Studies on Diastereoisomeric α-Amino Acids and Corresponding α-Hydroxy Acids. VIII. Configuration of the Isomeric Octopines

Structural basis for high specificity of octopine binding in the plant pathogen Agrobacterium tumefaciens

Agrobacterium pathogens of octopine- and nopaline-types force host plants to produce either octopine or nopaline compounds, which they use as nutrients. Two Agrobacterium ABC-transporters and their cognate periplasmic binding proteins (PBPs) OccJ and NocT import octopine and nopaline/octopine, respectively. Here, we show that both octopine transport and degradation confer a selective advantage to octopine-type A. tumefaciens when it colonizes plants. We report the X-ray structures of the unliganded PBP OccJ and its complex with octopine as well as a structural comparison with NocT and the related PBP LAO from Salmonella enterica, which binds amino acids (lysine, arginine and ornithine). We investigated the specificity of OccJ, NocT and LAO using several ligands such as amino acids, octopine, nopaline and octopine analogues. OccJ displays a high selectivity and nanomolar range affinity for octopine. Altogether, the structural and affinity data allowed to define an octopine binding signature in PBPs and to construct a OccJ mutant impaired in octopine binding, a selective octopine-binding NocT and a non-selective octopine-binding LAO by changing one single residue in these PBPs. We proposed the PBP OccJ as a major trait in the ecological specialization of octopine-type Agrobacterium pathogens when they colonize and exploit the plant host.

Uptake and conversion of D-amino acids in Arabidopsis thaliana

The D-enantiomers of proteinogenic amino acids fulfill essential functions in bacteria, fungi and animals. Just in the plant kingdom, the metabolism and role of D-amino acids (D-AAs) still remains unclear, although plants have to cope with significant amounts of these compounds from microbial decay in the rhizosphere. To fill this gap of knowledge, we tested the inhibitory effects of D-AAs on plant growth and established a method to quantitate 16 out of 19 proteinogenic amino acids and their D-enantiomers in plant tissue extracts. Therefore, the amino acids in the extracts were derivatized with Marfey's reagent and separated by HPLC-MS. We used two ecotypes (Col-0 and C24) and a mutant (lht1) of the model plant Arabidopsis thaliana to determine the influence and fate of exogenously applied D-AAs. All of them were found in high concentrations in the plant extracts after application, even in lht1, which points to additional transporters facilitating the import of D-AAs. The addition of particular amino acids (D-Trp, D-Phe, D-Met and D-His) led to the accumulation of the corresponding L-amino acid. In almost all cases, the application of a D-AA resulted in the accumulation of D-Ala and D-Glu. The presented results indicate that soil borne D-AAs can actively be taken up and metabolized via central metabolic routes.

N5-(1-carboxyethyl)-ornithine, a new amino acid from the intracellular pool of Streptococcus lactis

Intracellular concentrations of amino acids were determined in cells of Streptococcus lactis 133 during growth in complex, spent, and chemically defined media. Glutamic and aspartic acids represented the major constituents of the amino acid pool. However, organisms grown in spent medium or in defined medium supplemented with ornithine also contained unusually high levels of two additional amino acids. One of these amino acids was ornithine. The second compound exhibited properties of a neutral amino acid by coelution with valine from the amino acid analyzer. The compound did not, however, comigrate with valine or any other standard amino acid by two-dimensional thin-layer chromatography. The unknown amino acid was purified by paper and thin-layer chromatography, and its molecular structure was determined by 1H and 13C nuclear magnetic resonance spectroscopy. This new amino acid was shown to be N5-(1-carboxyethyl)-ornithine. The 14C-labeled compound was formed by cells of S. lactis 133 during growth in spent medium or defined medium containing [14C]ornithine. Formation of the derivative by resting cells required ornithine and the presence of a metabolizable sugar. N5-(1-Carboxyethyl)-ornithine was synthesized chemically from both poly-S-ornithine and (2S)-N2-carbobenzyloxy-ornithine as a 1:1 mixture of two diastereomers. The physical and chemical properties of the amino acid purified from S. lactis 133 were identical to those of one of the synthetic diastereomers. The bis-N-trifluoroacetyl-di-n-butyl esters of the natural and synthetic compounds generated identical gas chromatography-mass spectrometry spectra. A mechanism is suggested for the in vivo synthesis of N5-(1-carboxyethyl)-ornithine, and the possible functions of this new amino acid are discussed.

Structure and synthesis of histopine, a histidine derivative produced by crown gall tumors

Histopine, an unusual amino acid derivative of histidine isolated from crown gall tumors of sunflowers (Helianthus annus) inoculated with Agrobacterium tumefaciens strain B6, was previously assigned the gross structure N-(1-carboxyethyl) histidine (2). A diastereomeric mixture containing histopine (2a and 2b) was readily prepared by reductive alkylation of (S)-histidine (1) with pyruvic acid and sodium cyanoborohydride. The individual diastereomers were prepared by reaction of (S)-histidine with (R)- and (S)-2-bromopropionic acid. (R)-N-(1-Carboxyethyl)-(S)-histidine (2a) supports the growth of A. tumefaciens whereas (S)-N-(1-carboxyethyl)-(S)-histidine (2b) is inactive. Therefore, we assign structure 2a to histopine.

Multiple genes coding for octopine-degrading enzymes in Agrobacterium

Most biotype 2 strains of Agrobacterium tumefaciens and A. radiobacter which utilize nopaline also degrade octopine. In all such strains studied, the ability to degrade octopine did not appear to be transferred to plasmidless recipient cells under conditions of plasmid transfer in which the ability to utilize nopaline was transferred. An octopine-degrading mutant was isolated in a strain cured of its plasmid, suggesting that genes of octopine degradation may have a chromosomal location in some strains. In strains in which octopine utilization is coded by plasmid genes, octopine degradation was always inducible, whereas in strains which degrade both octopine and nopaline, octopine utilization was constitutive although nopaline degradation was inducible. When plasmids coding for octopine-utilizing ability were transformed into a strain containing either a nopaline- or null-type plasmid, transformants able to degrade octopine were either not observed or were unstable upon purification. All of these data suggest that plasmids associated with virulence are incompatible with one another, and therefore imply that the major groups of plasmids associated with virulence have a common origin.

Enzymic and chemical synthesis of epilson-N-(L-propionyl-2)-L-lysine

Pyruvate was shown to act as an oxo acid substrate in the reverse direction of saccharopine dehydrogenase [epsilon N-(L-glutaryl-2)-L-lysine: NAD oxidoreductase (L-lysine-forming)] reaction. The enzymic condensation product of lysine and pyruvate was isolated and identified as epsilon-N-(L-propionyl-2)-L-lysine by comparison with the synthetic compound. A method for the chemical preparation of diastereoisomers of epsilon-N-(propionyl-2)-L-lysine is also described.

Investigations on the kinetic mechanism of octopine dehydrogenase. 1. Steady-state kinetics

The kinetic mechanism of action of octopine dehydrogenase was investigated. This enzyme catalyses the reversible dehydrogenation of D-octopine to L-arginine and pyruvate, in the presence of nicotinamide-adenine dinucleotide. Initial velocity and product inhibition studies were carried out in both directions. Most of the results are consistent with a bi-ter sequential mechanism where NAD+ binds first to the enzyme followed by D-octopine, and the products are released in the order L-arginine, pyruvate and NADH. Various kinetic parameters were determined for each reactant at 33 degrees C, at pH 9.6 for NAD reduction, at pH 6.6 for NADH oxidation.