- Research article
- Open Access
Characterization of the biotin uptake system encoded by the biotin-inducible bioYMN operon of Corynebacterium glutamicum
© Schneider et al; licensee BioMed Central Ltd 2012
Received: 16 November 2011
Accepted: 13 January 2012
Published: 13 January 2012
The amino acid-producing Gram-positive Corynebacterium glutamicum is auxotrophic for biotin although biotin ring assembly starting from the precursor pimeloyl-CoA is still functional. It possesses AccBC, the α-subunit of the acyl-carboxylases involved in fatty acid and mycolic acid synthesis, and pyruvate carboxylase as the only biotin-containing proteins. Comparative genome analyses suggested that the putative transport system BioYMN encoded by cg2147, cg2148 and cg2149 might be involved in biotin uptake by C. glutamicum.
By comparison of global gene expression patterns of cells grown with limiting or excess supply of biotin or with dethiobiotin as supplement replacing biotin revealed that expression of genes coding for enzymes of biotin ring assembly and for the putative uptake system was regulated according to biotin availability. RT-PCR and 5'-RACE experiments demonstrated that the genes bioY, bioM, and bioN are transcribed from one promoter as a single transcript. Biochemical analyses revealed that BioYMN catalyzes the effective uptake of biotin with a concentration of 60 nM biotin supporting a half-maximal transport rate. Maximal biotin uptake rates were at least five fold higher in biotin-limited cells as compared to cells grown with excess biotin. Overexpression of bioYMN led to an at least 50 fold higher biotin uptake rate as compared to the empty vector control. Overproduction of BioYMN alleviated biotin limitation and interfered with triggering L-glutamate production by biotin limitation.
The operon bioYMN from C. glutamicum was shown to be induced by biotin limitation. Transport assays with radio-labeled biotin revealed that BioYMN functions as a biotin uptake system. Overexpression of bioYMN affected L-glutamate production triggered by biotin limitation.
Biotin is a vitamin in humans (vitamin H or B7). Biotin deficiency is rarely observed in humans, e.g. after prolonged consumption of raw egg whites that contains biotin-binding avidin , as the normal microflora of the large intestine is considered to provide sufficient supply of biotin. If biotin is lacking, multiple carboxylase deficiencies arise  because biotin is a cofactor of the biotin-dependent carboxylases, which occur in all domains of life . Many bacteria can synthesize biotin, but biotin auxotrophic bacteria such as Corynebacterium glutamicum require uptake of biotin from the habitat.
Biotin synthesis can be subdivided into synthesis of pimelic acid followed by the biotin ring assembly . Biotin ring assembly occurs via the well-studied enzymes 8-amino-7-oxononanoate synthase, 7,8-diaminononanoate synthase, dethiobiotin synthase and biotin synthase encoded by bioF, bioA, bioD and bioB, respectively . Pimelate synthesis occurs via two alternative routes as found in Bacillus subtilis and Escherichia coli, respectively . In B. subtilis, pimeloyl-CoA is generated by interception of fatty acid biosynthesis by P450-dependent BioI, which yields pimeloyl-ACP chains by oxidative cleavage of long-chain acyl-ACPs . In E. coli, malonyl-CoA methyl ester is generated by SAM-dependent methyltransferase BioC as a primer molecule and afterwards elongated in fatty acid biosynthesis to yield methyl-pimeloyl-ACP which finally is demethylated by carboxylesterase BioH . Other sources of pimeloyl-CoA are externally added pimelic acid which is activated by pimeloyl-CoA synthetase as e.g. in B. subtilis, yet uncharacterized biosynthetic pathways as proposed e.g. for Desulfovibrio species  or degradation of benzene as e.g. in Rhodopseudomonas palustris .
C. glutamicum is a Gram-positive biotin-auxotrophic bacterium that was originally isolated as an L-glutamate producer from soil samples . C. glutamicum lacks the ability to synthesize pimeloyl-CoA, but the enzymes for biotin ring assembly, BioA, BioD and BioB, are functional [9–11]. It has been proposed that biotin auxotrophy in C. glutamicum is due to the lack of a BioF homolog [9–11]. Accordingly, it has been found that biotin, dethiobiotin, and aminopelargonic acid derivatives effectively support growth when added in low concentrations, but not pimelic acid . Biotin auxotrophy of C. glutamicum elicits L-glutamate production, a characteristic which led to its discovery. L-Glutamate production by C. glutamicum can be triggered in number of alternative ways, e.g. by addition of ethambutol  or Tween  or by a temperature shift .
Triggering L-glutamate production by biotin limitation alters synthesis of fatty acids and mycolic acids  as a consequence of reduced activity of acyl-CoA carboxylases, which contain AccBC, one of the two biotin-containing enzymes of C. glutamicum  as α-subunit. Secretion of L-glutamate is mediated by a carrier [18, 19] involving the gene product of cg1434 , which encodes mechanosensitive channel MscS [21, 22]. Activation of MscS without osmotic downshock is thought to result in L-glutamate secretion [20–22].
L-Glutamate production occurs due to reduction of the activity of the tricarboxylic acid cycle enzyme oxoglutarate dehydrogenase (ODHC). The small inhibitory protein OdhI binds to ODHC and inhibits its activity unless it is phosphorylated by serine protein kinase PknG or PknA, PknB and PknL [23–25].
Biotin uptake has not yet been studied in C. glutamicum. A sodium-dependent multivitamin transporter and the monocarboxylate transporter 1 are involved in biotin uptake in mammalian cells . A proton symporter is required for biotin uptake in the biotin-auxotrophic yeasts Saccharomyces cerevisiae and Schizosaccharomyces pombe . In bacteria, several systems for uptake of biotin exist. One biotin uptake system is encoded by the genes bioM, bioN and bioY and mutations in these genes were shown to result in reduced biotin uptake [28, 29]. In bacteria containing only BioY, this protein functions as a high-capacity transporter on its own, while in combination with BioMN it also shows high-affinity towards its substrate biotin .
Comparative genome analyses revealed that actinobacteria including C. glutamicum possess gene clusters of bioY, bioM, and bioN and were proposed to import biotin via BioYMN transport systems. In this study, we characterized global gene expression changes due to altered biotin supply and demonstrated that biotin-inducible transport system BioYMN imports biotin.
Influence of biotin on global gene expression in wild type C. glutamicum
Gene expression differences of C. glutamicum WT in response to biotin limitation, biotin excess or supplementation with dethiobiotin
Relative mRNA level
1 μg/l biotin
20000 μg/l biotin
200 μg/l biotin
200 μg/l biotin
biotin synthase BioB
ABC-type transporter. permease component
ribosomal protein L15 RplO
lactam utilization protein
cysteine desulfhydrase/selenocysteine lyase NadS
quinolate synthase A NadA
ADP-ribose pyrophosphatase NdnR
Biotin transport protein BioY
Biotin transport protein BioM
Biotin transport protein BioN
predicted transcriptional regulator MarR family
isocitrate lyase AceA
putative dipeptide/tripeptide permease
adenosylmethionine-8-amino-7-oxononanoate aminotransferase BioA
thiol:disulfide interchange protein TlpA
Dethiobiotin, the substrate of biotin synthase BioB, is the immediate precursor of biotin. To compare global gene expression when C. glutamicum is supplemented with dethiobiotin or biotin, parallel cultures of C. glutamicum WT were grown in glucose minimal medium with either biotin or dethiobiotin at concentrations of 200 μg/l. In the presence of dethiobiotin, only 9 of the genes listed in Table 1 were differentially expressed, all showing an increased mRNA level similar to those under biotin limitation. The most strongly regulated genes were bioB, the gene encoding biotin synthase converting dethiobiotin to biotin (11.3 fold higher than with biotin), cg2884 (5.6 fold) and bioY (4.4 fold).
Transcriptional organisation of the putative bioYMNoperon
Since the RT-PCR data indicated that bioY, bioM and bioN are described as one transcript from one promoter, the RACE-PCR technique was applied to identify transcriptional start sites of bioY and bioM. Thereby, one transcription start point was identified for the transcription unit bioYMN (Figure 1 lower panel), being identical with the first nucleotide (nt) of the bioY translational start codon. Comparison of the sequence upstream of the transcriptional start site to the σ70 promoter consensus  revealed two hexamers (5'-TTGCTT-3' and 5'-TATGATT-3') which show similarity (9 of 12 identical bases) to the -35 and -10 promoter hexamers and are separated by a spacer of 19 bases (Figure 1 lower panel).
Characterization of biotin uptake by BioYMN
Effect of bioYMNoverexpression on L-glutamate production triggered by biotin-limitation
Here, we have shown that C. glutamicum shows biotin-dependent gene expression changes of the genes encoding the enzymes for biotin ring assembly and for biotin uptake. Moreover, the maximal biotin uptake rate was at least ten fold higher under biotin limitation conditions (1.3 pmol min-1 mg (dry weight)-1) as compared to biotin excess conditions (< 0.1 pmol min-1 mg (dry weight)-1). These findings are in contrast to the speculation that biotin-auxotrophic C. glutamicum has not only lost the ability to synthesize biotin, but also the ability for biotin-dependent gene regulation . BirA of C. glutamicum was characterized as monofunctional biotin protein ligase  and is not involved in biotin-dependent gene regulation as suggested previously based on bioinformatics analysis . In a similar bioinformatics analysis, a putative transcriptional regulator of the biotin synthesis genes, BioR, has been identified in α-proteobacteria . This GntR-type of transcriptional repressor is encoded together with bio genes and putative binding sites named BIOR boxes occur upstream of bio genes and upstream of the regulatory genes in α-proteobacteria . In actinobacteria, TetR-type transcriptional regulators named BioQ were found to be encoded in 11 of 27 genomes as well as a palindromic DNA motif upstream of the bio genes. The bioQ gene clustered with bioB in several genomes of the genera Nocardia, Rhodococcus, Propionibacterium and Mycobacterium . BioQ is also encoded in the genomes of four Corynebacterium species although not clustered with bio genes and the predicted BioQ binding sites (TGAAC-N3-GTTCA) occur upstream of the bio genes . Although the bioinformatics evidence is convincing, genetic, biochemical or physiologic characterization of this putative transcriptional regulator in actinobacteria has not yet been published.
The biotin-inducible bioYMN operon was shown here to encode a functionally active biotin uptake system. BioYMN of C. glutamicum likely is essential for survival of this biotin-auxotrophic species as various attempts to delete the operon failed although very high concentrations of biotin were supplemented (data not shown). Restoring biotin prototrophy of C. glutamicum has not been reported yet, but it is tempting to speculate that BioYMN is not essential in a biotin-prototrophic recombinant C. glutamicum strain. BioYMN from C. glutamicum belongs to a type of uptake systems that have been classified as energy-coupling factor (ECF) transporters [38, 39]. The core component BioY is active as high-capacity biotin uptake system. In conjunction with the ATP-binding-cassette ATPase BioM and the transmembrane protein BioN, the uptake system shows high affinity for its substrate biotin . E. coli cells containing BioY from R. capsulatus imported biotin with a Vmax of 60 pmol min-1 (mg protein)-1 and a Kt of 250 nM, whereas BioYMN-containing cells exhibited a 50-fold-lower Kt . The Kt of BioYMN from C. glutamicum is also in the nanomolar range, but around tenfold lower (60 and 77 nM, respectively, s. above). C. glutamicum cells overproducing endogenous BioYMN showed a Vmax of 8.4 pmol min-1 (mg protein)-1, which is comparable to that determined for E. coli cells containing BioYMN from R. capsulatus (6 pmol min-1 (mg protein)-1 ), but lower than that determined for E. coli cells containing only BioY from R. capsulatus (60 pmol min-1 (mg protein)-1 ).
Amino acid production by the biotin-auxotrophic C. glutamicum can be affected positively or negatively by the biotin supply in the medium. Biotin-sufficient conditions are employed for L-lysine production and it has been shown that increasing the biotin supply  or overproducing the biotin protein ligase BirA  improved L-lysine production. Under biotin-sufficient conditions, the biotin-containing enzyme pyruvate carboxylase is the major anaplerotic enzyme synthesizing oxaloacetate as precursor of L-lysine as deletion of the pyruvate carboxylase gene pyc negatively affected L-lysine production  whereas deletion of the PEP carboxylase gene ppc did not . Accordingly, overexpression of pyc improved L-lysine production . On the other hand, L-glutamate production can be triggered by biotin limitation and a role of BioYMN in L-glutamate production by C. glutamicum has been found here. Biotin limitation reduces/alters synthesis of fatty and mycolic acids  as a consequence of reduced levels of biotinylated AccBC, the α-subunit of the acyl-carboxylases. Moreover, under biotin limitation conditions anaplerosis is not fulfilled by biotin-containing pyruvate carboxylase [41, 43], but by PEP carboxylase . In line with the observation that L-glutamate production by C. glutamicum wild type is known to be suppressed by an excess of biotin , enhancing biotin uptake by overexpression of bioYMN decreased L-glutamate production (Figure 3). Thus, BioYMN plays a role in biotin-triggered L-glutamate production by C. glutamicum.
C. glutamicum showed biotin-dependent regulation of mRNA levels of bioA, bioB, bioY, bioM, and bioN. The genes bioY, bioM, and bioN are transcribed as an operon, bioYMN. Transport assays with radio-labeled biotin revealed that BioYMN functions as a biotin uptake system with an affinity for its substrate in the nanomolar range. Overepression of bioYMN alleviated biotin limitation and interfered with triggering L-glutamate production by biotin limitation.
Bacterial strains, plasmids, oligonucleotides, and culture conditions
Bacteria and plasmids used in this study
Strain, plasmid or oligonucleotide
Relevant characteristics or sequence
Source, reference, or purpose
E. coli strains
C. glutamicum strains
pEKEx3 containing bioY, bioM and bioN
cloning vector, AmpR
Determination of amino acid concentrations
During cultivation, samples (1 ml) were collected to determine biomass and amino acid concentrations. The optical density was determined by absorbance at 600 nm. After centrifugation of the sample (13,000 g, 5 min), aliquots of the supernatant were used for analysis. Amino acid concentrations in the culture supernatants were determined by automatic precolumn derivatization with ortho-phthaldialdehyde and reversed-phase high-performance liquid chromatography (RP-HPLC) (HP1100 series; Hewlett-Packard, Waldbronn, Germany) with fluorimetric detection (excitation at 230 nm; emission at 450 nm) as described previously . Hypersil ODS 5-mm columns were used (precolumn: 40 × 4 mm; column: 120 × 4 mm, Chromatographie Service GmbH, Langerwehe, Germany). The buffer gradient consisted of 0.1 M sodium acetate, pH 7.2 (with 0.03% sodium azide), as the polar phase and methanol as the nonpolar phase. Quantification was performed with L-asparagine as an internal standard and by comparison with external standards.
Construction of plasmids and strains
The oligonucleotides listed in Table 2 were obtained from Operon (Cologne, Germany) or MWG (Ebersberg, Germany). Standard methods such as PCR, restriction, and ligation were carried out as described previously . Plasmids were constructed in Escherichia coli DH5α from PCR-generated fragments (KOD, Novagen, Darmstadt, Germany) and isolated with the QIAprep spin miniprep kit (QIAGEN, Hilden, Germany). E. coli was transformed by the CaCl2 method , while C. glutamicum was transformed via electroporation . All cloned DNA fragments were shown to be correct by sequencing. For homologous overexpression of bioYMN the operon was amplified from genomic DNA of C. glutamicum WT by using primers bio-operon_fw and and bio-operon_rev, and was sub-cloned to pGEM-T-easy and cloned as 2235 bp-EcoRI-fragment into the expression vector pEKEx3 , which allows IPTG-inducible gene expression in C. glutamicum.
Comparative transcriptome analysis using DNA microarrays
Generation of C. glutamicum whole-genome DNA microarrays, total RNA preparation, synthesis of fluorescently labelled cDNA, microarray hybridization, washing, and statistical data analysis were performed as described previously [52, 53]. Genes exhibiting mRNA levels that were significantly changed (P ≤ 0.05 in Student's t test) by at least a factor of 2.0 were determined in three DNA microarray experiments performed with RNA isolated from three independent cultures.
RT-PCR analysis and 5'-RACE
RNA was prepared as described previously [52, 53] and incubated in 0.1 M sodium acetate, pH 3.0, 5 mM MgSO4, and 0.3 U/μl DNase I (Roche Diagnostics, Mannheim, Germany) for 30 min at 37°C. After heat inactivation for 5 min at 75°C, the RNA was precipitated with LiCl as described by . After denaturation for 5 min at 65°C, reverse transcription of 500 ng RNA was performed with Omniscript Reverse Transcriptase (QIAGEN, Hilden, Germany) according to the manufacturer's instructions by using random hexamer primers (Invitrogen, Karlsruhe, Germany). Subsequently, the cDNA was amplified using combinations of the primers A (bioY-RBS_fw, bioY_rev), B (bioY-int_fw, bioM-int_rev) and C (bioMN-RBS_fw, bioYMN_rev). As a control, cDNA of dnaE was amplified using primers RT-dnaE-fw and RT-dnaE-rev. To determine transcriptional starts by RACE-PCR RNA was prepared and purified as described above. Primers binding downstream of the annotated translational starts of bioY and bioM (bioY_rev, bioM_rev) along with 2.0 μg total RNA were used for cDNA synthesis reverse transcription with Superscript II (Invitrogen, Karlsruhe, Germany) according to the supplier's protocol. After RNA digestion with RNase H (Fermentas, St. Leon-Roth, Germany) and purification the cDNA was then modified by terminal deoxynucleotidyl transferase (Fermentas, St. Leon-Roth, Germany) and dATP respectively dCTP to determinate the transcriptional start accurately. Subsequently, the cDNA was amplified using combinations of oligo(dT) or oligo(dG) primer and either bioY-int_rev or bioM-int_rev. The obtained PCR products were cloned into the pGEM-T Easy vector (Promega, Mannheim, Germany) and transferred into E. coli DH5α cells. At least two different clones per gene were selected for plasmid preparation and DNA sequencing (BigDye Terminator v3.1 Cycle Sequencing Kit and ABI Prism Capillary Sequencer Model 3730, Applied Biosystems, Forster-City, USA).
Biotin-limited (2.5 μg/l) precultures of C. glutamicum WT(pEKEx3) and biotin-sufficient (200 μg/l) precultures of WT(pEKEx3) and WT(pEKEx3-bioYMN) were used to inoculate glucose minimal medium cultures with either 1 μg/l or 200 μg/l biotin and allowed to grow to mid-exponential phase in minimal medium CGXII supplied with glucose as the sole carbon source. 1 mM IPTG was used in this culture for 17 h for the induction of pEKEx3-bioYMN expression. Subsequently, cells were washed two times with the assay buffer (0.1 M sodium chloride, 25 mM potassium phosphate, pH 7.5) and incubated on ice until the measurement. The cells were energized by incubation for 3 min at 30°C with 20 mM glucose at an optical density (600 nm) of 5 in an assay volume of 2 ml before biotin was added. Finally, 7 kBq of 3H-labeled biotin (1.11-2.22 TBq/mmol, PerkinElmer, Rodgau, Germany) was applied in an 2 ml assay at concentrations indicated in the respective experiments, and 200 μl samples were taken at 15, 30, 45, 60, 90 s in order to determine initial uptake rates. Cells were collected on GF55 glass fiber filters (Millipore, Schwalbach, Germany) and washed twice with 2.5 ml of assay buffer. After the resuspension of cells in scintillation fluid (Rotiszinth, Roth, Germany) the radioactivity of the sample was counted in a scintillation counter (Beckman, Krefeld, Germany).
The authors would like to thank Lothar Eggeling (Jülich) for discussions during the initial phase of the project. We acknowledge support of the publication fee by Deutsche Forschungsgemeinschaft and the Open Access Publication Funds of Bielefeld University.
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