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Biosynthetic diversity in plant triterpene cyclizationDereth R Phillips, Jeanne M Rasbery, Bonnie Bartel and Seiichi PT Matsuda
Plants produce a wealth of terpenoids, many of which have
been the tools of healers and chefs for millennia. Recent
research has led to the identification and characterization of
many genes that are responsible for the biosynthesis of
triterpenoids. Cyclases that generate sterol precursors can be
recognized with some confidence on the basis of sequence;
several catalytically important residues are now known, and the
product profiles of sterol-generating cyclases typically reflect
their phylogenetic position. By contrast, the phylogenetic
relationships of cyclases that generate nonsteroidal triterpene
alcohols do not consistently reflect their catalytic properties
and might indicate recent and rapid catalytic evolution.
Addresses
Department of Biochemistry and Cell Biology and Department of
Chemistry, Rice University, 6100 Main Street, Houston, TX 77005, USA
Corresponding author: Matsuda, Seiichi PT ([email protected])
Current Opinion in Plant Biology 2006, 9:305–314
This review comes from a themed issue on
Physiology and metabolism
Edited by Eran Pichersky and Krishna Niyogi
Available online 3rd April 2006
1369-5266/$ – see front matter
# 2005 Elsevier Ltd. All rights reserved.
DOI 10.1016/j.pbi.2006.03.004
IntroductionPlants have long been known to synthesize a plethora of
small molecules, and plant genome sequencing is reinfor-
cing the view that plants devote considerable efforts
towards developing chemical solutions to biological prob-
lems. Terpenoids are metabolites of isopentenyl pyro-
phosphate (IPP) oligomers and comprise the largest group
of plant natural products, with over 20 000 known mem-
bers. Triterpenoids are synthesized from IPP via the 30-
carbon intermediate squalene, and include sterols, ster-
oids, and triterpenoid saponins (Figure 1). In addition to
sterols (which are 6,6,6,5-tetracycles derived from lanos-
terol or cycloartenol), nearly 100 additional triterpenoid
skeletons have been described [1��]. Cycloartenol and
lanosterol can serve as precursors to membrane sterols and
steroid hormones. Other triterpenes have less well-
defined roles, but many might act in plant defense.
Triterpenoid carbon frameworks are cyclized by mem-
bers of the oxidosqualene cyclase (OSC) family, which
has expanded greatly in plants. In this review, we
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highlight recent progress in the study of the enzyme
families that generate triterpene skeletal diversity.
Oxidosqualene cyclases that utilize theprotosteryl cationOxidosqualene cyclases (OSCs) convert oxidosqualene to
one or more cyclic triterpene alcohols with up to six
carbocyclic rings (Figure 1). Plants biosynthesize diverse
triterpenoids and encode multiple OSC enzymes to form
these skeletons (Table 1). For example, the sequenced
genomes of Arabidopsis thaliana and Oryza sativa (rice)
encode 13 [1��,2] and nine apparent OSC enzymes,
respectively. Genome mining, heterologous expression,
and biochemical characterization of the encoded proteins
(Table 1) have provided substantial insight into the
triterpenoid biosynthetic capabilities of plants.
Cycloartenol synthase (CAS) converts oxidosqualene to
cycloartenol through the protosteryl cation intermediate
(Figure 1) and was the basal plant OSC from which others
derived [3��]. The Arabidopsis CAS1 cDNA was cloned by
screening extracts from a yeast lanosterol synthase mutant
(erg7) that was transformed with random ArabidopsiscDNAs for the ability to cyclize oxidosqualene [4]. This
isolation facilitated the subsequent homology-based iden-
tification of other OSCs. Plant CAS genes have now been
cloned and characterized from numerous eudicots, several
monocots, and a gymnosperm (Table 1, Figure 2), consis-
tent with biochemical evidence of CAS activity throughout
seed plants [5–7]. The similarity of plant CAS genes to
those in amoebae [8] and bacteria [9] suggests that the
known cycloartenol synthases are orthologs, and that
cycloartenol synthase predates the emergence of plants.
Lanosterol is the initial carbocyclic sterol precursor in
animals, fungi, and trypanosomatids. Although substan-
tial labeling experiments support cycloartenol rather than
lanosterol as the major plant sterol precursor [5,10],
lanosterol biosynthesis has been demonstrated in a few
plants (e.g. in the latex of several Euphorbia species [11]).
Intriguingly, the Arabidopsis protein most similar to CAS1
(At3g45130, 65% identical) encodes a lanosterol synthase
(LSS) [12��]. The presence of probable At3g45130/LSS
orthologs in the asterids Taraxacum officinale and Panaxginseng and the eurosid Luffa cylindrica (66–69% identical;
Figure 2) suggests that lanosterol synthase is broadly
distributed among eudicots. The maintenance of CAS
in all examined plant lineages (Table 1), despite an
apparent ability of at least some plants to produce lanos-
terol [12��], implies that plants require some cycloartenol
metabolites that cannot be made from lanosterol. Muta-
tional analyses have shown that Tyr410, His477, and
Current Opinion in Plant Biology 2006, 9:305–314
306 Physiology and metabolism
Figure 1
A simplified scheme of plant triterpenoid biosynthesis. Farnesyl diphosphate synthase (FPS) isomerizes isopentenyl diphosphate (IPP) and
dimethylallyl diphosphate (DMAPP) to farnesyl diphosphate (FPP), which squalene synthase (SQS) converts to squalene. Squalene epoxidase
(SQE) oxidizes squalene to 2,3-oxidosqualene. OSC enzymes cyclize 2,3-oxidosqualene through cationic intermediates (e.g. the protosteryl cation,
the dammarenyl cation and others not shown) to triterpene alcohols or aldehydes. A few of the characterized OSC enzymes and products
listed in Table 1 are illustrated. OSC products can be further modified by multiple enzymes to form membrane sterols, brassinosteroids, saponins,
and other compounds. bAS1, b-amyrin synthase; LUP, lupeol synthase; MRN1, marneral synthase; PP, diphosphate; THA1, thalianol synthase.
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Biosynthetic diversity in plant triterpene cyclization Phillips et al. 307
Table 1
Characterized plant oxidosqualene cyclases.
Synthase Plant Name (Genbank accession)a Productsb (product identification method [reference[s]])
Cycloartenol Abies magnifica CAS1 (AAG44096) Cycloartenol (NMR, GC;c)
Cycloartenol A. thaliana At2g07050/CAS1 (P38605) Cycloartenol (NMR, IR, MS [4])
Cycloartenol B. platyphylla BPX1 (BAB83085)
BPX2 (BAB83086)
Cycloartenol (LC-MS [53])
Cycloartenol C. speciosus CSOSC1 (BAB83253) Cycloartenol (LC-MS [38])
Cycloartenol C. pepo CPX (BAD34644) Cycloartenol (LC-MS [17��])
Cycloartenol G. glabra GgCAS1 (BAA76902) Cycloartenol [54]
Cycloartenol L. cylindrica LcCAS1 (BAA85266) Cycloartenol [55]
Cycloartenol P. ginseng PNX (BAA33460) Cycloartenol (HPLC [56])
Cycloartenol P. sativum CASPEA (BAA23533) Cycloartenol [57]
Lanosterol A. thaliana At3g45130/LSS1/PEN7 Lanosterol (GC-MS, NMR [12��])
Cucurbitadienol C. pepo CPQ (BAD34645) Cucurbitadienol (LC-MS, NMR [17��])
b-Amyrin Avena strigosa AsbAS1 (CAC84558) b-Amyrin (Genetic analysis, HPLC [19])
b-Amyrin B. platyphylla BPY (BAB83088) b-Amyrin (LC-MS [53])
b-Amyrin Euphorbia tirucalli EtAS (BAE43642) b-Amyrin (GC-MS, NMR [58])
b-Amyrin G. glabra GgbAS1 (BAA89815) b-Amyrin (LC-MS [59])
b-Amyrin M. truncatula MtAMY1/bAS1 (CAD23247) b-Amyrin (GC-MS, NMR [23]; HPLC [24])
b-Amyrin P. ginseng PNY1 (BAA33461)
PNY2 (BAA33722)
b-Amyrin (HPLC, MS, NMR [56,60])
b-Amyrin P. sativum PSY (BAA97558) b-Amyrin (LC-MS, GC-MS, NMR [32])
Lupeol B. platyphylla BPW (BAB83087) Lupeol (LC-MS [53])
Lupeol G. glabra GgLUS1 (BAD08587) Lupeol (LC-MS [26��])
Lupeol O. europaea OEW (BAA86930) Lupeol (LC-MS, NMR [29])
Lupeol T. officinale TRW (BAA86932) Lupeol (LC-MS, NMR [29])
Thalianol A. thaliana At5g48010/THA1/PEN4 Thalianol (NMR [39��])
Marneral A. thaliana At5g42600/MRN1/PEN5 Marneral (NMR [40��])
Isomultiflorenol L. cylindrica LcIMS1 (BAB68529) Isomultiflorenol (LC-MS [30])
Mixed A. thaliana At1g78970/LUP1 Lupeol, 3b,20-dihydroxylupane, b-amyrin, germanicol, taraxasterol
and c-taraxasterol (GC, MS [33]; NMR [33–35])
Mixed A. thaliana At1g78960/LUP2/
YUP8H12R.43
b-Amyrin, taraxasterol, tirucalla-7,21-dien-3b-ol, lupeol, bauerenol,
butyrospermol, multiflorenol, a-amyrin and c-taraxasterol
(HPLC, NMR [2,36]; GC-MS [2]; LC-MS [36])
Mixed A. thaliana At1g66960/LUP5 Tirucalla-7,21-dien-3b-ol and additional uncharacterized (LC-MS [37])
Mixed A. thaliana At1g78500/PEN6 Bauerenol, lupeol, a-amyrin and additional uncharacterized (LC-MS [37])
Mixed C. speciosus CsOSC2 (BAB83254) Lupeol, germanicol, b-amyrin and additional uncharacterized (LC-MS [38])
Mixed L. japonicus AMY2 (AAO33580) Lupeol, b-amyrin and additional uncharacterized (HPLC [24])
Mixed P. sativum PSM (BAA97559) a-Amyrin, b-amyrin, d-amyrin, c- taraxasterol, butyrospermol,
lupeol, germanicol and taraxasterol (LC-MS, GC-MS, NMR [32])
a A. thaliana PEN and LUP designations are from [2].b For OSC enzymes with mixed products, major products are listed in bold text if known.c JBR Herrera, PhD thesis, Rice University, 1999. Abbreviations: GC, gas chromatography; HPLC, high pressure LC; IR, infrared spectroscopy; LC,
liquid chromatography; MS, mass spectrometry; NMR, nuclear magnetic resonance.
Ile481 cooperate to control product specificity in Arabi-dopsis CAS1 [13–15]. In fact, Arabidopsis CAS1 can be
converted to an accurate lanosterol synthase with only
two amino-acid substitutions: His477 to Asn and Ile481 to
Val [16��]. It is intriguing that Arabidopsis LSS contains
residues that correspond to these mutations. This pre-
cedent suggests that only a small evolutionary step could
convert CAS to lanosterol synthase if natural selection
favored a lanosterol route in plants.
Other enzymes that form the protosteryl cation have arisen
from CAS gene duplication and diversification. For exam-
ple, Cucurbita pepo cucurbitadienol synthase (CPQ) is
closely related (65–71% identical) to both cycloartenol
and lanosterol synthases (Figure 2) but produces cucurbi-
tadienol ([17��]; Figure 1), a precursor of cucurbitacins,
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which are bitter compounds that might act as antifeedants
(reviewed in [18]). The sequence similarity of plant
cycloartenol, lanosterol, and cucurbitadienol synthases
(Figure 2) is consistent with relatively recent divergence
of lanosterol and cucurbitadienol synthases from an ances-
tral CAS via an evolutionary route that maintained the
protosteryl cation intermediate (Figure 1).
Cyclases that generate single triterpenesthrough the dammarenyl cationSeveral oxidosqualene cyclases that function in secondary
metabolism also have been reported to generate single
products. Lupeol synthases cyclize oxidosqualene to the
dammarenyl cation, promote ring expansion and annula-
tion to the lupyl cation, and terminate by abstracting the
C-29 proton to form lupeol (Figure 1; [1��]). Lupeol
Current Opinion in Plant Biology 2006, 9:305–314
308 Physiology and metabolism
Figure 2
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Biosynthetic diversity in plant triterpene cyclization Phillips et al. 309
synthases are found in Glycyrrhiza glabra, Betula platy-phylla, T. officinale, and Olea europea (Table 1); these
enzymes are 74–81% identical to one another and form
a clade that is distinct from other characterized OSCs
(Figure 2). The presence of eurosid and asterid genes in
this clade suggests that an accurate lupeol synthase
evolved before the divergence of asterids and eurosids.
b-Amyrin synthases also form the lupyl cation, but allow
further ring expansion and some rearrangement before
deprotonation to b-amyrin [1��]. Several OSCs from
eudicots and monocots produce b-amyrin accurately
(Table 1). These b-amyrin synthases are considerably
more distant from one another (48–50% identical) than
are the CAS enzymes (70–79% identical), and indepen-
dent origins of b-amyrin synthases in eudicots and mono-
cots have been proposed [19,20��].
Lupeol, b-amyrin, and their diverse metabolites are
implicated in various plant processes. b-Amyrin is a
precursor of saponins, which are triterpene glycosides
such as the antifungal saponin avenacin found in Avenaroots [19,20��,21]. b-Amyrin and its metabolites tend to
accumulate in specific tissues (see [22��] for the localiza-
tion of 31 Medicago saponins). Some of this localization
could be transcriptional, as indicated by the tissue-spe-
cific expression of b-amyrin synthase genes in Medicago[23,24], Lotus [24], Pisum [24], Centella [25], Glycyrrhiza[26��], and Avena [19,20��]. Lupeol synthase expression is
associated with root nodulation in several plants. For
example, Glycyrrhiza lupeol synthase is expressed in
nodules and cultured cells, the same areas in which the
lupeol metabolite betulinic acid is detected [26��]. In
Vicia faba nodule outer cortex, 82% of the organic-soluble
material is betulin, a lupeol metabolite, and another 7% is
lupeol [27]. Moreover, a partial OSC sequence
(CAA75588), which was recovered in a screen for genes
that are induced during Medicago truncatula nodulation
[28], is closely related to lupeol synthases [24,29] and is
expressed most highly in root nodules [24]. The role of
lupeol in root nodule biology remains to be elucidated.
In addition to lupeol and b-amyrin synthases, less broadly
distributed enzymes can also have high product
(Figure 2 Legend) Predicted phylogenetic relationships among characterize
enzymes (colored) from Table 1 and uncharacterized enzymes (in black) we
using the Clustal W method. The untrimmed alignment was used to generate
using PAUP 4.05b [52]. The bootstrap method was performed for 100 replic
criterion. Bootstrap values are listed at nodes. Characterized enzymes and c
products are enclosed in similarly colored boxes. GenBank accession numb
CAC84559; Avena ventricosa CS1, AAT38892; Centella asiatica OSCCCS, A
ABB76767; Allium macrostemon ALLOSC1, BAA84603; Taraxacum officinal
LcOSC2, BAA85267; Cucurbita pepo CPR, BAD34646; Avena ventricosa bA
CabAS, AAS01523; Aster sedifolius OXA1, AAX14716; Ricinus communis L
enzymes are indicated by ’Arabidopsis’ followed by the gene locus number
of the respective colored box. Mixed dammarenyl compounds are labeled ‘
according to the cation intermediate through which they create their produc
inconsistent with the overall cation-intermediate type of the clade.
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selectivity. Luffa cylindrica isomultiflorenol synthase
(LcIMS1) cyclizes oxidosqualene through a dammarenyl
cation to make isomultiflorenol [30], a bryonolic acid
precursor [31]. Temporal expression studies in L. cylin-drica cell cultures indicate that LcIMS mRNA levels
correlate with bryonolic acid accumulation [30].
Multifunctional cyclases that generatetriterpenes through the dammarenyl cationThe diversity of plant triterpenes emanates not only from
the radiation of the OSC gene family but also from the
ability of some family members to contribute multiple
products (Table 1). Several subfamilies of multifunc-
tional triterpene synthases use dammarenyl cation inter-
mediates. Orthologous mixed-amyrin synthases have
been characterized from the legumes Pisum sativum(i.e. PSM) [32] and Lotus japonicus (i.e. AMY2) [24].
Arabidopsis encodes several paralogous multifunctional
enzymes that biosynthesize b-amyrin, lupeol, taraxas-
terol, and/or related dammarenyl-derived compounds
(Table 1): At1g78970/LUP1 [33–35], At1g78960/LUP2
[2,36], At1g66960/LUP5 [37], and At1g78500/PEN6 [37].
The legume mixed-amyrin synthases share a recent
common ancestor with accurate b-amyrin synthases;
the Arabidopsis mixed-amyrin synthases are more distant
(Figure 2).
Multifunctional OSC enzymes have arisen repeatedly
during angiosperm evolution (Figure 2). A distant exam-
ple is the Costus speciosus CsOSC2, which makes lupeol,
germanicol, and b-amyrin [38] from the dammarenyl
cation. Rather surprisingly, its closest relatives are
cycloartenol synthases (67–70% identical), which use
the protosteryl cation intermediate (Figure 2). This rela-
tionship implies a recent evolutionary transition that
involved a dramatic catalytic change from the protosteryl
cation to the dammarenyl cation [3��].
Discovery of new triterpene skeletons bygenome miningGenome mining in Arabidopsis has uncovered two
enzymes that generate incompletely cyclized structures
that have not been characterized by classical natural
product isolation. {At5g48010}/THA1 [39] converts
d and predicted plant oxidosqualene cyclases. Characterized
re aligned with the MegAlign program (DNASTAR, Inc., Madison, WI)
a phylogram rooted with Dictyostelium discoideum CAS1 (AAF80384) [8]
ates with all characters weighted equally and distance as the optimality
losely related uncharacterized enzymes that are predicted to have similar
ers for uncharacterized enzymes are as follows: Avena strigosa CS1,
AS01524; Oryza sativa CAS1, AAF03375; Ricinus communis CAS,
e TRV, BAA86933; Panax ginseng PNZ1, BAA33462; Luffa cylindrica
S1, AAT38898; Panax ginseng bAS1, BAD15332; Centella asiatica
UP, ABB76766; and Euphorbia tirucalli EtOSC, BAE43643. A. thaliana
. The product(s) made by each enzyme type are listed to the right
mixed’. The two plant clades separated with a dashed line are labeled
ts (protosteryl or dammarenyl). Asterisks mark products that are
Current Opinion in Plant Biology 2006, 9:305–314
310 Physiology and metabolism
Figure 3
Predicted phylogenetic relationships among enzymatically characterized
and putative squalene epoxidases from sequenced plant genomes.
Sequences are from M. truncatula (Medicago SE1, CAD23249 and
Medicago SE2, AD23248), O. sativa (Oryza 1, Os03g12900 and Oryza 2,
Os03g12910), A. thaliana (At1g58440, At2g22830, At4g37760,
At5g24140, At5g24150 and At5g24160), and Populus trichocarpa
(Populus 1, eugene3.04180003; Populus 2, estExt_Genewise1_v1.C
LG II0395; Populus 3, estExt_fgenesh1_pg v1.C LG V0617; Populus 4,
fgenesh1_pg.C LG XIX000144) accessed through the US Department
of Energy (DOE) Joint Genome Institute website (http://genome.jgi-
psf.org/Poptr1/Poptr1.home.html). They were aligned with the MegAlign
program (DNASTAR, Inc., Madison, WI) using the Clustal W method.
Amino-acid residues that correspond to positions 60–522 from
At1g58440 were used to generate a phylogram that is rooted with
Saccharomyces ERG1 (CAA97201) using PAUP 4.05b [52]. The
bootstrap method was performed for 1000 replicates with all characters
weighted equally and distance as the optimality criterion. Boostrap
values are listed at nodes. Characterized enzymes are in bold font.
The shaded region outlines enzymes that seem most likely to encode
genuine squalene epoxidases on the basis of their similarity to the
characterized Medicago enzymes.
oxidosqualene to the tricyclic alcohol thalianol (Figure 1).
Triterpenoids that have the methyl substitution and
olefinic position of thalianol have not been found in
nature. At5g42600/MRN1 [40��] catalyzes an unusual
cyclization reaction: oxidosqualene is converted to a
bicyclic cation that undergoes rearrangement and A-ring
cleavage to generate a monocyclic aldehyde (Figure 1).
Marneral also has not been isolated from any natural
source but is suggested as a biosynthetic precursor of
iridals found in sword lilies [41]; these monocots are only
distantly related to the eudicot Arabidopsis. These exam-
ples demonstrate that heterologous expression of novel
OSC enzymes can provide a means to mine plant gen-
omes for new biosynthetic pathways and low-abundance
natural products.
Squalene epoxidasesOSC enzymes are a major radiation point in the triterpe-
noid pathway and facilitate the production of numerous
and diverse triterpenoids. Interestingly, plants also have
multiple genes that are predicted to encode squalene
epoxidase (SQE) enzymes, also known as squalene mono-
oxygenases. SQEs catalyze the first oxygenation step in
triterpene biosynthesis, converting squalene into the
OSC precursor 2,3-oxidosqualene (Figure 1).
The first cloned SQE gene, from Saccharomyces cerevisiae,was identified by complementation of the yeast ergosterol
biosynthetic mutant erg1 [42]. Two Medicago squalene
epoxidases that were identified by sequence similarity are
able to rescue the yeast erg1 mutant defect when hetero-
logously expressed [23], indicating that the encoded
enzymes function as squalene epoxidases.
In addition to the two biochemically characterized Med-icago SQEs [23], the sequenced genomes of Oryza, Popu-lus, and Arabidopsis (Figure 3) encode multiple predicted
SQEs. Each of these plants possesses genes that are
closely related (63–82% identical) to the characterized
Medicago SQEs, but Arabidopsis also has three SQE-like
genes (At5g24140, At5g24150 and At5g24160) that are
more diverged (44–48% identical, Figure 3). It remains to
be determined which of these more distant enzymes are
genuine SQEs and whether any have adopted new cat-
alytic functions.
Functional implications of triterpenediversificationSeveral forces could drive expansion in the SQE and OSC
families. Phylogenic analyses of Arabidopsis and Oryzareceptor-like kinases reveal that the expansion of a parti-
cular sub-family after speciation can indicate that mem-
bers have evolved to act in defense or disease resistance
[43��]. Conversely, very little post-speciation expansion is
observed when sub-family members function in devel-
opment or central metabolism [43��]. This observation
might begin to explain the divergence patterns within the
Current Opinion in Plant Biology 2006, 9:305–314
plant OSC family. Minimal post-speciation duplication is
observed in the CAS subfamily (Figure 2), and CAS
enzymes from the eudicot Arabidopsis, the monocot C.speciosus, and the gymnosperm Abies have remained very
similar to one another (�75% identical). These observa-
tions are consistent with a housekeeping function for
cycloartenol as a precursor to bulk membrane sterols
and brassinosteroids. By contrast, substantial lineage-
specific expansion is apparent in plant OSC sub-families
that do not use the protosteryl cation intermediate
(Figure 2), consistent with known and postulated defense
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Biosynthetic diversity in plant triterpene cyclization Phillips et al. 311
roles for many non-steroidal triterpenes and suggesting
that plants derive advantage from synthesizing diverse
triterpene skeletons. Although the neighboring positions
of Arabidopsis LUP1 and LUP2 (80% identical) on chro-
mosome 1 imply recent duplication, the product profiles
of these multifunctional OSCs have already diverged
(Table 1).
Why some OSCs produce multiple products is not known
but some of these products might represent evolution in
progress. Numerous mutagenesis and directed evolution
experiments demonstrate that small changes in OSC
sequences can expand product diversity (reviewed in
[44]). If a new product confers an advantage, subsequent
mutations might enhance the production of the beneficial
product. Interestingly, Arabidopsis contains two subfami-
lies of enzymes for which orthologs from other plant
species have not been identified (Figure 2). Of the
characterized enzymes in these subfamilies, four are
multifunctional and two make compounds not yet found
in plants (Table 1).
Control of triterpene metabolismGene duplication, in addition to allowing for product
diversification, allows the differential expression of family
members in various plant tissues. For example, Arabidop-sis maintains two genes that encode farnesyl diphosphate
synthase (FPS), which acts early in terpene biosynthesis
(Figure 1). Arabidopsis FPS1 is expressed in most tissues,
whereas FPS2 expression is restricted to specific devel-
opmental stages [45]. Triterpene biosynthetic genes are
induced to produce terpenoids under specific conditions,
including various biotic stresses. For example, b-amyrin
synthases are induced by a yeast elicitor in Tabernaemon-tana divaricata [46] and M. truncatula [23] cultures, con-
sistent with a role for b-amyrin as a precursor to antifungal
saponins (Figure 1). In addition, treatment with methyl
jasmonate (MeJA), a phytohormone that is involved in
plant stress responses [47], increases the message levels of
confirmed and predicted b-amyrin synthase genes from
Medicago [23], Glycyrrhiza [26��], and Centella asiatica [25]
and is accompanied by increased production of triterpene
saponins [23,25,26��].
In some cases, genetic linkage could provide an efficient
mechanism for the transcriptional control of triterpenoid
biosynthetic genes. In Avena, a cluster of five loci that are
involved in avenacin biosynthesis [20��] is encoded near
the AsbAS1 b-amyrin synthase gene [19]. It will be
interesting to learn whether such clustering is found
for additional plant triterpene metabolic genes.
Metabolic channeling, in which biosynthetic enzymes are
co-localized within a cellular organelle or specific plant
organ, might contribute to pathway control. Substrate
channeling could promote efficient triterpenoid produc-
tion by protecting intermediates from seizure by other
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enzymes that make different products. Channeling might
provide a mechanism to isolate potentially toxic metabo-
lites within particular organelles or might confer benefits
to plants that are challenged with infectious agents or
changing environmental conditions (reviewed in [48��]).
Metabolic channeling may be facilitated by coordinate
expression of genes that encode different steps of a
pathway. For example, when Medicago cell cultures are
treated with MeJA, one squalene epoxidase gene (SE2) is
dramatically upregulated [23]. Genes encoding squalene
synthase and b-amyrin synthase, which precede and
follow SE2 in saponin production, are similarly MeJA-
induced, but SE1 and CAS are not [23]. This coordinate
regulation might indicate separate metabolic channels for
saponin and sterol production in this organism.
Conclusions and future prospectsThrough genome sequencing, heterologous expression,
enzymology, and analytical chemistry, a growing number
of plant triterpenes are being associated with the enzymes
that produce them. Although relatively few OSC
enzymes have been catalytically characterized
(Table 1), progress in this area is rapidly accelerating.
Most characterized plant OSCs are from angiosperms
(Table 1); future OSC characterizations from more basal
land plants would clarify orthologous relationships in the
family. As the number of sequenced and characterized
OSC and SQE enzymes increases, so will our under-
standing of the relationships between various enzyme
subfamilies, which in turn will allow more accurate pre-
dictions of the products of uncharacterized synthases and
more facile metabolic engineering for pharmaceutical or
agricultural benefit.
Compounding the challenge of completing triterpenoid
accounting is the complexity of the metabolism that can
follow oxidosqualene cyclization (reviewed in [49]). Elab-
orations of the triterpene skeleton can include hydrox-
ylation by P450-dependent monooxygenases, alkylation
by methyltransferases, and glycosylation by glycosyltrans-
ferases [50��]; these and other modifications can be
essential for bioactivity. For example, more than 20
enzymatic steps are needed to convert cycloartenol into
the active hormone brassinolide [49]. Although progress
has been made in a few pathways, many of the specific
enzymes that carry out these reactions remain to be
characterized.
The model plant A. thaliana was not known as a source of
novel triterpenes, but the study of its OSCs provided
several interesting observations. In addition to the first
cycloartenol synthase [4], Arabidopsis provided the first
characterized lanosterol synthase from the plant kingdom
[12��], and sequence comparisons suggest that this func-
tion might be shared by additional eudicots (Figure 2).
The characterization of the Arabidopsis thalianol [39��]
Current Opinion in Plant Biology 2006, 9:305–314
312 Physiology and metabolism
and marneral [40��] synthases led to the discovery of
compounds not yet found in nature, implying that our
list of known triterpene skeletons is far from complete
and demonstrating a new means of triterpene discovery.
The Arabidopsis LUP1 enzyme provided the first example
of a multifunctional OSC [33–35], and multifunctionality
is now established as a recurring theme in the OSC family
(Table 1; Figure 2). It is likely that additional insights will
arise from the characterization of the remaining five
Arabidopsis OSC family members (Figure 2).
Whereas the biological roles of sterols and brassinoster-
oids are well known (reviewed in [51]), the functions of
other triterpenoid skeletons are only beginning to be
elucidated. It will be informative to continue the exam-
ination of the expression patterns of triterpene biosyn-
thetic genes and proteins in the relevant plants during
development and in response to biotic and abiotic chal-
lenges. Moreover, phenotypic analysis of plants that lack
or overexpress particular triterpene biosynthetic genes
will be necessary to fully understand triterpene function.
An Avena mutant screen yielded eight loci that were
defective in saponin accumulation [21]; one of these is
defective in a b-amyrin synthase gene and is the only
published example of a plant OSC mutant [19]. The
saponin-deficient oat mutants are susceptible to infection
by Gaeumannomyces graminis, providing a biological role
for b-amyrin in fungal disease resistance [21]. Genetic
analyses of the roles of certain triterpenes in Arabidopsiswill probably be complicated by the genetic linkage of
some OSC genes and the partial redundancy of multi-
functional enzymes that synthesize both b-amyrin and
lupeol, among other products (Table 1). Nevertheless,
available evidence suggests that straightforward mutant
analysis might reveal the biological consequences of, for
example, losing cycloartenol or lanosterol synthase. The
remarkable diversity of plant triterpene products uncov-
ered to date suggests that a corresponding wealth of
triterpene function awaits discovery.
AcknowledgementsWe thank Diana Dugas, Mariya Kolesnikova, William K Wilson, AndrewWoodward, and Quanbo Xiong for comments on the manuscript andapologize to colleagues we were unable to cite due to space limitations.The authors’ triterpene research is supported by the US National ScienceFoundation (NSF) (MCB-0209769) and the Robert A Welch Foundation(C-1323 and C-1309). JMR was supported in part by a training grant fromthe National Institutes of Health (T32-GM08362).
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