arabidopsis thaliana type i isopentenyl diphosphate ... · insertion line 014625, exon 4, 1651...
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The Arabidopsis thaliana Type I Isopentenyl DiphosphateIsomerases Are Targeted to Multiple SubcellularCompartments and Have Overlapping Functions inIsoprenoid Biosynthesis W
Michael A. Phillips,a,1 John C. D’Auria,a Jonathan Gershenzon,a,2 and Eran Picherskyb
a Max Planck Institute for Chemical Ecology, D-07745 Jena, Germanyb Department of Molecular, Cellular, and Developmental Biology, University of Michigan, Ann Arbor, Michigan 48109-1048
To form the building blocks of isoprenoids, isopentenyl diphosphate (IPP) isomerase activity, which converts IPP to dimethylallyl
diphosphate (DMAPP), appears to be necessary in cytosol, plastids, and mitochondria. Arabidopsis thaliana contains only two
IPP isomerases (Isopentenyl Diphosphate Isomerase1 [IDI1] and IDI2). Both encode proteins with N-terminal extensions similar
to transit peptides and are expressed in all organs, with IDI1 less abundant than IDI2. Examination of enhanced green fluorescent
protein fusions established that IDI1 is mainly in the plastid, whereas IDI2 is mainly in the mitochondria. Both proteins are also in
the cytosol as a result of their translation from naturally occurring shorter transcripts lacking transit peptides, as demonstrated
by59 rapid amplificationofcDNAendscloning. IPP isomeraseactivity in the cytosol wasconfirmedbyuniform labelingof IPP-and
DMAPP-derived units of the cytoplasmic isoprenoid product, sitosterol, when labeled mevalonate was administered. Analysis of
mutant lines showed that double mutants were nonviable, while homozygous single mutants had no major morphological or
chemical differences from the wild type except for flowers with fused sepals and underdeveloped petals on idi2 mutants. Thus,
each of the two Arabidopsis IPP isomerases is found in multiple but partially overlapping subcellular locations, and each can
compensate for the loss of the other through partial redundancy in the cytosol.
INTRODUCTION
Isoprenoids are essential compounds in all organisms, but their
largest structural variety occurs in plants. There, they serve not
only universal roles as photosynthetic pigments, redox cofac-
tors, and hormones but also specialized ecological roles as
feeding deterrents, pollination vector attractants, and phyto-
alexins. Animals and fungi produce the precursors for isoprenoid
biosynthesis via the mevalonic acid pathway, and many bacteria
synthesize the same building blocks through the methylerythritol
phosphate (MEP) pathway. Plants, by contrast, possess both
pathways, with the mevalonic acid pathway operating in the
cytosol (McGarvey and Croteau, 1995) and the MEP pathway
operating in plastids (Rodrıguez-Concepcion and Boronat,
2002). Although proceeding via chemically distinct routes, the
two pathways converge at the formation of isopentenyl diphos-
phate (IPP). Isoprenoid biosynthesis also requires the formation
of dimethylallyl diphosphate (DMAPP), a double bond isomer of
IPP, as both of these C5 diphosphate compounds are used by
prenyltransferases to form the C10, C15, C20, and larger prenyl
diphosphates that serve as precursors in the monoterpene,
sesquiterpene, and diterpene biosynthetic pathways, respec-
tively. In each reaction series, DMAPP is the initial allylic diphos-
phate to which successive units of IPP are added via head-to-tail
condensations (Burke et al., 1999).
While the plastidic MEP pathway results in the synthesis of
both IPP and DMAPP (Hoeffler et al., 2002), the cytosol-localized
mevalonate pathway produces only IPP. IPP can be isomerized
to DMAPP by isopentenyl diphosphate isomerase (IDI), a divalent
metal ion–requiring enzyme found in all living organisms
(Gershenzon and Kreis, 1999). IDI can also catalyze the reverse
reaction from DMAPP to IPP, but the equilibrium favors the forward
reaction. Animals, fungi, and some bacteria contain an enzyme
designated type I IPP isomerase (Muehlbacher and Poulter, 1988;
Anderson et al., 1989; Carrigan and Poulter, 2003); other bacteria
have a nonhomologous type II IPP isomerase (Kaneda et al., 2001).
In plants, only DNA sequences encoding proteins homologous
with type I IPP isomerase have been identified to date (Blanc and
Pichersky, 1995; Campbell et al., 1997; Cunningham and Gantt,
2000; Nakamura et al., 2001; Page et al., 2004).
Based on the pathways of isoprenoid biosynthesis found in
plants, the molar ratio of IPP to DMAPP needed to make various
terpenoid classes varies from 1:1 for monoterpenes to 2:1 for
sesquiterpenes and sterols, 3:1 for diterpenes, carotenoids, and
phytol, and much higher for long-chain polyprenols and polyter-
penes (Gershenzon and Kreis, 1999) (Figure 1). Thus, by con-
trolling the conversion of IPP to DMAPP, IPP isomerase may
have an important role in regulating the biosynthesis of the major
1 Current address: Laboratori de Genetica Molecular Vegetal, ConsejoSuperior de Investigaciones Cientificas, Institut de Recerca i TecnologiaAgroalimentaries, Barcelona 08034, Spain.2 Address correspondence to [email protected] authors responsible for distribution of materials integral to thefindings presented in this article in accordance with the policy describedin the Instructions for Authors (www.plantcell.org) are: MichaelA. Phillips ([email protected]) and John C. D’Auria ([email protected]).W Online version contains Web-only data.www.plantcell.org/cgi/doi/10.1105/tpc.107.053926
The Plant Cell, Vol. 20: 677–696, March 2008, www.plantcell.org ª 2008 American Society of Plant Biologists
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types of isoprenoid products formed. In principle, DMAPP for
isoprenoid formation in nonplastidic compartments could arise
not only from IPP isomerase but also directly from the plastidial
MEP pathway via transport from plastids to other sites of
isoprenoid biosynthesis. However, since the IPP:DMAPP ratio
produced in vitro by 1-hydroxy-2-methylbutenyl 4-diphosphate
reductase, the last step in the MEP pathway, is 6:1 (Rohdich
et al., 2003; Eisenreich et al., 2004), IPP isomerase activity might
still be necessary to optimize the relative amounts of these two
C5 intermediates for efficient isoprenoid biosynthesis both in the
plastids and elsewhere in the cell.
With the distribution of the various branches of isoprenoid
biosynthesis in different subcellular locations, the compartmen-
tation of IPP isomerase could have a significant influence on the
flux to different end products. Intriguingly, most known plant
genes encoding type I IPP isomerases appear to encode pro-
teins with N-terminal transit peptides, suggesting organellar
localization (Figure 2). For example, Clarkia breweri IDI1 and
IDI2 have N-terminal extensions of 70 and 69 amino acids,
respectively, compared with Escherichia coli IDI (Blanc and
Pichersky, 1995), and Arabidopsis thaliana has been shown to
contain only two IPP isomerase genes (At5g16440, designated
IDI1, and At3g02780, designated IDI2), both of which encode a
protein with an N-terminal extension (compared with the E. coli
IPP isomerase) that has been shown to not be necessary for
catalytic activity (Campbell et al., 1997) (Figure 2). An exception
was found in tobacco (Nicotiana tabacum), in which two cDNAs,
designated IDI1 and IDI2, were obtained, one encoding a protein
with an apparent transit peptide, while the other did not. When
these proteins were expressed as GFP fusions in this plant, the
tobacco IDI1 protein was found to be targeted to the plastid,
while the IDI2 protein was found in the cytosol (Nakamura et al.,
2001). However, it was not conclusively demonstrated that the
tobacco IDI2 cDNA was in fact a copy of a full-length transcript
(e.g., by comparison with a genomic sequence or by primer
extension experiments).
The presence of N-terminal extensions on the IPP isomerases
found in Arabidopsis and other species suggests that they might
be directed to plastids or mitochondria, both sites of isoprenoid
formation in plants. Plastids, in addition to the MEP pathway,
also contain biosynthetic machinery for monoterpene, diterpene,
gibberellin, carotenoid, and phytol production. Mitochondria, on
the other hand, are sites of ubiquinone biosynthesis (Lutke-
Brinkhaus et al., 1984; Ohara et al., 2006) and form other iso-
prenoids in organisms outside the plant kingdom (Felkai et al.,
1999; Marbois et al., 2005). Curiously, in both C. breweri and
Arabidopsis, none of the IDI proteins appear to be targeted to the
cytosol (since they all appear to have transit peptides), even
though this compartment produces sesquiterpenes, sterols, and
dolichols and the cytosolic mevalonate pathway supplies only
IPP and not DMAPP. Conceivably, alternative splicing or alter-
native transcription start sites of the IDI genes could lead to
cytosolic protein targeting, as is known for another Arabidopsis
protein involved in isoprenoid biosynthesis, farnesyl diphosphate
synthase1, which can be located in both the cytosol and the
mitochondria (Cunillera et al., 1997). Thus, it is not clear at pres-
ent which plant compartments possess IPP isomerase activity
and whether such activity is essential for the synthesis of iso-
prenoid compounds in that compartment.
Here, we present evidence that in Arabidopsis, one IPP isom-
erase (IDI1) is targeted to plastids, the other (IDI2) is targeted to
mitochondria, and additional IPP isomerase activity encoded by
both genes is present in the cytoplasm. While even one func-
tional IDI gene is sufficient to support growth and development,
Figure 1. Overview of Isoprenoid Biosynthesis by Compartment in a Higher Plant Cell.
Indicated are the IPP and DMAPP requirements for various classes of isoprenoids. AcCoA, acetyl-CoA; FPP, farnesyl diphosphate; GPP, geranyl
diphosphate; GGPP, geranylgeranyl diphosphate; G3P, glyceraldehyde 3-phosphate; MEP, methylerythritol phosphate pathway; MVA, mevalonate
pathway; OPP, diphosphate moiety. The block arrows denote multiple steps, and the asymmetric arrows reflect the expected equilibrium of the
reversible IPP isomerase (IDI) reaction.
678 The Plant Cell
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we demonstrate that IDI1 and IDI2 are not completely redundant
and play distinct roles in isoprenoid metabolism.
RESULTS
Transcripts of Arabidopsis IDI1 and IDI2 Encode Proteins
with an N-Terminal Extension
The present annotation in The Arabidopsis Information Resource
(TAIR; http://www.plantgdb.org/AtGDB/) shows that the IDI1
gene contains six exons and five introns, as does IDI2 (Figure 3).
These two genes encode proteins of 291 and 284 amino acids,
respectively, which contain N-terminal extensions of 75 and 68
residues, respectively, compared with the sequence of E. coli IDI
(Figure 2). This extension, present in most plant IDI sequences
(Cunningham and Gantt, 2000), is quite variable, with the excep-
tion of the 16 residues just upstream of the Met residue in the
equivalent position to the starting Met in the E. coli sequence
(Figure 2). This 16-residue sequence starts with a Met that is
conserved in almost all known plant IDI sequences and contains
Figure 2. Amino Acid Sequence Alignment of Plant, Yeast, and E. coli Type I IPP Isomerase Proteins.
At, Arabidopsis thaliana IDI1 (At5g16440) and IDI2 (At3g02780); Cb, Clarkia breweri IPP isomerase 1 (X82627) and IPP isomerase 2 (U48963); Ec,
Escherichia coli IPP isomerase (NP_417365); Sc, Saccharomyces cerevisiae IPP isomerase (P15496). Residues in black are absolutely conserved in all
sequences shown, while those in dark gray and light gray are conserved among 70 and 50%, respectively. Alignments were performed using Blosum62
(AlignX, VectorNTI 10) with a gap-opening penalty of 10 and a gap-extension penalty of 0.1. Asterisks indicate Met residues conserved in nearly all
known plant species. The horizontal bar represents the conserved 16-residue region of the N-terminal extension (relative to E. coli IDI).
Figure 3. Genomic Structures of Arabidopsis IDI1 (At5g16440) and IDI2 (At3g02780).
Green arrows indicate exons, while the thin yellow lines in between indicate introns. The red boxes show the 59 untranslated regions. The 39 untranslated
regions are shown as yellow boxes. qRT-PCR forward and reverse primers are represented as black arrowheads. The insertion sites of the T-DNA
mutants used in this study are indicated with black vertical lines. They are idi1-1 (GABI insertion line 217HO4, exon 3, 799 nucleotides downstream of
the predicted start codon), idi1-2 (SALK insertion line 006330, intron 3, 841 nucleotides downstream of the predicted start codon), and idi2-1 (SALK
insertion line 014625, exon 4, 1651 nucleotides downstream of the predicted start codon).
The Role of IPP Isomerase in Arabidopsis 679
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a second conserved Met residue halfway through (Cunningham
and Gantt, 2000) (Figure 2). Interestingly, yeast IDI also contains
a large N-terminal extension relative to E. coli IDI, but this
sequence as a whole shows little similarity to the corresponding
plant sequences, with the exception of the above-mentioned
16-residue region. The yeast sequence does not contain any Met
residues in this region (Figure 2), but since some enzymes of the
mevalonate pathway have been associated with mitochondria in
yeast (Shimizu et al., 1971), it may indeed serve some non-
catalytic function. When the N-terminal extension upstream of
this 16-residue region, which is also highly variable between At
IDI1 and At IDI2, is discounted, At IDI1 and At IDI2 are 91%
identical to each other, 84 and 83% identical, respectively, to C.
breweri IDI1, 45 and 46% identical, respectively, to yeast IDI, and
27 and 26% identical, respectively, to E. coli IDI. Interestingly, the
first exon of At IDI1 and At IDI2 (236 and 215 nucleotides,
respectively, starting from the initiating ATG codon) encodes the
entire N-terminal part of the protein that has no equivalent in the
E. coli IDI protein plus a few additional amino acids.
The prediction of N-terminal extensions for both IDI1 and IDI2,
as outlined above, is consistent with other available sequence
information for these genes. For example, the starting codon of
IDI1 is likely to be as indicated in Figure 2 due to the presence of
an in-frame stop codon in the 59 untranslated region (UTR) of IDI1
at position �9 relative to the predicted initiating ATG in several
available cDNAs. For IDI2, available cDNAs include a maximum
of 26 nucleotides of 59 UTR sequence upstream of the predicted
ATG initiating codon, and this region does not include any
additional start codons or stop codons in-frame with the pro-
posed start codon. However, an in-frame stop codon is present
at �57 with no additional start codons in between, making it
extremely likely that the proposed start codon for IDI2 is also the
correct one. Examination of 36 cDNAs for IDI1 and 41 cDNAs for
IDI2 in the databases also supported the identification of all
introns as annotated in TAIR (except when the cDNAs were
incomplete). The sequences of RT-PCR products that we ob-
tained for IDI1 and IDI2 using oligonucleotides based on the
beginning and end of the open reading frames as annotated in
TAIR (idi1-attB1 and idi1-attB2 [for IDI1] or idi2-attB1 and idi2-
attB2 [for IDI2] [see Supplemental Table 1 online]) also confirmed
the intron–exon demarcation.
In order to gain insight into the possible subcellular localiza-
tions of the two IDI enzymes as directed by the N-terminal ex-
tensions, the full-length deduced amino acid sequences for the
two proteins were used to query several public servers, including
ChloroP (http://www.cbs.dtu.dk/services/ChloroP/) (Emanuelsson
et al., 1999), TargetP (http://www.cbs.dtu.dk/services/TargetP/)
(Emanuelsson et al., 2000), Predotar (http://urgi.versailles.inra.fr/
predotar/predotar.html), MitoProt (http://mips.gsf.de/cgi-bin/
proj/medgen/mitofilter) (Claros and Vincens, 1996), and PSORT
(http://wolfpsort.org/) (Nakai and Horton, 1999). Most algorithms
suggested plastid localization with a high level of certainty for
IDI1, although MitoProt also suggested mitochondrial localiza-
tion for this protein. There was less agreement regarding IDI2,
with targeting predictions roughly split between the mitochondria
and plastid. Interestingly, ChloroP predicted plastid localization
for both proteins, while MitoProt predicted mitochondrial local-
ization for both.
IDI1 Is Directed to the Plastid and IDI2 Is Directed to
the Mitochondrion
To determine the subcellular localization of both IDI proteins, we
transformed Arabidopsis with constructs in which the genomic
sequence for either IDI1 or IDI2 had been fused to enhanced
green fluorescent protein (eGFP) under the control of the cauli-
flower mosaic virus 35S promoter and visualized targeting by con-
focal and fluorescence microscopy. Two other transformed lines
were used as controls. First, we cloned the eGFP gene into the
sameeGFP-readyGatewayplant transformationvector (pB7FWG2)
(Karimi et al., 2002), producing an eGFP dimer lacking any transit
peptide, which served as a control for cytosolic localization.
Second, we used Arabidopsis plants transformed with a signal
peptide fused to eGFP, for which plastid localization of the eGFP
fusion protein had already been confirmed (Marques et al., 2004).
Comparisons of confocal micrographs of the plastid and
cytosolic controls (Figures 4B and 4C, respectively) and non-
transformed controls (Figure 4A) viewed under similar instrument
settings indicated that virtually no green fluorescence was de-
tectable in nontransformed controls, whereas red autofluores-
cence derived from chlorophyll was readily visible (Figure 4A). In
the plastid control, intense green fluorescence colocalized with
chloroplast autofluorescence (Figure 4B). However, in the cyto-
solic localization control, green fluorescence was visible in the
cytosol, the nucleus, and at the cell wall but not in the red
autofluorescent plastids (Figure 4C). Thus, under these experi-
mental conditions, plastid targeting could readily be distin-
guished from cytosolic localization.
Plant lines transformed with IDI1 were visualized in a similar
way and revealed eGFP fluorescence that colocalized with
plastids in roots, stems, and leaves (Figure 4D; localization in
stems and roots not shown). However, plants transformed with
IDI2 exhibited green fluorescence in discrete subcellular organ-
elles that did not colocalize with plastid autofluorescence (Figure
4E). When seedling roots from these same transformed lines
were stained with a mitochondria-specific orange fluorescent
dye, eGFP fluorescence was observed to colocalize with the
MitoTracker Orange–derived fluorescence (Figure 4F), confirm-
ing targeting to mitochondria.
The same transformation vectors containing the cDNAs in-
stead of the full-length genomic sequences were also tested in
this way. Cloning and sequencing of the transcripts using trans-
gene-specific primers showed that plants transformed with the
genomic sequence and cDNAs produced identical transcripts.
Although the cDNAs were found to have generally the same
localization patterns as the genomic sequences, some expres-
sion of the IDI1 cDNA was occasionally detected in both the
cytosol and plastid simultaneously (Figure 5A). A third set of
eGFP fusion constructs for IDI1 and IDI2 bearing the native
promoter was analyzed, but expression levels were too low to
visualize eGFP fluorescence.
At Least One IPP Isomerase Gene Is Required for
Arabidopsis Viability, and IDI2 Is Necessary for Normal
Flower Development
Lines of Arabidopsis with mutations at each IPP isomerase locus
were investigated to learn more about the roles of these genes in
680 The Plant Cell
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Figure 4. Subcellular Localization of IDI-eGFP Fusion Proteins in Transformed or Control Arabidopsis Leaf Tissue.
The first column shows green fluorescence from eGFP, the second shows red autofluorescence from chlorophyll, and the third shows an overlay of the
The Role of IPP Isomerase in Arabidopsis 681
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planta. Using publicly available T-DNA insertion line collections,
we obtained two lines with insertions in the IDI1 gene (idi1-1,
GABI 217_ H04, and idi1-2, SALK_006330, N506330) and one
line with an insertion in the IDI2 gene (idi2-1, SALK_014625,
N514625). The insertion in idi1-1 is in exon 3, the insertion in idi1-2
is after the fourth nucleotide in intron 3, and the insertion in idi2-1
is in exon 5 (Figure 3). RT-PCR revealed that none of these
mutant lines produced a functional full-length transcript from the
affected gene (Figure 6). All single idi mutants (Figure 3) were
confirmed as homozygous for their respective insertions in the T3
generation by DNA gel blot analysis, T-DNA–specific PCR, and
left border sequencing of the resulting PCR products. The
segregation of T-DNA insertions and associated herbicide re-
sistance markers was Mendelian in all cases.
Plants homozygous for idi1-1 or idi1-2 alleles showed no
obvious phenotype. However, plants homozygous for the idi2-1
allele formed flowers in which the sepals were fused and the
petals were highly underdeveloped (Figure 7A). The pollen from
these mutants was viable, and backcrossing of this mutant for
three generations to ecotype Columbia (Col-0) wild-type plants
followed by self-fertilization confirmed that the phenotype was
linked to the idi2-1 mutant allele.
We were unsuccessful in obtaining double homozygous mu-
tants by crossing either idi1 mutant with idi2-1. Following
screening of >400 progeny from each of these crosses (>800
plants total), no double homozygous plant was observed (1 in 16
was expected). In addition, we were unable to detect any plants
that were homozygous at one locus and heterozygous at an-
other. The expected frequency of this genotype, assuming
strictly Mendelian segregation, would be one in four plants.
In an attempt to rescue the double homozygous mutant
containing both the idi1-1 and idi2-1 alleles, we transformed
double heterozygous lines with a truncated version of the IDI1
cDNA lacking the putative signal peptide but fused to eGFP in an
effort to provide IPP isomerase activity to the cytosol (see kinetic
characterization for a description of the active, truncated forms
of IDI1 and IDI2). The retention of the truncated fusion protein
(cytIDI-eGFP) in the cytoplasm was confirmed by confocal
microscopy (Figure 5B). Transformed plants were screened by
PCR for the presence of the idi1-1 or idi2-1 allele. We determined
the genotypes of 40 plants by PCR and further monitored the
expression of the transgene in these plants by measuring GFP
fluorescence in crude protein extracts of seedlings (data not
shown). Based on this screening strategy, we selected six
Figure 4. (continued).
two channels. All confocal images were scanned using similar laser gain and offset settings. Confocal images are as follows: nontransformed
Arabidopsis (A), plastid localization–positive control ferredoxin NADP(H) oxidoreductase (Marques et al., 2004) (B), cytosolic eGFP expression (empty
vector control) (C), genomic IDI1-eGFP fusion (D), and genomic IDI2-eGFP fusion (E). (F) shows an epifluorescence micrograph of MitoTracker Orange–
stained root hairs of Arabidopsis stably transformed with the IDI2-eGFP construct. eGFP fluorescence is shown in the left column, MitoTracker Orange
fluorescence in the central column, and the overlay of the two in the right column. Bars ¼ 20 mm.
Figure 5. Confocal Micrographs Showing the Simultaneous Plastid and Cytosolic Localization of IDI1c-eGFP in the Stem of a Wild-Type Plant and of
the Truncated cytIDI-eGFP in the Cytoplasm of Leaf Tissue in the idi2-1 Mutant Background.
(A) IDI1c-eGFP expression in the stem (wild type).
(B) cytIDI-eGFP expression in leaf (idi2-1).
The first column shows green fluorescence from eGFP, the second shows red autofluorescence from chlorophyll, and the third shows an overlay of the
two channels. All confocal images were scanned using similar laser gain and offset settings. Cytosolic expression of IDI did not restore the fused-sepal
phenotype of the mutant plant but made possible the isolation of plants homozygous for the idi2 allele and heterozygous for the idi1 allele. Confocal
conditions were the same as those described for Figure 4. Bars ¼ 20 mm.
682 The Plant Cell
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independent lines from the T0 generation that were heterozy-
gous for both the idi1-1 and idi2-1 mutant alleles and had high
levels of expression of the truncated IDI1 (as determined by GFP
fluorescence) and allowed them to self-fertilize. Screening of 240
individuals in the T1 generation again failed to yield a double
homozygous mutant. However, we were able to find plants that
were heterozygous at the IDI1 locus and homozygous for idi2-1.
Of 240 plants, 36 had such a genotype. In nearly every case,
these plants displayed the same flower morphology defect as the
idi2-1 single mutant, although two lines (cytIDI-11 and cytIDI-14)
displayed partial restoration to the wild type (Figure 7B). No
plants homozygous for the idi1-1 mutant allele and heterozygous
at the IDI2 locus were isolated in this screen.
Transformation of the idi2-1 Mutant with the Full-Length
IDI2 cDNA but Not the Full-Length IDI1 cDNA Restores
the Wild-Type Floral Phenotype
Since the fused sepal phenotype was observed to segregate
with the idi2-1 allele, we attempted to restore the wild-type
phenotype in this mutant by transformation with vectors encod-
ing either the IDI1 or IDI2 full-length cDNA. T1 glufosinate
ammonium–resistant plants were allowed to self-fertilize, and
seeds were collected from individual transformed lines. T2 plants
were grown on sterile Murashige and Skoog (MS)–glufosinate
ammonium plates, and transformed lines with apparent single
inserts (as judged by a 3:1 resistant-to-susceptible ratio) were
transferred to soil and allowed to flower under long-day condi-
tions. Plants transformed with the IDI1 cDNA retained the mutant
phenotype (Figure 7C), while the flowers of those transformed
with the IDI2 cDNA were completely restored to the wild type
(Figure 7D). The subcellular localization of IDI2 in the rescued
mutant background was confirmed with confocal microscopy
and determined to be identical to that shown in Figure 4E.
LossofEither IDI1or IDI2 IndividuallyHasaMinimalEffecton
Isoprenoid Content in Leaf Tissue or in Flowers
The single homozygous mutants were subjected to chemical
analyses to quantify the major isoprenoid metabolites produced
in the chloroplasts and mitochondria. Chlorophyll and caroten-
oids are probably the most abundant isoprenoid products of the
chloroplasts, while ubiquinone is the major isoprenoid produced
in mitochondria. Given the role of carotenoids as photoprotec-
tants of the photosynthetic apparatus, we anticipated that if
either IDI protein played a limiting role in carotenoid production,
their absence would be most clearly noted under high light
conditions. Therefore, we compared carotenoid and chlorophyll
levels in acetone extracts of leaves from wild-type and mutant
plants grown under high light levels (600 mmol�m�2�s�1) as
measured by HPLC. A simple ion-trap liquid chromatography–
mass spectrometry (LC-MS) method was implemented to se-
lectively detect ubiquinone levels in the same extracts. We
detected no differences between wild-type plants and idi1-1
and idi1-2 mutant lines for any of the isoprenoids analyzed,
except that a slight decrease (20%) in both the carotenoids and
chlorophylls was noted for idi2-1 (Figure 8). A sample of the
plants used for HPLC analysis was also used to again confirm the
absence of functional transcripts in the mutant lines.
To examine whether the idi2-1 mutant flower phenotype was
due to a deficiency in a specific class of essential isoprenoids,
the above chemical analysis was repeated using wild-type and
idi2-1 flowers grown under normal conditions. No significant
differences were noted between the levels of carotenoids, chlo-
rophylls, phytosterols, or ubiquinone in flowers from the idi2-1
mutant versus those of wild-type flowers (Figure 9).
IDI2 Transcripts Are More Abundant Than Those of IDI1
Overall, but Both Genes Have Similar Organ-Specific
Expression Profiles
The organ-specific expression of IDI1 and IDI2 was monitored by
quantitative real-time PCR (qRT-PCR) using primers designed to
recognize a portion of the 39 UTR of each gene. Steady state
transcript levels of each gene in four organs (roots, stems,
leaves, and flowers) were measured and normalized to those of
leaves. Within a given organ, overall expression between IDI1
and IDI2 was also compared based on the Ct values of the
common normalizer gene. Qualitatively, expression of both
genes was detectable in all organs surveyed. Quantitatively,
expression of IDI1 was 4.1-fold higher in flowers than in leaves,
1.5-fold higher in roots than leaves, and about the same in stems
as in leaves (Figure 10A). Expression of IDI2 was about the same
in flowers and stems as in leaves but ;2.5-fold higher in roots, in
agreement with Campbell et al. (1997) (Figure 10A). When the
expression of the two IDI genes was compared within a given
organ, IDI2 was always more abundant, with IDI2 transcripts
outnumbering IDI1 by ;10-fold in leaves, 22-fold in roots, 4.9-
fold in flowers, and 4.6-fold in stems.
Figure 6. RT-PCR Analysis of Wild-Type and idi Mutant Lines.
Total RNA was converted to cDNA using a poly(dT) primer and then used in
a PCR either with primers that amplify the full-length transcript of IDI1
(columns A to C) or IDI2 (columns D and E) (top panel) or a normalizer gene
(RP2LS; bottom panel) to confirm the conversion of RNA into cDNA
template. cDNA templates are as follows: wild type (A), idi1-1 (B), idi1-2 (C),
wild type (D), and idi2-1 (E). IDI1 was amplified with primers flanking the
start and stop codons and is predicted to produce a product of 930 bp,
whereas IDI2 was amplified with primers that included a small portion of the
39 UTR and is thus predicted to amplify a slightly larger product of 988 bp.
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The steady state transcript level of the remaining functional IDI
gene in each mutant line was similarly measured. In this case,
whole mutant seedlings were used and compared with samples
obtained from wild-type seedlings. No mutant showed a signif-
icant increase in the remaining IDI gene relative to the wild type
(#1.5 fold increase; Figure 10B).
The IDI1 and IDI2 Proteins Have Similar Kinetic Properties
To look for further differences in the roles of the two genes, we
compared the catalytic properties of the encoded proteins
expressed in vitro. It was previously shown that the N-terminal
extensions of IDI1 and IDI2 were not required for catalytic activity
(Campbell et al., 1997). Therefore, we expressed both proteins in
truncated form based on their alignment to the start codon of
E. coli IDI (Figure 2). The purification of the recombinant proteins
was aided by expression with an N-terminal His tag. However,
due to the catalytic role of divalent metal ions in the IPP isom-
erase reaction (Carrigan and Poulter, 2003), the presence of
the His tag posed problems for accurately measuring the affinity
of each enzyme for IPP. Therefore, after introducing a thrombin
cleavage site, the His tags were removed by thrombolytic cleav-
age following purification on a charged Ni affinity column. The Km
values of IDI1 and IDI2 for IPP were determined to be 20 6 3.8
and 16 6 2.6 mM, respectively, while their kcat values were 2.24 6
0.1 and 0.89 6 0.04 min�1, consistent with previous literature
reports for this class of IDI enzymes (Muehlbacher and Poulter,
1988; Anderson et al., 1989; Street and Poulter, 1990; Carrigan
and Poulter, 2003). A pH optimum curve of each protein revealed
that both had a similar preference for a neutral pH (Figure 11).
Incorporation of [2-13C]Mevalonate into Sitosterol
Demonstrates IPP Isomerase Activity in the Cytosol
Except for the floral phenotype of the idi2 mutant, there were no
significant morphological or chemical alterations in the individual
idi mutants, making it hard to draw any conclusions about the
specific roles of these genes in isoprenoid metabolism. The nega-
tive impact of a single idi mutation may be ameliorated by DMAPP
supplied from the isomerase encoded by the other IDI gene. To
investigate this possibility, we compared the biosynthesis of
sitosterol, the most abundant plant sterol, in the wild type ver-
sus all three idi mutant lines. Sitosterol is known to be biosyn-
thesized in the cytosol. Thus, to assess the source of the IPP and
DMAPP for sitosterol biosynthesis, we labeled the cytosolic
mevalonate pathway by supplying [2-13C]mevalonate to plants
Figure 7. Phenotype of idi2-1 Mutant Flowers and Genetic Comple-
mentation.
Flowers from the idi2-1 mutant ([A], left) demonstrate a fused-sepal
phenotype with highly underdeveloped petals but produce fertile pollen
and can self-fertilize. A Col-0 wild-type flower ([A], right) is shown for
comparison. Two homozygous idi2 lines (out of 36) expressing cytosolic
IDI showed partial reversion to the wild-type flower morphology (B). The
black arrow in (B) indicates a mutant flower, whereas the white arrows
show wild-type flowers. The fused-sepal phenotype of the idi2-1 mutant
was not affected by transformation with the IDI1 cDNA (C), while this
phenotype was fully restored to that of the wild type by transformation of
this mutant with a cDNA encoding IDI2 (D). Shown are three independent
lines transformed with the IDI1 cDNA (C) and three lines transformed with
the IDI2 cDNA (D); a Col-0 wild-type flower is pictured at left in (D).
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in a MS growth medium while simultaneously administering
mevastatin, an inhibitor of an essential step in the mevalonate
pathway, HMG-CoA reductase, to block the endogenous for-
mation of unlabeled mevalonate (Rodrıguez-Concepcion et al.,
2004). The biosynthesis of a sitosterol molecule requires four IPP
units and two DMAPP units (see Supplemental Figure 1 online). If
there were a cytosolic IPP isomerase, all IPP and DMAPP units
should be labeled by [2-13C]mevalonate, resulting in an incorpo-
ration of five 13C atoms (one 13C atom is lost during demethyl-
ation of the cycloartenol intermediate) (Schaeffer et al., 2001).
However, if there is no IDI activity in the cytosol, only the IPP units
would be labeled directly from [2-13C]mevalonate, resulting in the
incorporation of four 13C atoms. The DMAPP would have to
come either from IPP generated in the cytosol and isomerized to
DMAPP in the plastids or mitochondria or from IPP generated in
the plastid that was isomerized there. In either case, the incor-
poration of label would be expected to be lower than for a
cytosol-generated DMAPP unit.
We detected high levels of [2-13C]mevalonate incorporation
into sitosterol in these experiments using GC-MS and 13C NMR.
The mass spectra for the trisilyl-sitosterol derivatives from the
wild type and idi mutant lines were identical (Figure 12). In
extracts from labeled plants (Figure 12B), a [M þ 5]þ� molecular
peak dominated the molecular ion cluster in the wild type and in
all three mutant lines, indicating the existence of a cytosolic IPP
isomerase activity in all of these plants. When spectra from plants
supplemented with [2-13C]mevalonate were compared with
those derived from unlabeled plants (Figures 12B versus 12A),
many differences in the fragmentation patterns were evident.
Aside from the dominant mass ions (m/z 491 versus 486),
sitosterol fragments from labeled plants bearing one (m/z 130
versus 129), two (m/z 161 versus 159), three (m/z 258 versus
255), four (m/z 361 versus 357), and five (m/z 401 vs. 396) 13C
labels were detected, corresponding to sitosterol fragments
containing one to five 13C-labeled isoprene units. The strongest
mass spectral evidence for a cytosolic isomerase comes from
the detection of 13C labeling in the aliphatic side chain of the
sitosterol skeleton, most of whose carbon atoms originate from
DMAPP. Specific fragments corresponding to this side chain
showed a significant enrichment of 1 mass unit (m/z 44 versus 43
and m/z 86 versus 85) in all samples supplemented with
[2-13C]mevalonate (Figure 12B) but not in the unlabeled controls
(Figure 12A), consistent with 13C labeling of the C26 position of
the aliphatic chain of sitosterol via a DMAPP unit derived from
[2-13C]mevalonic acid (see Supplemental Figure 1 online). The
absolute levels of sitosterol in the plants used in these experi-
ments were similar in mutant and wild-type lines grown on MS
medium alone (132 to 141 ng/mg fresh weight, based on com-
parison with the internal stigmastanol standard). Meanwhile,
plants grown in the presence of [2-13C]mevalonate and meva-
statin displayed a decrease of ;30% in the levels of sitosterol
(99 to 109 ng/mg fresh weight).
To confirm that the labeling of sitosterol mass spectral frag-
ments was due to DMAPP originating from an isomerase in the
cytosol, labeled sitosterol from wild-type and mutant plants was
purified by preparative HPLC and then measured by 13C NMR.
The incorporation of [2-13C]mevalonic acid would be expected to
label five specific carbon atoms in the sitosterol skeleton (see
Supplemental Figure 1 online). For sitosterol isolated from both
Figure 9. Analysis of Isoprenoid Levels in idi2-1 Mutant Flowers.
Carotenoid and chlorophyll levels were determined by HPLC analysis
(monitoring at 445 and 650 nm). An aliquot of the same sample was used
for the analysis of ubiquinone-9 levels by ion-trap LC-MS as described in
Methods. Quantification was based on external standard curves. Quan-
tification of sitosterol was based on the relative peak area of stigmas-
tanol added to flower tissue prior to extraction as an internal standard
(10 mg), while identification was based on comparison with a derivatized
authentic sitosterol standard. Error bars indicate SD from seven repli-
cates. Ubiquinone-9 levels are shown on the right vertical axis.
Figure 8. Carotenoid, Chlorophyll, and Ubiquinone Contents of Wild-
Type and idi Mutant Leaf Tissue Exposed to Continuous High Light (600
mmol�m�2�s�1).
Frozen, ground leaf tissue (500 mg) from six pooled individual plants was
extracted with 2.5 mL of acetone:water (9:1) and analyzed by HPLC (for
carotenoids and chlorophyll) or ion-trap LC-MS (for ubiquinone). Values
shown are averages 6 SD of eight replicates. Quantification was based
on external standard curves. Ubiquinone-9 levels are shown on the right
vertical axis.
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mutant and wild-type plants, each of these five atoms was
indeed found to be enriched (Figure 13). Most notable was the
strong enrichment of a signal at 19.82 ppm corresponding to
C26, a carbon atom in the side chain derived from DMAPP. This
furnished strong evidence that the DMAPP used in the formation
of sterols is derived from the cytosolic mevalonate pathway via a
cytosolic IPP isomerase.
Shortened Transcripts of Both IDI1 and IDI2 Are
Expressed That Lack the N-Terminal Transit Peptide for
Organellar Targeting
The presence of the IDI protein in the cytosol might be due to the
translation of a shorter transcript lacking the N-terminal signaling
peptide. To determine whether such alternative transcription
occurred at a significant rate, 59 rapid amplification of cDNA ends
(RACE) was employed to assess the lengths of the IDI1 and IDI2
transcripts. Using reverse primers for each gene optimized for 59
RACE (see Supplemental Table 1 online), we found two distinct
size classes of 59 RACE products for IDI1 and IDI2. Because the
reverse primers were designed to be complementary to exon 2
(IDI1) and exon 4 (IDI2), we were able to rule out genomic DNA
contamination as a possible source for these clones. Sequence
analysis of these fragments indicated that the longer 59 RACE
products from transcripts of both genes from both leaf and flower
tissues came from full-length transcripts that included the pro-
posed start codons (Figure 14; fragments 1 and 3 representing
IDI1 and IDI2, respectively). For IDI1, even longer transcripts than
those represented by fragment 1 were observed in both tissues.
Importantly, 59 RACE analysis and sequencing detected shorter
transcripts for both IDI1 and IDI2 (represented by fragments 2 and
5 for IDI1 in leaf and flowers, respectively, and by fragment 4 for
IDI2 in both tissues). Fragment 2 represents an IDI1 transcript that
begins 180 bp downstream from the predicted start codon, while
fragment 5 represents an IDI1 transcript beginning 48 bp down-
stream from the same position. Fragment 4 represents an IDI2
transcript that begins 52 bp from its start codon. The shorter
transcripts include the region encoding the Met-rich, conserved
portion of the N-terminal extension corresponding to Met codons
at positions�16 and�8 (IDI2 fragment 4 and IDI1 fragment 5) or
only at position�8 (IDI1 fragment 4) relative to the E. coli IDI start
codon (Figure 2). A highly truncated IDI1 RACE product was also
observed from leaf templates, which is unlikely to produce
functional proteins.
Figure 10. Steady State Transcript Levels of IDI1 and IDI2 in Arabidopsis
as Measured by qRT-PCR.
Relative quantification was performed according to the Pfaffl method
(Pfaffl, 2001). Error bars indicate SD.
(A) Organ-specific expression. Fold change values compare expression
levels of each gene with that in the leaf. When IDI1 and IDI2 were
compared in the same organ, IDI2 was found to be more abundant in all
organs surveyed (described in text). cDNA template loading was nor-
malized to the Ct value of the Arabidopsis RP2LS gene (At4g35800).
(B) Expression of the remaining IDI gene in idi mutant lines. Total RNA
was extracted from whole seedlings, converted to cDNA, and used in
relative quantification experiments with wild-type seedling extracts.
Figure 11. pH Optima of the Two Mature IDI Proteins from Arabidopsis.
Activity is based on the conversion of [1-14C]IPP to its acid-labile isomer,
DMAPP, and scintillation counting of an ether extract of the reaction
following acid hydrolysis. Error bars indicate SD of four replicates at each
pH. Linear conditions were established previously by assaying a range of
enzyme concentrations and incubation times. IDI1 and IDI2 are repre-
sented by open and closed circles, respectively.
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DISCUSSION
The Arabidopsis IDI1 and IDI2 Genes Encode Similar
Proteins with Divergent N Termini That Are Predicted to
Serve as Transit Peptides
Our studies of the two Arabidopsis IPP isomerase genes, IDI1 and
IDI2, indicated no great differences in organ expression patterns
between them, and the catalytic properties of the encoded pro-
teins were also similar. However, there are some distinctions in
their metabolic roles caused by differences in subcellular localiza-
tion resulting from divergence in their N-terminal sequences.
An analysis of the gene structure of IDI1 and IDI2, based on
available cDNAs and our own RT-PCR products, indicated that
the annotated versions available in public databases correctly
show the intron and exon structure of these genes and that
alternative splicing of primary transcripts, if it occurs, must be
rare. Furthermore, the presence of upstream in-frame stop
codons in the 59 UTR (or promoter region) of both genes strongly
suggested that the start codons shown in Figure 2 are the true
translational start signals used in planta for the complete tran-
script. The predicted amino acid sequences include the pres-
ence of a 65- to 75-residue N-terminal extension in both proteins
compared with the E. coli homolog. These extensions are highly
divergent from one another (and from the corresponding se-
quences in other plant IDI proteins) with the exception of the last
16 residues. This observation, together with the results of tar-
geting prediction software and the observation that both proteins
are catalytically active when expressed as truncations without
the extension (Campbell et al., 1997; this study), all indicated
likely organellar targeting of IDI1 and IDI2 when translated from
full-length complete transcripts.
The IDI1 Protein Participates in Plastid Isoprenoid
Formation, but Knocking Out the IDI1 Gene Has No
Morphological or Chemical Effects
Expression of the IDI1 gene fused to the eGFP open reading
frame in plants resulted in clear plastid localization of this protein
(Figure 4). While the terminal step of the MEP pathway produces
Figure 12. Sitosterol Mass Spectra from Arabidopsis Plants Grown in the Absence or Presence of [2-13C]Mevalonate and Mevastatin.
(A) Plants grown on MS medium.
(B) Plants grown on MS medium containing [2-13C]mevalonate mevastatin.
In each case, no difference was detected between spectra from wild-type or idi mutant plants (spectra from a wild-type plant are shown; see also
Supplemental Figure 2 online). The inset in (A) shows the mass spectrum of authentic sitosterol standard; the inset in (B) shows the incorporation of
[2-13C]mevalonate into sitosterol in wild-type and idi lines grown in the presence of mevastatin, as determined by the relative proportions of isotopomers
in the mass ion cluster representing [M]þ (m/z 486) through [Mþ5]þ (m/z 491) species after subtraction of the natural abundance of 13C in the control
samples. Error bars indicate SD of four replicates. Sterols were extracted from 2-week-old seedlings with methanol:CH2Cl2 (2:1, v/v) using stigmastanol
as an internal standard, derivatized with N-methyl-N- trimethylsilyltrifluoroacetamide, and analyzed by GC-MS.
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both IPP and DMAPP (Eisenreich et al., 2004), previous work has
suggested that IDI activity in the plastid is necessary for maximal
rates of synthesis of isoprenoids such as carotenoids (Albrecht
and Sandmann, 1994; Page et al., 2004). Furthermore, it has also
been shown that in E. coli cells that were engineered to synthe-
size carotenoids from DMAPP and IPP produced via the MEP
pathway, IDI activity was a limiting factor in carotenoid biosyn-
thesis (Kajiwara et al., 1997; Cunningham and Gantt, 2000). That
exogenously supplied mevalonate can complement a block in
1-deoxyxylulose 5-phosphate synthase activity and chlorophyll
biosynthesis (presumably following the transport of IPP to the
plastid) also suggests the presence of IDI activity in this com-
partment (Estevez et al., 2000; Nagata et al., 2002). Thus, plastid
localization for a plant IDI is not surprising. However, plants
homozygous for the idi1 null alleles are viable and contain wild-
type levels of carotenoids and chlorophylls even under high light
conditions (Figure 8), suggesting that IDI2 may somehow com-
pensate for the lack of IDI1.
The IDI2 Protein Participates in Mitochondrial Isoprenoid
Formation, and idi2 Mutants Have Abnormal
Floral Morphology
The expression in plants of IDI2 fused to eGFP unambiguously
demonstrated localization to a nonplastid organelle (Figure 4E).
Using a mitochondria-specific fluorescent dye, we were able to
show the site of IDI2 targeting as the mitochondria (Figure 4F). A
mitochondria-specific isoform of IPP isomerase is not surpris-
ing given the previously reported role of mitochondria in the bio-
synthesis of some essential isoprenoids, such as ubiquinone
(Lutke-Brinkhaus et al., 1984), and the targeting of a specific
isoform of FPP synthase to this compartment (Cunillera et al.,
1997). While IPP has been shown to be taken up by mitochondria
(Lutke-Brinkhaus et al., 1984), if DMAPP cannot similarly be
absorbed, then there would be an absolute requirement for
an IPP isomerase in the mitochondrion to provide DMAPP
for the construction of isoprenoids. Direct import of FPP into
Figure 13. Upfield Portion of the 13C NMR Spectra of Purified Sitosterol Extracted from Wild-Type and idi Mutant Arabidopsis Seedlings Cultivated in
the Presence of [2-13C]Mevalonate and Mevastatin.
Sitosterol from wild-type and mutant plants gave virtually identical spectra (see Supplemental Figure 3 online). The wild-type spectrum is shown above.
These signals were identified by previously published chemical shift values for sitosterol (Goad and Akihisa, 1997). These allowed unambiguous
assignment of all carbon atoms in the molecule. Labeling was found to occur at the predicted positions based on the scheme for sitosterol biosynthesis
from IPP and DMAPP shown in Supplemental Figure 1 online. The peaks at 24.31 (C15), 31.93 (C7), 33.96 (C22), and 37.27 (C1) ppm were enriched by
labeling via IPP. The peak at 19.82 ppm (C26) was enriched by labeling via DMAPP. Since the extent of IPP and DMAPP labeling of sitosterol, a cytosolic
isoprenoid product, is comparable, both substrates must come from the cytosol, indicating the presence of a cytosolic IPP isomerase. The structure
and carbon atom numbering of sitosterol are shown above the spectrum, with enriched carbons shown in boldface; numbers in parentheses indicate
the reported chemical shifts in parts per million.
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mitochondria, inferred from the observation that the administra-
tion of [3H]farnesol to cultured tobacco BY-2 cells resulted in
labeled ubiquinone (Hartmann and Bach, 2001), would obviate
the need for an IPP isomerase there. But it is possible that the
label from farnesol in this study was imported in a form other
than FPP, such as ubiquinone itself, which has been shown to be
imported into mitochondria in tobacco after assembly in the
endoplasmic reticulum (Swiezewska et al., 1993; Ohara et al.,
2004).
Compared with IDI1, IDI2 is more highly expressed overall. At
the organ level, we observed that IDI2 expression is highest in
roots but that IDI1 expression is highest in flowers. These results
partially agree with those of Campbell et al. (1997), who found
that IDI1 and IDI2 were both most highly expressed in roots. This
discrepancy may be due to cross-hybridization of the cDNA
probes used with RNA gel blots in the previous study, since the
portions of IDI1 and IDI2 that encode the mature protein share
89% identity at the nucleotide level. In our case, the design of
primers in the 39 UTR, where IDI1 and IDI2 share no similarity, and
the sequencing of multiple qRT-PCR products ensured the
specificity of IDI transcript measurements.
The mitochondrial localization of IDI2 and the fused-sepal
phenotype of the idi2-1 mutant (Figure 7) led us to speculate that
specific isoprenoid metabolites derived from the mitochondria
Figure 14. The 59 RACE Products of IDI1 and IDI2 in Leaves and Flowers of Wild-Type Arabidopsis Plants.
Nested RACE products were separated on a 4% agarose gel, excised, cloned, and sequenced. A nucleotide alignment of five representative RACE
products is shown for bands representing the IDI1 full-length transcript (1), the IDI1 short transcript (2 and 5), the IDI2 full-length transcript (3), and the
IDI2 short transcript (4). Alignments were performed using Blosum62 (VectorNTI 10) with a gap-opening penalty of 10 and a gap-extension penalty of
0.1. The presumed start codons for the full-length IDI1 and IDI2 proteins are boxed, while the dotted lines represent possible alternative start codons for
shortened transcripts, including that corresponding to the E. coli start codon (defined as Metþ1) and conserved Met codons at amino acid positions�8
and �16 relative to the E. coli start position. The sizes of representative marker bands are indicated in base pairs.
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are necessary for normal floral development. In addition to the
synthesis of ubiquinone, some protein prenylation is thought to
take place in the mitochondria of spinach (Spinacia oleracea)
(Shipton et al., 1995). However, in Arabidopsis, no protein
prenyltransferase activity is known to occur in this organelle
(Crowell, 2000). While mitochondria have previously been shown
to be involved in floral organ development in Nicotiana spp
(Bonnett et al., 1991), it is not currently clear why a lack of IDI2
activity in Arabidopsis would produce the observed floral phe-
notype.
Representative isoprenoids biosynthesized in the plastid, cy-
tosol, and mitochondrion were analyzed in idi2-1 flowers in an
attempt to identify the cause of the mutant phenotype. However,
these analyses failed to show any specific isoprenoid deficiency
in mutant flowers. Furthermore, transformation experiments in
which a truncated isomerase expressed in the idi2-1 mutant
background failed to fully restore the wild-type phenotype sug-
gest that the basis of the idi2-1 phenotype is not related to any of
the compounds we have examined here or to the lack of
cytosolic isomerase activity.
Single Mutants in IDI1 or IDI2 Are Rescued by the
Remaining IDI
Characterization of mutant lines in which the IDI genes had been
disrupted showed that the simultaneous loss of both genes
results in a lethal phenotype. However, there were no major
morphological or chemical abnormalities associated with the
loss of either gene singly, with the exception of the loss of IDI2 in
flowers. What is the source of DMAPP in these single idi mu-
tants? We can rule out the MEP pathway as a significant source
of DMAPP in the single mutant lines, because then the double idi
mutant (which should have a functioning MEP pathway) would
also be viable. By the same reasoning, we can exclude the
existence of a heretofore unrecognized type II IPP isomerase in
Arabidopsis or the presence of any other protein catalyzing the
conversion of IPP to DMAPP in planta. Other explanations for the
viability of the single idi mutant lines require the remaining IDI
protein to be the source of the DMAPP. Although it was impos-
sible to obtain viable plants with three idi null alleles in crosses
between the mutants, overexpressing IDI1 as a cytosolic protein
gave viable plants that were homozygous for the idi2 null allele
and heterozygous for an idi1 null allele. To be sure, there are
limits to the ability of one IDI activity to complement another, in
that expression of IDI1 as a plastidic protein or a cytosolic protein
completely failed to restore the idi2-1 flower phenotype to that of
the wild type (Figure 7). Nevertheless, it seems clear that a single
IDI gene is sufficient for plant viability, whether it encodes IDI1,
which we observed in the plastids, or IDI2, which was found in the
mitochondria. In both cases, the transport of DMAPP or later
intermediates between organelles would seem essential for
normal isoprenoid formation.
Scattered evidence suggests that isoprenoid biosynthetic in-
termediates can be transported among subcellular components.
For example, IPP import into mitochondria (Lutke-Brinkhaus
et al., 1984) and exchange of IPP between the cytosol and plastid
have been documented by inhibitor studies in Arabidopsis (Laule
et al., 2003) and in vivo feeding studies in several plant systems,
including tobacco BY-2 cultures (Hemmerlin et al., 2003), snap-
dragon (Antirrhinum majus) (Dudareva et al., 2005), chamomile
(Chamaemelum nobile) (Adam et al., 1999), and lima bean (Pha-
seolus lunatus) (Piel et al., 1998). In vitro studies with isolated
membranes also support the transport of IPP from plastids to the
cytosol (and possibly DMAPP, albeit at very low levels) (Bick and
Lange, 2003) and from the cytosol to plastids (Kreuz and Kleinig,
1984; Soler et al., 1993; Flugge and Gao, 2005). Among earlier
isoprenoid intermediates, exogenously supplied mevalonate, an
intermediate in the cytosolic IPP pathway, has been shown to par-
tially rescue a block in the plastidic MEP pathway (Estevez et al.,
2000; Nagata et al., 2002; Gutierrez-Nava et al., 2004; Rodrıguez-
Concepcion et al., 2004). The transport of bona fide MEP pathway
intermediates such as 1-deoxy D-xylulose 5-phosphate (DXP)
from the cytosol into plastids has been shown to proceed via an
inorganic phosphate antiport transporter (Flugge and Gao, 2005).
In fact, a cytosolic xylulose kinase was recently identified in
Arabidopsis that converts 1-deoxy D-xylulose to DXP (Hemmerlin
et al., 2006), although a role for DXP in the cytosol is unclear at
present.
To find the source of DMAPP in cytosolic isoprenoid formation,
we investigated the origin of the C5 units of a major cytosol-
produced isoprenoid, sitosterol, in both wild-type and single idi
mutant Arabidopsis plants. When [2-13C]mevalonate, an inter-
mediate of the cytosolic pathway, was supplied, all C5 units in all
idi1 and idi2 mutant lines were uniformly labeled whether derived
from IPP or DMAPP. These findings point to the existence of a
cytosolic IPP isomerase activity arising from both IDI1 and IDI2
and provide no support for the incorporation of DMAPP units
originating in another compartment (which would be unlabeled)
or for the transport of cytosolic IPP to the plastids or mitochon-
dria for the isomerization to DMAPP followed by incorporation
upon return to the cytosol (which would give lower specific
labeling).
Arabidopsis Has IPP Isomerase Activity in the Cytosol
Arising from Shorter Transcripts of IDI1 and IDI2
While the GFP studies indicated the localization of IPP isomerase
protein only in plastids (IDI1) or mitochondria (IDI2), inspection of
the gene sequences indicated additional downstream Met co-
dons of IDI1 and IDI2 that could serve as initiators of translation of
shortened proteins without signal peptides that might be local-
ized to the cytosol. Using 59 RACE, shorter transcripts were
isolated for both genes; these lacked the 59 UTR and 48 bp or
more of the coding sequence of the full-length transcripts. These
short transcripts can be expected to give shortened proteins
without transit peptides, providing further evidence of cytosol-
localized IPP isomerase. The fact that the in vitro activity of both
proteins has an optimum at pH 7.0 is also consistent with a
cytosolic location. However, in relation to mitochondrial and
plastidial IPP isomerase forms, such truncated cytosolic proteins
probably represent only a small proportion of total IPP isomerase
proteins. While 59 RACE is not a quantitative technique, it is
expected to favor the amplification of shorter fragments. Hence,
the observation that RACE products corresponding to full-length
transcripts are more abundant than RACE products representing
shorter ones (Figure 14) suggests that full-length transcripts
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predominate in planta. The greater proportion of longer plastid-
targeted (IDI1) or mitochondria-targeted (IDI2) transcripts versus
cytosolic transcripts (from both IDI1 and IDI2) may also explain
the general lack of cytosolic eGFP expression observed in IDI-
eGFP–transformed lines. Fluorescence from a small amount of
cytosolically localized fusion protein dispersed over the large
space of the cytosol is likely much less visible by confocal
microscopy than large amounts of plastidial and mitochondrial
fusion proteins accumulated in the smaller volumes of these
organelles. However, since our IDI-eGFP constructs did not
include the native 59 UTR sequences, the analysis of 59 RACE
products is probably a more physiologically relevant indicator of
protein targeting.
The presence of IPP isomerase activity in the cytosol is not
only consistent with the sitosterol feeding studies and the exis-
tence of shorter transcripts but also rationalizes the lack of gross
phenotypes in the idi mutants. It also provides a logical way to
support the formation of sesquiterpenes, sterols, dolichols, and a
range of other isoprenoids in this compartment, since the basic
isoprenoid pathway in the cytosol produces only IPP and not
DMAPP, the C5 starter unit for terpenoid construction.
The Properties and Localization of IDI May Vary among
Plant Species
While the IPP isomerase of E. coli is dispensable for this bacte-
rium (Hahn et al., 1999), plants require this activity to supply the
C5 starter units for isoprenoid chain elongation; indeed, most
plant species studied, like Arabidopsis, have at least two differ-
ent IDI genes (Cunningham and Gantt, 2000; Nakamura et al.,
2001). The products of multiple IDI genes may be targeted to
different subcellular locations, as shown here for Arabidopsis,
because isoprenoid formation in plants is typically distributed
among different subcellular compartments. Previous studies
with tobacco showed that two IDI cDNAs encode proteins that
are localized to the cytoplasm and the plastid, respectively
(Nakamura et al., 2001), although it remains to be determined
whether these cDNAs in fact represent actual transcripts of IDI
forms present in this species.
Interestingly, sequence analyses of IDI genes have demon-
strated that proteins from the same species are more similar to
each other than to IDI sequences of other species (Cunningham
and Gantt, 2000). This is also true in Arabidopsis, in which IDI1
and IDI2 share 92% identity when the N-terminal region is ex-
cluded from comparison but are only 84 to 90% identical to other
known plant IPP isomerase sequences. Hence, IDI gene dupli-
cation is relatively recent on the scale of higher plant evolution,
and there may be differences in IPP isomerase properties or
localization among different plant lineages (Ramos-Valdivia et al.,
1997a, 1998). For example, in Cinchona robusta cell cultures that
produce anthraquinones requiring a DMAPP unit, two IDI pro-
teins are known with different kinetic characteristics and patterns
of occurrence (Ramos-Valdivia et al., 1997b). These results are in
contrast with this study, in which it was shown that the two
Arabidopsis proteins have no significant differences in kinetic
properties but have different patterns of subcellular localization.
There are vast differences among plant species in the amounts
and types of terpenoid secondary metabolites they produce.
Given that particular terpene types differ in their relative require-
ments for IPP and DMAPP, and in the subcellular compartments
in which they are produced, various species may require distinct
types of IPP isomerases operating in separate compartments to
efficiently regulate their IPP and DMAPP pools. Arabidopsis, with
its relatively low output of terpenoid secondary metabolites
(Chen et al., 2003; D’Auria and Gershenzon, 2005) and two
biochemically similar IPP isomerases operating in various com-
partments, may provide a basic model for IPP isomerase diver-
sification and distribution in a plant species.
METHODS
Plant Materials and Treatments
Arabidopsis thaliana (ecotype Col-0) plants were grown on soil in a climate-
controlled growth chamber (228C, 55% RH, and 100 mmol�m�2�s�1 pho-
tosynthetically active radiation) under either short days (12 h of light/12 h
of dark) or long days (16 h of light/8 h of dark) for 4 to 6 weeks. The
three independent T-DNA insertion mutants used in this study were
idi1-1 (SALK_006330, N506330), idi1-2 (GABI 217_H04), and idi2-1
(SALK_014625, N514625). Seed stocks were obtained either from the
European Arabidopsis Stock Center or from the GABI-KAT consortium
(Bielefeld University). Initial segregation analysis was performed by
seeding plants on MS medium plates supplemented with either 50 mg/
mL kanamycin (SALK insertion lines) or 7.5 mg/mL sulfadiazine (GABI
insertion line) as described previously (Alonso et al., 2003; Rosso et al.,
2003). In addition, a PCR-based assay was designed to detect the
presence of the T-DNA insertion. The primers used for this assay con-
sisted of T-DNA left border–specific primers (SALK_LBb1or GABI_LBb1)
in combination with the gene-specific primers IDI1L, IDI1R, IDI2L, and
IDI2R (see Supplemental Table 1 online). Plants segregating as homozy-
gous as confirmed by herbicide resistance and PCR were further ana-
lyzed by DNA gel blot analysis performed as described previously
(D’Auria et al., 2007). Hybridization probes included either a HindIII frag-
ment from the genomic clone of IDI1 or the XbaI–NcoI fragment obtained
from the genomic clone of IDI2.
Homozygous idi2-1 plants were backcrossed for three generations to
Col-0 plants for confirmation of phenotype segregation. In every gener-
ation, 30 progeny were screened for the presence of the T-DNA insert,
and a minimum of five positive plants based on the PCR assay were used
as the pollen donors for backcrossing. Plants positive for a T-DNA insert
after the third generation of backcrossing were allowed to self-fertilize,
and their progeny were genotyped by DNA gel blot. In order to obtain
plant lines containing T-DNA insertion alleles for both IDI1 and IDI2,
homozygous mutants of each of the four insertion lines were crossed in a
reciprocal manner and analyzed in the self-fertilized F2 for a double
mutant genotype.
Isotopically Labeled Precursor Feeding and Sterol Analysis
Seeds of the four homozygous T-DNA insertion lines, along with
Col-0 seeds, were sterilized and plated on MS medium supplemented
with a combination of 10 mM mevastatin (Sigma-Aldrich) and 4.5 mM
[2-13C]mevalonolactone (Sigma-Aldrich) or with either compound alone
as controls. Plants were grown for 2 weeks. Sterols were then extracted
as follows: 100 mg of plant material (fresh weight) was ground in liquid N2
and extracted with 1.5 mL of methanol:CH2Cl2 (2:1) containing 10 mg of
stigmastanol (Sigma-Aldrich) as an internal standard. Samples were
incubated at 408C for 30 min and centrifuged at 4200g for 10 min. The
supernatant was removed and the pellet was reextracted twice with an
additional 1.5 mL of methanol:CH2Cl2, followed by pooling of the
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supernatants. These were then back-extracted with 2 mL of 0.8%
aqueous NaCl, and the lower organic phase was removed with a glass
pipette and transferred to a new glass vial. The aqueous phase was
extracted two additional times with 2 mL of CH2Cl2, and phases were
separated as before. The pooled organic fractions were dried under a
nitrogen stream and resuspended in 200 mL of CH2Cl2. After transfer to a
glass GC vial insert, the samples were dried again, redissolved with 70 mL
of tetrahydrofuran, incubated with 30 mL of N-methyl-N-trimethylsilyltri-
fluoroacetamide, and immediately analyzed.
The samples were analyzed on a Hewlett-Packard 6890 gas chromato-
graph coupled to a Hewlett-Packard 5973 quadrupole mass selective
detector. Separation was performed on a DB5 column (5% phenyl-
methylpolysiloxane; J&W Scientific) measuring 30 m 3 0.25 mm i.d. with
a 0.25-mm film thickness. Helium was utilized as the carrier gas at a
constant flow rate of 2 mL/min. A 1-mL aliquot of each sample was
injected in a splitless mode at 2508C. The temperature program was as
follows: 2-min hold at 2008C, then 158C/min to 2808C, followed by a
second gradient of 28C/min to 3008C, with a final 3-min hold. The mass
detector was run in scan mode from m/z 33 to 555 at 70 eV. Sitosterol, the
dominant phytosterol in Arabidopsis, eluted at 14.21 min (data not
shown). Isotopic labeling patterns and incorporation efficiencies were
determined for sitosterol following identification by retention time and
mass spectra compared with those of an authentic standard.
For NMR analysis, the methanol:CH2Cl2 plant extracts were concen-
trated and sitosterol was purified by preparative HPLC using a Supelcosil
LC-18 DB semipreparative HPLC column (Supelco) and a gradient
beginning at 10% water (solvent A) and 90% acetone (solvent B),
reaching 100% B at 11 min, followed by a hold at 100% B for 5 min
before a return to initial conditions at 20 min. Analytes were monitored at
210 nm, and sitosterol eluted as a minor peak at 10.65 min based on
comparison with an authentic standard. Sitosterol fractions from con-
secutive runs were pooled, evaporated under a nitrogen stream, and
resuspended in CDCl3. A Bruker DRX 500 NMR spectrometer was used
for recording of 1H and 13C NMR spectra of sitosterol. Operating fre-
quencies were 500.13 MHz for the acquisition of 1H spectra and 125.75
MHz for 13C spectra. CDCl3 was used as the solvent, and chemical shifts
were referenced to trimethylsilane added as an internal standard.
Vector Construction and Plant Transformation
Gateway technology (Invitrogen) was used for the generation of all
transformation constructs, which generally consisted of a target gene
bearing a C-terminal fusion to eGFP under the control of the cauliflower
mosaic virus 35S promoter for plant transformations or a target gene
bearing an N-terminal fusion to a His tag under the control of the T7
promoter for bacterial expression. attB adaptor–bearing PCR primers
(see Supplemental Table 1 online) were designed for the generation of
attB PCR products for recombination with the donor vector pDONR207
via BP Clonase reactions (Invitrogen). Primer and template combinations
used to generate the full-length cDNA or genomic clones for IDI1 and IDI2
are shown in Supplemental Table 1 online. Primers used to subclone IDI1
and IDI2 into the pB7FWG2 transformation vector (Karimi et al., 2002)
bearing a C-terminal eGFP fusion included the presumed start codon (but
none of the 59 UTR), encompassed the entire genomic sequence,
including all introns, and up to and including the last amino acid codon
of exon 6. However, the stop codons were left out to produce a
continuous open reading frame with eGFP fused to the C terminus of
either protein. The region connecting eGFP to IDI1 or IDI2 encoded a
short tether sequence (HPAFLYKVVIS) which is predicted to form a
random coil. Fully sequenced entry clones were recombined in LR
Clonase reactions with the pB7FWG2 vector (Karimi et al., 2002). After
each 10-mL recombination reaction, 3 mL was used to transform TOP10
chemically competent cells (Invitrogen), and the resulting transformed
cells were then used to inoculate 5-mL overnight cultures grown at 378C in
the presence of antibiotic (50 mg/mL gentamycin [Duchefa] for pDONR
entry clones or 100 mg/mL spectinomycin [Duchefa] for plant transfor-
mation expression vectors). Plant transformation vectors were intro-
duced into Agrobacterium tumefaciens strain GV3101 and used in
vacuum infiltration transformations with Arabidopsis (ecotype Col-0)
(Bechtold and Pelletier, 1998).
T0 seeds were sown in soil, stratified for 3 d at 48C, and sprayed with 50
mg/mL glufosinate ammonium two to three times daily starting at day 10.
Resistant plant lines were allowed to self-pollinate. Resulting T1 seeds
were characterized as follows. Single insert lines were identified by
segregation analysis based on resistance to glufosinate ammonium when
grown on sterile MS phytagar plates. Transgene expression levels of
independent lines were estimated by measuring the levels of green
fluorescence in seedling total protein extracts with a fluorescence plate
reader and a SYBR Green fluorescence filter. For this measurement, 100
mg of seedlings from each independent line was homogenized in tripli-
cate in a cold, 2-mL glass Tenbroek homogenizer containing 500 mL of
extraction buffer (100 mM Tris, pH 7.5, 10% glycerol, and 1 mM DTT). The
homogenate was spun at 48C in a benchtop microcentrifuge at maximum
speed for 10 min, and a 50-mL aliquot of each supernatant was trans-
ferred to a plate well for fluorescence measurement and compared with
wild-type (nontransformed) extracts. Apparent single insert lines (based
on 3:1 glufosinate ammonium resistance ratios) having the highest green
fluorescence values were carried on to the next generation and used in
confocal microscopy analysis. To confirm the presence of the full-length
transgene in each independent transformed line, total RNA was extracted
from each line used for microscopy and converted to cDNA as described
below in Gene Expression Measurements. This was then used as a
template in RT-PCR with the 35SF and eGFPR primers (see Supplemental
Table 1 online). Amplicons were cloned using the TOPO-TA-pCR4 cloning
kit (Invitrogen) and sequenced with M13, M13 reverse, and internal
primers to confirm that all plants used in microscopy expressed a full-
length transcript, including a complete transit peptide, that was in-frame
with the N terminus of eGFP.
Microscopy
Stably transformed Arabidopsis seedlings from the T2 or T3 generation
representing four transformation constructs (35S:IDI1c-eGFP, 35S:IDI2c-
eGFP, 35S:IDI1g-eGFP, and 35S:IDI2g-eGFP) were grown on sterile MS
agarose plates containing 25 mg/mL glufosinate ammonium (Sigma-
Aldrich) for 10 to 15 d. To test for chloroplast localization of eGFP fusion
proteins, true leaves, stems, and roots from each group were dissected
and mounted on a microscope slide with water and used in confocal
microscopy. Scans were performed on plants from three independent
lines per construct using a Zeiss LSM 510 Meta system, lasers specific for
eGFP (488-nm excitation, detection from 500 to 530 nm) and for chloro-
plast autofluorescence (561-nm excitation, 575-nm long-pass detection),
and a 403 LD C-Apochromat objective (water-corrected). To test for
mitochondrial localization, transformed Arabidopsis seedlings were
stained overnight in PBS, pH 7.2, containing 2% DMSO and 500 nM
MitoTracker Orange CMTMRos (Invitrogen) at 48C in light-protected
vessels with gentle shaking. Stained seedlings were washed two times
with PBS at 48C for 4 h with gentle shaking. Roots and stems were
mounted in PBS and visualized using a Zeiss Axiovert 200 inverted
fluorescence microscope, eGFP (filterset 38) and orange (filterset 20)
fluorescent filter blocks, an attached MRc5 Axiocam color digital camera,
and an LD Achroplan 403 objective.
Gene Expression Measurements
The expression of IDI1 and IDI2 in wild-type plant organs and homozy-
gous mutant seedlings was monitored by qRT-PCR and SYBR Green
assays. Primers were designed for each gene using Beacon Designer
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(version 5; PremierBiosoft) in the 39 UTR (IDI1utrF, IDI1utrR, IDI2utrF, and
IDI2utrR) (see Supplemental Table 1 online). The efficiencies of the
primers were determined by the standard curve method (Pfaffl, 2001)
and according to their individual amplification curves using the Lin-
RegPCR program (Ramakers et al., 2003). For comparative quantifica-
tion, six normalizer gene candidates were screened for similarity of overall
expression levels among different organs using purified cDNA from wild-
type Arabidopsis roots, stems, flowers, and leaves. For comparison of
organ-specific expression of IDI1 and IDI2, 2.0 mg of total RNA from each
of those tissues was reverse-transcribed using SuperScript III (Invitrogen)
in a 20-mL reaction according to the manufacturer’s instructions using
50 pmol of an anchored poly(dT) primer [d(T18V)]. For each tissue, four
independent biological replicates derived from individual soil-grown
plants were reverse-transcribed into cDNA. After 1 h at 508C, reactions
were diluted 1:10 with pure water. A 1-mL aliquot of this diluted template
containing ;0.2 ng of cDNA was analyzed in triplicate in 25-mL SYBR
Green assays in which leaves were used as a calibrator against each of
the other organs. Fold change differences for IDI1 and IDI2 expression in
each of the organs surveyed were calculated according to the efficiency-
corrected model (Pfaffl, 2001) using RP2LS (At4g35800) as a reference
gene. To measure IDI gene expression in homozygous knockout mutants,
whole plate-grown seedlings were used for total RNA extractions as
described above (four biological replicates and three technical replicates
of each), then analyzed by qRT-PCR as described above using wild-type
seedling transcript levels as a calibrator for fold change calculations.
Biochemical Characterization
For a comparison of the kinetic properties of the two IDI proteins, a
truncated version of each cDNA lacking the signal peptide but containing
a thrombin cleavage site was generated using the cytIDI1clv-attB1 and
cytIDI1stp-attB2 primers for idi1 and cytIDI2clv-attB1 and cytIDI2stp-
attB2 for idi2 (see Supplemental Table 1 online). Entry clones were
generated from these attB PCR products using pDONR207 as described
above. Fully sequenced entry clones were then used in LR Clonase
reactions with a Gateway-compatible form of the bacterial expression
vector pET28 (Yu and Liu, 2006) bearing nine N-terminal His residues to
yield cytIDI1-pH28 and cytIDI2-pH28. The truncation site was based on
the alignment of IDI1 and IDI2 to the start Met of the Escherichia coli IDI
protein (GI: 1789255). Following transformation of E. coli BL21(DE3)
competent cells with purified plasmids encoding cytIDI1-pET28 and
cytIDI2-pET28, a single colony of each was used to inoculate a 200-mL
culture of OverNight Express autoinduction medium (Novagen) supple-
mented with 1% (v/v) glycerol and 50 mg/mL kanamycin. Cultures were
grown at room temperature for 48 h (220 rpm), then centrifuged for 20 min
at 4400g and 48C. The pellet was resuspended in 10 mL of ice-cold 50 mM
Tris, pH 7.5, 10% (v/v) glycerol, 500 mM NaCl, 1 mM phenylmethylsul-
fonyl fluoride, 10 mM MgCl2, 10 mM imidazole, and 50 mg/mL lysozyme
and sonicated three times for 1 min each using a Bandelin HD2070
Sonoplus sonicator at 70% power. Lysates were centrifuged for 20 min at
31,000g and 48C. Crude extracts were purified on a Pharmacia His-
TrapHQ Ni affinity column using a fast protein liquid chromatography
protein purification system (Pharmacia-Amersham) by washing the
bound sample with resuspension buffer lacking phenylmethylsulfonyl
fluoride and lysozyme and eluting with the same buffer containing 125
mM imidazole.
Following affinity purification, the His tags were removed with a
thrombin cleavage capture kit (Novagen). The biotinylated thrombin
was removed with a strepavidin–agarose spin column, and the digested
proteins, judged to be >97% pure by SDS-PAGE, were subsequently
desalted into IDI assay buffer (50 mM Tris, pH 7.0, 10% [v/v] glycerol,
5 mM MgCl2, 200 mM KCl, 1 mM DTT, 0.1 mM MnCl2, and 0.1 mM ZnCl2)
using DG-10 desalting columns (Bio-Rad) and quantified using the
Bradford reagent (Bio-Rad). Proteins were diluted to 0.25 mg/mL and
assayed by the acid lability method (Satterwhite, 1985). For Km and kcat
measurements, reactions were performed in 100-mL volumes at six
different concentrations of [1-14C]IPP (American Radiochemicals; 50
mCi/mmol). For pH optima studies, a broad-range pH buffer consisting of
50 mM acetate, MES, and bis-Tris-propane was adjusted at whole pH
intervals from 4 to 10, and reactions were performed under linear
conditions at each pH in triplicate. Each reaction included 2.5 mg of
protein and took place at room temperature. After 15 min, reactions were
stopped by the addition of 1 volume of 1 N HCl and 1 mL of diethyl ether.
Hydrolysis of the acid-labile DMAPP isomer was performed at 378C for
30 min, followed by extraction two times with 1 mL of diethyl ether. The
organic phases were pooled, purified over a Pasteur pipette column
containing glass wool, silica gel, and anhydrous MgSO4, and finally
quantified by liquid scintillation counting. Km and kcat calculations were
determined using SigmaPlot version 7.0 and the Enzyme Kinetics module
version 1.1.
Isoprenoid Analysis
Five hundred milligrams of leaf tissue from wild-type and idi mutant plants
grown in 250-mL pots under continuous high light (600 mmol�m�2�s�1) at
258C was ground in liquid nitrogen and extracted with 2.5 mL of
acetone:water (9:1) in quadruplicate. For flower analysis, 100 mg of
wild-type or idi2-1 flowers was frozen, ground, and extracted in 1.0 mL
of CH2Cl2:acetone (1:1). A 300-mL aliquot of each floral extract was dried
under a nitrogen stream and resuspended in tetrahydrofuran. Sterols
were then derivatized with N-methyl-N-trimethylsilyltrifluoroacetamide
and analyzed by GC-MS. Both leaf and flower extracts were shielded
from light, and extraction was performed at 48C using a lab quake
followed by centrifugation at 16,000g (48C). A 10-mL aliquot of each
supernatant was analyzed by HPLC on an apparatus fitted with a diode
array detector using a Supelcosil C18 column (7.5 cm 3 4.6 mm) flowing
at 1.5 mL/min. The gradient consisted of water (A) and acetone (B),
running at 65% B for 4 min, then reaching 90% B at 12 min, and finally
100% B at 20 min, before returning to initial conditions. Carotenoids were
monitored at 445 nm and chlorophylls at 650 nm. Both classes of
compounds were identified based on their retention times and absorption
spectra compared with authentic standards.
For ubiquinone analysis, the same samples were analyzed on an 1100
series HPLC apparatus (Agilent Technologies) coupled to an Esquire
6000 ESI ion-trap mass spectrometer (Bruker Daltonics) operated in
positive mode in the range m/z 500 to 900. Specifics were as follows:
skimmer voltage, �40 eV; capillary exit voltage, �152.4 eV; capillary
voltage, �4000 V; nebulizer pressure, 35 p.s.i.; drying gas, 8 L/min; gas
temperature, 3308C. Elution was accomplished using a YMC-Pack C30
column (25 cm 3 4.6 mm, 5 mm; YMC) with a gradient of 99% methanol:
1% water (v/v) (solvent A) and tert-butyl-methylether (solvent B) at a flow
rate of 1.0 mL/min at 258C as follows: start, 0% B; 0 to 50% (v/v) B (25
min); 50 to 0% (v/v) B (1 min); 0% B (6 min). Flow coming from the column
was diverted in a ratio of 4:1 before entering the mass spectrometer
electrospray chamber. Ubiquinone-9 was detected in positive ion mode
and quantified by the integrated area of the extracted ion trace of the sum
of m/z 795.6 þ 817.6 þ 833.6 ([MþH]þ, [MþNa]þ, [MþK]þ).
59 RACE Cloning
Total RNA isolated from flowers or leaves was used to prepare RACE-
ready cDNA using the SMART RACE cDNA amplification kit (Clontech
Laboratories). Following a round of PCR using UPM and gene-specific
primers (IDI1RACE-R1 and IDI2RACE-R1), nested PCR was performed
using NUP and nested gene-specific primers (IDI1RACE-R2 and IDI2R-
ACE-R2). 59 RACE PCR products were purified on a 4% agarose gel,
excised, and cloned using the pCR4 TOPO-TA cloning kit (Invitrogen).
Cloning reaction products were used in transformations with TOP10 cells.
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Resulting positive colonies were grown in 5-mL Luria-Bertani cultures
containing 50 mg/mL kanamycin for plasmid mini-preps. Purified plas-
mids were sequenced using M13 and M13R primers.
Accession Numbers
Sequence data from this article can be found in the Arabidopsis Genome
Initiative or GenBank/EMBL databases under the following accession
numbers: Arabidopsis thaliana IDI1 (At5g16440), IDI2 (At3g02780), and
RP2LS (At4g35800); Clarkia breweri IPP isomerase 1 (X82627) and IPP
isomerase 2 (U48963); Escherichia coli IPP isomerase (NP_417365); and
Saccharomyces cerevisiae IPP isomerase (P15496).
Supplemental Data
The following materials are available in the online version of this article.
Supplemental Figure 1. Scheme for the Incorporation of [2-13C]
Mevalonate into Sitosterol.
Supplemental Figure 2. Sitosterol Mass Spectra from Mutant
Arabidopsis Plants.
Supplemental Figure 3. Upfield Portion of the 13C NMR Spectrum of
Purified Sitosterol Extracted from idi Mutant Arabidopsis Seedlings.
Supplemental Table 1. Primer Sequences Used in This Study.
ACKNOWLEDGMENTS
We thank Jenny Wrede, Katrin Luck, Claudia Wenderoth, Jana Pastuscheck,
and Martin Franke for their technical assistance and Andreas Weber and
the greenhouse staff at the Max Planck Institute for Chemical Ecology
(MPICE) for their assistance in caring for the Arabidopsis plants. Stefan
Opitz (MPICE) and Ales Svatos (MPICE) are thanked for their assistance
with phytosterol and ubiquinone analysis, respectively, and we thank
Joao Pedro Marques (Institut fur Pflanzenphysiologie, Halle, Germany)
for providing us with the ferredoxin-NADP(H) oxidoreductase-eGFP
positive control Arabidopsis line. We express our gratitude to Almut
Kießlich at the Carl Zeiss Applikationszentrum (Jena, Germany) for her
assistance with confocal microscopy. This work was carried out with
support from the Max Planck Society and a postdoctoral fellowship from
the Alexander von Humboldt Foundation (J.C.D.).
Received July 3, 2007; revised January 18, 2008; accepted February 7,
2008; published March 4, 2008.
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DOI 10.1105/tpc.107.053926; originally published online March 4, 2008; 2008;20;677-696Plant Cell
Michael A. Phillips, John C. D'Auria, Jonathan Gershenzon and Eran PicherskySubcellular Compartments and Have Overlapping Functions in Isoprenoid Biosynthesis
Type I Isopentenyl Diphosphate Isomerases Are Targeted to MultipleArabidopsis thalianaThe
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