Ökologie des Bodens, Botanisches Institut, RWTH-Aachen, Worringerweg 1, 52056 Aachen, Germany1
Division of Microbiology, School of AMS, University of Reading, Whiteknights, Reading RG6 6AJ, UK2
Author for correspondence: Jürgen Prell. Tel: +49 241 8026647. Fax: +49 241 8022637. e-mail: prell{at}bio1.rwth-aachen.de
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ABSTRACT |
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Keywords: carbon metabolism, GABA shunt, symbiotic expression, promoter-probe vector, pJP2
Abbreviations: GABA, -aminobutyrate; GUS, ß-D-glucuronidase; PEP, phosphoenolpyruvate; PNP, p-nitrophenol; SSDH, succinate semialdehyde dehydrogenase; TCA, tricarboxylic acid; X-Gal, 5-bromo-4-chloro-3-indolyl ß-D-galactopyranoside; X-Glc, 5-bromo-4-chloro-3-indolyl ß-D-glucuronic acid
The GenBank accession number for the sequence determined in this work is AF335502.
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INTRODUCTION |
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C4-dicarboxylic acids are thought to be the only source of carbon skeletons available to the bacteroids in sufficient amounts to support the energetically expensive process of nitrogen fixation. These dicarboxylic acids are derived from the plants glycolysis. Phosphoenolpyruvate (PEP) is carboxylated via PEP carboxylase (EC 4.1.1.31) to oxaloacetate and then further reduced by malate dehydrogenase (EC 1.1.1.37) to malate (Streeter, 1991 ; Vance & Heichel, 1991
). The C4-dicarboxylic acids are taken up by the bacteroids and presumably directly channelled into the TCA cycle. Atmospheric nitrogen is fixed to ammonia by the nitrogenase enzyme complex, which is expressed in the bacteroids in response to the low oxygen concentration present in the nodule. The majority of the ammonia produced is transported to the plant host cell, where it is assimilated and incorporated into amino acids. Part of the ammonia however appears to be assimilated by the bacteroids themselves in order to maintain their metabolism. Two potential ammonia-assimilating enzymes, alanine dehydrogenase (EC 1.4.1.1) and glutamate dehydrogenase (EC 1.4.1.2) both show high activities in mature bacteroids of Sinorhizobium meliloti (Miller et al., 1991
). Alanine is, as recently discovered, also an excretion product of anaerobically isolated mature bacteroids in soybean and pea (Waters et al., 1998
; Allaway et al., 2000
).
The role of glutamate, which generally appears in large quantities in the nodules (Miller et al., 1991 ; Vance & Heichel, 1991
; Salminen & Streeter, 1992
), remains unclear. A reason for glutamate accumulation could be the inhibition of the bacterial 2-oxoglutarate dehydrogenase complex during symbiosis. This complex is part of the TCA cycle and converts 2-oxoglutarate to succinyl-CoA. It is sensitive to the redox charge of the cell because of inhibition by the concentration of NADH (Streeter, 1991
). The high NADH level in bacteroids is probably due to oxygen limitation, which is also a prerequisite for effective functioning of the bacteroids nitrogenase (McDermott et al., 1989
; Dunn, 1998
; Poole & Allaway, 2000
). In symbiosis, 2-oxoglutarate could be directly aminated by glutamate dehydrogenase, or transaminated by any aminotransferase using 2-oxoglutarate as the receiving oxoacid. Consistent with this, mutations in the 2-oxoglutarate dehydrogenase complex in Rhizobium leguminosarum bv. viciae 3841 lead to the synthesis and excretion of large quantities of glutamate (Walshaw et al., 1997
).
A possible sink for glutamate in bacteroids includes the GABA shunt pathway. This is a theoretical bypass of the 2-oxoglutarate dehydrogenase complex, in which glutamate is decarboxylated to -aminobutyric acid (4-aminobutyrate; GABA) by glutamate decarboxylase (EC 4.1.1.15). The amino residue of GABA is removed by GABA aminotransferase (EC 2.6.1.19) leading to succinate semialdehyde, which is further oxidized to succinate by succinate-semialdehyde dehydrogenase (EC 1.2.1.16). The GABA aminotransferase is a pyridoxal-phosphate-dependent enzyme that transfers the amino residue of GABA to an oxoacid. In the case of 2-oxoglutarate as the receiving oxoacid, this reaction would also cover the first step of the pathway, the amination of 2-oxoglutarate to glutamate. The existence of a GABA shunt pathway in Rhizobium spp. has been often discussed (McDermott et al., 1989
; Miller et al., 1991
; Dunn, 1998
; Poole & Allaway, 2000
). However, it has never been confirmed to operate during symbiosis, as corresponding mutants were not available.
In this paper, we report the identification, cloning and analysis of the R. leguminosarum bv. viciae VF39 gabT gene, encoding 2-oxoglutarate-dependent GABA aminotransferase. We constructed mutants and analysed gabT expression in free-living state and in bacteroids. We show that while GabT is not essential for growth on GABA or symbiotic nitrogen fixation, it is specifically induced in the nodule, suggesting a role in bacteroid metabolism.
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METHODS |
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To adjust the pH, TY media were buffered with 50 mM MES (for pH 5·3 and 6·0), with 50 mM MOPS (pH 7·0) or with 50 mM TABS (pH 8·0). 5-Bromo-4-chloro-3-indolyl ß-D-galactopyranoside (X-Gal) was added at a final concentration of 40 µg ml-1.
For ß-D-glucuronidase (GUS) activity, TY solid media were supplemented with 5-bromo-4-chloro-3-indolyl ß-D-glucuronic acid (X-Glc) at a final concentration of 40 µg ml-1.
Antibiotics were used as needed for E. coli strains at the following final concentrations: ampicillin 100 µg ml-1; kanamycin 25 µg ml-1; tetracycline 10 µg ml-1. For R. leguminosarum, antibiotics were added at final concentrations of: 500 µg ml-1 (streptomycin); 80 µg ml-1 (neomycin) and 10 µg ml-1 (tetracycline).
Preparation of cell extracts.
Cultures of R. leguminosarum VF39 WT or mutant strains were grown overnight on AMS (400 ml) or VMM (250 ml), supplemented with GABA and glutamate and were harvested at an OD600 of approximately 0·5 by centrifugation (8000 r.p.m.; 10 min; 4 °C; Sorvall SLA-3000). The pellet was suspended in 50 ml 20 mM phosphate buffer (pH 7·2) and centrifuged again. Then the cells were resuspended in 48 ml breaking buffer (40 mM HEPES, 1 mM DTT at pH 7·0) and either crushed twice in a French pressure cell at 70 MPa or sonicated for 3 min at 90 W on ice. Cell debris was removed by centrifugation (17000 r.p.m.; 25 min; 4 °C; Sorvall SS34). The cell extracts were kept on ice and enzyme activities were measured within 2 h after preparation. Protein concentrations were determined by the method of Bradford (1976) and compared to a BSA standard (020 µg ml-1). Protein concentrations in the prepared cell extracts were between 1 and 3 mg ml-1.
Enzyme assays.
2-Oxoglutarate-dependent GABA aminotransferase was measured with 150 mM GABA and 50 mM 2-oxoglutarate (disodium salt) as substrates, as earlier described by Bartsch (1990) . The assay was performed in a final volume of 500 µl, using 250 µl cell extract. Glutamate formation was determined by reduction of NAD+ in a coupled glutamate dehydrogenase (GDH) assay. In a final volume of 1·5 ml [40 mM hydrazine; 50 mM glycine (pH 7·6); 2·7 mM NAD+; 3 units GDH (Sigma, G-2626)], the complete GABA aminotransferase sample (500 µl) was incubated for 1·5 h at 37 °C. NADH production was measured at 340 nm in a spectrophotometer. Assays were done in duplicate with a minus enzyme control for each extract. Results were compared to a standard curve (with 0120 nmol glutamate per sample in duplicate), prepared freshly every day.
Pyruvate-dependent GABA aminotransferase activity was measured with 150 mM GABA and 50 mM pyruvate (sodium salt) as substrates. The assay was performed as described for 2-oxoglutarate-dependent GABA aminotransferase with the following changes. Ten microlitres of cell extract was used in a final assay volume of 500 µl. Alanine production was measured in a final volume of 1·5 ml [40 mM hydrazine; 50 mM glycine (pH 9·0); 2·7 mM NAD+; 0·5 units alanine dehydrogenase (Sigma, A-7653)].
Succinate-semialdehyde dehydrogenase (SSDH) was measured with 2·5 mM succinate semialdehyde and 1 mM NAD+ as substrates (Laura Green, University of Missouri, personal communication). The assay was performed in 50 mM Tris buffer at pH 8·0, 1 mM DTT and 10 mM KCN, to avoid reoxidation of NADH by cytochrome c oxidase. Reduction of NAD+ was measured spectrophotometrically at 340 nm.
GUS and lacZ activity assays.
Precultures grown on TY medium were harvested and transferred to VMM containing the different substrates. The cultures were started at an OD600 of 0·2 and showed a basic level of induction of about 100 nmol p-nitrophenol (PNP) min-1 per OD600 unit (Fig. 3, t=0). GUS was assayed as previously described by Boesten et al. (1998) . After 20 min the assay was stopped and cleared of cell debris by centrifugation (13000 r.p.m.; 10 min). The release of PNP was measured spectrophotometrically at 415 nm. Enzyme activities were calculated and expressed in nmol PNP min-1 per OD600 unit.
ß-D-Galactosidase (lacZ) was assayed similarly, with 50 µl o-nitrophenyl ß-D-galactopyranoside. o-Nitrophenol was detected at 420 nm.
DNA techniques.
Standard DNA techniques were carried out according to Maniatis et al. (1982) . Total DNA was prepared by the CTAB method described by K. Wilson in Ausubel et al. (1987)
. Plasmid DNA from cultures was purified with the NucleoSpin Plasmid kit (Macherey-Nagel). DNA fragments from agarose gels were isolated using the NucleoSpin Extract kit (Macherey-Nagel) according to the manufacturers instructions.
Construction of the pJP2 promoter-probe vector.
The basis of the pJP2 promoter-probe vector is the broad-host-range, mobilizable plasmid pTR102 (Weinstein et al., 1992 ), a mini-RK2 derivative, containing par functions ensuring plasmid stability.
First, the BamHI, PstI and HindIII restriction sites of pTR102 were deleted by BamHI and HindIII restriction, Klenow fill-in and religation, leading to vector pTR102-d. Then a promoterless uidA gene (GUS) from pCCOGUS (Axelos et al., 1989 ) was cloned into the PstI and SacI sites of pTR102-d, leading to pTR102-GUS. An artificial multiple cloning site was inserted into the NcoI and KpnI sites of pTR102-GUS. Two complementary oligonucleotides with the following sequences were synthesized (MWG-Biotech): 5'-CAT GGA TCC AAG CTT CTC GAG CTC TAG ACT GAG GTA AT-3' and 5'-CAT GAT TAC CTC AGT CTA GAG CTC GAG AAG CTT GGA TCC ATG GTA C-3' (Fig. 1b
). The fragment contains a ribosome-binding sequence (GAGG, 5 bp upstream of the ATG), which was a consensus compiled from a number of known R. leguminosarum fix and nif genes. Stop codons were introduced in all reading frames to prevent translational gene fusions to the GUS protein. Finally several single-cutting restriction sites were added to facilitate cloning of DNA fragments.
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Sequence analyses.
Appropriate restriction sites within the gabT region were used to clone 300800 bp fragments into vector pUC19. Sequencing of the resulting recombinant plasmids was done for both strands by the chain-termination method using a Thermo Sequenase fluorescent labelled primer cycle sequencing kit with 7-deaza-dGTP (Amersham Pharmacia Biotech) and IRD700/800 labelled standard primers (universal and reverse) according to the manufacturers instructions. Extension products were separated and detected on a LI-COR 4200L sequencer. An IRD700-labelled IS50 primer (5'-CGG GAA AGG TTC CGT TCA GGA CG-3') was used to sequence fragments flanking the Tn5-B20.
Nucleotide sequence comparisons were done by the NCBI BLAST2 package (Altschul et al., 1997 ) against the NCBI-nr database.
Construction of plasmid integration mutants.
A 394 bp Ecl136II/EcoRI fragment (Fig. 2d) was used for the construction of the gabT integration mutant VF39-19T. The fragment was cloned into the SmaI/EcoRI sites of pK19mob, resulting in pK19mob-gabT. The plasmid was transferred from E. coli S17-1 to R. leguminosarum VF39 and recombined into the genomic gabT region via single crossover. Total DNA of the resulting clones was digested with SalI and with EcoRI, separated by gel electrophoresis, transferred onto Qiabrane nylon membranes (Qiagen) by vacuum blotting (Pharmacia) and correct integration was verified by Southern hybridization at 68 °C with a PCR-derived (using universal and reverse primers and pK19mob-gabT as template) and digoxigenin-11-dUTP-labelled gabT probe (DIG DNA Labelling Kit; Boehringer). The integration mutant was designated VF39-19T and used for further studies.
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Plant cultivation, thin sections and staining.
The pea Pisum sativum cv. Rondo was used as a host plant in this work. Seeds were sterilized in concentrated sulphuric acid for 15 min, washed three times with sterile water and germinated on sterile vermiculite. Five seedlings were then transferred to sterile vermiculite in 10x10 cm plastic boxes and grown for 3 d.
Bacteria were pre-grown on solid medium in the presence of the appropriate antibiotics. A loop of cells was resuspended in 3 ml sterile water and used for inoculation. Plants were grown at 22 °C under artificial light for 16 h a day.
Nodules were harvested after 28 d and prepared for GUS activity assays and histochemical staining.
Bacteroid suspensions for GUS assays were prepared as follows. Five to ten fresh nodules were collected in 1 ml 50 mM sodium phosphate buffer (pH 7·0). The nodules were crushed with an appropriately shaped metal rod. Plant tissue was removed by centrifugation (5 min; 1250 r.p.m.). The supernatant was cleared (5 min; 4500 r.p.m.) and the pellet resuspended in 500 µl sodium phosphate buffer. The resulting bacteroid suspension was directly used for GUS activity assays as described above.
For thin sectioning, fresh nodules were sliced under 50 mM sodium phosphate buffer (pH 7·0) into 80 µm sections using a Leica VT1000S vibratome. The sections were incubated in staining buffer (50 mM sodium phosphate buffer pH 7·0; 0·1% Triton X-100; 5 mM K3[Fe(CN)6]; 5 mM K4[Fe(CN)6]) containing 0·02% X-Glc until clear blue staining appeared. For strongly expressed fusions the staining time was about 3060 min. The reaction was stopped by fixing the sections in 1·25% glutaraldehyde in 50 mM sodium phosphate buffer (pH 7·0). Pictures were taken on an Olympus B201 bright-field microscope.
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RESULTS |
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In an initial approach to identify promoters and genes induced under acidic and/or alkaline conditions, about 11000 mutants were tested for growth and expression on solid TY medium at different pH values (pH 5·38·0). None of them was impaired in growth.
One mutant, PH10, showed a more intense blue staining on media containing X-Gal at pH 5·3 and was selected for further investigations. In liquid TY medium lacZ expression was induced twofold at pH 5·3 when compared with the expression level at pH 6·0 (V. Lipka, RWTH-Aachen, unpublished).
The Tn5-B20 transposon (8·2 kb) was cloned from the genome of mutant PH10 and was found to be located on a 10·7 kb SalI fragment (pSVB28-PH10SalI). After restriction analyses and further subcloning, the 2·5 kb of chromosomal DNA flanking the transposon insertion were sequenced entirely. The sequence has been deposited at the NCBI GenBank (accession no. AF335502).
An ORF encoding 426 aa interrupted by the Tn5-B20 insertion showed good homologies to several 4-aminobutyrate (GABA) aminotransferase genes and was therefore designated as gabT. The best homology was found to the Mesorhizobium loti mlr5521 gene annotated as 4-aminobutyrate aminotransferase (Kaneko et al., 2000 ; NCBI accession no. NP106172), which encodes a protein 81% identical over 429 aa to the R. leguminosarum gabT gene product. The E. coli goaG gene, located on the Kohara clone #257 at min 29·129·6 of the E. coli K-12 chromosome and annotated as GABA or ornithine aminotransferase (Jovanovic & Model, 1997
; NCBI accession no. P50457), showed the second-best result at the protein level, with 61% identity over 421 aa, and the third-best similarity was found with the Pseudomonas aeroginosa PAO1 gabT locus (Stover et al., 2000
; NCBI accession no. AAG03655), exhibiting 57% identity over 426 aa. A second E. coli GABA aminotransferase gene, located on the Kohara clone #443 at min 59·860·2 of the K-12 chromosome (NCBI accession no. P22256), showed the fourth-best homology. The identity was 56% over 426 aa. This gene is part of the gabCDTP region (Bartsch et al., 1990
), which encodes gene products responsible for uptake (gabP) and degradation (gabDT) of GABA.
Downstream of the R. leguminosarum gabT gene, the 5'-end of another ORF was discovered, encoding a putative protein with homologies to the N-terminus of several SSDHs (data not shown); SSDH is the next enzyme in the GABA shunt pathway. This ORF was therefore designated as gabD' (Fig. 2). A third ORF identified upstream of gabT and orientated in the opposite direction showed homologies to merR-type transcriptional regulators and thus may specify a regulator for gabTD expression. It was tentatively named as gabR'.
The phenotype of gabT mutants
The R. leguminosarum PH10 Tn5-B20 mutant was tested for growth in liquid VMM containing GABA as sole carbon and nitrogen source. Growth rates of the mutant showed no difference from the wild-type (Table 2).
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To confirm that the absence of 2-oxoglutarate-dependent GABA aminotransferase from the PH10 extracts was indeed due to the mutation in the gabT gene, a plasmid integration mutant (VF39-19T) was generated. This mutant showed the same phenotypes as the PH10 strain.
To see if the downstream gabD gene is similarly affected by the gabT mutation, SSDH activity was also measured. The wild-type strain and all mutants showed similar SSDH levels (Table 2).
In symbiosis with the host P. sativum both gabT mutants produced normal, pink nodules and showed nitrogen fixation activities comparable to the wild-type.
Free-living and symbiotic expression of gabT
To study gabT regulation, a 572 bp Sau3AI fragment (Fig. 2b) containing the putative gabT promoter region was cloned into the BamHI site of the promoter-probe vector pJP2. The Sau3AI fragment contains the complete intergenic region between gabT and the predicted gabR' gene. It also includes 77 nucleotides of the 5'-end of the gabT coding region.
The fusion plasmid pJP2-gabT was transferred into R. leguminosarum VF39 and the induction of the gabT promoter was monitored during growth on different carbon and nitrogen sources. As shown in Fig. 3, GABA, as the substrate for the GABA aminotransferase, induces transcription of gabT, although only transiently. An initial threefold induction was observed, which declined to the basal level within 24 h. Glutamate, which is thought to be an intermediate in the GABA shunt pathway and a possible precursor of GABA, did not induce the gabT promoter and neither did succinate, the end-product of the pathway. Succinate, however, caused a reduction of the basal level of transcriptional activity.
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The effect of dual carbon sources was also examined. In combination with GABA, glutamate led to prolonged expression of gabT (Fig. 3), compared to the transient expression with GABA alone. Succinate in combination with GABA decreased the induction seen with GABA alone.
The expression of the gabT promoter was also studied during symbiosis with pea as a host plant. It was found to be induced in the proximal part of the infection zone (II), next to interzone IIIII, and strongly expressed in the late symbiotic zone (results not shown). The symbiotic activity of the gabT::uidA fusion was 813±63 nmol PNP min-1 per OD600 unit (mean±SD; n=3), which is comparable to the magnitude of maximum free-living induction by GABA and glutamate (Fig. 3).
Role of gabR in gabT expression
To investigate a possible function of GabR in gabT regulation, a plasmid integration mutant of gabR (VF39-18R) was constructed (see Methods). When pJP2-gabT was introduced into this mutant derivative, deep blue colonies were formed on TY plates containing X-Glc, while the wild-type carrying this plasmid produced only slightly bluish colonies after several days of growth. Quantitative measurements of GUS activity confirmed a constitutively high activity of the gabT gene fusion in the gabR mutant background. Overnight cultures in liquid TY medium resulted in GUS activities of about 700 nmol PNP min-1 per OD600 unit, whereas the wild-type showed only about 100 nmol PNP min-1 per OD600 unit (Fig. 3; t=0). Consistent with this, 2-oxoglutarate-dependent GABA aminotransferase activity in protein extracts from the mutant was about five times higher than in the wild-type (Table 2
). These results indicate that gabT expression is significantly enhanced in a gabR mutant background and that GabR acts as a repressor modulating gabT transcription.
When tested for growth in VMM liquid medium containing GABA as a sole nitrogen and carbon source, the gabR mutant VF39-18R showed no difference from the wild-type or the gabT mutants (Table 2).
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DISCUSSION |
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E. coli K-12 wild-type strains (CS101A and CS8A) have been found to be unable to grow on GABA as a sole source of carbon and nitrogen (Dover & Halpern, 1971 ). However, UV-induced mutants are able to use GABA as a sole nitrogen source, and in these mutants GABA aminotransferase and SSDH activity were both increased six- to ninefold. These mutants were proposed to be regulatory mutants. A second generation of UV-induced mutations permitted growth on GABA as sole source of carbon and nitrogen (Dover & Halpern, 1971
), and led to increased uptake of GABA. These results indicate that in E. coli K-12 the GABA shunt can serve as a metabolic pathway for GABA degradation.
In contrast to E. coli, R. leguminosarum bv. viciae VF39 grows on GABA as a sole source of carbon and nitrogen. The gabT mutants are not impaired in growth on GABA even though the activity of 2-oxoglutarate-dependent GABA aminotransferase is absent. However, pyruvate-dependent GABA aminotransferase activity is unaffected by the gabT mutation and may be responsible for continued growth on GABA. This implicates the presence of at least two genes encoding GABA aminotransferases with distinct substrate specificities in R. leguminosarum bv. viciae.
Enzyme activities of 2-oxoglutarate and pyruvate-dependent GABA aminotransferase were earlier presented from Sinorhizobium meliloti bacteroids by Miller et al. (1991) and from Bradyrhizobium japonicum bacteroids by Kouchi et al. (1991)
. The question of whether one or two enzymes were responsible for the different activities was not solved in these reports.
The pyruvate-dependent GABA aminotransferase activity in the gabT mutants of R. leguminosarum VF39 maintains a functioning GABA shunt pathway. The GABA shunt has often been discussed to play a role in rhizobial carbon metabolism during symbiosis, as the 2-oxoglutarate dehydrogenase complex is thought to be inhibited by excess of reducing equivalents under the oxygen-limiting conditions present in the nodule (McDermott et al., 1989 ; Vance & Heichel, 1991
; Dunn, 1998
; Poole & Allaway, 2000
).
Miller et al. (1991) reported relatively high GABA concentrations [31 nmol (mg protein)-1] in bacteroids of S. meliloti. Similarly, Vance & Heichel (1991) found GABA to be present in whole root nodules at concentrations of about 4008000 nmol (g fresh wt)-1. They further discussed a role for GABA in regulation of cytoplasmic pH during microaerobic and anaerobic conditions. Assuming that
serves as a substrate for nodule PEP carboxylase, acidosis resulting in excess H+ produced during hydration of dark CO2 fixation could be toxic to host cells. Decarboxylation of glutamate to GABA could therefore be a significant sink for protons. This could explain why the gabT transposon mutant described here was initially identified by a screen for genes induced at low pH values.
To investigate gabT expression in R. leguminosarum bv. viciae during symbiosis, we constructed a new promoter-probe vector pJP2, which is maintained stably even in the absence of selective pressure. Vector stability is traditionally tested via re-isolation of rhizobia from crushed nodules and plating on selective media (Weinstein et al., 1992; Dombrecht et al., 2001 ). However, for S. meliloti the differentiation from free-living bacteria to bacteroids is irreversible and bacteroids do not regenerate viable cells on growth medium (McRae et al., 1989
). Re-isolation from crushed nodules only results in growth of free-living or transforming bacteria but not bacteroids. We therefore believe that plasmid loss can be best visualized in stained thin sections of whole nodules, and it was never observed in the case of pJP2.
In pea nodules, the R. leguminosarum VF39 gabT promoter is induced directly before interzone IIIII, and the gene is highly expressed throughout the late symbiotic zone III. This suggests a role of the GABA aminotransferase in the metabolism of the bacteroids. During symbiosis with the pea host, however, gabT mutants (PH10 and VF39-19T) did not show any phenotypes distinctly different from VF39. Also, expression of the gabT::uidA fusion in the mutant VF39-19T was not affected on the plant (data not shown).
To evaluate the possible role of the GABA shunt in bacteroid metabolism, a double mutant in both GABA aminotransferases may be required. Therefore a gabT deletion mutant is now being used as a recipient in a second transposon mutagenesis. Screening for mutants unable to grow on GABA may lead to a strain affected in pyruvate-dependent GABA aminotransferase activity.
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ACKNOWLEDGEMENTS |
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Received 16 July 2001;
revised 3 October 2001;
accepted 18 October 2001.