Translator Disclaimer
1 April 2010 The Biosynthetic Pathways for Shikimate and Aromatic Amino Acids in Arabidopsis thaliana
Author Affiliations +
Abstract

The aromatic amino acids phenylalanine, tyrosine and tryptophan in plants are not only essential components of protein synthesis, but also serve as precursors for a wide range of secondary metabolites that are important for plant growth as well as for human nutrition and health. The aromatic amino acids are synthesized via the shikimate pathway followed by the branched aromatic amino acid metabolic pathway, with chorismate serving as a major branch point intermediate metabolite. Yet, the regulation of their synthesis is still far from being understood. So far, only three enzymes in this pathway, namely, chorismate mutase of phenylalanine and tyrosine synthesis, tryptophan synthase of tryptophan biosynthesis and arogenate dehydratase of phenylalanine biosynthesis, proved experimentally to be allosterically regulated. The major biosynthesis route of phenylalanine in plants occurs via arogenate. Yet, recent studies suggest that an alternative route of phynylalanine biosynthesis via phenylpyruvate may also exist in plants, similarly to many microorganisms. Several transcription factors regulating the expression of genes encoding enzymes of both the shikimate pathway and aromatic amino acid metabolism have also been recently identified in Arabidopsis and other plant species.

INTRODUCTION

The aromatic amino acids (AAA), phenylalanine (Phe), tyrosine (Tyr) and tryptophan (Trp) (Fig. 1), are central molecules in plant metabolism. Besides their function as building blocks of proteins, the three AAA serve as precursors for a variety of plant hormones, such as auxin and salicylate, as well as for a very wide range of aromatic secondary metabolites with multiple biological functions and biotechnological value in the health promoting, medical and food industries (Bartel, 1997; Vogt, 2010). The AAA of plants are also essential nutritive compounds in the diets of humans and monogastric livestock, which are unable to synthesize them (Li and Last, 1996; Galili et al., 2002). Additionally, the shikimate pathway enzyme 5-enolpyruvylshikimate-3-phospate synthase (EPSP synthase) is the target of the glyphosate herbicide, and non-plant EPSP synthase provides the herbicide-resistance trait in a number of commercial transgenic crops (Duke and Powles, 2008). These important properties account for the major motivation to elucidate the regulation of the shikimate and AAA biosynthesis pathways in plants.

The biosynthesis of AAA from core primary metabolism initiates via the shikimate pathway, leading to the synthesis of chorismate (Fig. 2). Chorismate is the initial branch point metabolite in the synthesis of all three AAA (Fig. 2) and the wide range of aromatic secondary metabolites derived from it (Gilchrist and Kosuge, 1980; Herrmann, 1995). Hence, the shikimate and AAA biosynthesis pathways also represent a major regulatory link of primary and secondary metabolism in plants.

Figure 1.

Structures of chorismate and the three aromatic amino acids.

Despite the extreme significance of the AAA to the life cycles of plants, the regulation their biosynthesis via the shikimate and AAA biosynthesis pathways has been largely ignored and even not reviewed in the last decade. Yet, these biosynthesis pathways have been re-visited in recent years by a number of studies. The present review focuses on new insights into the regulation of AAA biosynthesis, which are based on: (i) recent studies, focusing mainly on Phe and to a smaller extent also on Tyr and Trp biosynthesis; and (ii) gene sequence data generated from the sequencing of the entire Arabidopsis thaliana (Arabidopsis) genome. A more extensive background on the biochemistry of the shikimate and AAA biosynthesis pathways is available in the following outstanding and most recent reviews dating to the years 1995 and 1999 (Herrmann, 1995; Herrmann and Weaver, 1999).

Figure 2.

The shikimate pathway. Enzymes involved in the biosynthesis of chorismate.

THE SHIKIMATE PATHWAY

The shikimate pathway, also known as the chorismate biosynthesis pathway, converts two metabolites, phosphoenolpyruvate (PEP) of the glycolysis pathway and erythrose 4-phosphate (E4-P) of the non-oxidative branch of the pentose phosphate pathway, into chorismate (Fig. 2). Genes encoding enzymes of the entire shikimate pathway have been identified in Arabidopsis and other plant species, mostly due to their homology to shikimate pathway genes from microbial organisms. The conversion of PEP and E4-P to chorismate comprises seven reactions catalyzed by six enzymes. The first enzyme of the shikimate pathway is 3-deoxyd-arabino-heptulosonate-7-phosphate synthase (DAHPS) (EC 2.5.1.54) converting PEP and E4-P into 3- dehydroquaianate (Fig. 2). Arabidopsis plants possess two known DAHPS genes: AtDAHPS1 (At4g39980) and AtDAHPS2 (At4g33510) in addition to one putative gene (At1g22410) with high similarity to AtDAHPS1. Expression of AtDAHPS1 in Escherichia coli showed that this enzyme requires Mn2+ and reduced thioredoxin (TRX) for activity, thereby, linking carbon flow into the shikimate pathway to electron flow from photosystem I (Entus et al., 2002). Despite the metabolic importance of DAHPS as a branch point metabolite converting primary carbon metabolism into the shikimate pathway, it is still unknown whether this enzyme serves as a major regulator of flux between primary and secondary metabolism in plants. DAHPS activity may however be central to the ability of the shikimate pathway to compete for PEP and E4-P with glycolysis as well as with the non-oxidative pentose phosphate pathway (Fig. 2).

The second enzyme of the shikimate pathway is 3-dehydroquinate synthase (DHQS; EC 4.2.3.4; At5g66120), which converts 3-deoxy-d-arabino-heptulosonate-7-phosphate into 3-dehydroquinate (Fig. 2). The third and fourth enzymatic steps are catalyzed by the bi-functional enzyme 3-dehydroquinate dehydratase/shikimate 5-dehydrogenase (DHQ/SDH; EC 4.2.1.10 and EC 1.1.1.25) (At3g06350), leading to the formation of shikimate (Fig. 2). This bifunctional enzyme has been characterized in tomato (Solanum lycopersicum) (Bischoff et al., 2001) and tobacco (Nicotiana tabacum) (Bonner and Jensen, 1994). A recent study showed that the Arabidopsis AtDHQ/SDH gene is required for female gametophyte development and function (Pagnussat et al., 2005). The crystal structure of Arabidopsis DHQ/SDH with shikimate bound at the SDH site and tartrate at the DHQ site has recently been elucidated (Singh and Christendat, 2006). The interactions observed in the DHQ-tartrate complex reveal a conserved mode for substrate binding between the plant and microbial DHQ dehydratase family of enzymes. The arrangement of the two functional domains of this enzyme suggests that the control of metabolic flux through the shikimate pathway is achieved by increasing the effective concentration of the intermediate substrate, 3-dehydroshikimate, through the proximity of the two sites (Singh and Christendat, 2006). While Arabidopsis plants possess only a single AtDHQ/SDH gene, tobacco plants possess two genes. RNAi-mediated suppression of either of the two tobacco DHQ/SDH-1 and NtDHQ/SDH-2 genes caused differential steady state levels of the pathway substrates dehydroquinate and shikimate (Ding et al., 2007).

The fifth enzymatic step of the shikimate pathway is catalyzed by shikimate kinase (SK) (EC 2.7.1.71), which converts shikimate to shikimate 3-phosphate (Fig. 1). Arabidopsis plants possess two SK isoforms: AtSK1 (At2g21940) and AtSK2 (At4g39540) as well as two additional SK-like genes that arose from an ancestral plant SK gene duplicates, but lost their SK activity (Fucile et al., 2008). It has been suggested that these two genes may have evolved a new enzymatic function that is not related to the shikimate pathway (Fucile et al., 2008). Several lines of evidence suggest that plant SK acts as a regulatory step for the shikimate pathway, facilitating metabolic flux towards specific pools of secondary metabolite. These include: (i) a rapid induction of plant SK transcripts by fungal elicitors (Gorlach et al., 1995); (ii) a significant sensitivity of plant SK activity to cellular ATP energy charge; and (iii) the differential expression of the three rice (Oryza sativa) SK genes in specific developmental stages and in response to biotic stress (Kasai et al., 2005).

Figure 3.

Chorismate, a central branch point metabolite in the synthesis of aromatic amino acids and secondary metabolites. First enzymes involved in several secondary pathways derived from chorismate.

The sixth enzymatic step of the shikimate pathway is catalyzed by 5-enolpyruvylshikimate 3-phosphate synthase (EPSPS) (CE 2.5.1.19), which leads to the synthesis of enolpyruvylshikimate 3-phosphate (EPSP) (Fig. 1). The Arabidopsis EPSPS is encoded by one functional gene (At2g45300) and perhaps also by a second putative gene (At1g48860) (Klee et al., 1987). This enzyme has been broadly studied for the last ∼30 years (for review see Duke and Powles, 2008) due to its association with resistance to the herbicide N-phosphonomethylglycine (glyphosphate, an analog of phosphoenylpyruvate), which is the basis for the Roundup-Ready transgenic crops (Singer and McDaniel, 1985; Smart et al., 1985; Stalker et al., 1985). The native plant EPSPS is competitively inhibited by the herbicide glyphosphate, the consequence of which is a diminished flux of the shikimate pathway (Healy-Fried et al., 2007).

The final step in the shikimate pathway is catalyzed by chorismate synthase (CS) (CE 4.2.3.5), which converts EPSP to chorismate (Fig. 2). This enzyme was first characterized in Corydalis semoervirens (Schaller et al., 1991) and is proposed to have been derived from a common ancestor for bacteria, plants and fungi (Macheroux et al., 1999). Arabidopsis possesses a single CS gene (At1g48850), in contrast to tomato plants, which possess two differentially expressed CS genes, termed LeCS1 and LeCS2 (Gorlach et al., 1993).

CHORISMATE, A CENTRAL BRANCH POINT METABOLITE IN THE SYNTHESIS OF AROMATIC AMINO ACIDS AND SECONDARY METABOLITES

Chorismate, the terminal metabolite of the shikimate pathway serves as the initiator metabolite for the synthesis of the three AAA (Fig. 3) and hence also for the various aromatic secondary metabolites derived from them. Yet, chorismate also serves one of the initiator substrate of the synthesis of a number of other aromatic metabolites, many of which are likely to be still unknown. Some examples of chorismate-derived metabolites are: (i) chorismate is one of the precursor metabolites for the synthesis of tetrahydrofolate (vitamin B9; also commonly termed folate), serving as the substrate of the aminodeoxychorismate synthase (Fig. 3) (Basset et al., 2004; Waller et al., 2010); (ii) chorismate is converted to isochorismate by isochorismate synthase (Wildermuth et al., 2001) on route to the production of salicylate (SA) (Fig. 3) (Garcion et al., 2008); and (iii) chorismate also serves the precursor metabolite for the synthesis of phylloquinone (vitamin K1) and many other plant pigments (Gross et al., 2006; Kim et al., 2008). Hence, chorismate is one of the central branch point metabolites in plant cells.

THE BIOSYNTHESIS NETWORK OF THE THREE AROMATIC AMINO ACIDS PHE, TYR AND TRP

The unsolved pathway of Phe biosynthesis: two possible metabolic routes using arogenate or phenylpyruvate as intermediates

The first committed step of Phe biosynthesis from chorismate is catalyzed by chorismate mutase (CM) (CE 5.4.99.5), which converts chorismate to prephenate (Fig. 4). Three CM genes have so far been described in Arabidopsis, namely AtCM1 (At3g29200), AtCM2 (At5g10870) and AtCM3 (At1g69370) (Mobley et al., 1999). The three genes are differentially expressed in various tissues and the expression of only AtCM1 is induced by various elicitors and pathogens (Mobley et al., 1999; Ehlting et al., 2005). The activities of the three Arabidopsis CM isoforms were demonstrated by complementing E. coli and yeast CM-deficient strains (Eberhard et al., 1993; Eberhard et al., 1996). The activities of AtCM1 and AtCM3 are inhibited by Phe and Tyr, whereas the activity of AtCM2 appears to be insensitive to these amino acids (Eberhard et al., 1996). The final two enzymatic steps converting prephenate to Phe in plants are still not entirely elucidated. The major route involves the conversion of chorismate via arogenate to Phe, catalyzed by respective enzymes prephenate aminotransferase (PAT) (CE 2.6.1.79) and arogenate dehydratase (ADT) (CE 4.2.1.49) (Cho et al., 2007; Yamada et al., 2008; Maeda et al., 2010) (Fig. 4). Yet, it is still not clear whether plants can also convert chorismate to Phe via phenylpyruvate (PPY), using enzymes with prephenate dehydratase (PDT) and Phe aminotransferase activities (Fig. 4) in a similar manner to E. coli and various other microorganisms. A PAT enzymatic activity, converting prephenate into arogenate (Fig. 4), has been reported in plants (Siehl et al., 1986; De-Eknamkul and Ellis, 1988). Yet, no plant gene encoding such an activity has so far been reported. An in silico data mining approach identified six putative ADT genes in Arabidopsis, namely, ADT1 (At1g11790), ADT2 (At3g07630), ADT3 (At2g27820), ADT4 (At3g44720), ADT5 (At5g22630) and ADT6 (At1g08250). Biochemical characterization of the recombinant enzymes encoded by these six Arabidopsis genes suggested that all of them possess arogenate dehydratase activity, converting arogenate into Phe (Fig. 4). Yet, three of them (ADT1, ADT2 and ADT6) can also utilize prephenate as a substrate and convert it to PPY (Fig. 4), even though they exhibit a preference for arogenate (Cho et al., 2007). A rice 5-methyl-Trp resistant mutant, called Mtr1, which over-accumulates Phe, Trp and several phenylpropanoids, appeared to result from a point mutation in a gene encoding an enzyme possessing both ADT and PDT activities, rending these activities insensitive to feedback inhibition by Phe (Yamada et al., 2008). Nevertheless, similar to the Arabidopsis enzymes that can utilize both ADT and PDT substrates, this rice enzyme possessed a preference to arogenate, implying that it functions primarily as an ADT. Recently, three genes encoding ADT enzymes were identified in petunia (Petunia hybrida). Similar to the Arabidopsis ADT isozymes, the three petunia ADT isozymes preferentially use arogenate as a substrate, but can also use prephenate as a substrate at a much lower efficiencies, supporting the hypothesis of preferential utilization of the arogenate route rather than the PPY route for Phe biosynthesis in plants (Maeda et al., 2010). However, feeding shikimate into petunia petals with suppressed expression of ADT1 (the major ADT enzyme in petunia) led to the accumulation of prephenate and PPY and also to partial recovery of the reduced Phe level, strongly indicating that petunia plants can also synthesize Phe via the PPY route.

Figure 4.

The pathway of Phe biosynthesis. Enzymes involved in the biosynthesis of Phe. N.D. not detected in Arabidopsis plants.

To study the consequence of producing PPY in plants by metabolic engineering, we have recently expressed a bacterial PheA gene encoding a bi-functional CM/PDT enzyme that converts chorismate via prephenate to PPY (Tzin et al., 2009). These Arabidopsis plants had a significant increase in the level of Phe, with no increase in the level of PPY. Although it is likely that a considerable amount of the prephenate, produced by the CM activity of the bacterial CM/PDT enzyme, was converted via arogenate to Phe using the ADT enzyme (Fig. 4), the fact that these plants showed no increased level of PPY suggests that Arabidopsis apparently possesses an endogenous AAAT activity that can use PPY as a substrate and covert it to Phe (Tzin et al., 2009) (Fig. 4). Yet, no gene encoding an aromatic amino acid aminotransferase (AAAAT) (CE 2.6.1.57) that can specifically convert PPY into Phe has so far been identified in plants. Hence, taken together, the studies described above imply that plants use primarily the arogenate route for the synthesis of Phe, although some minor function of the PPY route in Phe biosynthesis cannot be ruled out. This is also supported by the observation that a number of plants species contain PPY, which also serves as a precursor for a number of secondary metabolites such as phenylacetaldehyde, 2-phenylethanol and 2-phenylethyl b-d-glucopyranoside (Watanabe et al., 2002; Kaminaga et al., 2006).

The pathway of Tyr biosynthesis

The major route of Tyr biosynthesis initiates from chorismate, using the same first two enzymes of Phe biosynthesis, namely CM and PAT, to produce arogenate (Fig. 4 and 5). Arogenate is then converted into Tyr by arogenate dehydrogenase (TyrA) (CE 1.3.1.43) (Fig. 5). TyrA activity has been demonstrated in tobacco (Gaines et al., 1982), maize (Byng et al., 1981), sorghum (Connelly and Conn, 1986) and Arabidopsis (Rippert and Matringe, 2002b). In Arabidopsis plants, two genes encoding TyrA enzymes were identified TyrA1 (At5g34930) and TyrA2 (At1g15710) (Rippert and Matringe, 2002b, a; Rippert et al., 2009).

A second possible route of Tyr biosynthesis has also been suggested, which includes the conversion of prephenate to phydroxyphenylpyruvate (p-hydroxyPPY) by prephenate dehydrogenase (PDH) (CE 1.3.1.43), which may be catalyzed by TyrA2 (Rippert and Matringe, 2002b). Subsequently, p-hydroxyPPY converts to Tyr by a broad range AAAAT (Fig. 5). Nevertheless, at a non-saturating concentration of prephenate, TyrA2 enzyme activity is 2000 times less efficient in catalyzing the reaction with prephenate than with arogenate (Rippert and Matringe, 2002a), and therefore the possible existence of this alternative route for Tyr biosynthesis using PDH is still in doubt.

The pathway of Trp biosynthesis

The first committed step of Trp biosynthesis includes a transfer of an amino group of glutamine to chorismate to generate anthranilate and pyruvate, catalyzed by anthranilate synthase (AS) (CE 4.1.3.27) (Fig. 6). Purified plant AS holoenzymes are believed to be heterotetramers composed of two alpha and two beta subunits (Niyogi et al., 1993; Poulsen et al., 1993). The Arabidopsis genome possesses two functional genes encoding the AS alpha subunit, ASa1 (At5g05730) and ASa2 (At2g29290), as well as a single functional ASb1 gene (At1g25220) encoding the AS beta subunit. In addition, two other genes were putatively assigned as encoding ASa subunits (At2g28880 and At3g55870) and additional five genes were putatively assigned as encoding ASb subunits (At5g57890, At1g25155, At1g24807, At1g24909 and At1g25083). Interestingly, four of the putative genes encoding ASb are located on one cluster on chromosome 1 (for more details see  http://www.plantcyc.org). The alpha subunit possesses the catalytic activity and the beta subunit possesses an aminotransferase activity, which transfers an amino group from glutamine to the alpha subunit. AS activity in plants is feedback inhibited by Trp through binding of Trp to the alpha subunit. Expression of AS genes encoding feedback-insensitive enzymes in a variety of plant species generally increases the production of free Trp and secondary metabolites derived from it (Li and Last, 1996; Tozawa et al., 2001; Hughes et al., 2004). The trp4 mutation in the gene encoding the Arabidopsis ASb1 subunit suppresses accumulation of the product of this enzyme, anthranilate (Niyogi et al., 1993). Anthranilate possesses a strong blue fluorescence under UV light, which has been utilized as a phenotypic marker for indentifying Arabidopsis mutants in the Trp biosynthesis enzymes (Rose et al., 1992; Radwanski et al., 1995).

Figure 5.

The pathway of Tyr biosynthesis. Enzymes involved in the biosynthesis of Tyr. N.D. not detected in Arabidopsis plants

The second enzyme in the Trp biosynthesis pathway is anthranilate phosphoribosylanthranilate transferase (PAT1) (CE 2.4.2.18; At5g17990), which converts anthranilate and phosphoribosylpyrophosphate into phosphoribosylanthranilate and inorganic pyrophosphate (Fig. 6).

The third enzyme in the Trp biosynthesis pathway is phosphoribosylanthranilate isomerase (PAI) (CE 5.3.1.24), which converts phosphoribosylanthranilate into l-(O-carboxyphenylamino)-l-deoxyribulose-5-phosphate (CDRP) (Fig. 6). Arabidopsis possesses three genes encoding PAI isoforms; PAI1 (At1g07780), PAI2 (At5g05590) and PAI3 (At1g29410).

Figure 6.

The pathway of Trp biosynthesis. Enzymes involved in the biosynthesis of Trp.

The fourth enzyme of Trp biosynthesis is indole-3-glycerol phosphate synthase (IGPS) (EC 4.1.1.48), which catalyzes the conversion of 1-(O- carboxyphenylamino)-1-deoxyribulose-5-phosphate to indole-3-glycerol phosphate (Li et al., 1995a). Arabidopsis plants possess one gene encoding a functional IGPS (AT2G04400) and also a second gene (AT5G48220) encoding a putative IGPS (Li et al., 1995a). IGPS is an important enzyme in the biosynthesis of Trp and the hormone indole-3-acetic acid (IAA; auxin) because it is the only known enzyme that catalyzes the formation of the indole ring. Quantitative comparison of the relative levels of Trp and IAA content in different Arabidopsis Trp biosynthesis mutants as well as in transgenic plants expression an IGPS antisense construct indicates that indole-3-glycerol phosphate is the branch-point metabolite for a de novo Trp-independent IAA biosynthesis in Arabidopsis (Ouyang et al., 2000). Interestingly, in both fungi and bacteria, IGPS is synthesized as a fusion protein containing one or two other enzymes of the Trp biosynthesis pathway (Li et al., 1995b). However, in plants IGPS generally appears as a mono-functional enzyme based on its cDNA sequence and functional complementation analysis (Li et al., 1995a).

The last two steps in the Trp biosynthesis are catalyzed by Trp synthase (TS) (CE 4.2.1.20), which includes both alpha (TSa) and beta (TSb) subunits. Indole-3-glycerol phosphate is cleaved by TSa to indole and glyceraldehyde-3-phosphate (α-reaction). Then, indole is transported to TSb, which catalyzes its condensation with serine (β-reaction) to produce Trp (Miles, 2001; Weber-Ban et al., 2001). Arabidopsis possesses at least one functional gene encoding TSa (At3g54640). Yet, a gene encoding a putative TSa homolog (At4g02610), also named indole synthase, was identified and characterized in Arabidopsis. Indole synthase possesses ∼65% amino acid sequence identity to TSa (Zhang et al., 2008). Arabidopsis possess two genes encoding functional TSb subunits, namely, TSb1 (At5g54810) and TSb2 (At4g27070), as well as two additional genes encoding putative TSb subunits (At5g28237 and At5g38530). The function of TSa1 and TSb1 was demonstrated by the facultative Trp auxotroph mutants, trp3 and trp2, respectively (Last et al., 1991), and it was suggested that the TSa1 and TSb1 subunits form an active heterodimer (Radwanski et al., 1995). The Arabidopsis gene encoding TSa1 was cloned by functional complementation of an E. coli mutant and suggested to function as a monomer (Bohlmann et al., 1995; Radwanski and Last, 1995; Radwanski et al., 1995). Yet, whether TS activity operates as a monomer or as a multi-enzyme complex is still not clear (Kriechbaumer et al., 2008).

TRANSCRIPTIONAL AND POST TRANSCRIPTIONAL REGULATON OF THE SHIKIMATE PATHWAY AND AROMATIC AMINO ACID METABOLISM

Transcriptional regulation

Transcriptional regulation of the shikimate pathway and aromatic amino acid metabolism in plants has so far not been studied extensively. The expression of DAHPS encoding the first enzyme of the shikimate pathway (Fig. 2) is induced by physical wounding and methyl-jasmonate (Devoto et al., 2005; Yan et al., 2007), infiltration with pathogenic Pseudomonas syringae strains (Keith et al., 1991), redox state (Entus et al., 2002) and abscisic acid (Leonhardt et al., 2004; Catala et al., 2007). The expression of the gene encoding EPSPS is induced in response to infection by the necrotrophic fungal pathogen Botrytis cinerea (Ferrari et al., 2007) and by sulfate starvation (Nikiforova et al., 2003). Fungal elicitors also rapidly stimulate the production of mRNA of SK (Gorlach et al., 1995). Ozone treatment induces a significant part of the shikimate pathway genes in tomato (Bischoff et al., 1996; Bischoff et al., 2001), tobacco (Janzik et al., 2005) and in the European beech (Fagus sylvatica) (Betz et al., 2009). Oligogalacturonides that are released from plant cell walls upon infection with of the Botrytis cinerea pathogen stimulate a number of genes encoding enzymes of the shikimate and AAA biosynthesis pathways, as well as genes encoding enzyme of secondary metabolites derived from the AAA (Ferrari et al., 2007). The expression of the three Arabidopsis genes encoding the three PAI isoforms (Fig. 6) is differentially regulated under normal growth conditions, with PAI1 and PAI3 showing ∼10-fold higher expression level than PAI2 (He and Li, 2001). Expression of these three PAI genes also respond differentially to environmental stresses, such as UV irradiation and treatment with the abiotic elicitor silver nitrate in a tissue- and cell-type-specific manner (Li et al., 1995b; He and Li, 2001). Deletion of the Arabidopsis gene encoding PAI1 causes some abnormal growth (He and Li, 2001) which indicates its predominant importance in Trp biosynthesis. Interestingly, the Arabidopsis PAI gene family is regulated by methylation in the Wassilewskija, but not Columbia ecotypes (Bender and Fink, 1995; Melquist et al., 1999). The PAI genes of Wassilewskija contain inverted repeats, which provide a trigger for their methylation (Bender and Fink, 1995; Melquist et al., 1999; Bartee and Bender, 2001; Melquist and Bender, 2003).

The Arabidopsis gene encoding IGPS of Trp biosynthesis (Fig. 6) is regulated by the hormones jasmonate (Sasaki-Sekimoto et al., 2005; Dombrecht et al., 2007) and salicylate (Rajjou et al., 2006), and also in seeds and seedlings by various defense mechanisms (Job et al., 2005; Chibani et al., 2006). In addition, expression of the Arabidopsis gene encoding PAT1 is apparently controlled by regulatory elements located inside introns, as inclusion of introns was shown to enhance the expression of PAT1-GUS fusion constructs that were stably transformed into Arabidopsis (Rose and Beliakoff, 2000).

Recently, in the frame of the AtGenExpress project, the response of the global Arabidopsis transcriptome to a variety of abiotic and biotic stresses was studied in roots and shoots, using the Affymetrix ATH1 microarray (NASC;  http://affymetrix.arabidopsis.info/) (Kilian et al., 2007). The database of these experiments was used in a bioinformatics study to analyze of the response of genes encoding biosynthesis enzymes as well as enzymes responsible for the first catabolic enzymes of the different amino acid in a variety of amino acid metabolic pathways (Less and Galili, 2008). The results showed that genes encoding amino acid catabolic enzymes principally respond in shorter time periods and are much more sensitive to abiotic stresses than genes encoding biosynthetic (allosteric and non-allosteric) enzymes. These responses also operated in a pathway-specific manner in response to different stress conditions (Less and Galili, 2008). These results imply that the catabolic genes play major regulatory roles in amino acid metabolism upon exposure to these stresses (Less and Galili, 2008). Interestingly, the Trp and Phe/Tyr branches of the AAA biosynthesis pathway responded differently to UV-B stress. In the Trp biosynthesis pathway, UV-B stress stimulated the expression of the genes encoding both the biosynthesis enzymes and the catabolic enzymes CYP79B2 and CYP79B3. In contrast, this stress did not affect the expression of the genes encoding the biosynthesis enzymes of the Phe/Tyr branch, while it stimulated the expression of only the gene encoding the Tyr catabolism enzyme Tyr-aminotransferase, but not the Phe catabolism enzyme Phe-ammonia lyase (PAL). Interestingly, exposure of Arabidopsis plants to various stresses, including amino acid starvation, as well as to treatments with the oxidative stress-inducing herbicide acifluorfen and the abiotic elicitor alphaamino butyric acid, also induce the expression of genes encoding Trp biosynthesis enzymes (Zhao et al., 1998). Overexpression of members of two clades of Arabidopsis genes, encoding “altered Trp regulation1” [ATR1]-like and MYB28-like transcription factors in transgenic Arabidopsis stimulates the expression of specific genes belonging to both the shikimate and Trp biosynthesis pathways, as well as genes encoding enzymes of Trp-derived secondary metabolites (Malitsky et al., 2008). Similar results were also obtained upon expression of the petunia ODORANT1 gene, encoding a R2R3-type MYB transcription factor in petunia flowers (Colquhoun et al., 2010). Down-regulation of ODORANT1 in transgenic petunia plants strongly reduced the abundance of transcripts and metabolites from the shikimate pathway (Verdonk et al., 2003). A functional homolog of ODORANT1 was not yet been identified in Arabidopsis.

Figure 7.

Post-transcriptional regulation of the shikimate pathway and aromatic amino acid metabolism. Key enzymes and metabolites are shown. Known allosteric regulation by compounds within the pathway is shown, activation with a green arrow, inhibition with a red line and bar, and putative allosteric inhibition with a dashed red line. DAHPS, 3-deoxy-d-arabino-heptulosonate-7-phosphate synthase; ASa, anthranilate synthase alpha subunit; CM, chorismate mutase; PDT, prephenate dehydratase ; ADT, arogenate dehydratase; TyrA, arogenate dehydrogenase.

Post-translational regulation by enzyme feedback-inhibition loops

The activities of DAHPS enzymes (the first enzymatic step of the shikimate pathway; see Fig. 2) from various microorganisms are generally regulated by allosteric feedback inhibition by the different AAA (Byng et al., 1983; Knaggs, 2001). In contrast, there is no published evidence showing that plant DAHPS enzymes are strongly allosterically inhibited in vivo by any of the AAA, and it is generally assumed that DAHPS activity in higher plants is not subject to a major allosteric control (Gilchrist and Kosuge, 1980; Herrmann and Weaver, 1999). Yet, the in vitro activities of DAHPSs from different plant species are weakly inhibited by Trp (Graziana and Boudet, 1980; Rubin and Jensen, 1985) and Tyr (Reinink and Borstap, 1982), or even can also be weakly activated by either Trp or Tyr (Suzich et al., 1984; Pinto et al., 1986) (Fig. 7). The activity of Vigna radiate (bean) DAHPS is weakly inhibited by prephenate and arogenate, the precursor metabolites of Phe and Tyr biosynthesis (Fig. 7) (Rubin and Jensen, 1985), but whether this is due to inhibition of enzyme level or activity is still unknown (Herrmann, 1995). It has also been suggested that the Petroselinum crispum (parsley) DAHPS activity results from several different isoforms, whose activities may be dependent on Mn2+ or Co2+ ions (McCue and Conn, 1989; Gorlach et al., 1993). In addition, the Mn2+-dependent regulation of DAHPS activity by arogenate was proposed as one of the key circuits in the overall pattern of allosteric control for the entire network of the shikimate and AAA biosynthesis (Doong et al., 1992; Doong et al., 1993). All in all, the above results imply that the shikimate pathway in plants is mostly regulated at the gene expression level rather than by post-translational controls.

The Regulation of AAA biosynthesis from chorismate by feedback inhibition loops is primarily associated with: (i) the branch point enzymes AS and CM, which utilize the substrate chorismate; (ii) the branch point enzyme ADT catalyzing the final step in Phe biosynthesis; and (iii) the branch point enzyme TyrA catalyzing the final step of Tyr biosynthesis (Fig. 7). AS, the first enzyme specific for Trp biosynthesis, is feedback-inhibited by Trp (Fig. 7). Arabidopsis trp5 mutants, producing an ASa1 subunit that is insensitive to feedback inhibition by Trp, were isolated in the 1990s either by screening for accumulation of the intermediate metabolite anthranilate (through measuring its fluorescent properties) or by resistance to toxic Trp analogs, such as 6-methyltryptophan (Kreps et al., 1996; Li and Last, 1996). CM, the first specific enzyme for Phe and Tyr biosynthesis, is normally feedback inhibited by Phe and Tyr and induced by Trp (Eberhard et al., 1996) (Fig. 7). To investigate the enzymatic properties of the three Arabidopsis CM isoforms, the Arabidopsis CM1, CM2 or CM3 cDNAs were expressed in yeast (Mobley et al., 1999). The activities of both the CM1 and CM3 isozymes were feedback inhibited by Phe and Tyr, while stimulated by Trp. In contrast, CM2 activity was insensitive to feedback inhibition by any of the AAA (Mobley et al., 1999). The activity of TyrA, the last enzyme of Tyr biosynthesis, is feedback inhibited by Tyr (Fig. 7) in Arabidopsis (Rippert and Matringe, 2002b) and Sorghum bicolor (Connelly and Conn, 1986). In addition, ADT activity from tobacco, spinach, and S. bicolor was shown to be positively regulated by Tyr and negatively regulated by Phe (Jung et al., 1986; Siehl and Conn, 1988). However, the allosteric regulation has not yet been characterized in Arabidopsis plants (Cho et al., 2007). In addition, the rice ADT is negatively regulated by Phe (Yamada et al., 2008), while its potential regulation by Tyr has not yet been elucidated.

Comparison of these feedback regulation loops shows that the flux from chorismate towards Phe and Tyr biosynthesis is generally significantly stronger than the flux towards Trp biosynthesis, and the flux from arogenate towards Phe biosynthesis is significantly stronger than that into Tyr biosynthesis (Rippert et al., 2004) (Fig. 7). This may also reflect the fact that Phe produces a significantly larger variety of secondary metabolites than Tyr and Trp.

The enzymes of the shikimate and AAA biosynthesis pathways are generally synthesized as precursors containing a plastid transit peptide that directs them to the plastid, the organelle in which these two essential pathways operate (Mustafa and Verpoorte, 2005; Weber et al., 2005; Zybailov et al., 2008). However, the intra-cellular localization of two enzymes, CM2 and ADT3, is still under some debate. Sub-cellular fractionation analysis suggested that the tobacco CM2 isozyme is localized in the cytosol (d'Amato et al., 1984), but whether this polypeptide indeed possesses CM activity has not been confirmed. Although in vitro studies showed that AtCM2 possesses CM activity (Eberhard et al., 1993; Eberhard et al., 1996), the physiological significance of AtCM2 still remains questionable (Rippert et al., 2009). In addition, an Arabidopsis polypeptide termed PDT1 (which corresponds to the ADT3 isozyme of Phe biosynthesis, characterized by Cho et al. 2007), was suggested to be a component of the heterotrimeric G-protein complex that is associated with the plasma membrane (Warpeha et al., 2006). This observation is in contrast to a more recent report, using an in situ microscopy analysis, which showed that all of the Arabidopsis ADT isozymes are localized in the plastid (Rippert et al., 2009). Thus, the current dogma is that all ADT isozymes are generally localized to the plastid, although it cannot be ruled out that under specific growth stages or physiological conditions, ADT3 may also be associated with other complexes before it is post-translationally transported into the plastid.

Influence of genetic, metabolic and environmental factors on the regulation of AAA metabolism

Several mutants and transgenic plants with modified shikimate and AAA biosynthesis pathways were used to elucidate the regulation of the biosynthesis of the three AAA. A rice 5-methyl Trp-resistant mutant (Mtr1), apparently encoding a feedback-insensitive PDT/ADT, was shown to over-accumulate Phe and Trp in both callus tissue and leaves (Wakasa and Widholm, 1987; Yamada et al., 2008). Expression of a bacterial PheA* gene, encoding a bifunctional CM/PDT enzyme that is feedback insensitive to Phe, in transgenic Arabidopsis plants, caused: (i) significant increases in the levels of Phe as well as a number of Phe-derived and Tyr-derived secondary metabolites; and (ii) significant decreases of Trp-derived secondary metabolites (Tzin et al., 2009). This implied a regulatory cross-interaction between the biosynthesis fluxes of the three AAA from chorismate, which also influence the rates of their conversion into various secondary metabolites. An Arabidopsis double mutant lacking PAL1 and PAL2 activities has an ∼100-fold increase in Phe and a 4-fold increase in Trp levels (Rohde et al., 2004). This pal1 and pal2 double mutant also influences the transcription of genes associated with the AAA biosynthesis network as well as genes associated phenylpropanoid secondary metabolites (Rohde et al., 2004). Arabidopsis and rice mutants with a feedback-insensitive ASa of Trp biosynthesis generally accumulate Trp, but not Phe or Tyr (Kreps et al., 1996; Li and Last, 1996; Bender and Fink, 1998; Tozawa et al., 2001; Ishihara et al., 2006). Exposure of Arabidopsis seedlings to sulfate starvation triggers an increase in the level of shikimate as well as the Phe and Trp and secondary metabolites derived from them (Nikiforova et al., 2003; Nikiforova et al., 2004; Nikiforova et al., 2006).

CATABOLISM OF THE AROMATIC AMINO ACIDS INTO SECONDARY METABOLITES

Phe catabolism

Phe serves as a precursor for a large family of secondary metabolites. The major group of these secondary metabolites is the phenylpropanoids, whose biosynthesis is initiated by the activity of Phe-ammonia lyase (PAL) (CE 4.3.1.5) (Fig. 8). Arabidopsis possesses four genes encoding the PAL1-PAL4 isozymes (At2g37040, At3g53260, At5g04230 and At3g10340, respectively). The phenylpropanoids possess multiple functions, particularly protecting against various abiotic and biotic stresses, and their production is generally stimulated by such stresses (Dixon and Paiva, 1995; Dixon, 2001; Casati and Walbot, 2005). The transcription of the PAL genes is generally highly regulated by biotic and abiotic stresses, as well as by conditions that demand increased production of the cell wall component lignin in various tissues (Anterola and Lewis, 2002). Genetic mutations that affect the production of PAL generally cause significant alteration in the levels of many phenylpropanoids (Shadle et al., 2003; Rohde et al., 2004). The major sub-groups of phenylpropanoids include the flavonoids, the lignin cell wall components, and the anthocyanins. The metabolite composition of the phenylpropanoids, as well as genes encoding enzymes and regulatory proteins associated with their synthesis, have been recently discussed in several excellent reviews, examples of which are (Weisshaar and Jenkins, 1998; Pichersky and Gang, 2000; D'Auria and Gershenzon, 2005; Boudet, 2007; Vogt, 2010). Some decisive steps in phenylpropanoid biosynthesis were resolved only recently, such as the 2-hydroxylation involved in coumarate biosynthesis (Kai et al., 2008). In addition, genomics approaches revealed new organ-specific pathways, such as the formation of tapetum-specific trisacyl-polyamine conjugates of Arabidopsis flower buds (Alves-Ferreira et al., 2007; Ehlting et al., 2008; Fellenberg et al., 2009; Matsuno et al., 2009). The fine regulation of phenylpropanoid biosynthesis is achieved by combinatorial actions of transcription factors, expressed in a spatially and temporally controlled manner as exemplified in the following reports: (Ramsay and Glover, 2005; Lepiniec et al., 2006; Stracke et al., 2007). A group of volatile compounds, including methylbenzoate, phenylethylacetate and isoeugenol, is also among the phenylpropanoids produced by PAL (Verdonk et al., 2003; Schuurink et al., 2006; Wildermuth, 2006; Ben Zvi et al., 2008).

Figure 8.

Phe catabolism. Only the first enzymes involved in several secondary metabolism pathways derived from Phe are indicated. A putative pathway in Arabidopsis is marked with a dashed grey line. PAL, Phe-ammonia lyase; AADC, aromatic amino acid decarboxylase.

Another class of sulfur-rich Phe-derived secondary metabolites includes the Phe-glucosinolates, whose basic skeleton consists of a b-thioglucose residue, an N-hydroxyiminosulfate moiety and a variable side chain (Reichelt et al., 2002). Phe-glucosinolates are generally not widespread in Arabidopsis, but some Arabidopsis ecotypes do synthesize these compounds, such as phenylethylglucosinolate in the leaves (Mikkelsen et al., 2004) and benzoyloxyglucosinolates in seeds (Kliebenstein et al., 2007). The committing gene in the biosynthesis of Phe-glucosinolates is the cytochrome P450, CYP79A2 (At5g05260), encoding an N-hydroxylase (CE 1.14.13) (Fig. 8) that converts Phe into phenylacetaldoxime, the precursor of benzylglucosinolate (Wittstock and Halkier, 2000).

Some plant species also produce the volatile Phe-derived secondary metabolite 2-phenylethanol (Facchini et al., 2000; Watanabe et al., 2002; Baldwin et al., 2004; Kaminaga et al., 2006; Tieman et al., 2006; Gonda et al., 2010). However, 2-phenylethanol is produced in flowers and/or fruits of specific plants, such as petunia, rose and tomato, and so far this volatile has not been detected in Arabidopsis.

Tyr catabolism

Tyr serves as a precursor of several families of secondary metabolites, including tocochromanols (vitamin E), plastoquinones, isoquinoline alkaloids and non-protein amino acids, and it has also been speculated that Tyr may also lead to the production of some phenylpropanoids (Fig. 9). The tocochromanols, which include both tocopherols and tocotrienols, are essential antioxidants in the diets of human and farm animals (Schneider, 2005; Della-Penna and Pogson, 2006; Mene-Saffrane and Dellapenna, 2009). The first committed enzyme of tocochromanols biosynthesis from Tyr is Tyr-aminotransferase (CE 2.6.1.5) (At5g53970) (Lopukhina et al., 2001), which produces p-hydroxyPPY (Fig. 9) (Norris et al., 1995; Garcia et al., 1999). It has been suggested that p-hydroxyPPY can also be synthesized from prephenate via an alternative biosynthesis pathway (Fig. 5) (Rippert and Matringe, 2002b; Rippert et al., 2004). If such a pathway indeed naturally exists, then p-hydroxyPPY can also be used for tocochromanols biosynthesis, bypassing Tyr (Fig. 5).

The Tyr catabolism pathway also produces isoquinoline alkaloids, which represent a large, diverse group of natural products found in ∼20% of all plant species (Facchini et al., 2004). In Arabidopsis, Tyr is also catabolized into tyramine by Tyr/L-dopa decarboxylase (TYDC) (EC 4.1.1.25), which is encoded by two genes (At2g20340, At4g28680). Tyramine is a precursor for benzyl-isoquinoline alkaloids, as well as cell wall-bound hydroxycinnamic acid amides (Facchini et al., 2000). It has been suggested that tyramine in involved in the Arabidopsis defense response (Trezzini et al., 1993).

Figure 9.

Tyr catabolism. Only the first enzymes involved in several secondary metabolism pathways derived from Tyr are indicated. Putative pathways in Arabidopsis are marked with dashed grey lines TyrAT, Tyr-aminotransferase; TYDC, Tyr/L-dopa decarboxylase; PDH, prephenate dehydrogenase; TAL, Tyr-ammonia lyase.

Figure 10.

Trp catabolism. Only the first enzymes involved in several secondary metabolism pathways derived from Trp are indicated. The numbers within the Trp catabolism pathway indicate: 1) the indole-3-acetaldoxime (IAOx) pathway catalyzed by two cytochrome P450s (CYP79B2 and CYP79B3); 2) the tryptamine (YUCCA) pathway catalyzed by Trp decarboxylase (TDC); 3) the indole-3-pyruvate (IPyA) pathway catalyzed by Trp aminotransferase (TAA); and 4) the indoleacetamide (IAM) pathway which initiates directly from Trp via either IAOx or indole-3-acetonitrile (IAN).

Even though phenylpropanoids are classically synthesized from Phe, it has also been proven that in several plant species the second metabolite of the phenylpropanoid pathway, namely coumarate, can also be synthesized directly from Tyr by Tyr ammonia-lyase (TAL) (EC 4.3.1.) (Neish, 1961; Beaudoin-Eagan and Thorpe, 1985; Guerra et al., 1985; Rosler et al., 1997; Khan et al., 2003; MacDonald and D'Cunha, 2007). All four isoforms of Arabidopsis PAL, the first enzyme of phenylpropanoid biosynthesis from Phe (Fig. 8), exhibit higher affinity for Phe than for Tyr (Cochrane et al., 2004). However, a point mutation in the Arabidopsis gene encoding the PAL1 isoform resulted in a lower PAL activity and a compensatory increase in TAL activity (Watts et al., 2006), supporting the potential use of TAL in the phenylpropanoid biosynthesis pathway.

Trp catabolism

Trp is catabolized into many indole-containing secondary metabolites, such as indole-3-acetic acid (IAA, auxin) (Ostin et al., 1998; Davies, 2004), indole glucosinolates (Halkier, 1999), phytoalexins (Pedras et al., 2000), terpenoid indole alkaloids (De Luca and St Pierre, 2000; Facchini et al., 2004), and tryptamine derivatives (Facchini et al., 2000) (Fig. 10). Auxins are some of the key metabolites synthesized from Trp. However, the biosynthetic pathway(s) leading to IAA, the main auxin metabolite, are not well understood. Although there is good evidence that IAA is synthesized from Trp (Gibson et al., 1972; Wright et al., 1991; Tsurusaki et al., 1997), several different routes of IAA biosynthesis from Trp have been proposed (Fig. 10) (Strader and Bartel, 2008; Quittenden et al., 2009). These include: 1) the indole-3-acetaldoxime (IAOx) pathway catalyzed by two cytochrome P450s (CE 1.14.13) (CYP79B2 and CYP79B3; At4g39950 and At2g22330) (Hull et al., 2000; Bartel et al., 2001); 2) the tryptamine (YUCCA) pathway catalyzed by Trp decarboxylase (TDC) (CE 4.1.1.28) (Facchini et al., 2000; Quittenden et al., 2009); 3) the indole-3-pyruvate (IPyA) pathway catalyzed by Trp aminotransferase (TAA)(CE 2.6.1.1) (At1g70560) (Stepanova et al., 2008; Tao et al., 2008); and 4) the indoleacetamide (IAM) pathway which initiates directly from Trp via either IAOx or indole-3-acetonitrile (IAN) (Pollmann et al., 2002). In addition, a possible additional, Trp-independent pathway of IAA biosynthesis directly from indole has been proposed (Normanly et al., 1993; Radwanski et al., 1996).

Table 1.

Arabidopsis thaliana genetic loci and enzyme activities mentioned in this review.

continued

Another important group of secondary metabolites derived from Trp includes the glucosinolates, which are amino acid-derived natural plant products containing a thio-Glc moiety and a sulfonate moiety bound to an oxime function (Halkier and Gershenzon, 2006). They are implicated in plant-insect and plant-pathogen interactions, and also recently attracted attention as cancer-preventive agents in humans (Halkier, 1999). Glucosinolates are found almost exclusively in the Brassicales and have been widely studied in Arabidopsis and in other species of the Brassicaceae family (Rask et al., 2000; Reichelt et al., 2002; Yatusevich et al., 2009). The IAOx, described above is also channeled by the oxime-metabolizing CYP83B1 enzyme into the biosynthetic pathway of indole glucosinolates (Naur et al., 2003).

The Trp catabolic pathway also synthesizes camalexin, the major indolic phytoalexin in Arabidopsis accumulating upon infection with plant pathogens and abiotic elicitors (Zhao and Last, 1996; Bottcher et al., 2009). Camalexin originates from IAOx (Fig. 10) (Hull et al., 2000; Mikkelsen et al., 2000; Zhao et al., 2002). In addition, the Trp catabolic pathway also leads to the synthesis of indole alkaloids via tryptamine (Fig. 10). One example of the Trp-derived indole alkaloids is vindoline, an important metabolite in human health (Facchini et al., 2000; Facchini et al., 2004; Malitsky et al., 2008; Sugawara et al., 2009). However, indole alkaloids are generally not found in Arabidopsis.

FUTURE PROSPECTS

The entire set of genes and enzymes associated with the shikimate pathway have been elucidated (Table 1). However, elucidation of the regulation of this pathway is still in its infancy, requiring future studies. Even though, there were significant discoveries associated with genes and enzymes of the biosynthesis of the AAA in recent years, there are still missing links and debates about some key regulatory steps The major route of Phe biosynthesis occurs through arogenate, but gene(s) encoding prephenate aminotransferase have yet to be identified. In addition, due to the fact that some plant arogenate dehydratase isozymes also possess residual prephenate dehydrate activities, as well as the observation that plants apparently possess aminotransferase activity that can convert PPY into Phe, one cannot rule out a minor contribution of a bacterial-like PPY route to Phe biosynthesis in plants. In addition, future studies should identify whether arogenate is the precursor for Tyr biosynthesis or whether an alternative bacterial-like route of Try biosynthesis via p-hyroxyPPY also exists. The regulation of the flux balance in the conversion of chorismate into Trp and Phe/Tyr has already been extensively studied. Yet, the flux balance regulating the conversion of arogenate into either Phe or Tyr is still unknown, requiring future studies. Although relatively old studies suggest the presence of several enzyme feedback inhibition loops within the AAA biosynthesis pathway, some studies provide clues for additional ones (Fig. 7), which require future confirmation. Finally, a number of transcription factors have been proven to control different steps in the biosynthesis of AAA and secondary metabolites derived from them. Yet, it is likely that these do not represent the full set and additional studies are required to address this issue. Interestingly, some transcription factors regulate genes encoding both primary and secondary metabolism associated with the AAA, and an exciting prospect for future research would to test whether the primary metabolism enzymes regulated by these transcription factors represent key regulatory enzymes connecting primary and secondary metabolism.

REFERENCES

1.

M. Alves-Ferreira , F. Wellmer , A. Banhara , V. Kumar , J. Riechmann , and E. Meyerowitz (2007). Global expression profiling applied to the analysis of Arabidopsis stamen development. Plant Physiol. 145: 81747–762. Google Scholar

2.

A. Anterola , and N. Lewis (2002). Trends in lignin modification: a comprehensive analysis of the effects of genetic manipulations/mutations on lignification and vascular integrit. Phytochem. 61: 81221–294. Google Scholar

3.

E. Baldwin , K. Goodner , A. Plotto , K. Pritchett , and M. Einstein (2004). Effect of volatiles and their concentration on perception of tomato descriptors. J. Food Science 69: 81310–318. Google Scholar

4.

L. Bartee , and J. Bender (2001). Two Arabidopsis methylation-deficiency mutations confer only partial effects on a methylated endogenous gene family. Nucleic Acids Res. 29: 812127–2134. Google Scholar

5.

B. Bartel (1997). Auxin biosynthesis. Annual Review of Plant Physiology and Plant Mol. Biol. 48: 8151–66. Google Scholar

6.

B. Bartel , S. LeClere , M. Magidin , and BK. Zolman . (2001). Inputs to the active indole-3-acetic acid pool: de novo synthesis, conjugate hydrolysis, and indole-3-butyric acid β-oxidation. J. Plant Growth Regul. 20: 81198–216. Google Scholar

7.

G. Basset , E. Quinlivan , S. Ravanel , F. Rebeille , B. Nichols , K. Shinozaki , M. Seki , L. Adams-Phillips , J. Giovannoni , J. Gregory , and A. Hanson (2004). Folate synthesis in plants: the p-aminobenzoate branch is initiated by a bifunctional PabA-PabB protein that is targeted to plastids. Proc. Natl. Acad. Sci. USA. 101: 811496–1501. Google Scholar

8.

L.D. Beaudoin-Eagan , and T.A. Thorpe (1985). Tyrosine and phenylalanine ammonia lyase activities during shoot initiation in tobacco callus cultures. Plant Physiol. 78: 81438–441. Google Scholar

9.

M.M. Ben Zvi , F. Negre-Zakharov , T. Masci , M. Ovadis , E. Shklarman , H. Ben-Meir , T. Tzfira , N. Dudareva , and A. Vainstein (2008). Interlinking showy traits: co-engineering of scent and colour biosynthesis in flowers. Plant Biotechnol. J. 6: 81403–415. Google Scholar

10.

J. Bender , and G.R. Fink (1995). Epigenetic control of an endogenous gene family is revealed by a novel blue fluorescent mutant of Arabidopsis. Cell. 83: 81725–734. Google Scholar

11.

J. Bender , and G.R. Fink (1998). A Myb homologue, ATR1, activates tryptophan gene expression in Arabidopsis. Proc. Natl. Acad. Sci. USA 95: 815655–5660. Google Scholar

12.

G.A. Betz , E. Gerstner , S. Stich , B. Winkler , G. Welzl , E. Kremmer , C. Langebartels , W. Heller , H. Sandermann , and D. Ernst (2009). Ozone affects shikimate pathway genes and secondary metabolites in saplings of European beech (Fagus sylvatica L.) grown under greenhouse conditions. Trees-Structure And Function. 23: 81539–553. Google Scholar

13.

M. Bischoff , J. Rösler , H. Raesecke , J. Görlach , N. Amrhein , and J. Schmid (1996). Cloning of a cDNA encoding a 3-dehydroquinate synthase from a higher plant, and analysis of the organ-specific and elicitor-induced expression of the corresponding gene. Plant. Mol. Biol. 31: 8169–76. Google Scholar

14.

M. Bischoff , A. Schaller , F. Bieri , F. Kessler , N. Amrhein , and J. Schmid (2001) Molecular characterization of tomato 3-dehydroquinate dehydratase-shikimate:NADP oxidoreductase. Plant Physiol. 125, 811891–1900. Google Scholar

15.

J. Bohlmann , V. DeLuca , U. Eilert , and W. Martin (1995). Purification and cDNA cloning of anthranilate synthase from Ruta graveolens: modes of expression and properties of native and recombinant enzymes. Plant J. 7: 81491–501. Google Scholar

16.

C.A. Bonner , and R.A. Jensen (1994). Cloning of cDNA encoding the bifunctional dehydroquinase.shikimate dehydrogenase of aromaticamino-acid biosynthesis in Nicotiana tabacum. Biochem. J. 302: 8111–14. Google Scholar

17.

C. Bottcher , L. Westphal , C. Schmotz , E. Prade , D. Scheel , and E. Glawischnig (2009). The multifunctional enzyme CYP71B15 (PHYTOALEXIN DEFICIENT3) converts cysteine-indole-3-acetonitrile to camalexin in the indole-3-acetonitrile metabolic network of Arabidopsis thaliana. Plant Cell. 21: 811830–1845. Google Scholar

18.

A. Boudet (2007). Evolution and current status of phenolic compounds. Phytochem. 68: 812722–2735. Google Scholar

19.

G.S. Byng , R.J. Whitaker , C. Flick , and R.A. Jensen (1981). Enzymology of L-Tyrosine biosynthesis in corn (Zea mays). Phytochem. 20: 811289–1292. Google Scholar

20.

G.S. Byng , J.L. Johnson , R.J. Whitaker , R.L. Gherna , and R.A. Jensen (1983). The evolutionary pattern of aromatic amino acid biosynthesis and the emerging phylogeny of pseudomonad bacteria. J. Mol. Evol. 19: 81272–282. Google Scholar

21.

P. Casati , and V. Walbot (2005). Differential accumulation of maysin and rhamnosylisoorientin in leaves of high-altitude landraces of maize after UV-B exposure. Plant Cell Environ. 28: 81788–799. Google Scholar

22.

R. Catala , J. Ouyang , I.A. Abreu , Y. Hu , H. Seo , X. Zhang , and N.H. Chua (2007). The Arabidopsis E3 SUMO ligase SIZ1 regulates plant growth and drought responses. Plant Cell. 19: 812952–2966. Google Scholar

23.

K. Chibani , S. Ali-Rachedi , C. Job , D. Job , M. Jullien , and P. Grappin (2006). Proteomic analysis of seed dormancy in Arabidopsis. Plant Physiol. 142: 811493–1510. Google Scholar

24.

M. Cho , O. Corea , H. Yang , D. Bedgar , D. Laskar , A. Anterola , F. Moog-Anterola , R. Hood , S. Kohalmi , M. Bernards , C. Kang , L. Davin , and N. Lewis (2007). Phenylalanine biosynthesis in Arabidopsis thaliana identification and characterization of Arogenate dehydratases. J. Biol. Chem. 282: 8130827–30835. Google Scholar

25.

F.C. Cochrane , L.B. Davin , and N.G. Lewis (2004). The Arabidopsis phenylalanine ammonia lyase gene family: kinetic characterization of the four PAL isoforms. Phytochem. 65: 811557–1564. Google Scholar

26.

T.A. Colquhoun , J.C. Verdonk , B.C. Schimmel , D.M. Tieman , B.A. Underwood , and D.G. Clark (2010). Petunia floral volatile benzenoid/phenylpropanoid genes are regulated in a similar manner. Phytochem. 71: 81158–167. Google Scholar

27.

J.A. Connelly , and E.E. Conn (1986).Tyrosine biosynthesis in Sorghum bicolor: isolation and regulatory properties of arogenate dehydrogenase. Z. Naturforsch. 41: 8169–78. Google Scholar

28.

T.A. d'Amato , R.J. Ganson , C.G. Gaines , and R.A. Jensen (1984). Subcellular localization of chorismate-mutase isoenzymes in protoplasts from mesophyll and suspension-cultured cells of Nicotiana silvestris Planta. 162: 81104–108. Google Scholar

29.

J. D'Auria , and J. Gershenzon (2005). The secondary metabolism of Arabidopsis thaliana: growing like a weed. Curr. Opin. Plant Biol. 8: 81308– 316. Google Scholar

30.

P. Davies (2004). Plant hormones - biosynthesis, signal transduction, action! pgs. 8136–62. (Kluwer Academic Publishers, Netherlands). Google Scholar

31.

V. De Luca , and B. St Pierre (2000). The cell and developmental biology of alkaloid biosynthesis. Trends Plant Sci. 5: 81168–173. Google Scholar

32.

W. De-Eknamkul , and B.E. Ellis (1988). Purification and characterization of prephenate aminotransferase from Anchusa officinalis cell cultures. Arch. Biochem. Biophys. 267: 8187–94. Google Scholar

33.

D. DellaPenna , and B. Pogson (2006). Vitamin synthesis in plants: tocopherols and carotenoids. Annu. Rev. Plant Biol. 57: 81711–738. Google Scholar

34.

A. Devoto , C. Ellis , A. Magusin , H. Chang , C. Chilcott , T. Zhu , and J. Turner (2005). Expression profiling reveals COI1 to be a key regulator of genes involved in wound- and methyl jasmonate-induced secondary metabolism, defence, and hormone interactions Plant Mol. Biol. 58: 81497–513. Google Scholar

35.

L. Ding , D. Hofius , M.R. Hajirezaei , A.R. Fernie , F. Bornke , and U. Sonnewald (2007). Functional analysis of the essential bifunctional tobacco enzyme 3-dehydroquinate dehydratase/shikimate dehydrogenase in transgenic tobacco plants. J. Exp. Bot. 58: 812053–2067. Google Scholar

36.

R. Dixon , and N. Paiva (1995). Stress-induced phenylpropanoid metabolism. Plant Cell. 17: 811085–1097. Google Scholar

37.

R.A. Dixon (2001). Natural products and plant disease resistance. Nature. 411: 81843–847. Google Scholar

38.

B. Dombrecht , G.P. Xue , S.J. Sprague , J.A. Kirkegaard , J.J. Ross , J.B. Reid , G.P. Fitt , N. Sewelam , P.M. Schenk , J.M. Manners , and K. Kazan (2007). MYC2 differentially modulates diverse jasmonate-dependent functions in Arabidopsis. Plant Cell. 19: 812225–2245. Google Scholar

39.

R. Doong , R. Ganson , and R. Jensen (1993). Plastid-localized 3-deoxy-d-arabino-heptulosonate 7-phosphate synthase (DS-Mn): the early-pathway target of sequential feedback inhibition in higher plants. Plant, Cell Environ. 16: 81393–402. Google Scholar

40.

R. Doong , J. Gander , R. Ganson , and R. Jensen (1992).The cytosolic isoenzyme of 3-deoxy-o-arabino-heptulosonate 7-phosphate synthase in Spinacia oleracea and other higher plants: Extreme substrate ambiguity and other properties. Plant Physiol. 84: 81351–360. Google Scholar

41.

S.O. Duke , and S.B. Powles (2008). Glyphosate: a once-in-a-century herbicide. Pest Manag. Sci. 64: 81319–325. Google Scholar

42.

J. Eberhard , H.R. Raesecke , J. Schmid , and N. Amrhein (1993). Cloning and expression in yeast of a higher plant chorismate mutase. Molecular cloning, sequencing of the cDNA and characterization of the Arabidopsis thaliana enzyme expressed in yeast. FEBS Lett. 334: 81233– 236. Google Scholar

43.

J. Eberhard , T.T. Ehrler , P. Epple , G. Felix , H.R. Raesecke , N. Amrhein , and J. Schmid (1996). Cytosolic and plastidic chorismate mutase isozymes from Arabidopsis thaliana: molecular characterization and enzymatic properties. Plant J. 10: 81815–821. Google Scholar

44.

J. Ehlting , V. Sauveplane , A. Olry , J. Ginglinger , N. Provart , and D. Werck-Reichhart (2008). An extensive (co-)expression analysis tool for the cytochrome P450 superfamily in Arabidopsis thaliana.BMC Plant Biol. 8: 811–19. Google Scholar

45.

J. Ehlting , N. Mattheus , D.S. Aeschliman , E. Li , B. Hamberger , I.F. Cullis , J. Zhuang , M. Kaneda , S.D. Mansfield , L. Samuels , K. Ritland , B.E. Ellis , J. Bohlmann , and C.J. Douglas (2005). Global transcript profiling of primary stems from Arabidopsis thaliana identifies candidate genes for missing links in lignin biosynthesis and transcriptional regulators of fiber differentiation. Plant J. 42: 81618–640. Google Scholar

46.

R. Entus , M. Poling , and K.M. Herrmann (2002). Redox regulation of Arabidopsis 3-deoxy-d-arabino-heptulosonate 7-phosphate synthase. Plant Physiol. 129: 811866–1871. Google Scholar

47.

P.J. Facchini , K.L. Huber-Allanach , and L.W. Tari (2000). Plant aromatic L-amino acid decarboxylases: evolution, biochemistry, regulation, and metabolic engineering applications. Phytochem. 54: 81121–138. Google Scholar

48.

P.J. Facchini , D.A. Bird , and B. St-Pierre (2004). Can Arabidopsis make complex alkaloids? Trends Plant Sci. 9: 81116–122. Google Scholar

49.

C. Fellenberg , C. Bottcher , and T. Vogt (2009). Phenylpropanoid polyamine conjugate biosynthesis in Arabidopsis thaliana flower buds. Phytochem. 70: 811392–1400. Google Scholar

50.

S. Ferrari , R. Galletti , C. Denoux , G. Lorenzo , F. Ausubel , and J. Dewdney (2007). Resistance to Botrytis cinerea induced in Arabidopsis by elicitors is independent of salicylic Acid, ethylene, or aasmonate signaling but requires PHYTOALEXIN DEFICIENT3. Plant Physiol. 144: 81367–379. Google Scholar

51.

G. Fucile , S. Falconer , and D. Christendat (2008). Evolutionary diversification of plant shikimate kinase gene duplicates. PLoS Genet. 4: 81e1000292. Google Scholar

52.

C.G. Gaines , G.S. Byng , R.J. Whitaker , and R.A. Jensen (1982). L-Tyrosine regulation and biosynthesis via arogenate dehydrogenase in suspension-cultured cells of Nicotiana silvestris Speg. et Comes Planta. 156: 81233–240. Google Scholar

53.

G. Galili , S. Galili , E. Lewinsohn , and Y. Tadmor (2002). Genetic, molecular and genomic approaches to improve the value of plant foods and feeds. Crit. Rev. Plant Sci. 21: 81167–204. Google Scholar

54.

I. Garcia , M. Rodgers , R. Pepin , T. Hssich , and M. Matringe (1999). Characterization and subcellular compartmentation of recombinant 4-hydroxyphenylpyruvate dioxygenase from Arabidopsis in transgenic tobacco. Plant Physiol. 119: 811507–1516. Google Scholar

55.

C. Garcion , A. Lohmann , E. Lamodiere , J. Catinot , A. Buchala , P. Doermann , and J.P. Metraux (2008). Characterization and biological function of the ISOCHORISMATE SYNTHASE2 gene of Arabidopsis. Plant Physiol. 147: 811279–1287. Google Scholar

56.

R. Gibson , E. Schneider , and F. Wightman (1972). Biosynthesis and metabolism of indol-3yl-acetic acid. II. In vivo experiments with 14C-labelled precursors of IAA in tomato and barley shoots. J. Exp. Bot. 23: 81381–399. Google Scholar

57.

D. Gilchrist , and T. Kosuge (1980). Aromatic amino acid biosynthesis and its regulation. In BN Miflin , ed, the Biochemistry of Plants, Academic Press, New York. 5: 81507–531. Google Scholar

58.

I. Gonda , E. Bar , V. Portnoy , S. Lev , J. Burger , A.A. Schaffer , Y. Tadmor , S. Gepstein , J.J. Giovannoni , N. Katzir , and E. Lewinsohn (2010). Branched-chain and aromatic amino acid catabolism into aroma volatiles in Cucumis melo L. fruit. J. Exp. Bot 61: 811111–1123. Google Scholar

59.

J. Gorlach , J. Schmid , and N. Amrhein (1993). Differential expression of tomato (Lycopersicon esculentum L.) genes encoding shikimate pathway isoenzymes. II. Chorismate synthase. Plant Mol. Biol. 23: 81707–716. Google Scholar

60.

J. Gorlach , H.R. Raesecke , D. Rentsch , M. Regenass , P. Roy , M. Zala , C. Keel , T. Boller , N. Amrhein , and J. Schmid (1995). Temporally distinct accumulation of transcripts encoding enzymes of the prechorismate pathway in elicitor-treated, cultured tomato cells. Proc. Natl. Acad. Sci. USA 92: 813166–3170. Google Scholar

61.

A. Graziana , and A. Boudet (1980). 3-Deoxy-d-arabino-heptulosonate 7-phosphate synthase from Zea mays: general properties and regulation by tryptophan. Plant Cell Physiol. 21: 81793–802. Google Scholar

62.

J. Gross , W.K. Cho , L. Lezhneva , J. Falk , K. Krupinska , K. Shinozaki , M. Seki , R.G. Herrmann , and J. Meurer (2006). A plant locus essential for phylloquinone (vitamin K1) biosynthesis originated from a fusion of four eubacterial genes. J. Biol. Chem. 281: 8117189–17196. Google Scholar

63.

D. Guerra , A.J. Anderson , and F.B. Salisbury (1985). Reduced phenylalanine ammonia-lyase and tyrosine ammonia-lyase activities and lignin synthesis in wheat grown under low pressure sodium lamps. Plant Physiol. 78: 81126–130. Google Scholar

64.

B. Halkier (1999). Glucosinolates. (New York: John Wiley & Sons Ltd.). Google Scholar

65.

B.A. Halkier , and J. Gershenzon (2006). Biology and biochemistry of glucosinolates. Annu Rev Plant Biol. 57: 81303–333. Google Scholar

66.

Y. He , and J. Li (2001). Differential expression of triplicate phosphoribo-sylanthranilate isomerase isogenes in the tryptophan biosynthetic pathway of Arabidopsis thaliana (L.) Heynh. Planta. 212: 81641–647. Google Scholar

67.

M.L. Healy-Fried , T. Funke , M.A. Priestman , H. Han , and E. Schonbrunn (2007). Structural basis of glyphosate tolerance resulting from mutations of Pro101 in Escherichia coli 5-enolpyruvylshikimate-3-phosphate synthase. J. Biol. Chem. 282: 8132949–32955. Google Scholar

68.

K.M. Herrmann (1995). The shikimate pathway early steps in the biosynthesis of aromatic compounds. Plant Cell. 7: 81907–919. Google Scholar

69.

K.M. Herrmann , and L.M. Weaver (1999). The shikimate pathway. Annu Rev Plant Physiol. Plant Mol. Biol. 50: 81473–503. Google Scholar

70.

E.H. Hughes , S.B. Hong , S.I. Gibson , J.V. Shanks , and K.Y. San (2004). Metabolic engineering of the indole pathway in Catharanthus roseus hairy roots and increased accumulation of tryptamine and serpentine. Metab. Eng. 6: 81268–276. Google Scholar

71.

A. Hull , R. Vij , and J. Celenza (2000). Arabidopsis cytochrome P450s that catalyze the first step of tryptophan-dependent indole-3-acetic acid biosynthesis. Proc. Natl. Acad. Sci. USA 97: 812379–2384. Google Scholar

72.

A. Ishihara , Y. Asada , Y. Takahashi , N. Yabe , Y. Komeda , T. Nishioka , H. Miyagawa , and K. Wakasa (2006). Metabolic changes in Arabidopsis thaliana expressing the feedback-resistant anthranilate synthase alpha subunit gene OASA1D. Phytochem. 67: 812349–2362. Google Scholar

73.

I. Janzik , S. Preiskowski , and H. Kneifel (2005). Ozone has dramatic effects on the regulation of the prechorismate pathway in tobacco (Nicotiana tabacum L. cv. Bel. W3. Planta. 223: 8120–27. Google Scholar

74.

C. Job , L. Rajjou , Y. Lovigny , M. Belghazi , and D. Job (2005). Patterns of protein oxidation in Arabidopsis seeds and during germination Plant Physiol. 138: 81790–802. Google Scholar

75.

E. Jung , L.O. Zamir , and R.A. Jensen (1986). Chloroplasts of higher plants synthesize L-phenylalanine via L-arogenate. Proc. Natl. Acad. Sci. USA 83: 817231–7235. Google Scholar

76.

K. Kai , M. Mizutani , N. Kawamura , R. Yamamoto , M. Tamai , H. Yamaguchi , K. Skata , and B. Shimizu (2008). Scopoletin is biosynthesized via ortho-hydroxylation of feruloyl CoA by a 2-oxolutarate-dependent dioxygenase in Arabidopsis thaliana. Plant J. 55: 81989–999. Google Scholar

77.

Y. Kaminaga , J. Schnepp , G. Peel , C.M. Kish , G. Ben-Nissan , D. Weiss , I. Orlova , O. Lavie , D. Rhodes , K. Wood , D.M. Porterfield , A.J. Cooper , J.V. Schloss , E. Pichersky , A. Vainstein , and N. Dudareva (2006). Plant phenylacetaldehyde synthase is a bifunctional homotetrameric enzyme that catalyzes phenylalanine decarboxylation and oxidation. J. Biol. Chem. 281: 8123357–23366. Google Scholar

78.

K. Kasai , T. Kanno , M. Akita , Y. Ikejiri-Kanno , K. Wakasa , and T. Y (2005). Identification of three shikimate kinase genes in rice characterization of their differential expression during panicle development and of the enzymatic activities of the encoded proteins. Planta 222: 81438–447. Google Scholar

79.

B. Keith , X.N. Dong , F.M. Ausubel , and G.R. Fink (1991). Differential induction of 3-deoxy-d-arabino-heptulosonate 7-phosphate synthase genes in Arabidopsis thaliana by wounding and pathogenic attack. Proc. Natl. Acad. Sci. USA. 88: 818821–8825. Google Scholar

80.

W. Khan , B. Prithiviraj , and D.L. Smith (2003). Chitosan and chitin oligomers increase phenylalanine ammonia-lyase and tyrosine ammonia-lyase activities in soybean leaves. J. Plant Physiol. 160: 81859–863. Google Scholar

81.

J. Kilian , D. Whitehead , J. Horak , D. Wanke , S. Weinl , O. Batistic , C. D'Angelo , E. Bornberg-Bauer , J. Kudla , and K. Harter (2007). The AtGenExpress global stress expression data set: protocols, evaluation and model data analysis of UV-B light, drought and cold stress responses. Plant J. 50: 81347–363. Google Scholar

82.

H. Kim , C. van Oostende , G. Basset , and J. Browse (2008). The AAE14 gene encodes the Arabidopsis o-succinylbenzoyl-CoA ligase that is essential for phylloquinone synthesis and photosystem-I function. Plant J. 54: 81272–283. Google Scholar

83.

H.J. Klee , Y.M. Muskopf , and C.S. Gasser (1987). Cloning of an Arabidopsis thaliana gene encoding 5-enolpyruvylshikimate-3-phosphate synthase: sequence analysis and manipulation to obtain glyphosatetolerant plants. Mol. Gen. Genet. 210: 81437–442. Google Scholar

84.

D.J. Kliebenstein , J.C. D'Auria , A.S. Behere , J.H. Kim , K.L. Gunderson , J.N. Breen , G. Lee , J. Gershenzon , R.L. Last , and G. Jander (2007). Characterization of seed-specific benzoyloxyglucosinolate mutations in Arabidopsis thaliana. Plant J. 51: 811062–1076. Google Scholar

85.

A.R. Knaggs (2001). The biosynthesis of shikimate metabolites. Nat. Prod. Rep. 18: 81334–355. Google Scholar

86.

J.A. Kreps , T. Ponappa , W. Dong , and C.D. Town (1996). Molecular basis of alpha-methyltryptophan resistance in amt-1, a mutant of Arabidopsis thaliana with altered tryptophan metabolism. Plant Physiol. 110, 811159–1165. Google Scholar

87.

V. Kriechbaumer , L. Weigang , A. Fiesselmann , T. Letzel , M. Frey , A. Gierl , and E. Glawischnig (2008). Characterisation of the tryptophan synthase alpha subunit in maize. BMC Plant Biol. 8: 8144. Google Scholar

88.

R. Last , P. Bissinger , D. Mahoney , E. Radwanski , and G. Fink (1991). Tryptophan mutants in Arabidopsis: the consequences of duplicated tryptophan synthase beta genes. Plant Cell. 3: 81345–358. Google Scholar

89.

N. Leonhardt , J.M. Kwak , N. Robert , D. Waner , G. Leonhardt , and J.I. Schroeder (2004). Microarray expression analyses of Arabidopsis guard cells and isolation of a recessive abscisic acid hypersensitive protein phosphatase 2C mutant. Plant Cell. 16: 81596–615. Google Scholar

90.

L. Lepiniec , I. Debeaujon , J.M. Routaboul , A. Baudry , L. Pourcel , N. Nesi , and M. Caboche (2006). Genetics and biochemistry of seed flavonoids. Annu. Rev. Plant Biol. 57: 81405–430. Google Scholar

91.

H. Less , and G. Galili (2008). Principal transcriptional programs regulating plant amino acid metabolism in response to abiotic stresses. Plant Physiol. 147: 81316–330. Google Scholar

92.

J. Li , and R.L. Last (1996). The Arabidopsis thaliana trp5 mutant has a feedback-resistant anthranilate synthase and elevated soluble tryptophan. Plant Physiol. 110: 8151–59. Google Scholar

93.

J. Li , S. Chen , L. Zhu , and R.L. Last (1995a). Isolation of cDNAs encoding the tryptophan pathway enzyme indole-3-glycerol phosphate synthase from Arabidopsis thaliana. Plant Physiol. 108: 81877–878. Google Scholar

94.

J. Li , J. Zhao , A. Rose , R. Schmidt , and R. Last (1995b). Arabidopsis thaliana phosphoribosylanthranilate isomerase: molecular genetic analysis of triplicate tryptophan pathway genes. Plant Cell. 7; 81447–461. Google Scholar

95.

A. Lopukhina , M. Dettenberg , E. Weiler , and H. Hollander-Czytko (2001). Cloning and characterization of a coronatine-regulated tyrosine aminotransferase from Arabidopsis. Plant Physiol. 126: 811678–1687. Google Scholar

96.

M.J. MacDonald , and G.B. D'Cunha (2007). A modern view of phenylalanine ammonia lyase. Biochem Cell Biol. 85: 81273–282. Google Scholar

97.

P. Macheroux , J. Schmid , N. Amrhein , and A. Schaller (1999). A unique reaction in a common pathway mechanism and function of chorismate synthase in the shikimate pathway. Planta. 207: 81325–334. Google Scholar

98.

H. Maeda , A.K. Shasany , J. Schnepp , I. Orlova , G. Taguchi , B.R. Cooper , D. Rhodes , E. Pichersky , and N. Dudareva (2010). RNAi suppression of arogenate dehydratase1 reveals that phenylalanine is synthesized predominantly via the arogenate pathway in petunia petals. Plant Cell. (In Press). Google Scholar

99.

S. Malitsky , E. Blum , H. Less , I. Venger , M. Elbaz , S. Morin , Y. Eshed , and A. Aharoni (2008). The transcript and metabolite networks affected by the two clades of Arabidopsis glucosinolate biosynthesis regulators. Plant Physiol. 148: 812021–2049. Google Scholar

100.

M. Matsuno , V. Compagnon , G.A. Schoch , M. Schmitt , D. Debayle , J.E. Bassard , B. Pollet , A. Hehn , D. Heintz , P. Ullmann , C. Lapierre , F. Bernier , J. Ehlting , and D. Werck-Reichhart (2009). Evolution of a novel phenolic pathway for pollen development. Sci 325: 811688–1692. Google Scholar

101.

K. McCue , and E. Conn (1989). Induction of 3-deoxy-arabino-beptulosonate 7-pbosphate syntbase activity by fungal elicitor in cultures of Petroselinum crispum. Proe. Natl. Acad. Sci. 86: 817374–7377. Google Scholar

102.

S. Melquist , and J. Bender (2003). Transcription from an upstream promoter controls methylation signaling from an inverted repeat of endogenous genes in Arabidopsis. Genes Dev. 17: 812036–2047. Google Scholar

103.

S. Melquist , B. Luff , and J. Bender (1999). Arabidopsis PAI gene arrangements, cytosine methylation and expression. Genetics 153: 81401–413. Google Scholar

104.

L. Mene-Saffrane , and D. Dellapenna (2009). Biosynthesis, regulation and functions of tocochromanols in plants. Plant Physiol. Biochem. (In Press). Google Scholar

105.

M. Mikkelsen , C. Hansen , U. Wittstock , and B. Halkier (2000). Cytochrome P450 CYP79B2 from Arabidopsis catalyzes the conversion of tryptophan to indole-3-acetaldoxime, a precursor of indole glucosinolates and indole-3-acetic acid. J. Biol. Chem. 275: 8133712–33717. Google Scholar

106.

M.D. Mikkelsen , P. Naur , and B.A. Halkier (2004). Arabidopsis mutants in the C-S lyase of glucosinolate biosynthesis establish a critical role for indole-3-acetaldoxime in auxin homeostasis. Plant J. 37: 81770–777. Google Scholar

107.

E.W. Miles (2001). Tryptophan synthase: a multienzyme complex with an intramolecular tunnel. Chem. Rec. 1: 81140–151. Google Scholar

108.

E. Mobley , B. Kunkel , and B. Keith (1999). Identification, characterization and comparative analysis of a novel chorismate mutase gene in Arabidopsis thaliana. Gene 240: 81115–123. Google Scholar

109.

N.R. Mustafa , and R. Verpoorte (2005). Chorismate derived C6C1 compounds in plants. Planta. 222: 811–5. Google Scholar

110.

P. Naur , B.L. Petersen , M.D. Mikkelsen , S. Bak , H. Rasmussen , C.E. Olsen , and B.A. Halkier (2003). CYP83A1 and CYP83B1, two nonredundant cytochrome P450 enzymes metabolizing oximes in the biosynthesis of glucosinolates in Arabidopsis. Plant Physiol. 133: 8163–72. Google Scholar

111.

A. Neish (1961). Formation of M- and P-coumaric acids by enzymatic deamination of the corresponding isomers of tyrosine. Phytochem. 1: 811–24. Google Scholar

112.

V. Nikiforova , J. Freitag , S. Kempa , M. Adamik , H. Hesse , and R. Hoefgen (2003). Transcriptome analysis of sulfur depletion in Arabidopsis thaliana: interlacing of biosynthetic pathways provides response specificity. Plant J. 33: 81633–650. Google Scholar

113.

V. Nikiforova , B. Gakière , S. Kempa , M. Adamik , L. Willmitzer , H. Hesse , and R. Hoefgen (2004). Towards dissecting nutrient metabolism in plants: a systems biology case study on sulfur metabolism. J. Exp. Bot. 55: 811861–1870. Google Scholar

114.

V.J. Nikiforova , M. Bielecka , B. Gakiere , S. Krueger , J. Rinder , S. Kempa , R. Morcuende , W.R. Scheible , H. Hesse , and R. Hoefgen (2006). Effect of sulfur availability on the integrity of amino acid biosynthesis in plants. Amino Acids. 30: 81173–183. Google Scholar

115.

K.K. Niyogi , R.L. Last , G.R. Fink , and B. Keith (1993). Suppressors of trp1 fluorescence identify a new Arabidopsis gene, TRP4, encoding the anthranilate synthase beta subunit. Plant Cell. 5: 811011–1027. Google Scholar

116.

J. Normanly , J.D. Cohen , and G.R. Fink (1993). Arabidopsis thaliana auxotrophs reveal a tryptophan-independent biosynthetic pathway for indole-3-acetic acid. Proc. Natl. Acad. Sci. USA. 90: 8110355–10359. Google Scholar

117.

S. Norris , T. Barrette , and D. DellaPenna (1995). Genetic dissection of carotenoid synthesis in Arabidopsis defines plastoquinone as an essential component of phytoene desaturation. Plant Cell. 7: 812139–2149. Google Scholar

118.

A. Ostin , M. Kowalyczk , R.P. Bhalerao , and G. Sandberg (1998). Metabolism of indole-3-acetic acid in Arabidopsis. Plant Physiol. 118: 81285–296. Google Scholar

119.

J. Ouyang , X. Shao , and J. Li (2000). Indole-3-glycerol phosphate, a branchpoint of indole-3-acetic acid biosynthesis from the tryptophan biosynthetic pathway in Arabidopsis thaliana. Plant. J. 24: 81327–333. Google Scholar

120.

G.C. Pagnussat , H.J. Yu , Q.A. Ngo , S. Rajani , S. Mayalagu , C.S. Johnson , A. Capron , L.F. Xie , D. Ye , and V. Sundaresan (2005). Genetic and molecular identification of genes required for female gametophyte development and function in Arabidopsis. Development 132: 81603–614. Google Scholar

121.

M. Pedras , F. Okanga , I. Zaharia , and A. Khan (2000). Phytoalexins from crucifers: synthesis, biosynthesis, and biotransformation. Phytochem. 53: 81161–176. Google Scholar

122.

E. Pichersky , and D. Gang (2000). Genetics and biochemistry of secondary metabolites in plants: an evolutionary perspective. Trends Pl. Sci. 4: 81439–445. Google Scholar

123.

J.E. Pinto , J.A. Suzich , and K.M. Herrmann (1986). 3-Deoxy-d-arabino-heptulosonate 7-phosphate synthase from potato tuber (Solanum tuberosum L.). Plant Physiol. 82: 811040–1044. Google Scholar

124.

S. Pollmann , A. Muller , M. Piotrowski , and E.W. Weiler (2002). Occurrence and formation of indole-3-acetamide in Arabidopsis thaliana. Planta 216: 81155–161. Google Scholar

125.

C. Poulsen , R.J. Bongaerts , and R. Verpoorte (1993). Purification and characterization of anthranilate synthase from Catharanthus roseus. Eur. J. Biochem. 212: 81431–440. Google Scholar

126.

L.J. Quittenden , N.W. Davies , J.A. Smith , P.P. Molesworth , N.D. Tivendale , and J.J. Ross (2009). Auxin biosynthesis in pea: characterization of the tryptamine pathway. Plant Physiol. 151: 811130–1138. Google Scholar

127.

E. Radwanski , A. Barczak , and R. Last (1996). Characterization of tryptophan synthase alpha subunit mutants of Arabidopsis thaliana. Mol. Gen. Genet. 253: 81353–361. Google Scholar

128.

E.R. Radwanski , and R.L. Last (1995). Tryptophan biosynthesis and metabolism biochemical and molecular genetics. Plant Cell. 7: 81921–934. Google Scholar

129.

E.R. Radwanski , J. Zhao , and R.L. Last (1995). Arabidopsis thaliana tryptophan synthase alpha gene cloning, expression, and subunit interaction. Mol Gen. Genet. 248: 81657–667. Google Scholar

130.

L. Rajjou , M. Belghazi , R. Huguet , C. Robin , A. Moreau , C. Job , and D. Job (2006). Proteomic investigation of the effect of salicylic acid on Arabidopsis seed germination and establishment of early defense mechanisms. Plant Physiol. 141: 81910–923. Google Scholar

131.

N.A. Ramsay , and B.J. Glover (2005). MYB-bHLH-WD40 protein complex and the evolution of cellular diversity. Trends Plant Sci. 10: 8163–70. Google Scholar

132.

L. Rask , E. Andreasson , B. Ekbom , S. Eriksson , B. Pontoppidan , and J. Meijer (2000). Myrosinase: gene family evolution and herbivore defense in Brassicaceae. Plant Mol. Biol. 42: 8193–113. Google Scholar

133.

M. Reichelt , P.D. Brown , B. Schneider , N.J. Oldham , E. Stauber , J. Tokuhisa , D.J. Kliebenstein , T. Mitchell-Olds , and J. Gershenzon (2002). Benzoic acid glucosinolate esters and other glucosinolates from Arabidopsis thaliana. Phytochem. 59: 81663–671. Google Scholar

134.

M. Reinink , and A. Borstap (1982). 3-Deoxy-d-arabino-heptulosonate 7-phosphate synthase from pea leaves: inhibition by L-tyrosine. Plant Sci. Lett. 26: 81167–171. Google Scholar

135.

P. Rippert , and M. Matringe (2002a). Molecular and biochemical characterization of an Arabidopsis thaliana arogenate dehydrogenase with two highly similar and active protein domains. Plant Mol. Biol. 48: 81361– 368. Google Scholar

136.

P. Rippert , and M. Matringe (2002b). Purification and kinetic analysis of the two recombinant arogenate dehydrogenase isoforms of Arabidopsis thaliana. Eur. J. Biochem. 269: 814753–4761. Google Scholar

137.

P. Rippert , C. Scimemi , M. Dubald , and M. Matringe (2004). Engineering plant shikimate pathway for production of tocotrienol and improving herbicide resistance. Plant Physiol. 134: 8192–100. Google Scholar

138.

P. Rippert , J. Puyaubert , D. Grisollet , L. Derrier , and M. Matringe (2009). Tyrosine and phenylalanine are synthesized within the plastids in Arabidopsis. Plant Physiol. 149: 811251–1260. Google Scholar

139.

A. Rohde , K. Morreel , J. Ralph , G. Goeminne , V. Hostyn , R. De Rycke , S. Kushnir , J. Van Doorsselaere , J.P. Joseleau , M. Vuylsteke , G. Van Driessche , J. Van Beeumen , E. Messens , and W. Boerjan (2004). Molecular phenotyping of the pal1 and pal2 mutants of Arabidopsis thaliana reveals far-reaching consequences on phenylpropanoid, amino acid, and carbohydrate metabolism. Plant Cell. 16; 812749–2771. Google Scholar

140.

A. Rose , A. Casselman , and R. Last (1992). A phosphoribosylanthranilate transferase gene is defective in blue fluorescent Arabidopsis thaliana tryptophan mutants. Plant Physiol. 100: 81582–592. Google Scholar

141.

A.B. Rose , and J.A. Beliakoff (2000). Intron-mediated enhancement of gene expression independent of unique intron sequences and splicing. Plant Physiol. 122: 81535–542. Google Scholar

142.

J. Rosler , F. Krekel , N. Amerhein , and J. Schmid (1997). Maize phenylalanine ammonia-lyase has tyrosine ammonia-lyase activity. Plant Physiol. 113: 81175–179. Google Scholar

143.

J.L. Rubin , and R.A. Jensen (1985). Differentially regulated isozymes of 3-deoxy-d-arabino-heptulosonate-7-phosphate synthase from seedlings of Vigna radiata [L.] Wilczek. Plant Physiol. 79: 81711–718. Google Scholar

144.

Y. Sasaki-Sekimoto , N. Taki , T. Obayashi , M. Aono , F. Matsumoto , N. Sakurai , H. Suzuki , M. Hirai , M. Noji , K. Saito , T. Masuda , K. Takamiya , D. Shibata , and H. Ohta (2005). Coordinated activation of metabolic pathways for antioxidants and defence compounds by jasmonates and their roles in stress tolerance in Arabidopsis. Plant J. 44: 81653–668. Google Scholar

145.

A. Schaller , J. Schmid , U. Leibinger , and N. Amrhein (1991). Molecular cloning and analysis of a cDNA coding for chorismate synthase from the higher plant Corydalis sempervirens Pers. J. Biol. Chem. 266: 8121434–21438. Google Scholar

146.

C. Schneider (2005). Chemistry and biology of vitamin E. Mol. Nutr. Food Res. 49: 817–30. Google Scholar

147.

R.C. Schuurink , M.A. Haring , and D.G. Clark (2006). Regulation of volatile benzenoid biosynthesis in petunia flowers. Trends Plant Sci. 11: 8120–25. Google Scholar

148.

G.L. Shadle , S.V. Wesley , K.L. Korth , F. Chen , C. Lamb , and R.A. Dixon (2003). Phenylpropanoid compounds and disease resistance in transgenic tobacco with altered expression of L-phenylalanine ammonia-lyase. Phytochem. 64: 81153–161. Google Scholar

149.

D.L. Siehl , and E.E. Conn (1988). Kinetic and regulatory properties of arogenate dehydratase in seedlings of Sorghum bicolor (L.) Moench. Arch. Biochem. Biophys. 260: 81822–829. Google Scholar

150.

D.L. Siehl , J.A. Connelly , and E.E. Conn (1986).Tyrosine biosynthesis in Sorghum bicolor: characteristics of prephenate aminotransferase. Z Naturforsch C. 41: 8179–86. Google Scholar

151.

S.R. Singer , and C.N. McDaniel (1985). Selection of glyphosate-tolerant tobacco calli and the expression of this tolerance in regenerated plants. Plant Physiol. 78: 81411–416. Google Scholar

152.

S.A. Singh , and D. Christendat (2006). Structure of Arabidopsis de-hydroquinate dehydratase-shikimate dehydrogenase and implications for metabolic channeling in the shikimate pathway. Biochem. 45: 817787– 7796. Google Scholar

153.

C.C. Smart , D. Johanning , G. Muller , and N. Amrhein (1985). Selective overproduction of 5-enol-pyruvylshikimic acid 3-phosphate synthase in a plant cell culture which tolerates high doses of the herbicide glyphosate. J. Biol. Chem. 260: 8116338–16346. Google Scholar

154.

D.M. Stalker , W.R. Hiatt , and L. Comai (1985). A single amino acid substitution in the enzyme 5-enolpyruvylshikimate-3-phosphate synthase confers resistance to the herbicide glyphosate. J. Biol. Chem. 260: 814724–4728. Google Scholar

155.

A. Stepanova , J. Robertson-Hoyt , J. Yun , L. Benavente , D. Xie , K. Doležal , A. Schlereth , G. Jürgens , and J. Alonso (2008). TAA1-mediated auxin biosynthesis is essential for hormone crosstalk and plant development. Cell 133: 81177–191. Google Scholar

156.

R. Stracke , H. Ishihara , G. Huep , A. Barsch , F. Mehrtens , K. Niehaus , and B. Weisshaar (2007). Differential regulation of closely related R2R3-MYB transcription factors controls flavonol accumulation in different parts of the Arabidopsis thaliana seedling. Plant J. 50: 81660–677. Google Scholar

157.

L.C. Strader , and B. Bartel (2008). A new path to auxin. Nat. Chem. Biol. 4: 81337–339. Google Scholar

158.

S. Sugawara , S. Hishiyama , Y. Jikumaru , A. Hanada , T. Nishimura , T. Koshiba , Y. Zhao , Y. Kamiya , and H. Kasahara (2009). Biochemical analyses of indole-3-acetaldoxime-dependent auxin biosynthesis in Arabidopsis. Proc. Natl. Acad. Sci. USA 106: 815430–5435. Google Scholar

159.

J. Suzich , R. Ranjeva , P. Hasegawa , and K. Herrmann (1984). Regulation of the shikimate pathway of carrot cells in suspension culture. Plant Physiol. 75: 81369–371. Google Scholar

160.

Y. Tao , J.L. Ferrer , K. Ljung , F. Pojer , F. Hong , J.A. Long , L. Li , J.E. Moreno , M.E. Bowman , L.J. Ivans , Y. Cheng , J. Lim , Y. Zhao , C.L. Ballare , G. Sandberg , J.P. Noel , and J. Chory (2008). Rapid synthesis of auxin via a new tryptophan-dependent pathway is required for shade avoidance in plants. Cell. 133: 81164–176. Google Scholar

161.

D. Tieman , M. Taylor , N. Schauer , A.R. Fernie , A.D. Hanson , and H.J. Klee (2006). Tomato aromatic amino acid decarboxylases participate in synthesis of the flavor volatiles 2-phenylethanol and 2-phenylacetaldehyde. Proc. Natl. Acad. Sci. USA. 103: 818287–8292. Google Scholar

162.

Y. Tozawa , H. Hasegawa , T. Terakawa , and K. Wakasa (2001). Characterization of rice anthranilate synthase alpha-subunit genes OASA1 and OASA2. Tryptophan accumulation in transgenic rice expressing a feedback-insensitive mutant of OASA1. Plant Physiol. 126: 811493–1506. Google Scholar

163.

G.F. Trezzini , A. Horrichs , and I.E. Somssich (1993). Isolation of putative defense-related genes from Arabidopsis thaliana and expression in fungal elicitor-treated cells. Plant Mol. Biol. 21: 81385–389. Google Scholar

164.

K. Tsurusaki , K. Takeda , and A. Sakurai (1997). Conversion of indole-3-acetaldehyde to indole-3-acetic acid in cell-wall fraction of barley (Hordeum vulgare) seedlings. Plant Cell Physiol. 38: 81268–273. Google Scholar

165.

V. Tzin , S. Malitsky , A. Aharoni , and G. Galili (2009). Expression of a bacterial bi-functional chorismate mutase/prephenate dehydratase modulates primary and secondary metabolism associated with aromatic amino acids in Arabidopsis. Plant J. 60: 81156–167. Google Scholar

166.

J.C. Verdonk , C.H. Ric de Vos , H.A. Verhoeven , M.A. Haring , A.J. van Tunen , and R.C. Schuurink (2003). Regulation of floral scent production in petunia revealed by targeted metabolomics. Phytochem. 62: 81997–1008 Google Scholar

167.

T. Vogt (2010). Phenylpropanoid biosynthesis. Mol. Plant 3: 812–20. Google Scholar

168.

K. Wakasa , and J. Widholm (1987). A 5-methyltryptophan resistant rice mutant, MTR1, selected in tissue culture. Theor. Appl. Genet. 74: 8149–54. Google Scholar

169.

J.C. Waller , T.A. Akhtar , A. Lara-Nunez , J.F. Gregory , 3rd, R.P. McQuinn , J.J. Giovannoni , and A.D. Hanson (2010). Developmental and feedforward control of the expression of folate biosynthesis genes in tomato fruit. Mol. Plant 3: 8166–77. Google Scholar

170.

K.M. Warpeha , S.S. Lateef , Y. Lapik , M. Anderson , B.S. Lee , and L.S. Kaufman (2006). G-protein-coupled receptor 1, G-protein alphasubunit 1, and prephenate dehydratase 1 are required for blue light-induced production of phenylalanine in etiolated Arabidopsis. Plant Physiol. 140: 81844–855. Google Scholar

171.

S. Watanabe , K. Hayashi , K. Yagi , T. Asai , H. MacTavish , J. Picone , C. Turnbull , and N. Watanabe (2002). Biogenesis of 2-phenylethanol in rose flowers: incorporation of [2H8]L-phenylalanine into 2-phenylethanol and its beta-D-glucopyranoside during the flower opening of Rosa ‘Hoh-Jun’ and Rosa damascena Mill. Biosci. Biotechno. Biochem. 66: 81943–947. Google Scholar

172.

K.T. Watts , B.N. Mijts , P.C. Lee , A.J. Manning , and C. Schmidt-Dannert (2006). Discovery of a substrate selectivity switch in tyrosine ammonia-lyase, a member of the aromatic amino acid lyase family. Chem. Biol. 13: 811317–1326. Google Scholar

173.

A. Weber , R. Schwacke , and U. Flügge (2005). Solute transporters of the plastid envelope membrane. Annual Review of Plant Biol. 56: 81133– 164. Google Scholar

174.

E. Weber-Ban , O. Hur , C. Bagwell , U. Banik , L.H. Yang , E.W. Miles , and M.F. Dunn (2001). Investigation of allosteric linkages in the regulation of tryptophan synthase: the roles of salt bridges and monovalent cations probed by site-directed mutation, optical spectroscopy, and kinetics. Biochem. 40: 813497–3511. Google Scholar

175.

B. Weisshaar , and G. Jenkins (1998). Phenylpropanoid metabolism and its regulation. Curr. Opin. Plant Biol. 1: 81251–257. Google Scholar

176.

M. Wildermuth (2006). Variations on a theme synthesis and modification of plant benzoic acids. Curr. Opin. Plant Biol. 9: 81288–296. Google Scholar

177.

M. Wildermuth , J. Dewdney , G. Wu , and F. Ausubel (2001). Isochorismate synthase is required to synthesize salicylic acid for plant defence. Nature. 414: 81562–565. Google Scholar

178.

U. Wittstock , and B.A. Halkier (2000). Cytochrome P450 CYP79A2 from Arabidopsis thaliana L. catalyzes the conversion of L-phenylalanine to phenylacetaldoxime in the biosynthesis of benzylglucosinolate. J. Biol. Chem. 275, 8114659–14666. Google Scholar

179.

A. Wright , M. Sampson , M. Neuffer , L. Michalczuk , J. Slovin , and J. Cohen (1991). Indole-3-acetic acid biosynthesis in the mutant maize orange pericarp, a tryptophan auxotroph. SCi. 254: 81998–1000. Google Scholar

180.

T. Yamada , F. Matsuda , K. Kasai , S. Fukuoka , K. Kitamura , Y. Tozawa , H. Miyagawa , and K. Wakasa (2008). Mutation of a rice gene encoding a phenylalanine biosynthetic enzyme results in accumulation of phenylalanine and tryptophan. Plant Cell. 20: 811316–1329. Google Scholar

181.

Y. Yan , S. Stolz , A. Chetelat , P. Reymond , M. Pagni , L. Dubugnon , and E.E. Farmer (2007). A downstream mediator in the growth repression limb of the jasmonate pathway. Plant Cell. 19: 812470–2483. Google Scholar

182.

R. Yatusevich , S.G. Mugford , C. Matthewman , T. Gigolashvili , H. Frerigmann , S. Delaney , A. Koprivova , U.I. Flugge , and S. Kopriva (2010). Genes of primary sulfate assimilation are part of the glucosinolate biosynthetic network in Arabidopsis thaliana. Plant J. 62: 811–11. Google Scholar

183.

R. Zhang , B. Wang , J. Ouyang , J. Li , and Y. Wang (2008). Arabidopsis indole synthase, a homolog of tryptophan synthase alpha, is an enzyme involved in the Trp-independent J. Integr. Plant Biol. 50: 811070–1077. Google Scholar

184.

J. Zhao , and R.L. Last (1996). Coordinate regulation of the tryptophan biosynthetic pathway and indolic phytoalexin accumulation in Arabidopsis. Plant Cell. 8: 812235–2244. Google Scholar

185.

J. Zhao , C.C. Williams , and R.L. Last (1998). Induction of Arabidopsis tryptophan pathway enzymes and camalexin by amino acid starvation, oxidative stress, and an abiotic elicitor. Plant Cell. 10: 81359–370. Google Scholar

186.

Y. Zhao , A. Hull , N. Gupta , K.A. Goss , J. Alonso , J. Ecker , J. Normanly , J. Chory , and J. Celenza (2002). Trp-dependent auxin biosynthesis in Arabidopsis: involvement of cytochrome P450s CYP79B2 and CYP79B3. Genes Dev. 16: 813100–3112. Google Scholar

187.

B. Zybailov , H. Rutschow , G. Friso , A. Rudella , O. Emanuelsson , Q. Sun , and K.J. van Wijk (2008). Sorting signals, N-terminal modifications and abundance of the chloroplast proteome. PLoS One. 3: 81e1994. Google Scholar
© 2010 American Society of Plant Biologists
Vered Tzin and Gad Galili "The Biosynthetic Pathways for Shikimate and Aromatic Amino Acids in Arabidopsis thaliana," The Arabidopsis Book 2010(8), (1 April 2010). https://doi.org/10.1199/tab.0132
Published: 1 April 2010
JOURNAL ARTICLE
PAGES


SHARE
ARTICLE IMPACT
Back to Top