Phytochemistry Reviews

, Volume 6, Issue 2, pp 277–305

Catharanthus terpenoid indole alkaloids: biosynthesis and regulation

Open AccessOriginal Paper

DOI: 10.1007/s11101-006-9047-8

Cite this article as:
El-Sayed, M. & Verpoorte, R. Phytochem Rev (2007) 6: 277. doi:10.1007/s11101-006-9047-8

Abstract

Catharanthus roseus is still the only source for the powerful antitumour drugs vinblastine and vincristine. Some other pharmaceutical compounds from this plant, ajmalicine and serpentine are also of economical importance. Although C. roseus has been studied extensively and was subject of numerous publications, a full characterization of its alkaloid pathway is not yet achieved. Here we review some of the recent work done on this plant. Most of the work focussed on early steps of the pathway, particularly the discovery of the 2-C-methyl-d-erythritol 4-phosphate (MEP)-pathway leading to terpenoids. Both mevalonate and MEP pathways are utilized by plants with apparent cross-talk between them across different compartments. Many genes of the early steps in Catharanthus alkaloid pathway have been cloned and overexpressed to improve the biosynthesis. Research on the late steps in the pathway resulted in cloning of several genes. Enzymes and genes involved in indole alkaloid biosynthesis and various aspects of their localization and regulation are discussed. Much progress has been made at alkaloid regulatory level. Feeding precursors, growth regulators treatments and metabolic engineering are good tools to increase productivity of terpenoid indole alkaloids. But still our knowledge of the late steps in the Catharanthus alkaloid pathway and the genes involved is limited.

Keywords

Indole alkaloidsBiosynthesisCatharanthusIndole pathwayMEP pathwayRegulationTerpenoids

Abbreviations

AACT

Acetoacetyl-CoA thiolase

ABA

Abscisic acid

AS

Anthranilate synthase

AVLB

Anhydrovinblastine

CMS

4-Cytidyl diphospho-2 C-methyl-d-erythritol synthase

CPR

Cytochrome P450 reductase

CR

Cathenamine reductase

DAT

Acetyl CoA:deacetylvindoline 17-O-acetyltransferease

D4H

Desacetoxyvindoline 4-hydroxylase

DMAPP

Dimethylallyl diphosphate

DXP

1-Deoxy-d-xylulose-5-phosphate

DXR

1-Deoxy-d-xylulose-5-phosphate reducto isomerase

DXS

1-Deoxy-d-xylulose-5-phosphate synthase

GAP

Glyceraldehyde-3-phosphate

G10H

Geraniol 10-hydroxylase

GPP

Geranyl diphosphate

HMG-CoA

3-Hydroxy-3-methylglutaryl-CoA

HMGS

3-Hydroxy-3-methylglutaryl-CoA synthase

HMGR

3-Hydroxy-3-methylglutaryl-CoA reductase

IPP

Isopentenyl diphosphate

Km

Michaelis–Menten constant

LAMT

Loganic acid methyltransferase

MCS

2-C-Methyl-d-erythritol 2,4-cyclodiphosphate synthase

MEP

2-C-methyl-d-erythritol 4-phosphate

MVAK

Mevalonate kinase

MJ

Methyljasmonates

Mr

Relative molecular weight

MVA

Mevalonic acid

MVAPK

5-Diphosphomevalonate kinase

NMT-SAM

Methoxy 2,16-dihydro-16-hydroxytabersonine N-methyltransferase

OMT

O-Methyltransferase

ORCA

Octadecanoid-responsive Catharanthus AP2/ERF-domain

SAM

S-Adenosyl-l-methionine

SGD

Strictosidine β-d-glucosidase

SLS

Secologanin synthase

STR

Strictosidine synthase

T16H

Tabersonine 16-hydroxylase

THAS

Tetrahydroalstonine synthase

TIA

Terpenoid indole alkaloids;

TDC

Tryptophan decarboxylase

Introduction

Plant cells are considered to be excellent producers of a broad variety of chemical compounds. Many of these compounds are of high economic value such as various drugs, flavours, dyes, fragrances and insecticides. These compounds usually play a role in the interaction of the plant with its environment, e.g. as toxins to defend the plant against micro-organisms or various predators, as messengers, attractants, repellents or as camouflage (Verpoorte 1998).

Alkaloids are one of the largest classes of secondary metabolites. They contain a heterocyclic nitrogen usually with basic properties that makes them particularly pharmacologically active. Among them are the indole alkaloids which are found mainly in plants belonging to the families: Apocynaceae, Loganiaceae, Rubiaceae and Nyssaceae (Verpoorte et al. 1997).

Catharanthus roseus (L.) G. Don (Madagascar Periwinkle) is one of the most extensively investigated medicinal plants. The importance of this plant is due to the presence of two antitumour alkaloids, vinblastine and vincristine found in the leaves, and ajmalicine, an alkaloid found in the roots. All parts of this plant contain a variety of alkaloids, even seeds that were thought to have no alkaloids until Jossang et al. (1998) isolated two binsidole alkaloides from the seeds, vingramine and methylvingramine. Cell suspension cultures of C. roseus are an alternative means for the production of economically important terpenoid indole alkaloids (TIAs). However, the yields are too low to allow commercial application. The more than 100 C. roseus alkaloids that have been identified share many biosynthetic steps. The early stages of alkaloid biosynthesis in C. roseus involve the formation of secologanin derived from the terpenoid (isoprenoid) biosynthesis and its condensation with tryptamine to produce the central intermediate strictosidine, the common precursor for the monoterpenoid indole alkaloids (Fig. 1).
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Fig. 1

Different Catharanthus indole alkaloids biosynthetic pathways

The terpenoid pathway

Terpenoids are the largest family of natural products with over 30,000 compounds. They are known to have many biological and physiological functions. Formation of terpenoids proceeds via two different pathways, the classical mevalonate and the newly discovered 2-C-methyl-d-erythritol 4-phosphate (MEP) pathway leading to isopentenyl diphosphate (IPP). In higher plants, the mevalonate pathway operates mainly in the cytoplasm and mitochondria. The MEP pathway operates in the plastids with a cross-talk between the two pathways where at least one metabolite can be exchanged.

Formation of IPP

The mevalonate pathway

The early steps in the isoprenoid pathway comprise the enzymatic conversions involved in the synthesis of IPP. The mevalonate pathway starts with the coupling of two molecules of acetyl-CoA to form acetoacetyl-CoA. This step is catalysed by the enzyme acetoacetyl-CoA thiolase (AACT). Condensation of acetoacetyl-CoA with another molecule of acetyl-CoA to form 3-hydroxy-3-methylglutaryl-CoA (HMG-COA), is catalysed by HMG-CoA synthase (HMGS). Reduction of HMG-CoA by HMG-CoA reductase (HMGR) leads to the formation of mevalonate. Phosphorylation of mevalonate to 5-diphosphomevalonate is catalysed by mevalonate kinase (MVAK) and 5-diphosphomevalonate kinase (MVAPK), then 5-diphosphomevalonate is decarboxylated by 5-diphosphomevalonate decarboxylase to IPP.

Isopentenyl diphosphate is considered as a building block of isoprenoids. The isomerization of IPP to form dimethylallyl diphosphate (DMAPP) is a key step in the biosynthesis of isoprenoids. This step is catalysed by IPP isomerase (E.C. 5.3.3.2; Ramos-Valdivia et al. 1997; Verpoorte et al. 1997). DMAPP is condensed with one IPP in a head-to-tail fashion generating geranyl diphosphate (GPP), the precursor for the monoterpenes including iridoids such as secologanin (Verpoorte et al. 1997; Contin 1999). The coupling reaction is catalysed by a prenyltransferase while the enzymatic cyclization of GPP is catalysed by a monoterpene synthase, GPP synthase (Chappell 1995).

The mevalonate-independent pathway leading to the formation of IPP (MEP pathway)

The biosynthesis of IPP, the central precursor of all isoprenoids, proceeds via two separate pathways in plants. The mevalonate pathway leads to the formation of triterpenes (sterols) and certain sesquiterpenes (Newman and Chappell 1999; Lange and Croteau 1999). The second pathway is mevalonate-independent (MEP pathway) and leads to the formation of monoterpenes, diterpenes, tetraterpenes (carotenoids) and the prenyl side chains of chlorophyll (Eisenreich et al. 1996, 1997; Arigoni et al. 1997; Rohmer 1999).

The discovery of the MEP pathway for isoprenoid biosynthesis was reviewed by Rohmer (1999), Lichtenthaler (1999), Rohdich et al. (2001), Rodriguez-Concepcion and Boronat (2002) and Dubey et al. (2003). The pathway was first discovered in studies of the biosynthesis of bacterial hopanoids that are similar to sterols produced by eukaryotes and act as membrane stabilizers. As hopanoids are chemically stable and easily isolated, they are very suited for labelling experiments using stable isotopes followed by NMR to determine the sites of incorporation in the molecules. Through the labelling experiments, it was thought to be trivial to identify the isoprenoid units resulting from the mevalonic acid (MVA) route but, the pattern of the labels was completely different and did not fit the classical MVA pathway.

Sprenger (1996), in his labelling experiments on bacteria that utilize only hexoses, and especially glucose as a carbon source, determined the origin of isoprenic units of hopanoids as derived from glucose. The labelling pattern was in accordance with pyruvate as a precursor of a C2 subunit and a triose phosphate derivative as precursor of a C3 subunit.

For the MEP pathway, the biosynthetic sequence leading to the formation of IPP in plants is still not completely identified (Fig. 2). The complete pathway has been elucidated, including the late steps in bacteria (for review see Rodriguez-Concepcion and Boronat 2002).
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Fig. 2

The biosynthesis of IPP via mevalonate pathway and MEP pathway with involved enzymes

The initial step of the pathway involves a condensation of pyruvate (C2 and C3) with d-glyceraldehyde 3-phosphate to yield 1-deoxy-d-xylulose-5-phosphate (DXP). Chahed et al. (2000) isolated and characterized the cDNA (crdxs) encoding for 1-deoxy-d-xylulose-5-phosphate synthase (DXS) from C. roseus. The enzyme that catalyses this reaction belongs to a family of transketolases. In the second step of this pathway, rearrangement and reduction of DXP to MEP takes place. The enzyme catalysing this step is DXP reducto isomerase (DXR). Grolle et al. (2000) cloned the gene encoding this enzyme from the bacterium Zymomonas mobilis. Veau et al. (2000) reported the cloning and expression of cDNAs encoding crdxr and crmecs (reducto isomerase and 2-C-methyl-d-erythritol-2,4-cyclodiphosphate synthase) from C. roseus. The IPP is formed finally in low rate from isopentenyl monophosphate via a step catalysed by the enzyme isopentenyl monophosphate kinase. Contin et al. (1998) proved that the terpenoid moiety of the TIAs, secologanin is not derived from the mevalonate pathway but instead from the MEP pathway using a cell suspension culture of C. roseus. The late steps are not characterized yet in C. roseus. 4-Cytidyl diphospho-2 C-methyl-d-erythritol synthase was first cloned from Arabidopsis thaliana and expressed in Escherichia coli (Rohdich et al. 2000). Although there are few radiotracer studies in plants which demonstrated the possible phophorylation role of 4-diphosphocytidyl-2-C-methyl-d-erythritol kinase (CMK) in the pathway, the complete enzymology and its molecular analysis is not available in a plant system. The gene encoding 2-C-methyl-d-erythritol 2,4-cyclodiphosphate synthase has been demonstrated in Arabidopsis but the enzyme was not fully characterized.

The iridoid pathway

The first steps in the pathway leading to the formation of secologanin are the formation of geraniol followed by hydroxylation into 10-hydroxylgeraniol, catalysed by the cytochrome P450 enzyme geraniol 10-hydroxylase (G10H). In the presence of NAD+ or NADP+, 10-hydroxygeraniol is oxidized into 10-oxogeranial. The enzyme responsible for this step is an oxidoreductase (Madyastha and Coscia 1979). 10-Oxogeraniol is converted to iridodial by cyclization. NADPH:cytochrome P450 reductase (CPR) is essential for the G10H catalysed reaction. In the formation of 7-deoxyloganic acid from iridodial, so far, no enzymes have been described (Contin 1999). Methylation of loganic acid to form loganin is catalysed by S-adenosyl-l-methionine:loganic acid methyltransferase (LAMT). Finally the cleavage of the cyclopentane ring of loganin forms the secologanin (Fig. 3). Conversion of loganin to secologanin is of particular interest, the enzyme catalysing this reaction is secologanin synthase (SLS). In C. roseus, Contin (1999) attempted to identify the enzyme involved in bioconversion of loganin to secologanin with no success. She reported that the conversion probably involves a cytochrome P450 enzyme. This enzyme was finally detected and characterized in a cell suspension culture of Lonicera japonica (Yamamoto et al. 2000). It is a membrane-associated enzyme belonging to the group of cytochrome P450 monooxygenases and its reaction requires NADPH and oxygen. Irmler et al. (2000) reported that the activities of CYP72A1 from C. roseus expressed in E. coli converts loganin into secologanin and confirmed it as SLS. This enzyme was previously purified from C. roseus by Mangold et al. (1994) and thought to have G10H activity but did not show any hydroxylase activity with 11 substrates for cytochrome P450 reactions.
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Fig. 3

The biosynthesis of secologanin from geraniol. G10H geraniol 10-hydroxylase, LAMT loganic acid methyltransferase, SLS secologanin synthase

Characterized enzymes involved in the biosynthetic pathway leading to the formation of secologanin

AACT (E.C. 2.3.1.9) and HMGS (E.C. 4.1.3.5)

Both AACT and HMGS activities were found to be present in C. roseus by using an HPLC method specially developed to determine HMG-CoA metabolizing enzyme activities. Using this method, three HMG-CoA catabolizing activities were discovered in C. roseus suspension cultured cells in addition to HMGR (Van der Heijden et al. 1994). These enzymes are instable and sensitive to high salt concentrations. AACT and HMGS were partially purified from a cell suspension culture of C. roseus (Van der Heijden and Verpoorte 1995).

3-Hydroxy-3-methylglutaryl-CoA reductase (E.C. 1.1.1.34)

The HMG reductase has been purified from a number of species besides C. roseus and its characteristics and regulation mechanisms have been the subject of extensive reviews (Chappell 1995; Bach 1995; Stermer et al. 1994; Verpoorte et al. 1997; Schulte 1998). Overexpression of the hmgr gene in C. roseus hairy roots resulted in an increase in alkaloid levels. A clone with high hybridization signal produced more ajmalicine and catharanthine than the control, whereas the clone with low hybridization signal increased the production of serpentine up to sevenfold (Ayora-Talavera et al. 2002).

MVAK (E.C. 2.7.1.36) and MVAPK (E.C. 2.7.4.2)

The phosphorylation of MVA to the mono- and di-phosphate ester (MVAP and MVAPP) has been extensively studied in C. roseus plants and cell cultures (Schulte 1998). MVAK from C. roseus cell cultures was purified to homogeneity and characterized. The enzyme showed to be quite stable. It is strongly inhibited by farnesyl diphosphate. MVAK activity depends on the presence of the divalent ions, Mg2+ and Mn2+ which are effective in sustaining the activity. It also has a broad pH optimum between 7 and 10 with a maximum activity around pH 9 (Schulte et al. 2000). MVAPK from C. roseus was also purified and characterized (Schulte et al. 1999).

5-Diphosphomevalonate decarboxylase (MVAPP decarboxylase, E.C. 4.1.1.33)

The MVAPP decarboxylase that forms IPP from MVAPP has not yet been given much attention and has only been characterized in a few plant species (Verpoorte et al. 1997; Contin 1999). The formation of IPP was reviewed by Ramos-Valdivia et al. (1997).

IPP isomerase (E.C. 5.3.3.2)

Isopentenyl diphosphate isomerase was partially purified from C. roseus cultures (Ramos-Valdivia et al. 1998). IPP-isomerase activity was also determined in 5-day-old C. roseus suspension cultured cells, treated with Pythium aphanidermatum elicitor preparation. A slight inhibition of the enzyme was observed during the first 120 h after elicitor treatment (Moreno et al. 1996).

Geranyl diphosphate synthase (E.C. 5.1.1.1)

The enzyme GPP synthase is not yet investigated in C. roseus (Contin 1999).

Geraniol 10-hydroxylase

This enzyme is a cytochrome P450 monooxygenase dependent on NADPH. G10H is regarded as a potential site for regulatory control in the biosynthesis of secologanin. Studies by Schiel et al. (1987) showed that G10H activity is induced when C. roseus cell cultures are transferred to an induction medium known to enhance alkaloid accumulation and that there is a close relationship between G10H activity and alkaloid accumulation. Also McFarlane et al. (1975) demonstrated that G10H is feedback inhibited by the TIAs catharanthine, vinblastine and vindoline. The Ki of catharanthine inhibition (1 mM) is in the range of alkaloid concentration in C. roseus (0.3–1 mM). Madyastha et al. (1976) partially purified G10H from C. roseus seedlings. Meijer et al. (1993a) purified G10H from C. roseus suspension cultured cells in a four-step procedure after solublization with cholate. The protein showed a Mr of 56,000 and a Km of 5.5 μM geraniol and 11 μM nerol. Also, Collu et al. (2001) purified this enzyme from C. roseus cell cultures following the method developed by Meijer et al. (1993a) with some modifications.

NADPH:cytochrome P450 reductase (E.C. 1.6.2.4)

Cytochrome P450 reductase functions in electron transfer from NADPH and is essential for all cytochrome P450 monooxygenases. It was purified from C. roseus plants (Madyastha and Coscia 1979) and from cell cultures (Meijer et al. 1993b). The protein showed a Mr of 79,000 and the activity is dependent on NADPH, FAD and FMN as cofactors. In C. roseus the CPR mRNA level is enhanced by fungal elicitor treatments (Meijer et al. 1993a, b, Lopes Cardoso et al.,1997). Like the yeast and animal CPRs, C. roseus protein contains a hydrophobic domain close to the N-terminus which serves as a membrane anchor. Steady-state mRNA levels observed in C. roseus plants were higher in flowers and much lower in leaves and stems while intermediate in the roots.

Cyclase

The dialdehyde (10-oxogeranial/10-oxoneral) is cyclized to iridodial. The enzyme responsible for the cyclization has not yet been purified from C. roseus but was obtained from Rauwolfia serpentina (Uesato et al. 1986, 1987; Verpoorte et al. 1997).

Loganic acid methyltransferase (E.C. 2.1.1.50)

In the formation of 7-deoxyloganic acid from iridodial, so far no enzymes have been described (Contin 1999). The 7-hydroxylation to afford loganic acid must precede its methylation, as suggested by enzymatic studies with the S-adenosyl-l-methionine:LAMT partially purified from C. roseus seedlings (Madyastha et al. 1973). This enzyme catalyses the transfer of a methyl group to loganic acid to form loganin. Contin (1999) measured the activity of LAMT in C. roseus cells cultured on three different media and found that the activity is restricted to the early period of growth similarly to the results obtained by Guarnaccia et al. (1974) and Madyastha and Coscia (1979) in C. roseus seedlings where maximum activity of the enzyme was recorded just after germination.

Secologanin synthase (E.C. 1.3.3.9)

Secologanin synthase belongs also to the cytochrome P450 family. This gene was cloned 12 years ago from C. roseus and was first thought to encode G10H (Vetter et al. 1992) but recently it was shown that it encodes the enzyme that converts loganin to secologanin (Irmler et al. 2000). This cytochrome P450 enzyme accepts only loganin as substrate with an optimum catalysing reaction at a pH of 7.5 (Yamamoto et al. 2000).

Enzymes involved in the MEP pathway leading to the formation of IPP

1-Deoxy-d-xylulose 5-phosphate synthase (E.C. 4.1.3.37)

Bacteria, fungi, yeasts and plants are capable of synthesizing 1-deoxy-d-xylulose (DX) or its 5-phosphate (DXP) from pyruvate and from d-glyceraldehyde or from its phosphate (GAP). The enzymatic activity in this step is thiamine diphosphate dependent and probably related to pyruvate dehydrogenase. As the reaction is not specific, the system can accept acyloins in place of pyruvate as acetyl donor and also different aldoses, yielding 1-deoxyketoses with C5, C6 or C7 skeletons.

The enzyme catalyses the concomitant decarboxylation of pyruvate and the condensation of the resulting (hydroxyethyl) thiamine on free GAP, yielding deoxyxylulose or its phosphate (DXP). As free glyceraldehyde is not a usual cellular metabolite, GAP and DXP are thought to be the normal substrate and product of the synthase.

1-Deoxy-d-xylulose 5-phosphate reducto isomerase (E.C. 1.1.1.267)

The rearrangement of DX or DXP yields 2-C-methyl-d-erythrose or its 4-phosphate and the reduction of these products yields 2-C-methyl-d-erythritol (ME) or its 4-phosphate (MEP; Duvold et al. 1997a,b, Sagner et al. 1998).

Using E. coli mutants that were auxotrophic to ME, a gene that complemented in these mutants the region coding for IPP biosynthesis was cloned and led to the identification of the enzyme responsible for the conversion of DXP into MEP (Takahashi et al. 1998). This reducto-isomerase enzyme is NADPH-dependent and requires Mn2+ as cofactor. It catalyses two consecutive steps: the rearrangement of DXP into 2-C-methyl-d-erythrose and the reduction of this aldose to MEP. The free aldose phosphate was not detected and the presence of the 5-phosphate group on DXP was required for the enzymatic conversion.

Isopentenyl monophosphate kinase (E.C. 2.7.1.)

Lange and Croteau (1999) reported the cloning of the gene encoding IPK from peppermint and E. coli. This kinase catalyses the phosphorylation of isopentenyl monophosphate as the last step of the biosynthetic sequence to IPP. This enzyme belongs to a conserved class of the GHMP family of kinases that includes galactokinase, homoserine kinase, MVAK and phosphomevalonate kinase. This enzyme was thought to catalyse the last step in the MEP pathway, however Rohdich et al. (2000) showed that the overexpressed CMK protein from tomato does not have any IPK activity, even if very high concentrations of recombinant enzyme were used. The detected IPK activity could not be metabolically relevant and cannot confirm the final steps leading to IPP synthesis.

Localization of the enzymes involved in the pathways leading to the formation of secologanin

In the mevalonate pathway, the enzymes are localized in the cytosol and produce the precursor of triterpenes and sesquiterpenes. Nothing has been reported on the localization of AACT/HMGS enzymes in C. roseus although they were purified from a cell suspension cultures (Van der Heijden et al. 1994; Van der Heijden and Verpoorte 1995). The radish AACT and HMGS have been reported as membrane-associated enzymes (Weber and Bach 1994; Bach et al. 1994). It has been suggested that HMGR might be located in mitochondria and plastids of plants (Gary 1987; Stermer et al. 1994). The regulated degradation of HMGR has been indicated to be completely localized in the endoplasmic reticulum in yeast (Hampton and Rine 1994). Evidence that HMGR is located within endoplasmic reticulum as well as in spherical, vesicular structures derived from endoplasmic reticulum has been recently given (Leivar et al. 2005).

The plant enzymes MVAK and MVAPK were presumed to be predominantly cytosolic but have been proven to be present in plastids as well (McKaskill and Croteau 1995; Albrecht and Sandmann 1994). The subcellular localization of MVAK and MVAPK was studied in suspension cultured cells of C. roseus and it was shown that most of the activity of both enzymes was located in the cytosolic fraction. MVAK activity was also recovered from an organellar and microsomal fraction. MVAPK activity was detected in the organelle fraction (Schulte et al. 1999, 2000).

The localization of IPP isomerase in C. roseus has not been determined yet but in Castor beans, a mitochondrial and proplastidial IPP isomerase have been detected (Green et al. 1975). In glandular trichomes of peppermint, it was found that the cytoplasmic MVA pathway was blocked at the level of HMGR and that the IPP utilized for both plastidial monoterpene and cytosolic sesquiterpene biosynthesis is synthesized exclusively in the plastids. A connection of the pathway was proposed at the level of IPP that requires translocation of IPP to the different compartments and the presence of an isoform of IPP isomerase in each compartment (McKaskill and Croteau 1995). Ramos-Valdivia et al. (1997) extensively reviewed the IPP isomerase.

In Lithospermum erythrorhizon, the enzyme GPP synthase involved in the biosynthesis of naphthoquinones was found to be present in the cytosol (Sommer et al. 1995).

The enzyme G10H is associated with (pro)vacuolar membranes (Madyastha et al. 1977) rather than with endoplasmic reticulum where many P450s are found (Nebert 1979). Collu (1999), studied the localization of G10H in C. roseus cell suspension cultures and confirmed that this enzyme is localized in vacuolar membranes. The CPR catalysing cytochrome P450 monooxygenase reactions is a membrane-bound flavoprotein, closely linked to the P450 protein. The expression of the three identified C. roseus MEP pathway genes and the G10H genes was found to be in internal phloem parenchyma, i.e. in cells different than the other known alkaloid biosynthesis related genes (Burlat et al. 2004).

Localization of the non-mevalonate pathway leading to the formation of IPP

The biosynthesis of mono-, di- and tetraterpenoids in plants seems to occur in plastids, where the MEP pathway is localized (Rohmer 1999; Lange and Croteau 1999). In plastids, the DXP pathway operates to supply IPP for the synthesis of monoterpenes, diterpenes and carotenoids. Table 1 summarizes the information about the known enzymes involved in TIA biosynthesis in C. roseus.
Table 1

Enzymes involved in biosynthesis of indole alkaloids of C. roseus

Enzyme

Abbreviation

Cofactors

Product

Localization

Anthranilate synthase

AS

Mg2+

Anthranilate

Plastid

Tryptophan decarboxylase

TDC

PP, PQQ

Tryptamine

Cytosol

Isopentenyl diphosphate isomerase

IPP isomerase

Mg2+, Mn2+

3,3-Dimethylallyl diphosphate

Plastid

Geraniol 10-hydroxylase

G10H

Haeme

10-Hydroxygeraniol

Provacuolar membrane

NAPDH:cytochrome P450 reductase

CPR

NADPH, FAD, FMN

Provacuolar membrane

SAM:loganic acid methyltransferease

LAMT

SAM

Loganin

Secologanin synthase

SLS

NADPH

Secologanin

Strictosidine synthase

STR

Strictosidine

Vacuole

Strictosidine β-glucosidase

SGD

[Cathenamine]

Endoplasmic reticulum

Cathenamine reductase

CR

NADPH

Ajmalicine

Geissoschizine dehydrogenase

NADP+

4,21-Dehydrogeissoschizine

Tetrahydroalstonine synthase

THAS

NADPH

Tetrahydroalstonine

Tabersonine 16-hydroxylase

T16H

Haeme, NADPH

16-Hydroxytabersonine

Endoplasmic reticulum

11-Hydroxytabersonine O-methyltransferase

OMT

16-Methoxytabersonine

SAM:methoxy 2,16-dihydro-16-hydroxytabersonine N-methyltransferase

NMT

SAM

Desacetoxyvindoline

Thylakoid membranes

Desacetoxyvindoline 17-hydroxylase

D4H

2-Oxoglutarate, Fe2+, ascorbate

Desacetylvindoline

Cytoplasm

Acetyl CoA:deacetylvindoline 17-O-acetyltransferase

DAT

Acetyl CoA

Vindoline

Cytoplasm

Acetyl CoA:minovincinine-O-acetyltransferase

MAT

Acetyl CoA

Echitovenine

Cytoplasm

Anhydrovinblastine synthase

AVLB synthase

Anhydrovinblastine

Vacuole

Genes-encoding enzymes involved in the biosynthesis of secologanin

A cDNA clone for radish AACT has been cloned by complementation in yeast (Vollack and Bach 1995). Using the radish cDNA as a probe to screen an A. thaliana cDNA library, four positive clones have been isolated of which three were identical and the fourth shown to be an antisense (Piñas et al. 1997). The presence of antisense mRNA could indicate a regulatory mechanism of controlling translation of AACT mRNA.

A cDNA encoding the A. thaliana HMGS has been cloned (Montamat et al. 1995) and expressed in E. coli (Diez et al. 1997). In addition to the A. thaliana HMGS gene, also the HMGS gene has been cloned from Schizosaccharomyces pombe (Katayama et al. 1995).

Plants have a small gene-family of HMGR isoenzymes that are differentially expressed and respond to a variety of developmental and environmental signals (Stermer et al. 1994; Enjuto et al. 1994; Weissenborn et al. 1995; Korth et al. 1997). HMGR genes have been well studied in Solanaceae species. Four HMGR genes have been isolated from tomato. One of them, the hmg1 gene has been found to be involved in aspects related to primary metabolism like sterol biosynthesis and cell growth. The activation pattern of the second HMGR gene hmg2 by wounding and elicitation has suggested a role in the plant’s defence (Weissenborn et al. 1995). Also potato, has at least three HMGR genes (Stermer et al. 1994). A C. roseushmg cDNA has been cloned (Maldonada-Mendosa et al. 1992). In C. roseus cell suspensions, methyl jasmonate has been shown to be able to increase HMGR mRNA levels after a transient suppression (Maldonada-Mendosa et al. 1994).

The gene of deoxyxylulose 5-phosphate synthase has been isolated from E. coli (Sprenger et al. 1997; Lois et al. 1998) and cloned from higher plants, Mentha × piperita (Lange et al. 1998) and C. roseus (Chahed et al. 2000; Veau et al. 2000). The gene encoding the DXR enzyme was cloned from higher plants such as peppermint (Lange and Croteau 1999), A. thaliana (Lange and Croteau 1999; Schwender et al. 1999) and C. roseus (Veau et al. 2000).

Molecular cloning of G10H has been previously attempted using several different approaches. Differential screening of a C. roseus cDNA library resulted in the isolation of two highly homologous cytochrome P450 cDNAs and their corresponding mRNAs were induced in alkaloid production when compared to normal growth medium (Vetter et al. 1992). Measuring the expression of the gene in different parts of the plant showed that mRNA levels were highest in the flowers. Attempts to clone the G10H gene by immunoscreening of a C. roseus cDNA library were not successful because the antibodies raised against the purified G10H protein were not sufficiently specific (Meijer et al. 1993a). Multiple cDNAs encoding P450s from A. thaliana were isolated by employing a PCR strategy with degenerate oligonucleotide primers designed on amino acid sequences conserved between plant cytochrome P450s (Mizutani et al. 1998). The gene was cloned by Collu et al. (2001) and expressed in C. roseus and yeast cells. It is strongly induced by methyljasmonate (MJ). Transgenic C. roseus cells showed that G10H activity is correlated to the ability of the cells to accumulate TIAs, although the increased G10H is not the only requirement for increased alkaloid accumulation (Collu et al. 2002). This gene was classified as a new member of the CYP76B plant P450 family.

Cytochrome P450 reductase is cloned from C. roseus cell cultures by Meijer et al. (1993b). Immunoscreening of a C. roseus cDNA expression library resulted in the isolation of a partial NADPH:CPR clone. The clone was identified on the basis of sequence homology with CPRs from yeast and animals. The gene is encoded by a single copy and the protein consists of 714 amino acids.

The indole pathway

Biosynthesis of tryptophan

Tryptophan is an aromatic amino acid derived from chorismate via anthranilate. Chorismate originates from the shikimate pathway (Fig. 4).
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Fig. 4

Biosynthesis of l-tryptophan through the chorismate pathway. 1 anthranilate synthase, 2 phosphoribosyl diphosphate (PR) anthranilate transferase, 3 PR-anthranilate isomerase, 4 indole-3-glycerol phosphate synthase, 5 tryptophan synthase α, 6 tryptophan synthase β

l-Tryptophan is formed through a biosynthetic pathway consisting of five enzymatically controlled steps (Poulsen and Verpoorte 1991; Verpoorte et al. 1997; Bongaerts 1998; Whitmer 1999). The first step is formation of anthranilate from chorismate. This step is catalysed by the enzyme anthranilate synthase (AS, E.C. 4.1.3.27). The second step is formation of N-(5-phosphoribosyl) anthranilate and this step is catalysed by the enzyme phosphoribosyl diphosphate (PR)-anthranilate transferase (E.C. 4.1.1.48). The third step is formation of 1-(O-carboxyphenylamino)-1-deoxyribulose phosphate. This step is catalysed by the enzyme PR-anthranilate isomerase (E.C. 5.3.1.24). The following step is formation of indole-3-glycerol phosphate. This step is catalysed by the enzyme indole-3-glycerol phosphate synthase (E.C. 4.1.1.48). The next step is formation of indole which is catalysed by the enzyme tryptophan synthase α (E.C. 4.2.1.20). The last step is formation of l-tryptophan which is catalysed by the enzyme tryptophan synthase β (E.C. 4.2.1.20). This enzyme was detected in the proteomics approach as being induced when alkaloid production is induced (Jacobs et al. 2005).

Enzymes involved in the biosynthesis of l-Tryptophan

Anthranilate synthase (E.C. 4.13.27)

Anthranilate synthase was first isolated and purified to apparent homogeneity from C. roseus (Poulsen et al. 1993). It is a tetramer, consisting of two large and two small subunits. The large α-subunit is responsible for the conversion of chorismate into anthranilate while the smaller β-subunits are responsible for the generation of the substrate NH3 from glutamine (Verpoorte et al. 1997). So far, none of the enzymes leading to tryptophan after AS has been studied in C. roseus (Moreno et al. 1995; Verpoorte et al. 1997).

Only a time course of tryptophan synthase (E.C. 4.2.1.20) activity during the growth of suspension cultured and immobilized cells of C. roseus has been determined (Facchini and DiCosmo 1991). Lower tryptophan synthase activity was present in immobilized cells than in suspension cultured cells. Using a proteomics approach, Jacobs (Jacobs 2003; Jacobs et al. 2005) identified the β-subunit tryptophan synthase in C. roseus cell suspension cultures which was detected during a short time of growth period and seemed to be correlated with alkaloid production.

Bongaerts (1998) reported the isolation and characterization of a full-length C. roseus cDNA encoding a functional AS α subunit. He found that AS activity is highest in roots compared with other organs of C. roseus and correlated well with the abundance of AS α transcripts in this organ. Expressing an AS α subunit insensitive to ajmalicine feedback in C. roseus hairy roots increases the production of tryptophan, tryptamine and lochnericine (Hughes et al. 2004a, b).

Biosynthesis of tryptamine

Tryptophan decarboxylase (E.C. 4.1.1.28)

Tryptamine is derived from primary metabolism by a single enzymatic conversion of the amino acid l-tryptophan, catalysed by tryptophan decarboxylase (TDC, E.C. 4.1.1.28). This enzyme was purified first by Noe and Berlin (1984), later this protein was extensively characterized (Fernandez et al. 1989; Pennings et al. 1989a, b). The enzyme is a soluble protein consisting of two identical subunits containing two molecules of pyridoxal phosphate (Pennings et al. 1989a). It was observed that TDC activity can be induced when suspension cultures of C. roseus are transferred from growth medium to alkaloid induction medium that contains a high concentration of sugar and low levels of hormones, nitrogen and phosphate (Knobloch et al. 1981). This enzyme is located on the interface between primary and secondary metabolism. It is considered a putative site for regulatory control of TIAs. However, generally there is no clear correlation between TDC activity and TIA biosynthesis in cell cultures of C. roseus (Knobloch and Berlin 1983; Merillon et al. 1986; Eilert et al. 1987; Facchini and DiCosmo 1991; Whitmer 1999).

Localization of TDC was shown to be in the cytosol (De Luca and Cutler 1987; Stevens et al. 1993). The expression of the tdc gene was restricted to the upper epidermis of cotyledons in C. roseus (Vasquez-Flota et al. 2000).

Tryptophan decarboxylase cDNA has been cloned from C. roseus (De Luca et al. 1989). The tdc gene was found to occur as a single copy in the C. roseus genome (Goddijn 1992). Expression of tdc appeared to be highly regulated at the transcriptional level. In cell suspension cultures tdc mRNA levels were shown to be downregulated by auxins and induced by fungal elicitors (Goddijn et al. 1992; Pasquali et al. 1992). The specific mRNAs encoding TDC enzyme activity, appear to be present in low quantities in developing seedlings if compared with the high levels of transcripts that occur in elicitor-induced cell suspension cultures of C. roseus by the fungus P. aphanidermatum. When tdc upstream sequences from −1,818 to +198 relative to the transcriptional start site were analysed to identify cis-acting elements that determine basal expression or respond to elicitor, it was found that there were three functional regions in the −160 promoter. The region between −160 and −99 was shown to act as the main transcriptional enhancer while the other two elements (between −99 to −87 and between −87 to −37) were found to be not redundant in the tdc promoter (Ouwerkerk and Memelink 1999). As TDC seems to represent an important site for regulatory control of alkaloid production, it was examined whether overexpression of tdc affects alkaloid accumulation (Goddijn 1992). The TDC cDNA driven by the strong Cauliflower Mosaic Virus 35S promoter was introduced into C. roseus by means of an oncogenic Agrobacterium tumefaciens strain. Overexpression appeared not to result in an increased alkaloid accumulation but only enhanced tryptamine levels (Goddijn et al. 1995; Verpoorte et al. 1998). Expressing tdc cDNA from C. roseus in a Nicotiana tabacum cell suspension culture (Hallard et al. 1997), resulted in the formation of tryptamine (about 10 μg/g fresh weight). This level of tryptamine is similar to that found in leaves of tdc transgenic tobacco plants (ranging from 18 to 66 μg/g FW, Lopes Cardoso 1995).

Biosynthesis of strictosidine

Strictosidine is the central intermediate in the biosynthesis of many alkaloids. It is formed by coupling of the iridoid glycoside secologanin and tryptamine. The enzyme condensing both secologanin and tryptamine is strictosidine synthase (STR, E.C. 4.3.3.2, Stöckigt 1980; Pennings et al. 1989c; Kutchan 1993; Verpoorte et al. 1997).

Strictosidine synthase (E.C. 4.3.3.2)

The purification of STR from C. roseus was first described by Treimer and Zenk (1979) and Mizukami et al. (1979) with an estimated molecular weight between 34 and 38 kDa. There are seven STR isoforms of which four were characterized by Zenk’s group. Those four isoforms differ in pI (4.3–4.8) and Km value for tryptamine (from 0.9 to 6.6 mM) where the activity was inhibited at high levels. Also, De Waal et al. (1995), purified and characterized this enzyme from C. roseus cell suspension cultures. In that study, four out of six isoforms were purified to homogeneity while two others were nearly homogeneous. The isoforms have a broad pH range (6–7.5) and all of them have similar kinetics. No inhibition could be observed for up to 5 mM tryptamine. The Km value determined for all isoforms is around 8.2–9.4 which is higher than that reported by Zenk’s group.

Recently, Jacobs (2003) and Jacobs et al. (2005) detected seven isoforms of STR in C. roseus cell suspension cultures by western blotting and two-dimensional electrophoresis. Expression of those isoforms varies upon elicitation with P. aphanidermatum.

Strictosidine synthase activity could not be inhibited by the end product alkaloids: vindoline, catharanthine and ajmalicine (Mizukami et al. 1979).

Early studies on localization of STR indicated that it is a cytosolic protein (Deus-Neumann and Zenk 1984; De Luca and Cutler 1987). But, McKnight et al. (1991) clearly demonstrated that STR protein is located in the vacuoles of C. roseus cells and it was further confirmed that STR activity is located in this compartment (Stevens et al. 1993).

A partial str cDNA clone was isolated from C. roseus by McKnight et al. (1990) but the complete genomic sequence for STR from C. roseus was reported by Pasquali et al. (1992). It is encoded by a single gene. Overexpression of the str gene in C. roseus resulted in a number of cases in an increase in alkaloid biosynthesis (Canel et al. 1998; Whitmer 1999) but this gradually decreased upon subculturing despite a high level of STR activity.

Cellular investigation showed that tdc and str1 mRNAs were present in the epidermis of stems, leaves, flower buds and appeared in most protoderm and cortical cells of the apical meristem of root tips. The mRNAs of genes-encoding enzymes involved in vindoline biosynthesis are associated with laticifer and idioblast cells of the shoots which is clearly different from TDC and STR localization (St-Pierre et al. 1999).

Biosynthesis of indole alkaloids

As strictosidine is considered to be a central intermediate in the biosynthetic pathway of monoterpenoid indole alkaloids in C. roseus, somewhere beyond this stage in the biosynthesis, routes towards the different specific end products are thought to diverge. Strictosidine-β-d-glucosidase (SGD) might be the enzyme playing an important role in steering the monoterpenoid indole alkaloid biosynthesis in a specific direction.

Strictosidine-β-d-glucosidase (E.C. 3.2.1.105)

The enzyme SGD was first described by Scott et al. (1977). It was thought that this enzyme was present as a large enzyme complex, so-called ajmalicine synthase, capable to form ajmalicine from tryptamine and secologanin. Hemscheidt and Zenk (1980) reported the presence of two specific β-glucosidases from C. roseus and both accepted strictosidine as substrate. A partial purification scheme for SGD has been presented by Stevens (1994) using C. roseus and Tabernaemontana divaricata cell cultures as source for the SGD enzyme. Luijendijk et al. (1998) purified the SGD enzyme to apparent homogeneity from C. roseus cell suspension cultures. It was reported that SGD has a very high molecular mass but under denaturing conditions a molecular mass of 63 kDa is found suggesting that the native enzyme is occurring as an aggregate where many subunits are bound. Kinetic parameters showed that it has a strong affinity for strictosidine as substrate. It shows a remarkable stability towards proteases as it plays a role in plant’s defence.

Subcellular localization studies showed that SGD is most likely associated with the endoplasmic reticulum and this is consistent with the presence of a putative signal sequence for targeting of the protein to the endoplasmic reticulum (Geerlings et al. 2000).

Geerlings et al. (2000) cloned the gene encoding this enzyme from C. roseus cell suspension cultures. A full-length clone gave rise to SGD activity when expressed in yeast. SGD is encoded by single copy gene and showed up to 60% homology at the amino acid level to other β-glucosidases from plants.

Biosynthesis of ajmalicine, serpentine and tetrahydroalstonine

The removal of the glucose moiety of strictosidine by SGD leads to an unstable highly reactive aglucon which was thought to be converted into 4,21-dehydrogeissoschizine. The latter was believed to be converted by cathenamine synthase to cathenamine (Rüffer et al. 1979). However, following the conversion of strictosidine by C. roseus purified glucosidase by 1H-NMR did not show any 4,21-dehydrogeissoschizine. The carbinolamine was the intermediate rather than 4,21-dehydrogeissoschizine. Apparently the formation of cathenamine from strictosidine does not need cathenamine synthase but only the glucosidase (Stevens 1994).

Cathenamine is reduced to form ajmalicine (Fig. 5). There are two different cathenamine reductases (CRs), one converts cathenamine into ajmalicine and the other converts the iminium form of cathenamine into tetrahydroalstonine (Hemscheidt and Zenk 1980). Ajmalicine is converted into serpentine by basic peroxidase isolated from C. roseus vacuoles (Blom et al. 1991). Sierra (1991) found a close correlation between the peroxidase activity and serpentine accumulation. Light grown cell cultures had a 20-fold higher vacuolar peroxidase activity compared to those of dark-grown cells and the accumulation of serpentine in light grown cells was higher.
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Fig. 5

Biosynthesis of ajmalicine, serpentine and tetrahydroalstonine in C. roseus. SGD strictosidine glucosidase, CR cathenamine reductase, POD peroxidase, THAS tetrahydroalstonine synthase

Enzymes involved in the biosynthesis of ajmalicine, serpentine and tetrahydroalstonine pathways

CR and tetrahydroalstonine synthase

The reduction of cathenamine to form ajmalicine is catalysed by the enzyme CR. Early studies by Hemscheidt and Zenk (1985) described this enzyme which used cathenamine as a substrate and NADPH as cofactor resulting in the formation of ajmalicine and 19-epi-ajmalicine. Tetrahydroalstonine synthase (THAS) from C. roseus used the iminium form of cathenamine as substrate and NADPH to form tetrahydroalstonine (Hemscheidt and Zenk 1985). This enzyme showed a Km of 62 μM for this substrate and the enzyme molecular mass was estimated to be 81 kDa. Both CR and THAS were detected in low levels in C. roseus cell cultures (Luijendijk 1995).

Localization of the enzymes involved in ajmalicine, serpentine and tetrahydroalstonine pathways

The subcellular localization of the enzymes involved in the biosynthesis of ajmalicine and tetrahydroalstonine in C. roseus cell cultures was studied by Luijendijk (1995). Assays after subcellular fractionation suggested a vacuolar localization of THAS. The CR activity was mostly below the detection limit making it impossible to draw any conclusions.

Ajmalicine is channelled across the plasma membrane until it is trapped in a low-pH vacuole by an ion-trap mechanism. The oxidation of ajmalicine to serpentine was shown to be catalysed by a vacuolar peroxidase (Blom et al. 1991).

Catharanthine pathway

The information on catharanthine biosynthesis is very limited. Battersby and Hall (1969) reported that geissoschizine fed to C. roseus plants was incorporated into catharanthine. Brown et al. (1971) suggested that geissoschizine could be converted into stemmadenine or akuammicine. Feeding stemmadenine to C. roseus cell suspension cultures resulted in the formation of catharanthine and tabersonine in few hours (El-Sayed et al. 2004). Condylocarpine was also formed after feeding as an oxidation product but not as an intermediate in the pathway.

Enzymes and genes involved in the catharanthine pathway have not been isolated or cloned yet.

Vindoline pathway

It has been established that tabersonine is transformed into vindoline by a sequence of six steps (Fig. 6). These steps include: aromatic hydroxylation, O-methylation, hydration of the 2,3-double bond, N(1)-methylation, hydroxylation at position 4 and 4-O-acetylation (Balsevich et al. 1986; De Luca et al. 1986). The first reaction is catalysed by tabersonine 16-hydroxylase (T16H) yielding 16-hydroxytabersonine. The second step is catalysed by O-methyltransferase (OMT) resulting in the formation of 16-methoxytabersonine. De Luca et al. (1987) established that the third step in vindoline biosynthesis is catalysed by an unidentified hydroxylase to form 16-methoxy−2,3-dihydro-3-hydroxytabersonine. The subsequent step is N-methylation of 16-methoxy-2,3-dihydro-3-hydroxytabersonine by N-methyltransferase (NMT) forming desacetoxyvindoline. The latter is hydroxylized by desacetoxyvindoline-4-hydroxylase (D4H) into deacetylvindoline. The last step in the biosynthesis of vindoline is acetylation of deacetylvindoline by deacetylvindoline-4-O-acetyltransferase (DAT) to form vindoline.
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Fig. 6

Vindoline biosynthesis pathway. T16H tabersonine 16-hydroxylase, OMTO-methyltransferase, NMTN-methyltransferase, D4H desacetoxyvindoline 4-hydroxylase, DAT deacetylvindoline-4-O-acetyltransferase

Enzymes involved in the biosynthesis of vindoline

T16H and OMT

Tabersonine 16-hydroxylase and OMT catalyse the first two steps in the vindoline biosynthesis pathway. Characterization of both enzymes was reported by St-Pierre and De Luca (1995). T16H was identified as a membrane-bound cytochrome P450-dependent enzyme with low activity in etiolated seedlings but strongly induced activity by light. OMT used 16-hydroxytabersonine as a natural substrate. These enzymes were recently reported to be localized in leaf epidermal cells, identifying these cells as the major site of vindoline precursor biosynthesis (Murata and De Luca 2005).

N-Methyltransferase

This enzyme has been partially purified by high-performance anion exchange chromatography on a mono-Q column and has an apparent Mr of 60,000 (Dethier and De Luca 1993). The enzyme has a high substrate specificity where the reduced 2,16 double bond in the tabersonine skeleton is essential.

Desacetoxyvindoline-4-hydroxylase

The hydroxylation of desacetoxyvindoline is catalysed by a 2-oxoglutarate-dependent dioxygenase D4H. This enzyme was purified to homogeneity and characterized by De Carolis et al. (1990) and De Carolis and De Luca (1993). It requires alkaloid substrate, 2-oxoglutarate, ascorbate, ferrous ions and molecular oxygen for the activity. Exposure of the etiolated seedlings to light or red-light induced the activity of the enzyme (Vasquez-Flota et al. 2000). MJ increased the activity of D4H in etiolated seedlings of C. roseus in light conditions but not in the absence of light (Vasquez-Flota and De Luca 1998).

Deacetylvindoline-4-O-acetyltransferase

Acetyl coenzyme A:DAT catalyses the biosynthesis of vindoline from acetyl coenzyme A and deacetylvindoline. The purified enzyme is strongly inhibited by tabersonine and coenzyme A (50% inhibition at 45 and 37 μM, respectively) and weakly inhibited by tryptamine, secologanin and vindoline (Power et al. 1990). The original purification of DAT led to an incorrect conclusion that the enzyme consists of two subunits with molecular weight of 33 and 21 kDa. The isolated dat gene encodes a 50 kDa polypeptide suggesting that the protein was cleaved during purification.

Genes-encoding enzymes involved in the vindoline pathway

A T16H cDNA was cloned from C. roseus cell suspension cultures by Schröder et al. (1999) and expressed in E. coli. The protein (CYP71D12) showed 47–52% identity with the other members of the CYP71D subfamily with unknown functions.

Vasquez-Flota et al. (1997) reported on the cloning of D4H gene from C. roseus. Three oligopeptides were isolated from the tryptic digest of the purified protein and microsequenced. One oligopeptide showed significant homology to hyoscyamine 6-β-hydroxylase. The three clones were confirmed to be authentic d4h clones as the heterologous expression of the recombinant protein showed D4H activity. Southern blot analysis suggested that the d4h is present as a single copy-gene. Hydroxylation activity and RNA blot hybridization studies showed that the enzyme activity followed closely the levels of d4h transcripts, occurring predominantly in young leaves and much lower in stems and fruits. Etiolated seedlings had undetectable activity but rapid increase of enzyme activity of D4H was shown after exposure to light.

The dat gene was cloned by St-Pierre et al. (1998) from C. roseus leaf extract. The genomic clone encoded a 50 kDa polypeptide. Cleavage of DAT protein to yield a heterodimer appears to be an artefact of the protein purification procedure. The study showed that the induced dat mRNA, protein accumulation and the enzyme activity occurred in leaves and cotyledons of light-treated seedlings. The southern blot of genomic DNA isolated from C. roseus indicated that the dat occurs as a single copy-gene.

Localization of the enzymes involved in the vindoline biosynthesis pathway

Tabersonine 16-hydroxylase is a cytochrome P450-dependent monooxygenase associated with the external face of the endoplasmic reticulum while OMT is believed to occur in the cytosol (St-Pierre and De Luca 1995). NMT is associated with the chloroplast thylakoids (De Luca 1993). D4H and DAT are cytosolic enzymes (St-Pierre et al. 1998; Vasquez-Flota et al. 1997). St-Pierre et al. (1999) reported that D4H and DAT mRNAs were associated with the laticifer and idioblast cells of the leaves, stems and flower buds. These results suggest that the late steps of vindoline biosynthesis occur in a specific tissue, explaining that the attempts to produce vindoline by cell culture technology have failed so far.

Biosynthesis of bisindole alkaloids

The bisindole alkaloids vinblastine and vincristine are of great interest. They are synthesized from the coupling of the monomeric alkaloids catharanthine and vindoline. The product resulting from the coupling is α-3′,4′-anhydrovinblastine which is converted into vinblastine which is further converted into vincristine (for review, see Verpoorte et al. 1997). The coupling process is catalysed by the enzyme anhydrovinblastine synthase (AVLBS). These dimeric alkaloids are used as antitumour agents and produced in trace amounts (0.003% dry weight). The natural high abundance of vindoline and catharanthine in C. roseus plants led to the establishment of a semisynthetic process for coupling the monomers either chemically (Langlois et al. 1976; Kutney et al. 1976) or enzymatically using horseradish peroxidase (Goodbody et al. 1988).

The basic peroxidase enzyme catalysing the dimerization process

The search of the enzyme responsible for the dimerization reaction using crude enzyme extracts failed to detect any significant dimerization activity. This was referred to the presence of enzyme inhibitors released from the different cellular compartments during homogenization (Sottomayor et al. 1996). After purification of the protein extracts, dimerization was detected in the fractions containing peroxidase activity and dependent on the presence of H2O2, this enzyme was identified as AVLBS (Sottomayor et al. 1998). Coupling vindoline with catharanthine by a peroxidase into anhydrovinblastine which is a reduction product from a highly instable dihydropyridinium, an iminium, is the true precursor to the other bisindole alkaloids vinblastine, vincristine and leurosine (Fig. 1). The purified protein showed a specific activity of 1.8 nkat/mg. Molecular weight was estimated to be 45.4 kDa and the pI of the protein around 10.7. The enzyme was a high spin ferric haem protein belonging to the class III peroxidase family.

The localization of the enzyme has been reported to occur in the vacuole associated to specific spots of the internal face of the tonoplast (Sottomayor et al. 1996).

Gene encoding basic peroxidase

Beginning with purified CRPRX1 (basic peroxidase) protein, the polypeptide N-terminal region was sequenced. By this process 11 N-terminal amino acids were identified. Further molecular strategies failed to give more cloning information results. A PCR strategy followed by screening of a cDNA library prepared from C. roseus leaf tissue enabled the preparation of a full-length cDNA clone which considered to be CrPrx1 cDNA (Hilliou et al. 2002).

Regulation of TIA biosynthesis

Regulation of TIAs can be controlled either by developmental or exogenous signals. Light is thought to have an effect on enzyme induction and activation. Stimulation of serpentine accumulation in cells and tissue cultures and oxidation of ajmalicine depends on light (Loyola-Vargas et al. 1992). Part of the vindoline biosynthetic pathway is also regulated by light (St-Pierre and De Luca 1995). In C. roseus callus cultures, Zhao et al. (2001a) found that light significantly influenced the biosynthesis of vindoline. In the same study, the group confirmed that stimulation of plastidial basic and acidic peroxidases by light led to induction of serpentine accumulation. Shanks and Bhadra (1997) established a light-adapted C. roseus hairy root culture that exhibited green pigmentation but with lower tabersonine, hörhammericine and lochnericine levels and an increase in specific yields of ajmalicine and serpentine compared to dark-grown cultures.

Application of various exogenous chemicals can improve the alkaloid production of C. roseus. Betaine, malic acid, tetramethyl ammonium bromide and rare elements increased the yields of ajmalicine and catharanthine in cell cultures about five- to sixfold (Zhao et al. 2000a, b). Zheng and Wu (2004) found that treating C. roseus cell suspension cultures with cadmium resulted in enhancement of ajmalicine content as well as TDC enzyme activity. The use of oxygenase inhibitors in hairy root cultures inhibited the accumulation of lochnericine and hörhammericine suggesting that these chemicals influenced the cytochrome P450 enzymes that may be responsible for the formation of these alkaloids (Morgan and Shanks 1999). G10H, a cytochrome P450 enzyme activity increased by addition of phenobarbital and decreased by ketoconazole (Contin et al. 1999).

Increasing the substrate supply via precursor feeding overcomes the rate-limiting steps in the production of alkaloids. Particularly the terpenoid pathway seems rate limiting for alkaloid production and feeding with secologanin or loganin has proven to be an efficient way to improve accumulation of alkaloids (Moreno et al. 1993; Whitmer et al. 1998 and Contin 1999). Feeding both tryptamine and loganin to transgenic cell cultures resulted in very high production levels (Whitmer et al. 1998). Feeding either geraniol, 10-hydroxygeraniol or loganin to a C. roseus hairy root culture resulted in significant increases in the accumulation of tabersonine (Morgan and Shanks 2000). But addition of tryptophan or tryptamine separately had no effect. It seems that a part of the pathway is present in the plant cell cultures. These enzymes do have a considerable capacity for alkaloid production. The flux is thus determined in an early phase of the pathway. Particularly the terpenoid part of the pathway seems limiting for the alkaloid production.

Plant growth regulators

The role of growth hormones in regulation of C. roseus indole alkaloids has been extensively studied (for review see Moreno et al. 1995 and Verpoorte et al. 1997). They affect both culture growth and secondary metabolite production. Auxins negatively influence alkaloid biosynthesis at all levels. Subculturing cells on an auxin-free medium, results in increased Tdc and Str mRNA levels, while addition of auxins rapidly decreases the Tdc mRNA level. 2,4-D strongly inhibits alkaloid production essentially during the growth phase (Arvy et al. 1994). Cytokinins are very important growth regulators which regulate many aspects of plant growth and differentiation. Addition of zeatin to an auxin-free C. roseus cell cultures resulted in an increase in alkaloid accumulation (Decendit et al. 1992). Zeatin enhanced the activity of G10H and the bioconversion of secologanin to ajmalicine in C. roseus cultures (Decendit et al. 1993). Exogenously applied cytokinins to untransformed C. roseus callus or cell suspension cultures increased the content of ajmalicine and serpentine (Garnier et al. 1996; Yahia et al. 1998).

Abscisic acid (ABA) regulates various aspects of plant growth and development including seed maturation and dormancy, as well as adaptation to abiotic environmental stresses (Davies and Jones 1991; Beaudoin et al. 2000). Smith et al. (1987) reported that ABA stimulated accumulation of catharanthine and vindoline in C. roseus. Treatment of precursors fed C. roseus cells with ABA did not induce the accumulation of alkaloids but it delayed the catabolism of strictosidine (El-Sayed and Verpoorte 2002).

Jasmonate

Jasmonic acid or MJ are used as exogenous signal transduction compounds (reviewed by Reymond and Farmer 1998). Addition of jasmonic acid to C. roseus hairy root cultures increased the yield of alkaloids (Rijhwani and Shanks 1998).

Treatment of C. roseus seedlings with MJ resulted in doubling of alkaloid accumulation (Aerts et al. 1994). Upon feeding precursors to C. roseus cell cultures and treating with MJ, strictosidine and ajmalicine accumulation was increased (El-Sayed and Verpoorte 2002). Octadecanoid-responsive Catharanthus AP2/ERF-domain (ORCA) transcription factors have been shown to regulate the JA-responsive activation of several TIA biosynthetic genes (Van der Fits and Memelink 2000; Memelink et al. 2001). ORCA2, a transcription factor of AP2/ERF domain transactivated str promoter activity by sequence-specific binding to the JERE (Menke et al. 1999). ORCA3, a novel jasmonate-responsive AP2-domain transcriptive factor was isolated from C. roseus by T-DNA tagging (Van der Fits and Memelink 2000). It is similar to ORCA2 in the AP2/ERF DNA-binding domain. Also expression of the gene was induced by MJ with similar kinetics as ORCA2. The ORCA3 protein binds to the promoter regions of the TIA biosynthetic genes str, tdc and cpr, the CPR (Van der Fits and Memelink 2001). Overexpression of ORCA3, resulted in induction of expression of many secondary and primary metabolite biosynthetic genes, though TIAs production increased only upon feeding loganin to the ORCA3 overexpressing cells (Van der Fits and Memelink 2000). Again this shows the important role of the iridoid pathway for determining the final alkaloid levels.

Salicylic acid

Salicylic acid has been shown to be an important compound in the defence system of plants. However, addition of SA to C. roseus, either seedlings (Aerts et al. 1996) or cell cultures (El-Sayed and Verpoorte 2002) did not affect the yield of alkaloids. A weak inducing effect on Str and Tdc steady-state mRNA levels was observed in C. roseus after addition of 0.1 mM SA (Pasquali 1994).

Fungal elicitation

The biosynthesis of TIAs can be stimulated by addition of exogenous elicitors such as fungal preparations. Many studies reveal that fungal elicitors profoundly affect regulation of indole alkaloid biosynthesis (for review see Verpoorte et al. 1997). In the past 20 years, plant microbe interactions and plant defence responses have been studied extensively. Pathogen recognition at the cell surface or in the cytosol initiates various cellular signalling processes that activate multi-component plant defence responses, such as oxidative burst defence gene activation and accumulation of defence-related compounds (Mehdy 1994; Chandra et al. 1997; Scheel 1998). Menke et al. (1999) reported induction of the tdc and str genes in C. roseus cells by fungal elicitors suggesting that the octadecanoid pathway may be involved in fungal elicitor-induced indole alkaloid production. In C. roseus, Moreno et al. (1996) measured activities of some enzymes involved in secondary metabolism before and after fungal elicitation and found that TDC activity is highly induced while G10H and IPP-isomerase activities are slightly decreased by elicitation. Although the strong and rapidly stimulating effect of fungal elicitors on plant secondary metabolite accumulation attracts considerable attention, contradictory results are sometimes observed. Great efforts are being made to investigate the mechanism of fungal elicitors at physiological and molecular levels. The mechanism of elicitation in plants is based on elicitor–receptor interaction after which a rapid array of biochemical responses occur (Radman et al. 2003). Figure 7 shows the possible elicitor mechanism of action. The mechanism includes: (1) binding of the elicitor to plasma membrane receptor. (2) Changes in Ca2+ influx to the cytoplasm from extracellular and intracellular pools. (3) Changes in the protein phosphorylation patterns and protein kinase activation. (4) Decrease of pH of the cytoplasm and activation of NADPH oxidases. (5) Changes in cell wall structure (lignification) through generating reactive oxygen species. (6) Synthesis of jasmonic acid and salicylic acid as secondary messengers. (7) Accumulation of defence-related proteins. (8) Synthesis of plant defence molecules such as phytoalexins. (9) Systemic acquired resistance.
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Fig. 7

Elicitor action mechanism in plant cell

Zhao et al. (2001c) screened 12 fungal elicitors to improve indole alkaloid production in C. roseus cell suspension cultures. Different kinds of alkaloids are induced by different fungal elicitors and different elicitor dosages. Combination of abiotic and biotic elicitors added to C. roseus cell suspension cultures resulted in improvement of TIA production. Ajmalicine and catharanthine are induced by addition of tetramethyl ammonium bromide and Aspergillus niger homogenate (Zhao et al. 2001b).

Metabolic engineering

Recently a number of examples of plant transformation were addressed (for review, see Verpoorte et al. 2000, 2002; Verpoorte and Alfermann 2000). Single or multiple steps of the pathway can be introduced in the plant genome to improve productivity of secondary metabolites. C. roseus is a model from which genes encoding key enzymes (TDC, STR and G10H) involved in TIAs were overexpressed in different plants. Strictosidine production, the central intermediate in the TIA pathway can be achieved in tobacco expressing Catharanthustdc and str genes upon feeding secologanin (Hallard et al. 1997). Expression of those genes in Morinda citrifolia cells also resulted in strictosidine formation when the cells were fed with tryptamine and secologanin (Hallard 2000). Hairy roots of Weigela ‘styriaca’ expressing str and tdc cDNAs from C. roseus are able to produce tryptamine and ajmalicine (Hallard 2000). In C. roseus, overexpression of the gene encoding the enzyme STR resulted in some cases in an increase in alkaloid biosynthesis. Although those transgenic cell lines of C. roseus overexpressing tdc and str lost their capacity to produce high levels of alkaloids after 2 years subculturing, the enzymes of both transgenes remained high (Whitmer 1999). Feeding such cell cultures with loganin increased alkaloid production considerably, by adding also tryptamine, high levels (ca 400 mg/l) of alkaloids could be obtained (Whitmer et al. 2002a,b). Overexpressing AS in hairy roots resulted in an increased level of tryptophane and tryptamine, but no increase of the major alkaloids. Again confirming the limiting role of the iridoid pathway (Hughes et al. 2004a). In combination with TDC a similar result was obtained, whereas overexpression of TDC alone gave an increase in serpentine (Hughes et al. 2004b).

Conclusions

There are over 100 indole alkaloids produced by C. roseus but the biosynthetic pathway to these alkaloids is not fully characterized yet. Recently, much progress was achieved in the terpenoid pathway especially the discovery of the MEP pathway leading to the isoprenoid formation. It was confirmed that in C. roseus, secologanin is derived from this pathway and the enzyme converting loganin to secologanin was characterized. Although the MEP pathway was given much attention in microbes, in C. roseus so far only three early steps in the pathway including enzymes and gene cloning were reported. In the last few years, the majority of work done in C. roseus focussed on the regulation of alkaloid production via many different applications such as feeding precursors, elicitation or metabolic engineering. Jasmonate is a well-established general inducer of a large number of genes in the pathway resulting in an improved alkaloid production. Overexpression of biosynthetic genes in C. roseus has so far failed to significantly increase sustainable production of the desired alkaloids. Joining expression of regulatory genes together with those controlling limiting steps that are not upregulated by the regulatory genes in the pathway may be of interest to overcome these problems. Still several parts of the pathway need to be elucidated at the level of intermediates. Proteomics and metabolomics approaches may be useful to identify the genes and enzymes involved. However, one need to consider also the involvement of transport in the regulation of the biosynthesis as different parts of the pathway are present in different cellular compartments and even different cells.

Copyright information

© Springer Science+Business Media B.V. 2007

Authors and Affiliations

  1. 1.Department of Pharmacognosy, Section of Metabolomics, Institute of Biology LeidenLeiden UniversityLeidenThe Netherlands
  2. 2.Department of Botany, Aswan Faculty of ScienceSouth Valley UniversityAswanEgypt