rob J. L. Willems

Affiliation: Department of Medical Microbiology, University Medical Center Utrecht, Utrecht, The Netherlands

Willem van Schaik

Affiliation: Department of Medical Microbiology, University Medical Center Utrecht, Utrecht, The Netherlands

Introduction

Enterococci are facultative anaerobic Gram-positive bacteria commonly found in the gastrointestinal tracts of humans and animals [1]. In the last twenty years, E. faecium has emerged as a clinical pathogen of major importance. This development has been linked to its ability to efficiently acquire antibiotic resistance genes and genetic elements that may contribute to virulence [2,3].

The ability of both commensal and clinical E. faecium strains to effectively colonize the intestinal tract determines the ecological success of this species. Therefore, understanding the mechanisms of successful host colonization is important for the development of novel strategies to prevent or treat infections with these opportunistic pathogens. The metabolism of carbohydrates in the complicated food webs of the mammalian intestinal tract is crucially important for gut colonization of commensals and opportunistic pathogens [4–8]. Carbohydrate utilization of E. faecium remains poorly understood despite its potential importance in colonization and adaptation to healthy individuals [9] and hospitalized patients [10].

One of the main energy and carbon sources for bacteria in the intestine originates from complex polysaccharides, such as starch [4]. Starch is a plant storage glycan that consists of glucose monomers joined via α-1,4 glycosidic linkages with additional branches introduced by α-1,6 linked glucose moieties. In the human intestinal tract, starch is digested by host-derived and microbial amylases. Its breakdown products (mainly maltose and maltodextrins) can be absorbed by the host small intestine [11], but can also reach the colon [12,13] where they can be metabolized by bacteria from several genera [14,15]. The metabolism of maltodextrin has been investigated in Escherichia coli [16,17] and in several Gram-positive bacteria, including Bacillus subtilis [18,19], Listeria monocytogenes [20] and Streptococcus pyogenes [21,22]. The maltose/maltodextrin regulon in E. coli consists of ten genes encoding four glycoside hydrolases, a maltodextrin phosphorylase, a maltodextrin glucosidase, a periplasmic α-amylase, together with an ATP-binding cassette (ABC) transporter [16,17]. In B. subtilis, maltose and maltodextrin are separately transported by a maltose-specific phosphotransferase system and a maltodextrin-specific ABC transporter, respectively [18], while in L. monocytogenes both maltose and maltodextrin are taken up by the same ABC transporter [20]. In this study, we identified the determinants of maltodextrin uptake and metabolism in E. faecium.

Materials and Methods

Bacterial strains, plasmids and growth conditions

E. faecium strains, E. coli strains and plasmids used or generated in this study are listed in Table 1. The E. faecium strain E1162 (with sequence type 17) was used throughout this study. This strain was isolated from a bloodstream infection in France in 1996 and its genome has previously been sequenced [23]. Unless otherwise mentioned, E. faecium was grown in brain heart infusion broth (BHI; Oxoid) at 37° C. The E. coli strains DH5α (Invitrogen) and EC1000 [24] were grown in Luria-Bertani medium. Where necessary, antibiotics were used at the following concentrations: gentamicin at 300 µg ml−1 for E. faecium and 25 µg ml−1 for E. coli, spectinomycin at 300 µg ml−1 for E. faecium and 100 µg ml−1 for E. coli. All antibiotics were obtained from Sigma-Aldrich (Saint Louis, MO). Growth of cultures was determined by measuring the optical density at 660 nm (OD660).

Strain or plasmid Relevant characteristic(s) Source or reference

E. faecium

E1162 Clinical isolate (bloodstream infection), isolated in France, 1996 [23]

ΔmdxR Markerless deletion mutant of mdxR of E1162 This study

ΔmdxABCD-pulA Markerless deletion mutant of the mdxABCD-pulA gene cluster of E1162 This study

ΔmdxR+mdxR Complementation strain of ΔmdxR; ΔmdxR harboring pEF25-mdxR This study

E. coli strains

DH5α E. coli host strain for routine cloning Invitrogen

EC1000 MC1000 glgB::repA; host strain for pWS3 derived vectors [24]

Plasmids

pWS3 Gram-positive thermosensitive origin of replication; Spcr [9]

pDEL1a pWS3 carrying the 5′ and 3′ flanking regions of mdxR for mutant construction This study

pDEL2a pWS3 carrying the 5′ and 3′ flanking regions of mdxABCD-pulA gene cluster for mutant construction This study

pDEL1b pDEL1a with a Genr cassette which was flanked by lox66- and lox71-sites cloned between the 5′ and 3′ flanking regions This study

pDEL2b pDEL2a with a Genr cassette which was flanked by lox66- and lox71-sites cloned between the 5′ and 3′ flanking regions This study

pWS3-Cre pWS3 derivative expressing Cre in E. faecium [26]

pEF25 Shuttle plasmid pAT18 with spectinomycin resistance cassette cloned in the EcoRI site; Spcr Eryr [27]

pEF25-mdxR Complementation plasmid for ΔmdxR; pEF25 carrying gene mdxR This study

Table 1. Strains and plasmids used in this study.

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Construction of deletion mutants and in trans complementation

Markerless gene deletion mutants in the mdxR gene (locustag: EfmE1162_2133) and the mdxABCD-pulA gene cluster (locustag: EfmE1162_0366 - EfmE1162_0370) were created via the Cre-lox recombination system as previously described [25,26]. Briefly, the 5′ and 3′ flanking regions (approximately 500 bp each) of the target genes were PCR amplified with the primers in Table 2. The two flanking regions were then fused together by fusion PCR (generating an EcoRI site between both fragments) and cloned into pWS3 [9], resulting in pDEL1a and pDEL2a. Then a gentamicin-resistance cassette which was flanked by lox66- and lox71-sites [26] was cloned into the EcoRI site that was generated between the 5′ and 3′ flanking regions in pDEL1a and pDEL2a, respectively. The resulting plasmids pDEL1b and pDEL2b were then electrotransformed into E. faecium E1162. Marked mutants were obtained by growing the gentamicin-resistant transformants at appropriate temperatures supplemented with appropriate antibiotics [26]. The plasmid pWS3-Cre [26], carrying a gene encoding Cre recombinase, was introduced into the marked mutant by electroporation and further culturing for the removal of the gentamicin resistance cassette and subsequent loss of pWS-Cre was performed as previously described [26]. Excision of the gentamicin resistance cassette and loss of pWS3-Cre was verified by PCR using primers listed in Table 2.

Primer Sequencea

delete_XhoI_mdxR_up_F 5′-CCGCTCGAGcctgcacctttggaatatgg-3′

delete_EcoRI_mdxR_up_R 5′-AACCTTGACTCGCCCCTTGAATTCacgttttgcaacatctgct-3′

delete_EcoRI_mdxR_dn_F 5′-GAATTCaaggggcgagtcaaggttat-3′

delete_XmaI_mdxR_dn_R 5′-CCCCCCGGGtgattggtaatggccggtat-3′

check_mdxR_up 5′-catgatcagcttgcagttgg-3′

check_mdxR_dn 5′-gtgtcaacagatgcgtttcg-3′

delete_XhoI_mdxABCD-pulA_up_F 5′-CCGCTCGAGtgcttgctgataagcatcgt-3′

delete_EcoRI_mdxABCD-pulA_up_R 5′-cgaccggaaagtgaaGAATTCaataggttccatggcagcag-3′

delete_EcoRI_mdxABCD-pulA_dn_F 5′-ggaacctattGAATTCttcactttccggtcgatgat-3′

delete_XmaI_mdxABCD-pulA_dn_R 5′-CCCCCCGGGttcctagaccgctgacacct-3′

check_mdxABCD-pulA_up 5′-tctttctttggcagccattt-3′

check_mdxABCD-pulA_dn 5′-gacagacaacaaccgatctgaa-3′

qPCR_mdxR_F 5′-agccgacagcaacagtctga-3′

qPCR_mdxR_R 5′-gctcgccgttcaagcattat-3′

qPCR_malP_F 5′-agcgcagcaagcagaaaaag-3′

qPCR_malP_R 5′-cttccatcgttctgcccaag-3′

qPCR_malT_F 5′-gaatcggtgcgctttcttgt-3′

qPCR_malT_R 5′-cgtggcattgattcttgctg-3′

qPCR_tuf_F 5′-TACACGCCACTACGCTCAC-3′

qPCR_tuf_R 5′-AGCTCCGTCCATTTGAGCAG-3′

pAT392_EcoRI_lox66_genta_F 5′-AGGGAATTCTACCGTTCGTATAGCATACATTATACGAAGTTATG ATAAACCCAGCGAACCATTTGAGG-3′

pAT392_EcoRI_lox71_genta_R 5′-CTCCGAATTCTACCGTTCGTATAATGTATGCTATACGAAGTTATT CAATCTTTATAAGTCCTTTTATAA-3′

Table 2. Primers used in this study.

aRestriction sites are underlined.

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An in trans complementated strain (ΔmdxR+mdxR) of the mdxR deletion mutant (ΔmdxR) was generated as previously described [26,27]. The gene mdxR was amplified by PCR from the genomic DNA of E1162 using the primers listed in Table 2. The PCR product was cloned into the shuttle vector pEF25 [27]. The resulting plasmid, pEF25-mdxR, was introduced into the ΔmdxR mutant strain by electroporation as described above [26].

Determination of growth curves

A BioScreen C instrument (Oy Growth Curves AB, Helsinki, Finland) was used to determine the growth of E. faecium strains on starch, maltodextrin, maltose and glucose. Strains were grown overnight in BHI containing appropriate antibiotics at 37° C. Subsequently, cells were inoculated at an initial OD660 of 0.0025 in M1 medium. M1 is a semi-defined medium in which E. faecium is hardly able to grow when no carbon source is added to the medium [9]. Here, M1 medium was supplemented with starch, the maltodextrin maltoheptaose and maltotetraose, maltose or glucose (2.5 g/l) as carbon sources (all carbohydrates were purchased from Sigma-Aldrich). Cultures were incubated in the Bioscreen C system at 37° C with continuous shaking. The absorbance at 600nm (A600) was recorded every 15 min for 12 hours. Each experiment was performed in triplicate.

Transcriptome profiling

Transcriptome comparisons were performed between the parental strain wild-type E1162 and mutant strain ΔmdxR in two conditions. Both strains were grown to mid-exponential (OD660 = 0.3) phase in BHI and in M1 supplemented with maltose (M1+maltose), and then RNA isolation, cDNA synthesis and hybridization were performed as described in our previous work [26]. Analysis for statistical significance were performed using the Web-based VAMPIRE microarray suite (http://sasquatch.ucsd.edu/vampire/) as described previously [28,29]. A gene of which all four probes on the microarray were identified as differentially expressed with a false discovery rate <0.05, was classified as significantly differentially expressed between samples. In addition, genes which exhibited an expression between 0.5- and 2-fold different from the wild-type were deemed biologically insignificant and were filtered out. This experiment was performed with four biological replicates.

The microarray data generated for the transcriptome analysis in this study have been deposited in the ArrayExpress database (http://www.ebi.ac.uk/arrayexpress) under accession numbers E-MEXP-3759 (M1+maltose) and E-MEXP-3760 (BHI).

Quantitative real-time RT-PCR (qRT-PCR)

The total RNA samples of the transcriptome profiling experiment were also used for qRT-PCR. The absence of genomic DNA was verified by PCR prior to reverse transcription. The cDNA was synthesized from total RNA (~1.0 µg) by using the Superscript III First-Strand Synthesis System (Invitrogen, Breda, The Netherlands) according to the manufacturer’s instructions. Using synthesized cDNAs, qRT-PCR was performed using Maxima SYBR Green/ROX qPCR Master Mix (Fermentas, Sankt Leon-Rot, Germany) and a StepOnePlus instrument (Applied Biosystems, Nieuwekerk a/d IJssel, The Netherlands) with the following program: 95° C for 10 min, and subsequently 40 cycles of 95° C for 15 sec, 55° C for 1 min. The expression of tufA was used as a housekeeping control [28]. The Ct value of each sample was normalized by the amplification efficiency. The relative transcript level (fold difference relative to tufA) of the tested genes were calculated by using the normalized Ct value of the tufA housekeeping control minus the normalized Ct value of the tested genes. The resulting value represents a log2 transformed fold difference in gene expression. Statistical significance between wild-type and mutant was assessed by the unpaired two-tailed Student’s t-test. This experiment was performed with four biological replicates.

Results

Identification of genes putatively involved in maltodextrin utilization in E. faecium

The genome sequence of E. faecium strain E1162 was analyzed to identify genes potentially responsible for the utilization of maltodextrin and maltose in E. faecium. A search of the E1162 genome for the orthologs of the L. monocytogenes and B. subtilis maltodextrin utilization proteins led to the identification of a gene cluster (locus tags EfmE1162_0366 - EfmE1162_0370; here termed mdxABCD-pulA), that is predicted to encode maltose/maltodextrin ABC transporter proteins and a neopullulanase which is predicted to hydrolyze the α-1,4 linkages in starch. The encoded proteins are homologous to the maltodextrin utilization proteins of L. monocytogenes EGD-e (amino acid identity: 31%-79%) [20] and B. subtilis 168 (amino acid identity: 25%-72%) [18] (Figure 1). In L. monocytogenes EGD-e, a regulator gene lmo2128 is located immediately upstream of the maltodextrin utilization gene cluster. In E. faecium E1162, a gene (locus tag: EfmE1162_2133, here termed mdxR) encoding a LacI family transcriptional regulator shares the highest amino acid identity (53%) with Lmo2128. The mdxR gene is located on a different contig and consequently is not in the immediate vicinity of the mdxABCD-pulA gene cluster. Analysis of the complete genome sequence of E. faecium Aus0004 [30] showed that mdxR and the mdxABCD-pulA gene cluster are located at a distance of 28 kb. The last gene (lmo2121) in the maltodextrin utilization gene cluster of L. monocytogenes EGD-e encodes a maltose phosphorylase, however the gene (EfmE1162_1486, termed malP here) that is homologous to lmo2121 is not part of the mdxABCD-pulA gene cluster in E1162. In E. faecium Aus0004, malP and the mdxABCD-pulA gene cluster are spaced 48 kb apart. Evidently, there are major differences in genomic organization between the maltodextrin utilization gene clusters of E. faecium and L. monocytogenes, possibly reflecting functional differences in the metabolism of maltodextrins and maltose between the two organisms.

[Figure omitted. See PDF.]

Figure 1. Schematic representation of the gene clusters involved in maltodextrin and maltose utilization of E. faecium E1162.

Genes are represented by arrows (drawn to scale). Genes putatively encoding proteins involved in maltodextrin transport and/or metabolism are indicated in blue or in red. Genes predicted to be involved in the uptake and/or metabolism of maltose are indicated in green or in purple. The genes that encode putative transcriptional regulators are indicated in red or purple. The grey arrows represent the adjacent genes that are not predicted to be involved in maltodextrin or maltose utilization. Gene names, without the EfmE1162-prefix (omitted for reasons of space), are indicated in the arrows and the gene locus tags are indicated above or below the arrows. The homologs in L. monocytogenes EGD-e or in E. faecalis V583 are shown with corresponding colors above or below the gene clusters of E. faecium. The gene locus tags of the homologs are indicated in the arrows. Lines link the homologous genes with corresponding genes in E. faecium and amino acid identities are indicated.

https://doi.org/10.1371/journal.pone.0072285.g001

BLAST analysis showed that all genes of the mdxABCD-pulA gene cluster are conserved (with amino acid identities >82%) in 66 of the 68 E. faecium genomes available (on 16 October 2012) at NCBI Genomes, but no homologous gene cluster is present in E. faecalis. The observation that E. faecalis strains without this gene cluster could also grow in M1 with maltodextrin (data not shown) indicates that E. faecalis has different maltodextrin utilization mechanisms than E. faecium. The functional conservation of maltodextrin utilization in E. faecium and E. faecalis indicates that these traits have been conserved throughout the evolution of these organisms and thus likely contribute to fitness of these commensal bacteria.

Deletion of mdxR and the mdxABCD-pulA gene cluster impair growth on maltodextrin

To determine the role of the mdxABCD-pulA gene cluster in the ability to grow on maltodextrin, a markerless deletion mutant (ΔmdxABCD-pulA) of all five genes in the mdxABCD-pulA gene cluster was constructed in E. faecium E1162. Additionally, a deletion mutant of the gene (mdxR) putatively encoding a transcriptional regulator involved in regulating expression of the mdxABCD-pulA gene cluster was also generated to characterize its role in gene regulation and carbohydrate utilization in E. faecium E1162. The mutant ΔmdxR was complemented in trans (ΔmdxR+mdxR), but the in trans complemented strain for mutant ΔmdxABCD-pulA could not be constructed, presumably due to the large size (6.3 kb) of the DNA fragment encompassing this gene cluster. Growth of E. faecium E1162 wild-type (WT), the isogenic mutants and the complemented strain on M1 [9] supplemented with starch, maltodextrin (in the form of maltotetraose), maltose or glucose were determined (Figure 2). The strains did not exhibit appreciable growth on M1 with starch, demonstrating that E1162 could not directly utilize starch. All strains showed identical growth in M1 with glucose, indicating that the introduced mutations did not cause a general growth defect. However, in M1 supplemented with maltotetraose, the growth of the ΔmdxR and ΔmdxABCD–pulA mutants were impaired, while in M1 supplemented with maltose the growth of these two mutants was comparable to wild-type and the complemented strain. The growth of the ΔmdxR and ΔmdxABCD–pulA mutants was also impaired in M1 supplemented with maltoheptaose and other maltodextrins with dextrose equivalents of 4.0-7.0, 13-17 and 16.5-19.5 (data not shown). These results show that the mdxABCD-pulA gene cluster of E. faecium is essential for the metabolism of maltodextrin but not for maltose.

[Figure omitted. See PDF.]

Figure 2. Growth of E. faecium on starch, maltotetraose, maltose and glucose.

Growth curves of E. faecium E1162 wild-type (black), its isogenic mutants ΔmdxR (red) and ΔmdxABCD-pulA (blue), and the in trans complemented strain ΔmdxR+mdxR (green) on starch (panel A), maltotetraose (panel B), maltose (panel C) and glucose (panel D) are shown. The growth curve of E1162 wild-type in M1 was shown in grey as a negative control. Overnight cultures were inoculated at an initial OD660 of 0.0025 into 300 µl semi-defined minimal medium M1 [9], M1 supplemented with 2.5 g/l of starch, maltotetraoise, maltose or glucose as sole carbon source, respectively, and then incubated in the Bioscreen C system at 37° C with continuous shaking. The absorbance of 600nm (A600) was recorded every 15 min for 12 hours. Growth curves are mean data of three independent experiments. Note that A600 at the start of the experiment is higher in M1 + starch than in the other conditions, due to increased turbidity of the medium containing starch.

https://doi.org/10.1371/journal.pone.0072285.g002

MdxR positively regulates the gene expression of the mdxABCD-pulA gene cluster

In L. monocytogenes and B. subtilis, the expression of the maltodextrin/maltose utilization systems is induced by maltose or maltodextrin [18,20]. To identify the genes that are controlled by MdxR in E. faecium, the transcriptome of the ΔmdxR mutant was first compared to the transcriptome of its parental strain E. faecium E1162 grown to mid-exponential phase in M1 supplemented with maltose (Table 3). We observed eight genes that were significantly lower expressed and four genes that were significantly higher expressed in the ΔmdxR mutant strain in comparison to the parental strain during growth in M1 with maltose. Almost all of these genes have a putative role in carbohydrate metabolism, indicating that MdxR does not act globally but rather is specific for a relatively small number of genes. All the genes of the mdxABCD-pulA gene cluster were expressed at lower levels in the ΔmdxR mutant, which confirmed the prediction that MdxR regulates the transcription of this cluster of genes. Three other genes (EfmE1162_1270, EfmE1162_1401, and EfmE1162_1402, which are not located in the immediate vicinity of the mdxABCD-pulA gene cluster were also expressed at lower levels in the mdxR deletion mutant. EfmE1162_1270 and EfmE1162_1401 were annotated as encoding oligo-1,6-glucosidases that share 43% and 51% amino acid identity with the MalL protein of B. subtilis 168. MalL is involved in the breakdown of maltodextrin in B. subtilis 168 [18] which suggests that EfmE1162_1270 and EfmE1162_1401 also have a role in the metabolism of maltodextrins in E. faecium. EfmE1162_1402 is predicted to encode a β-glucosidase that hydrolyzes the β-1,4 bonds of sugars like cellobiose, thereby releasing glucose. There were four genes expressed at higher levels in ΔmdxR than in wild-type E1162 during growth in M1+maltose. Three of these genes (EfmE1162_1412 - EfmE1162_1414) were predicted to be involved in glycerol utilization. However, both wild-type E1162 and ΔmdxR were unable to grow in M1 supplemented with glycerol in aerobic or anaerobic conditions (data not shown), which was consistent with the previously reported inability of E. faecium to grow on glycerol as carbon source [31]. Possibly, E. faecium may be able to grow on glycerol in conditions that were not tested in this or previous studies and the functions of EfmE1162_1412 - EfmE1162_1414 thus remain to be determined.

LocusTaga Accession code Gene name Annotation Expression ratio ΔmdxR/WT

M1+maltose BHI

EfmE1162_0366 ZP_06676211 mdxA conserved hypothetical protein 0.16 -b

EfmE1162_0367 ZP_06676212 mdxB maltose/maltodextrin ABC transporter, permease protein 0.12 -

EfmE1162_0368 ZP_06676213 mdxC maltose/maltodextrin ABC transporter, permease protein 0.27 -

EfmE1162_0369 ZP_06676214 mdxD maltose/maltodextrin ABC transporter, binding protein 0.27 -

EfmE1162_0370 ZP_06676215 pulA Neopullulanase 0.34 -

EfmE1162_1270 ZP_06677115 oligo-1,6-glucosidase 0.23 -

EfmE1162_1401 ZP_06677246 oligo-1,6-glucosidase 0.13 -

EfmE1162_1402 ZP_06677247 beta-glucosidase 0.16 -

EfmE1162_0373 ZP_06676218 conserved hypothetical protein 2.40 -

EfmE1162_1412 ZP_06677257 glycerol kinase 3.05 -

EfmE1162_1413 ZP_06677258 aerobic glycerol-3-phosphate dehydrogenase 3.56 -

EfmE1162_1414 ZP_06677259 glycerol uptake facilitator protein 3.94 -

EfmE1162_0318 ZP_06676163 hypothetical protein - 0.46

EfmE1162_0408 ZP_06676253 hypothetical protein - 0.46

EfmE1162_0932 ZP_06676777 hypothetical protein - 0.40

Table 3. Comparative transcriptome analysis of E. faecium E1162 and the ΔmdxR mutant during mid-exponential growth in M1+maltose and BHI.

aGenes (excluding mdxR) exhibiting significantly different (False Discovery Rate <0.05 and fold-change in expression <0.5 or >2) expression between E1162 wild-type and ΔmdxR during mid-exponential growth (OD660 = 0.3) in M1+maltose or in BHI are included. This experiment was performed with four biological replicates.

bNo significant difference in gene expression.

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As a control, we also performed a transcriptome comparison analysis between the wild-type E1162 and the ΔmdxR mutant strain in BHI (which we routinely use to culture E. faecium and contains 2 g/l glucose). Only three genes encoding hypothetical proteins were expressed at slightly lower levels in ΔmdxR than in wild-type E1162, indicating that regulation by MdxR is unimportant in a rich, glucose-containing medium.

The transcription of a putative maltose utilization gene cluster was induced in M1+maltose and expressed independently of mdxR

Our results above showed that inactivation of the mdxABCD-pulA gene cluster of E1162 impaired the growth on maltodextrin but had no effect on the growth on maltose, suggesting that E1162 possesses a maltose utilization system which works independently of the maltodextrin utilization system. In E. faecalis a gene cluster composed of five genes has been identified as being responsible for maltose uptake and utilization [32,33]. A homology search in E1162 for the orthologs of this gene cluster identified a gene cluster (EfmE1162_1485 - EfmE1162_1489; here named malRMBPT) which is predicted to encode five proteins with amino acid identities ranging from 59% to 87% to their homologs in E. faecalis V583 (Figure 1), and this gene cluster is conserved among all the available genomes of E. faecium (amino acid identities >96%).

We used qRT-PCR to analyze the expression of mdxB (putatively encoding the permease component of the maltodextrin ABC transporter) and two genes (malT and malP) of the maltose utilization gene cluster in wild-type E1162 and its isogenic mutant ΔmdxR grown in BHI and in M1+maltose (Figure 3). We found that, in both wild-type and mutant, the transcription of mdxB was at equally low level when grown in BHI, but was strongly upregulated when grown in M1+maltose. Consistent with the observations in the transcriptome analysis, the transcription of mdxB was significantly lower (0.14 fold) in ΔmdxR than in wild-type E1162 when grown in M1+maltose. In both E1162 and the mdxR mutant, the transcription of malT and malP was greatly induced in M1+maltose compared to BHI. These qPCR data indicate that the EfmE1162_1485 - EfmE1162_1489 gene cluster is regulated independently of MdxR and may be involved in maltose utilization in E. faecium, similar to its homologous gene cluster in E. faecalis [32].

[Figure omitted. See PDF.]

Figure 3. qRT-PCR analysis of mdxB, malT and malP expression ratios in wild-type E1162 and its isogenic mutant ΔmdxR grown in BHI and maltose.

The data from the qRT-PCR were normalized using tufA as an internal standard [28]. The differences in gene expression (log2-transformed data) relative to tufA are shown. Error bars represent the standard deviation of the mean of four biological replicates. Asterisks represent significant differences (*: P<0.01, **: P<0.001, ***: P<0.0001, as determined by an unpaired two-tailed Student’s t-test) between the indicated samples.

https://doi.org/10.1371/journal.pone.0072285.g003

Discussion

Carbohydrate utilization is a fundamental metabolic function in bacteria and is an important determinant for niche-adaptation by commensal bacteria [9,34,35]. In this work, we have identified the genetic determinants of E. faecium that contribute to its ability to metabolize maltodextrin which is present as a breakdown product of starch in the digestive tract of humans and animals. Our results confirm previous data by showing that E. faecium cannot grow on starch [36], indicating that E. faecium can only benefit from the degradation products of starch due to the action of amylolytic enzymes, which are produced by the host and other gut commensals. We show that the mdxABCD-pulA gene cluster of E. faecium confers the ability to grow on maltodextrin. The deletion of mdxABCD-pulA did not affect the growth rate on maltose, suggesting that E. faecium has an independent system for the utilization of maltose. Similarly in B. subtilis, maltose is transported by maltose-specific phosphotransferase system, while maltodextrin is transported by a maltodextrin-specific ABC transporter [18]. In contrast, L. monocytogenes takes up both maltose and maltodextrin by the same ABC transporter [20]. Therefore, we propose that, similar to the situation in B. subtilis, the proteins encoded by the mdxABCD-pulA gene cluster are exclusively involved in maltodextrin transport and metabolism, and do not have a role in maltose metabolism.

Our transcriptome analysis and qRT-PCR experiments showed that the expression of the mdxABCD-pulA gene cluster and the putative maltose utilization gene cluster malRMBPT is induced by maltose and repressed in medium which contains a rapidly-metabolized sugar such as glucose. The expression level of the putative maltose utilization gene cluster is considerably higher in M1+maltose than in BHI, but is unaffected by the deletion of mdxR. The mdxB gene of the maltodextrin transport and metabolism gene cluster was expressed at significantly higher levels in wild-type E1162 than in ΔmdxR when grown in M1+maltose, but, interestingly, in ΔmdxRexpression of mdxB is still higher in M1+maltose than in BHI, suggesting that MdxR is not the sole regulator governing expression of the mdxABCD-pulA gene cluster. A possible explanation is that transcription of the mdxABCD-pulA gene cluster is coregulated by MdxR and HPr kinase/P-Ser-HPr phosphatase (HPrK/P) systems, which in L. monocytogenes [20] and L. lactis [37] represses the expression of genes involved in maltodextrin or maltose utilization in the presence of glucose. Consequently, upregulation of mdxB in M1+maltose may partially result from the release of glucose-mediated repression rather than stimulation by maltose. However, this upregulation is insufficient to support the effective growth on maltodextrin, for which MdxR is absolutely required.

E. faecium possesses a wide range of carbohydrate metabolic pathways [23] allowing utilization of a variety of sugars. In this study, we have identified an E. faecium gene cluster that is responsible for utilization of maltodextrin, a potential important carbon source for E. faecium in the gut. These data could contribute to the mechanistic understanding of the lifestyle of E. faecium as a gut commensal.

Author Contributions

Conceived and designed the experiments: XZ WvS. Performed the experiments: XZ MR DB. Analyzed the data: XZ RJLW WvS. Wrote the manuscript: XZ RJLW MJMB WvS.

Citation: Zhang X, Rogers M, Bierschenk D, Bonten MJM, Willems RJL, van Schaik W (2013) A LacI-Family Regulator Activates Maltodextrin Metabolism of Enterococcus faecium. PLoS ONE 8(8): e72285. https://doi.org/10.1371/journal.pone.0072285

References

1. Top J, Willems R, Bonten M (2008) Emergence of CC17 Enterococcus faecium: from commensal to hospital-adapted pathogen. FEMS Immunol Med Microbiol 52: 297-308. doi:10.1111/j.1348-0421.2008.00039.x. PubMed: 18279340.

2. Willems RJ, Top J, van Schaik W, Leavis H, Bonten M et al. (2012) Restricted Gene Flow among Hospital Subpopulations of Enterococcus faecium. MBio 3(4): e00151-12. PubMed: 22807567.

3. Willems RJ, van Schaik W (2009) Transition of Enterococcus faecium from commensal organism to nosocomial pathogen. Future Microbiol 4: 1125-1135. doi:10.2217/fmb.09.82. PubMed: 19895216.

4. Koropatkin NM, Cameron EA, Martens EC (2012) How glycan metabolism shapes the human gut microbiota. Nat Rev Microbiol 10: 323-335. PubMed: 22491358.

5. Chang DE, Smalley DJ, Tucker DL, Leatham MP, Norris WE et al. (2004) Carbon nutrition of Escherichia coli in the mouse intestine. Proc Natl Acad Sci U S A 101: 7427-7432. doi:10.1073/pnas.0307888101. PubMed: 15123798.

6. Marco ML, Peters TH, Bongers RS, Molenaar D, van Hemert S et al. (2009) Lifestyle of Lactobacillus plantarum in the mouse caecum. Environ Microbiol 11: 2747-2757. doi:10.1111/j.1462-2920.2009.02001.x. PubMed: 19638173.

7. Thomas M, Wrzosek L, Ben-Yahia L, Noordine ML, Gitton C et al. (2011) Carbohydrate metabolism is essential for the colonization of Streptococcus thermophilus in the digestive tract of gnotobiotic rats. PLOS ONE 6: e28789. doi:10.1371/journal.pone.0028789. PubMed: 22216112.

8. Sonnenburg ED, Zheng H, Joglekar P, Higginbottom SK, Firbank SJ et al. (2010) Specificity of polysaccharide use in intestinal Bacteroides species determines diet-induced microbiota alterations. Cell 141: 1241-1252. doi:10.1016/j.cell.2010.05.005. PubMed: 20603004.

9. Zhang X, Vrijenhoek JE, Bonten MJ, Willems RJ, van Schaik W (2011) A genetic element present on megaplasmids allows Enterococcus faecium to use raffinose as carbon source. Environ Microbiol 13: 518-528. doi:10.1111/j.1462-2920.2010.02355.x. PubMed: 20946531.

10. Zhang X, Top J, de Been M, Bierschenk D, Rogers M et al. (2013) Identification of a Genetic Determinant in Clinical Enterococcus faecium Strains That Contributes to Intestinal Colonization During Antibiotic Treatment. J Infect Dis 207: 1780-1786. doi:10.1093/infdis/jit076. PubMed: 23447698.

11. Gray GM (1992) Starch digestion and absorption in nonruminants. J Nutr 122: 172-177. PubMed: 1729468.

12. Englyst HN, Cummings JH (1986) Digestion of the carbohydrates of banana (Musa paradisiaca sapientum) in the human small intestine. Am J Clin Nutr 44: 42-50. PubMed: 3014853.

13. Englyst HN, Cummings JH (1987) Digestion of polysaccharides of potato in the small intestine of man. Am J Clin Nutr 45: 423-431. PubMed: 3812341.

14. Cotta MA (1992) Interaction of ruminal bacteria in the production and utilization of maltooligosaccharides from starch. Appl Environ Microbiol 58: 48-54. PubMed: 1539992.

15. Wang X, Conway PL, Brown IL, Evans AJ (1999) In vitro utilization of amylopectin and high-amylose maize (Amylomaize) starch granules by human colonic bacteria. Appl Environ Microbiol 65: 4848-4854. PubMed: 10543795.

16. Boos W, Shuman H (1998) Maltose/maltodextrin system of Escherichia coli: transport, metabolism, and regulation. Microbiol Mol Biol Rev 62: 204-229. PubMed: 9529892.

17. Dippel R, Boos W (2005) The maltodextrin system of Escherichia coli: metabolism and transport. J Bacteriol 187: 8322-8331. doi:10.1128/JB.187.24.8322-8331.2005. PubMed: 16321936.

18. Schönert S, Seitz S, Krafft H, Feuerbaum EA, Andernach I et al. (2006) Maltose and maltodextrin utilization by Bacillus subtilis. J Bacteriol 188: 3911-3922. doi:10.1128/JB.00213-06. PubMed: 16707683.

19. Kamionka A, Dahl MK (2001) Bacillus subtilis contains a cyclodextrin-binding protein which is part of a putative ABC-transporter. FEMS Microbiol Lett 204: 55-60. doi:10.1111/j.1574-6968.2001.tb10862.x. PubMed: 11682178.

20. Gopal S, Berg D, Hagen N, Schriefer EM, Stoll R et al. (2010) Maltose and maltodextrin utilization by Listeria monocytogenes depend on an inducible ABC transporter which is repressed by glucose. PLOS ONE 5: e10349. doi:10.1371/journal.pone.0010349. PubMed: 20436965.

21. Shelburne SA 3rd, Keith DB, Davenport MT, Horstmann N, Brennan RG et al. (2008) Molecular characterization of group A Streptococcus maltodextrin catabolism and its role in pharyngitis. Mol Microbiol 69: 436-452. doi:10.1111/j.1365-2958.2008.06290.x. PubMed: 18485073.

22. Shelburne SA 3rd, Fang H, Okorafor N, Sumby P, Sitkiewicz I et al. (2007) MalE of group A Streptococcus participates in the rapid transport of maltotriose and longer maltodextrins. J Bacteriol 189: 2610-2617. doi:10.1128/JB.01539-06. PubMed: 17259319.

23. van Schaik W, Top J, Riley DR, Boekhorst J, Vrijenhoek JE et al. (2010) Pyrosequencing-based comparative genome analysis of the nosocomial pathogen Enterococcus faecium and identification of a large transferable pathogenicity island. BMC Genomics 11: 239. doi:10.1186/1471-2164-11-239. PubMed: 20398277.

24. Leenhouts K, Buist G, Bolhuis A, ten Berge A, Kiel J et al. (1996) A general system for generating unlabelled gene replacements in bacterial chromosomes. Mol Gen Genet 253: 217-224. doi:10.1007/s004380050315. PubMed: 9003306.

25. Sauer B (1987) Functional expression of the cre-lox site-specific recombination system in the yeast Saccharomyces cerevisiae. Mol Cell Biol 7: 2087-2096. PubMed: 3037344.

26. Zhang X, Paganelli FL, Bierschenk D, Kuipers A, Bonten MJ et al. (2012) Genome-wide identification of ampicillin resistance determinants in Enterococcus faecium. PLOS Genet 8: e1002804. PubMed: 22761597.

27. Top J, Sinnige JC, Majoor EA, Bonten MJ, Willems RJ et al. (2011) The recombinase IntA is required for excision of esp-containing ICEEfm1 in Enterococcus faecium. J Bacteriol 193: 1003-1006. doi:10.1128/JB.00952-10. PubMed: 21148730.

28. Lebreton F, van Schaik W, Sanguinetti M, Posteraro B, Torelli R et al. (2012) AsrR is an oxidative stress sensing regulator modulating Enterococcus faecium opportunistic traits, antimicrobial resistance, and pathogenicity. PLOS Pathog 8: e1002834. PubMed: 22876178.

29. Hsiao A, Ideker T, Olefsky JM, Subramaniam S (2005) VAMPIRE microarray suite: a web-based platform for the interpretation of gene expression data. Nucleic Acids Res 33: W627-W632. doi:10.1093/nar/gki443. PubMed: 15980550.

30. Lam MM, Seemann T, Bulach DM, Gladman SL, Chen H et al. (2012) Comparative analysis of the first complete Enterococcus faecium genome. J Bacteriol 194: 2334-2341. doi:10.1128/JB.00259-12. PubMed: 22366422.

31. Huycke MM (2002) Physiology of enterococci. In: MS GilmoreDB ClewellP. CourvalinGM DunnyBE Murray, The Enterococci: Pathogenesis, Molecular Biology, and Antibiotic Resistance. Washington, DC: ASM Press. pp. 133-176.

32. Le Breton Y, Pichereau V, Sauvageot N, Auffray Y, Rincé A (2005) Maltose utilization in Enterococcus faecalis. J Appl Microbiol 98: 806-813. doi:10.1111/j.1365-2672.2004.02468.x. PubMed: 15752325.

33. Mokhtari A, Blancato VS, Repizo GD, Henry C, Pikis A et al. (2013) Enterococcus faecalis utilizes maltose by connecting two incompatible metabolic routes via a novel maltose 6'-phosphate phosphatase (MapP). Mol Microbiol 88: 234-253. doi:10.1111/mmi.12183. PubMed: 23490043.

34. Cantarel BL, Lombard V, Henrissat B (2012) Complex carbohydrate utilization by the healthy human microbiome. PLOS ONE 7: e28742. doi:10.1371/journal.pone.0028742. PubMed: 22719820.

35. Abubucker S, Segata N, Goll J, Schubert AM, Izard J et al. (2012) Metabolic reconstruction for metagenomic data and its application to the human microbiome. PLOS Comput Biol 8: e1002358. PubMed: 22719234.

36. Deibel RH, Lake DE, Niven CF Jr. (1963) Physiology of the enterococci as related to their taxonomy. J Bacteriol 86: 1275-1282. PubMed: 14086101.

37. Monedero V, Kuipers OP, Jamet E, Deutscher J (2001) Regulatory functions of serine-46-phosphorylated HPr in Lactococcus lactis. J Bacteriol 183: 3391-3398. doi:10.1128/JB.183.11.3391-3398.2001. PubMed: 11344147.