Inactivation of an aminoaldehyde dehydrogenase is responsible for fragrance in rice
Rice (Oryza sativa) has two betaine aldehyde dehydrogenase homologs, BAD1 and BAD2, encoded on chromosome four and chromosome eight respectively. BAD2 is responsible for the characteristic aroma of fragrant rice. Complementary DNA clones of both BAD1 and BAD2 were isolated and expressed in E. coli. BAD2 had optimum activity at pH 10, little to no affinity towards N-acetyl-γ-aminobutyraldehyde (NAGABald) with a Km of approximately 10 mM and moderate affinity towards γ-guanidinobutyraldehyde (GGBald) and betaine aldehyde (bet-ald) with Km values of approximately 260 μM and 63 μM respectively. A lower Km of approximately 9 μM was observed with γ-aminobutyraldehyde (GABald), suggesting BAD2 has a higher affinity towards this substate in vivo. The enzyme encoded on chromosome four, BAD1, had optimum activity at pH 9.5, showed little to no affinity towards bet-ald with a Km of 3 mM and had moderate affinity towards GGBald, NAGABald and GABald with Km values of approximately 545, 420 and 497 μM respectively. BAD1 had a half life roughly double that of BAD2. We discuss the implications of these findings on the pathway of fragrance generation in Basmati and Jasmine rice and the potential of rice to accumulate the osmoprotectant glycine betaine.
KeywordsAminoaldehyde dehydrogenase Betaine aldehyde dehydrogenase Basmati Rice Fragrance Jasmine
Jasmine and basmati style rice has a pleasant aroma due to the accumulation of the volatile compound 2-acetyl-1-pyrroline (2AP) (Buttery et al. 1983a; Lorieux et al. 1996; Widjaja et al. 1996; Yoshihashi 2002a) in all aerial parts of the plant including the leaves and grain (Yoshihashi et al. 2002b). As well as being the major chemical component of fragrance in rice (Buttery et al. 1983a), 2AP is a significant aroma chemical in a number of organisms and foodstuffs including Pandanus (Buttery et al. 1983b; Laohakunjit and Noomhorm 2004; Thimmaraju et al. 2005), popcorn (Schieberle 1995), corn tortillas (Buttery and Ling 1995), baguettes (Zehentbauer and Grosch 1998), ham (Carrapiso et al. 2002), cheese (Zehentbauer and Reineccius 2002), mung bean (Brahmachary and Ghosh 2002), green tea (Kumazawa and Masuda 2002), bread flowers (Vallaris glabra Ktze) (Wongpornchai et al. 2003) some yeasts (Snowdon et al. 2006) and select bacteria (Romanczyk et al. 1995; Costello et al. 2001; Rungsardthong and Noomhoom 2005; Snowdon et al. 2006; Adams and De Kimpe 2007) including the wine spoilage bacteria Lactobaccillus hilgardii (Costello et al. 2001; Snowdon et al. 2006).
Studies into the biological formation of 2AP have shown it can be derived from either proline or ornithine in rice (Yoshihashi et al. 2002b), Pandanus (Thimmaraju et al. 2005) and L. hilgardii (Costello et al. 2001). In rice the nitrogen in the pyrroline ring of proline becomes the nitrogen in the pyrroline ring of 2AP while the carboxyl group of proline is removed and replaced with an acetyl group from another source (Yoshihashi et al. 2002b). Costello et al. (2001) found that in L. hilgardii the acetyl group of 2AP can be derived from fructose when either ethanol or acetaldehyde are supplied in excess. They further suggested Δ1pyrroline, a product of proline catabolism via putrescine oxidation, is the immediate precursor of the pyrroline ring of 2AP and the acetyl group was most likely formed from reaction with acetyl-CoA or acetaldehyde in either a chemical or enzymatic reaction. Additionally, detailed precursor studies have revealed that the formation of 2AP in Bacillus cerus proceeds via acetylation of Δ1pyrroline (Adams and De Kimpe 2007).
Several independent lines of evidence suggest the genetic cause of rice fragrance is due to the loss of function of the betaine aldehyde dehydrogenase (BAD) homolog. Fragrance is a recessive trait (Lorieux et al. 1996; Garland et al. 2000; Jin et al. 2003) which suggests it is a loss, rather than gain, of gene function that is responsible for fragrance. Several mapping studies have independently identified BAD2 as the candidate gene responsible for fragrance (Bradbury et al. 2005a, b; Vanavichit et al. 2006; Amarawathi et al. 2008; Shi et al. 2008) and sequencing of BAD2 in each case found a deletion within the gene which would render the gene non-functional. Bradbury et al. (2005a) identified an eight base pair deletion in BAD2 which leads to the generation of a premature stop codon that would, if translated, produce a truncated non-functional protein. A variation of this deletion was reported in some Basmati varieties where a five base pair deletion was present at the same location in exon eight rather than the eight base pair deletion (Amarawathi et al. 2008) and Shi et al. (2008) identified a seven base pair deletion in exon two that also renders the BAD2 gene product non-functional and generates fragrance. The accumulated data shows that the generation of fragrance in rice is due to loss of function of the BAD2 gene product and not due to gain of a novel function.
Betaine aldehyde dehydrogenase is an enzyme capable of converting betaine aldehyde (bet-ald), a product of choline oxidation, into the osmoprotectant glycine betaine (Ishitani et al. 1993; Russell et al. 1998; Shirasawa et al. 2006), however, reports of BADs in non glycine betaine accumulating species, including rice, (Ishitani et al. 1993; Nakamura et al. 1997; Mohanty et al. 2002; Niu et al. 2007) suggest BAD enzymes have a role other than the generation of glycine betaine. Many recent studies have found plant BADs are capable of metabolising a range of substrates including omega-aminoaldehydes, often more efficiently than bet-ald (Trossat et al. 1997; Incharoensakdi et al. 2000; Livingstone et al. 2003; Oishi and Ebina 2005), while others report enzymes with aminoaldehyde dehydrogenase (AAD) activity that have high homology to BADs but no affinity for bet-ald (Sebela et al. 2000), leading to the suggestion BADs and AADs are the same enzyme and should be reclassified as such (Sebela et al. 2000; Livingstone et al. 2003; Reumann 2004).
Some of the chemicals other than bet-ald that are substrates of BADs and AADs include; 3-aminopropanaldehyde, 3-dimethylsulfoniopropionaldehyde, γ-guanidinobutyraldehyde (GGBald) and γ-aminobutyraldehyde (GABald) (Trossat et al. 1997; Incharoensakdi et al. 2000; Sebela et al. 2000; Oishi and Ebina 2005). The latter of these, GABald, is a four carbon aminoaldehyde derived from proline via putrescine oxidation that in solution exists in equilibrium with its cyclic form, Δ1-pyrroline (Struve and Christophersen 2003), a precursor of 2AP in B. cerus (Adams and De Kimpe 2007). GABald is the immediate precursor of γ-aminobutyric acid (GABA) a four carbon amino acid that purportedly plays a role as a natural pesticide (Shelp et al. 2006) and has been shown to play a role in pollen tube growth and guidance (Palanivelu et al. 2003).
It seems plausible that the cDNAs annotated as encoding enzymes with BAD activity in rice, BAD1 and BAD2, actually encode enzymes with AAD activity and that inactivation of BAD2, encoded from chromosome eight, leads to the accumulation of GABald/Δ1-pyrroline, the immediate precursor of 2AP. In order to explore this question further, BAD1 and BAD2 cDNAs were isolated and expressed in E. coli and the purified enzymes analysed for affinity to a range of substrates including bet-ald and GABald.
Materials and methods
Plant materials and RNA extraction
Oryza sativa cv. Nipponbare was obtained as seed from the Australian Plant DNA Bank (www.biobank.com) and grown in sterile tap water for two to four weeks before extraction of total RNA using a Qiagen RNeasy® Plant Mini Kit (50) according to the manufacturer’s instructions. Total RNA quantity and quality was assessed by gel electrophoresis and absorbance at 260 nm. Prior to cDNA synthesis, total RNA was incubated for 30 min at 25°C with 1U DNase (Roche)/ μg RNA in a 1/10th volume 10× DNase 1 reaction buffer (Invitrogen).
First strand cDNA synthesis utilised the Transcriptor™ First Strand cDNA synthesis Kit (Roche, Mannheim, Germany) according to the manufacturer’s instructions. Reactions contained 0.5–1 μg total RNA, 10U Transcriptor™ reverse transcriptase and 50 pmol Anchored-oligo(dT)18 primer supplied with the kit. Reactions were incubated at 55°C for 30 min and stopped by incubating at 85°C for 5 min. Subsequent PCR amplification used between 1 μl and 5 μl of the first strand cDNA per 50 μl reaction.
PCR amplification and cloning
As BAD1 and BAD2 have previously been identified as full length cDNAs of known sequence, both were initially amplified in two halves utilising the primers 5′-CCAAGGTCCGGGACAAC-3′ and 5′-GCACCGGCACATCTTGCTGT-3′ for the first half of BAD1, 5′-TAGCTTCACATCCCCATGTG-3′ and 5′-TTCTGTCCGTCCGTTCTG-3′ for the second half of BAD1, 5′-GATGGCCACGGCGATC-3′ and 5′-TTTCTCCAGATGCTTGGGTC-3′ for the first half of BAD2 and 5′-CTGGTAAAAAGATTATGGCTTCA-3′ and 5′-CCGTCATACTATGGCCTCTTA-3′ for the second half of BAD2. These products were then used in a PCR amplification of the full length cDNAs using primers which contained Nde1 and BamH1 restriction sites. BAD1 full-length cDNA was amplified by PCR using the sense primer 5′-ATATCCATATGATGGCCGCGCCGTCGGCGATCCC-3′ and antisense primer 5′-AATTCGGATCCTGACGTGCTCCGTCGCTCTTG-3′. BAD2 full-length cDNA was amplified by PCR using the sense primer 5′-ATATCCATATGATGGCCACGGCGATCCCGCAG-3′ and antisense primer 5′-AATTCGGATCCACGATCAGAACAGATGGGCGTGTC-3′. PCRs were performed using Platinum® Taq DNA Polymerase High Fidelity from Invitrogen™. Reactions contained 0.2 μM of each primer, 2 μl cDNA, 2 mM MgSO4, 5% DMSO, 3% glycerol and 2 units of HiFi Taq in 1× buffer to a volume of 50 μl. Thermal cycling parameters were as follows: 94°C, 2 min for one cycle; 94°C, 30 s; 58°C, 30 s; 68°C, 1 min 40 s for 30 cycles. Analysis of PCR products on a 1% agarose gel revealed single bands of appropriate size. Prior to ligation into pGEM®-T vector (Promega), A overhangs were added by incubation of cDNAs with 5 mM dATP, 1× PCR buffer 5 mM MgCl2 and Platinum Taq DNA polymerase at 95°C for 5 min followed by 70°C for 30 min. Following ligation into pGEM®-T (Promega) restriction digests with Nde1 and BamH1 were performed which allowed directional cloning into pET-19b expression vector (Novagen) following the manufacturer’s instructions.
Cloned cDNAs were sequenced using the BigDye® Terminator v3.1 Cycle Sequencing Kit (Applied Biosystems, Foster, CA., USA) and the labelled DNA fragments separated and analysed with an ABI 3730 48 capillary DNA analyser (Applied Biosystems). All sequence analysis and alignments were undertaken using ChromasPro software (Technelysium Pty Ltd).
Recombinant protein expression and purification
Full length BAD1 and BAD2 cDNAs were directionally cloned into the Nde1 and BamH1 restriction sites of the bacterial expression plasmid pET19b (Novagen) to enable addition of a 10× Histidine tag to the C terminus of both enzymes. E. coli strain BL21 (Novagen, Madison, WI, USA) was transformed with the pET19b-BAD1 and pET19b-BAD2 vector constructs and grown in Luria-Bertani medium supplemented with appropriate antibiotics according to the manufacturer’s instructions. One hundred ml of an overnight culture was transferred to 500 ml fresh Luria-Bertani medium and grown for a further 3 h. The expression of recombinant protein was then induced by the addition of 1 mM isopropyl β-D-thiogalactoside (IPTG) and the cells were allowed to grow for a further 3 h at 37°C with shaking (210 rpm) before harvesting by centrifugation at 4°C. The cells were lysed in lysis/bind buffer (300 mM NaCl, 50 mM sodium phosphate buffer (pH 8.0), 10 mM imidazole, 1/10th volume 10× BugBuster® Protein Extraction Reagent (Novagen, Darmstadt, Germany), Complete, EDTA-free protease inhibitor cocktail (Roche, Mannheim, Germany), 100 μM sodium orthovanadate, 100 μM sodium molybdate and 100 μM sodium tartrate. Insoluble material was pelleted by centrifugation at 15,000g for 30 min at 4°C and the resulting supernatant was incubated on ice in the presence of 500 μl Ni-NTA His·Bind® Resin (Novagen) for 60 min with gentle shaking. The resin was washed 5× in 10 ml wash buffer (300 mM NaCl, 50 mM sodium phosphate buffer, 20 mM imidazole, pH 8.0) to remove contaminating proteins. Recombinant His-BAD protein was eluted by 7× 500 μl washes in elution buffer (300 mM NaCl, 50 mM sodium phosphate buffer, 250 mM imidazole, pH 8.0). Elutions were pooled and dialysed against 50 mM HEPES buffer (pH 7.5) for 24 h at 4°C. Following dialysis the protein was concentrated 10 fold by centrifugation using a 12–14 kDa cut-off spin column and stored at −80°C with the addition of 10% glycerol. The presence of recombinant protein was confirmed by SDS/PAGE.
Synthesis of substrates
Betaine aldehyde was obtained from Sigma-Aldrich. GABald/ Δ1-pyrroline was synthesised to 86% purity by the method of Struve and Christophersen (2003). GGBald was synthesised by a modification of the method of Vanderbilt et al. (1975) by bubbling nitrogen gas through a 20 ml (1.0 mmol) solution of arginine in water for 5 min, heating to 30°C before adding, while mixing, chloramine-T hydrate to a concentration of 1.0 mmol. This mixture was incubated at 30°C for 30 min, cooled on ice and filtered. The filtrate was then purified to 81% by separation on a preparative Phenomenex LunaC18 100A, 5u, 150 × 25.4 mm I.D. HPLC column using Gilson 306 gradient pumps, Gilson 155 UV/Vis detector, Gilson 204 fraction collector and controlled using Gilson Unipoint software. The mobile phase was an acetonitrile/water mixture with 0.05% trifluoroacetic acid, at a flow rate of 15 ml/min starting at 1% acetonitrile and holding for 5 min before ramping up to 90% acetonitrile over 15 min. Selected fractions were pooled and dried under vacuum on a BÜCHI Rotorvapor R-114 rotary evaporator. NAGABald diethyl acetal was synthesised by modification of the method of Rajabi and Saidi (2005). Briefly, 250 μl of GABald diethylacetal was mixed with an equimolar volume of acetic anhydride and microwaved (on high) for 5 × 3 s. The diethylacetal groups were removed by the method of Struve and Christophersen (2003) to leave NAGABald of 73% purity as determined by LCMS.
Purity of GGBald and NAGABald was assessed by LCMS using a Phenomenex AquaC18 125A, 5u, 150 × 4.6 mm I.D. HPLC column on an Agilent 1100 LC and an Agilent 1100 MSD controlled by chemstation software. The mobile phase was an acetonitrile/water mix with 0.05% trifluoroacetic acid, at a flow rate of 1 ml/min starting at 1% acetonitrile and holding for 5 min before ramping up to 90% acetonitrile over 15 min. The MS was run in atmospheric pressure chemical ionisation (APCI) mode, had an ionisation voltage of 150 V, capillary voltage of 2000 V, drying gas temperature of 345°C, vaporiser temperature of 395°C, nebuliser pressure of 60 psig and a gas flow rate of 5 l/min. The purity of Δ1-pyrroline was assessed on an Agilent 6890 Series GC system with an Agilent 5973 Network Mass Selective Detector using an SGE BPX5 capillary column 50.0 m × 0.22 mm ID × 1 μm film thickness. One μl of sample was injected at an inlet temperature of 280°C and 25:1 split ratio. Helium was used as the carrier gas with a constant flow of 1.5 ml/min. The oven was held at 50°C for 5 min before ramping up to 300°C at a rate of 4°C/min.
Enzyme assay mixtures (1 ml total volume) were based on the work of Yorifuji et al. (1986), Trossat et al. (1997), Valenzuela-Soto et al. (2003) and Oishi and Ebina (2005) and contained 50 mM HEPES, MES or Glycine Buffer, 20 mM β-mercaptoethanol, 2 mM NAD+, with 10 ug of enzyme (BAD1 or BAD2) and varying concentrations of substrates. HEPES and MES buffers were obtained from Sigma, glycine buffer consisted of 50 mM glycine, 1 mM MgSO4, 0.1 mM ZnSO4. Buffers were adjusted to the required pH by addition of KOH. The reaction was followed by monitoring the conversion of NAD+ to NADH (340 nm) on a Hewlett Packard 8453 UV/vis spectrophotometer controlled by ChemStation software. For determination of optimum pH, 5 mM GABald was used as the final substrate concentration and this was confirmed by replacing GABald with 5 mM bet-ald as the final substrate concentration. All enzyme assays were performed a minimum of three times.
Purification of recombinant rice BADs expressed in E. coli
SDS gel analysis showed rice BAD1 and BAD2 purified from E. coli have subunits of approximately 56 kDa. Final enzyme concentrations were adjusted to 10 μg/μl as determined by Bradford assay.
Synthesis of aldehyde substrates
Purity of synthesised substrates was analysed via GCMS. The GABald preparation displayed two main peaks with molecular weights of 69 and 87 corresponding to the circular Δ1-pyrroline form and the linear GABald form respectively. Likewise the N-acetyl- γ-aminobutyraldehyde (NAGABald) preparation showed a large peak with a molecular weight of 129 corresponding to the linear form of NAGABald and a smaller peak with a molecular weight of 113 corresponding to the circular form N-acetylpyrroline. Δ1-pyrroline was taken to be 86% pure based on the method of Struve and Christophersen (2003) while GGBald and NAGABald were determined by GCMS and LCMS analysis to be 81% and 73% pure respectively.
pH optimum and half life of BADs
Substrate specificity and activity of BADs
Km and kcat/Km values of BAD1 and BAD2 at optimum pH towards various substrates
Enzyme Km (μM)
Enzyme kcat/Km (M−1 s−1)
Enzyme half life and pH optima
In the absence of beta-mercaptoethanol the half life of BAD1 was approximately ten minutes while BAD2 had a half life of approximately five minutes. This stability difference could lead to an overestimation of the concentration of active BAD2 enzyme in comparison to BAD1 in corresponding assays, leading to an underestimation of BAD2 activity. This would not affect the reported Km values but would lead to larger kcat/Km values suggesting that our estimates of BAD2 kcat/Km are conservative.
Optimum activity of BAD1 and BAD2 towards bet-ald was found to be at pH 9.5 and pH 10 respectively. High pH optima have been reported for many AAD and BAD enzymes including BAD from oats (Livingstone et al. 2003), Zoysia tenuifolia (Oishi and Ebina 2005) and AAD from pea (Sebela et al. 2000). Both rice BAD1 and BAD2 are believed to be directed to the peroxisome (Nakamura et al. 1997; Bradbury et al. 2005a). Although no data are available on the pH of plant peroxisomes, Dansen et al. (2000) has shown that human fibroblast peroxisomes have a basic pH of around 8.2 ± 0.3. Struve and Christophersen (2003) investigated the influence of pH on structural forms of GABald and found that at pHs of 9–10 GABald exists almost entirely as the ring form, Δ1-pyrroline, and so BAD enzymes may therefore be active toward the ring form of this aldehyde. Alternatively, BADs may be active towards the linear form, GABald, which at high pH would have existed in the reaction mixture at very low concentrations. If this is the case, the Km values of both BADs towards the linear GABald would be significantly lower than those reported here. Studies on 2AP formation from proline in Maillard reactions have shown more 2AP is formed at pH 8 than is formed at pH 6 (Blank et al. 2003) suggesting a possible link between BAD location, GABald/Δ1-pyrroline isomeric form and 2AP formation.
Role of BAD2 and GABald accumulation in fragrance
Radio-labelling studies have shown the nitrogen in the pyrroline ring of proline becomes the nitrogen in the pyrroline ring of fragrant rice 2AP (Yoshihashi et al. 2002b). The compound Δ1-pyrroline is identical to the ring component of 2AP and has been shown to be a precursor of 2AP in Maillard reactions (Hofmann and Schieberle 1998) and more recently in B. cereus (Adams and De Kimpe 2007). Δ1-pyrroline exists in equilibrium with its linear form of GABald which is part of the proline catabolism pathway via oxidation of putrescine. GABald has been shown to be a substrate of BADs and AADs from various plants (Trossat et al. 1997; Sebela et al. 2000; Livingstone et al. 2003; Oishi and Ebina 2005) and a non-functional BAD2 is responsible for fragrance in rice (Bradbury et al. 2005a, b; Vanavichit et al. 2006; Amarawathi et al. 2008; Shi et al. 2008). Because of the associations between Δ1-pyrroline and 2AP and between GABald and BADs as well as the ability of GABald to spontaneously cyclise into Δ1-pyrroline, we focused on GABald as our primary substrate of interest. The other aldehyde substrates were chosen because of their similarity to GABald and occurrence in related pathways of proline/arginine catabolism. Bet-ald was chosen because of the homology based annotation of the gene responsible for fragrance in rice (Bradbury et al. 2005a).
Putrescine is found in high levels in actively growing tissues where cells are rapidly dividing (Kakkar et al. 2000) and is catabolised to GABald by diamine oxidase (DAO) during the processes of lignification and cell wall stiffening (Sebela et al. 2001), after the majority of cell division has taken place. Formation of GABald is therefore likely to occur in young tissue that has stopped actively dividing and is undergoing cell wall stiffening. Tips of rice leaves contain higher levels of 2AP than the base of the leaf (data not shown) while young leaves are more aromatic than old ones (Lorieux et al. 1996), which correlates with the proposed pathway of 2AP formation occurring shortly after putrescine catabolism (Fig. 4). Dissipation of 2AP in older tissue is most likely due to the volatile nature of the chemical (Yoshihashi et al. 2005).
BAD1 has a low affinity to GABald with a Km of 498 μM but a high kcat/Km of 27 M−1 s−1 suggesting that despite the large Km, GABald may still be a substrate for BAD1 in vivo and that the presence of BAD1 may diminish the pool of GABald available to form 2AP. The similarity of preferred substrates of BAD1 and BAD2 makes it unclear as to why a non-functional BAD2 has such a major impact on the fragrance phenotype of rice. Fitzgerald et al. (2008) have shown BAD1 accounts for at most 30% of total BAD gene expression within the leaves of non-fragrant rice, although this is increased by exposure to salt stress. It is therefore conceivable the fragrance phenotype of rice is altered by the action/inactivation of the BAD2 enzyme via a combination of its higher transcript levels, higher catalytic efficiency and higher substrate specificity towards GABald in comparison to that of BAD1. An absence of BAD2 is likely to cause an accumulation of GABald leading to higher 2AP production.
BAD1 may influence fragrance in rice, especially in saline conditions when BAD1 mRNA expression is higher and, perhaps more importantly, when levels of GABald are closer to that of the Km of BAD1. Lorieux et al. (1996) identified a minor locus for fragrance in rice located on chromosome four most likely between molecular markers RG214 and RG788. These markers are very close to molecular marker RZ675, located at 23,974,544 bp on chromosome four. The gene encoding the BAD1 enzyme is located on chromosome four between 23,146,445 and 23,150,872 bp (NCBI; http://www.ncbi.nlm.nih.gov/). This fragrance locus had less influence on 2AP accumulation in the varieties studied than BAD2 and it was only identified by Lorieux et al. (1996) when the BAD2 locus on chromosome eight was accounted for. More recent work has further narrowed down this region and suggested a role for BAD1 on the level of fragrance in Basmati rice (Amarawathi et al., 2008). With their similar activities and with BAD1 being associated with a fragrance allele, it seems likely that both BAD1 and BAD2 have an influence on 2AP accumulation in rice. Mutations that lead to a non-functional BAD1 or a reduction in expression levels of BAD1 may cause an increase in 2AP accumulation and could explain the minor fragrance allele identified by Lorieux et al. (1996) and Amarawathi et al. (2008).
Does fragrance affect plant performance?
The identification of a perturbation of one of the GABA synthesis pathways being key to 2AP accumulation in rice leads to the question; does this perturbation lead to a decrease in plant performance? BAD expression has previously been linked to salt tolerance in numerous plants (Ishitani et al. 1995; Harinasut et al. 1996; Wood et al. 1996) and the gene expression of BAD2 (Fitzgerald et al. 2008) and the concentration of GABA (Kim et al. 2007) has been found to increase in rice under salt stress. BAD2 has been shown to play a role in salt tolerance in rice, yet does not accumulate glycine betaine (Ishitani et al. 1993; Rathinasabapathi et al. 1993) and we have shown that GABald is the preferred substrate of BAD2. The predominant pathway to GABA formation in plants is via direct decarboxylation of glutamate (Narayan and Nair 1990; Snedden et al. 1995) and alternative pathways of GABA synthesis are from either arginine or ornithine decarboxylases via putrescine (Narayan and Nair 1990; Kakkar et al. 2000). A GABA gradiant has been shown to play an essential role in pollen tube growth and guidance in Arabidopsis (Palanivelu et al. 2003) and interruption of this gradient inhibits pollen tube growth. Reports of low yield in fragrant rice parallel reports of sterility in fragrant Pandanus (Stone 1978), a plant that is often grown in environments that are subject to water or salinity stress. BAD2 may play a role in the generation of a GABA gradient in rice panicles, under stress conditions, and disruption of this process may inhibit plant performance, including grain yield.
Betaine aldehyde accumulation
Rice does not accumulate glycine betaine, reportedly because its genome encodes a choline monooxygenase (CMO) that is non-functional due to aberrant stop codons (NCBI accession number P0545E05.33 chromosome 6) (Shirasawa et al. 2006). Although there have been no reports of a CMO being isolated or characterised from any plant in the Poaceae to date (Jagendorf and Takabe 2001; Oishi and Ebina 2005), the NCBI database records the isolation of an apparently complete CMO cDNA from rice (AJ578494) (Niu et al. 2007). If this putative rice CMO is fully functional then a new theory as to why rice does not accumulate glycine betaine is called for. Perhaps rice CMO is expressed at low levels. Alternatively, CMO and BAD expression maybe spatially or temporally separated, the apparent localisation of BAD in the peroxisome and CMO in the cytoplasm may separate the pool of the toxic intermediate bet-ald from BAD.
Efforts to engineer glycine betaine accumulation in fragrant rice need to ensure the pool of GABald is maintained at levels which result in the formation of detectable levels of 2AP. This could be achieved by the use of the codA gene which produces an enzyme that converts choline directly to glycine betaine, and probably has very low affinity for GABald. Furthermore, targeting this enzyme to the chloroplast could maximise salt tolerance and isolate the action of this enzyme from the pool of GABald, there by maintaining 2AP levels in fragrant rice while increasing salt tolerance. Transformation of a fragrant rice variety, Pusa Basmati 1, with codA has resulted in glycine betaine accumulation and enhanced salt tolerance (Mohanty et al. 2002), however, since the close association between glycine betaine and fragrance was unknown at that time, the effect of codA expression on fragrance was not assessed.
We have shown that two enzymes previously annotated as BADs actually have a greater affinity towards aminoaldehydes and as such should be reclassified AADs. We have demonstrated for the first time the biochemical function of an enzyme produced from a gene which has previously been linked to the fragrance phenotype in rice (Bradbury et al. 2005a). The accumulation of 2AP in rice is explained by the absence of BAD2 activity leading to an increased level of its preferred substrate, GABald/Δ1-pyrroline, the immediate precursor of 2AP. This work has also provided insights which are applicable to efforts to engineer glycine betaine accumulation in rice which would enhance stress tolerance.
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- Brahmachary RL, Ghosh M (2002) Vaginal pheromone and other compounds in mung-bean aroma. J Sci Ind Res (India) 61:625–629Google Scholar
- Buttery RG, Juliano BO, Ling LC (1983b) Identification of rice aroma compound 2-Acetyl-1-Pyrroline in Pandan Leaves. Chem Ind (Lond) 478–479Google Scholar
- Fitzgerald TL, Waters DLE, Henry RJ (2008) The affect of salt on betaine aldehyde dehydrogenase transcript levels and 2-acetyl-1-pyrroline concentration in fragrant and non-fragrant rice (Oryza sativa). Plant Sci. doi: 10.1016/j.plantsci.2008.06.005
- Harinasut P, Tsutsui K, Takabe T, Nomura M, Takabe T, Kishitani S (1996) Exogenous glycine betaine accumulation and increased salt-tolerance in rice seedlings. Biosci Biotechnol Biochem 60:366–368Google Scholar
- Incharoensakdi A, Matsuda N, Hibino T, Meng YL, Ishikawa H, Hara A et al (2000) Overproduction of spinach betaine aldehyde dehydrogenase in Escherichia coli. Structural and functional properties of wild-type, mutants and E. coli enzymes. Eur J Biochem 267:7015–7023. doi: 10.1046/j.1432-1327.2000.01797.x PubMedCrossRefGoogle Scholar
- Ishitani M, Arakawa K, Mizuno K, Kishitani S, Takabe T (1993) Betaine aldehyde dehydrogenase in the Gramineae. Levels in leaves of both betaine accumulating and non-accumulating cereal plants. Plant Cell Physiol 34:493–495Google Scholar
- Nakamura T, Yokota S, Muramoto Y, Tsutsui K, Oguri Y, Fukui K et al (1997) Expression of a betaine aldehyde dehydrogenase gene in rice, a glycine betaine nonaccumulator, and possible localization of its protein in peroxisomes. Plant J 11:1115–1120. doi: 10.1046/j.1365-313X.1997.11051115.x PubMedCrossRefGoogle Scholar
- Niu XL, Zheng WJ, Lu BR, Ren GJ, Huang WZ, Wang SH et al (2007) An unusual post-transcriptional processing in two Betaine aldehyde dehydrogenase loci of cereal crops directed by short, direct repeats in response to stress conditions. Plant Physiol 143:1929–1942. doi: 10.1104/pp.107.095752 PubMedCrossRefGoogle Scholar
- Rathinasabapathi B, Gage DA, Mackill DJ, Hanson AD (1993) Cultivated and wild rices do not accumulate glycine betaine due to deficiencies in two biosynthetic steps. Crop Sci 33:534–538Google Scholar
- Sebela M, Brauner F, Radova A, Jacobsen S, Havlis J, Galuszka P et al (2000) Characterisation of a homogeneous plant aminoaldehyde dehydrogenase. Biochim Biophys Acta Protein Struct Mol Enzymol 1480:329–341Google Scholar
- Shi W, Yang Y, Chen S, Xu M (2008) Discovery of a new fragrance allele and the development of functional markers for the breeding of fragrant rice varieties. Mol Breed (Published Online)Google Scholar
- Stone BC (1978) Studies in Malesian Pandanaceae XVII on the taxonomy of ‘Pandan Wangi’ a Pandanus cultivar with scented leaves. Econ Bot 32:285–293Google Scholar
- Thimmaraju R, Bhagyalakshmi N, Narayan MS, Venkatachalam L, Ravishankar GA (2005) In vitro culture of Pandanus amaryllifolius and enhancement of 2-acetyl-1-pyrroline, the major flavouring compound of aromatic rice, by precursor feeding of L-proline. J Sci Food Agric 85:2527–2534. doi: 10.1002/jsfa.2286 CrossRefGoogle Scholar
- Valenzuela-Soto EM, Velasco-Garcia R, Mujica-Jimenez C, Gaviria-Gonzalez L, Munoz-Clares RA (2003) Monovalent cations requirements for the stability of betaine aldehyde dehydrogenase from Pseudomonas aeruginosa, porcine kidney and amaranth leaves. Chem Biol Interact 143:139–148. doi: 10.1016/S0009-2797(02)00198-9 PubMedCrossRefGoogle Scholar
- Vanavichit A, Yoshihashi T, Wanchana S, Areekit S, Saengsraku D, Kamolsukyunyong W et al (2006) Positional cloning of Os2AP, the aromatic gene controlling the biosynthetic switch of 2-acetyl-1-pyrroline and gamma aminobutyric acid (GABA) in rice (abstract). In 5th International rice genetics symposium. Manila, PhilippinesGoogle Scholar
- Yorifuji T, Koike K, Sakurai T, Yokoyama K (1986) 4-Aminobutyraldehyde and 4-guanidinobutyraldehyde dehydrogenases for arginine degradation in Pseudomonas putida. Agric Biol Chem 50:2009–2016Google Scholar
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