A single gene encodes isopentenyl diphosphate isomerase isoformstargeted to plastids, mitochondria and peroxisomesin Catharanthus roseus
Gregory Guirimand • Anthony Guihur • Michael A. Phillips • Audrey Oudin •
Gaelle Glevarec • Celine Melin • Nicolas Papon • Marc Clastre • Benoit St-Pierre •
Manuel Rodrıguez-Concepcion • Vincent Burlat • Vincent Courdavault
Received: 17 February 2012 / Accepted: 5 May 2012 / Published online: 26 May 2012
� Springer Science+Business Media B.V. 2012
Abstract Isopentenyl diphosphate isomerases (IDI) cat-
alyze the interconversion of the two isoprenoid universal
C5 units, isopentenyl diphosphate and dimethylally
diphosphate, to allow the biosynthesis of the large variety
of isoprenoids including both primary and specialized
metabolites. This isomerisation is usually performed by
two distinct IDI isoforms located either in plastids/
peroxisomes or mitochondria/peroxisomes as recently
established in Arabidopsis thaliana mainly accumulating
primary isoprenoids. By contrast, almost nothing is known
in plants accumulating specialized isoprenoids. Here we
report the cloning and functional validation of an IDI
encoding cDNA (CrIDI1) from Catharanthus roseus that
produces high amount of monoterpenoid indole alkaloids.
The corresponding gene is expressed in all organs
including roots, flowers and young leaves where transcripts
have been detected in internal phloem parenchyma and
epidermis. The CrIDI1 gene also produces long and short
transcripts giving rise to corresponding proteins with and
without a N-terminal transit peptide (TP), respectively.
Expression of green fluorescent protein fusions revealed
that the long isoform is targeted to both plastids and
mitochondria with an apparent similar efficiency. Deletion/
fusion experiments established that the first 18-residues of
the N-terminal TP are solely responsible of the mitochon-
dria targeting while the entire 77-residue long TP is needed
for an additional plastid localization. The short isoform is
targeted to peroxisomes in agreement with the presence of
peroxisome targeting sequence at its C-terminal end. This
complex plastid/mitochondria/peroxisomes triple targeting
occurring in C. roseus producing specialized isoprenoid
secondary metabolites is somehow different from the sit-
uation observed in A. thaliana mainly producing house-
keeping isoprenoid metabolites.
Keywords Catharanthus roseus � Dual targeting �Isoprenoid � Isopentenyl diphosphate isomerase �Methylerythritol phosphate pathway � Mevalonate pathway
Introduction
Isoprenoids encompass an extraordinary variety of essen-
tial (primary) and specialized (previously named second-
ary) metabolites in bacteria, animals, and fungi and also in
plants in which more than 30,000 different molecules have
been identified to date. These molecules originate from
the head-to-tail condensation of the basic five-carbon units
isopentenyl diphosphate (IPP) and its allylic isomer
dimethylallyl diphosphate (DMAPP) (Sacchettini and
Electronic supplementary material The online version of thisarticle (doi:10.1007/s11103-012-9923-0) contains supplementarymaterial, which is available to authorized users.
G. Guirimand � A. Guihur � A. Oudin � G. Glevarec �C. Melin � N. Papon � M. Clastre � B. St-Pierre �V. Courdavault (&)
EA2106 ‘‘Biomolecules et Biotechnologies Vegetales’’,
Universite Francois Rabelais de Tours, 37200 Tours, France
e-mail: [email protected]
M. A. Phillips � M. Rodrıguez-Concepcion
Department of Molecular Genetics, Centre for Research
in Agricultural Genomics (CRAG), CSIC-IRTA-UAB,
08034 Barcelona, Spain
V. Burlat
Laboratoire de Recherche en Sciences Vegetales, Universite de
Toulouse, UPS, UMR 5546, BP 42617, 31326 Castanet-Tolosan,
France
V. Burlat
CNRS, UMR 5546, BP 42617, 31326 Castanet-Tolosan, France
123
Plant Mol Biol (2012) 79:443–459
DOI 10.1007/s11103-012-9923-0
Poulter 1997). Sequential condensations of IPP to DMAPP
lead to the synthesis of polyprenyl diphosphates of
increasing size such as geranyl diphosphate (C10), farnesyl
diphosphate (C15) or geranylgeranyl diphosphate (C20),
which could be further metabolized to monoterpenes, ses-
quiterpenes and diterpenes, respectively. While fungi and
animals synthesize both IPP and DMAPP via the mevalo-
nate (MVA) pathway, most of bacteria produce these pre-
cursors through the 2-C-methyl-D-erythritol 4-phosphate
(MEP) pathway. Interestingly, plants harbor both pathways
giving rise to specific end-products including phytosterols,
sesquiterpenes, triterpenes and the side-chain of ubiqui-
none for the MVA pathway (Bouvier et al. 2005) and
monoterpenes, diterpenes, carotenoids as well as the side-
chain of chlorophylls and tocopherols for the MEP pathway
(Rodrıguez-Concepcion and Boronat 2002). These specific
biosyntheses result from a complex subcellular compart-
mentalization within plant cells. Indeed, the MEP pathway
enzymes have been exclusively localized in plastids (Hsieh
et al. 2008) while the MVA pathway has been considered
until recently to occur mainly in the cytosol (Tholl and Lee
2011). However, the specific localization of the final steps
of the MVA pathway within peroxisomes has revealed a
more complex organization than previously supposed
(Sapir-Mir et al. 2008; Simkin et al. 2011). Both pathways
also differ by their terminal products since the MEP
pathway directly synthesizes both IPP and DMAPP (6:1
mixture) while the MVA pathway produces only IPP
(Bloch et al. 1959; Hoeffler et al. 2002; Rohdich et al.
2003). Due to the molar ratio required to synthesize the
different polyprenyl diphosphates, isomerization of IPP to
DMAPP is needed to allow an efficient isoprenoid bio-
synthesis, especially for the MVA pathway. The enzyme
IPP isomerase (IDI; EC 5.3.3.2) catalyzes the reversible
conversion of IPP to DMAPP and is found in all living
organisms (Ramos-Valdivia et al. 1997). Depending on the
cofactor required for activity, IDIs have been classified into
two types. Type I IDIs are zinc metalloproteins also
needing Mg2? for their catalytic activity (Muehlbacher and
Poulter 1988; Anderson et al. 1989; Carrigan and Poulter
2003; Lee and Poulter 2006). Type II IDIs are flavoproteins
requiring the reduced form of flavin mononucleotide and
Mg2? for activity and they have been identified in archaea
and some bacteria (Kaneda et al. 2001; Sharma et al. 2010).
Therefore, plants only display type I IDIs that are usually
encoded by two distinct genes (Campbell et al. 1998;
Cunningham and Gantt 2000; Nakamura et al. 2001). In
Arabidopsis thaliana, both genes (AtIDI1, At5g16440 and
AtIDI2, At3g02780) are expressed as long and short tran-
scripts encoding proteins that differ in length at their
N-terminal end (Phillips et al. 2008). Such mechanism
engenders a complex subcellular localization of the cor-
responding isoenzymes since AtIDI1 and AtIDI2 long
isoforms are targeted to plastids and mitochondria,
respectively (Phillips et al. 2008; Okada et al. 2008), while
both short isoforms are directed to peroxisomes (Sapir-Mir
et al. 2008) reflecting the compartmentalization of the MEP
and MVA pathways and the central role of IDI in iso-
prenoid biosynthesis. These combined studies have largely
contributed to the re-evaluation of the first model of type I
IDIs subcellular distribution in plant cells proposing a dual
localization within plastids and cytosol (Nakamura et al.
2001). In addition, by contrast with type II IDIs organized
in tetramers, elucidation of the crystal structure of the
Escherichia coli type I IDI indicates that they mainly
operate as monomers in agreement with plant IDI purifi-
cation (Ramos-Valdivia et al. 1997; Durbecq et al. 2001;
Kaneda et al. 2001). However, an elegant and sensitive
analysis of the yeast proteome complexes has revealed the
existence of type I IDIs self interactions in multi-protein
structures suggesting the existence of higher levels of
association (Gavin et al. 2002).
The current knowledge concerning the architecture of
the isoprenoid biosynthetic pathways and the IPP/DMAPP
isomerization in plant cells mainly relies on results
obtained in A. thaliana. However, a growing set of results
has been also produced during the last 10 years in plants
such as Catharanthus roseus displaying a particularly
active production of specialized isoprenoids (Hemmerlin
et al. 2012). C. roseus, also called Madagascar periwinkle,
is known to produce valuable monoterpenoid indole
alkaloids (MIA; Guirimand et al. 2010a), which contain an
isoprenoid moiety synthesized by the MEP pathway. In
C. roseus, we previously demonstrated that MEP pathway
genes and geraniol 10-hydroxylase gene (CrG10H) were
mainly expressed in a specialized tissue of aerial organs,
the internal phloem associated parenchyma (IPAP; Burlat
et al. 2004; Courdavault et al. 2005; Oudin et al. 2007)
and that a MEP pathway enzyme and geranylgeranyl
diphosphate synthase accumulated in the stroma of plas-
tids and in long stroma-filled chlorophyll-free protrusion
budding from plastids named stromules (Oudin et al.
2007; Guirimand et al. 2009; Thabet et al. 2012). In
addition, we have also recently established the pivotal role
of peroxisomes in isoprenoid production by the localiza-
tion of the enzymes catalyzing the final steps of the MVA
pathway in this subcellular compartment as well as those
of a farnesyl diphosphate synthase involved in sesquit-
erpenoid biogenesis (Clastre et al. 2011; Simkin et al.
2011; Thabet et al. 2011; Guirimand et al. 2012). To gain
further insight into the role of the enzyme compartmen-
talization during isoprenoid biosynthesis in plants dis-
playing an active production of specialized isoprenoids,
we describe here the characterization of C. roseus type I
IDI (CrIDI1), including the cloning and functional vali-
dation of the enzyme, the CrIDI1 transcript distribution
444 Plant Mol Biol (2012) 79:443–459
123
studied by real-time PCR and RNA in situ hybridization,
the IDI subcellular localization analyzed by fluorescent
protein fusion approaches and its propensity to self
interact in vivo using bimolecular complementation
assays. These analyses indicate that CrIDI1 displays a
triple subcellular localization in plastids/mitochondria and
peroxisomes suggesting that this single protein allows the
biosynthesis of distinct isoprenoids originated from either
the MVA or MEP pathways in three distinct subcellular
compartments.
Methods
Plant material and cell culture conditions
Mature C. roseus (L.) G. Don, cultivar Pacifica Pink
(Apocynaceae) plants grown from seeds (Ball Ducrettet,
Thonon, France) in the botanical garden of Tours were
harvested in summer for microscopy fixation (RNA in situ
hybridization experiments) and RNA extraction (cloning
experiments and gene expression measurements). C. roseus
cell suspensions used for subcellular localization studies
(C20A chlorophyll-free cells and CR6 chlorophyll con-
taining cells) were propagated in Gamborg B5 medium
(Duchefa) at 24 �C under continuous shaking (100 rpm)
for 7 days (C20A cells) or 14 days (CR6 cells) as previ-
ously described (Merillon et al. 1989; Kodja et al. 1989;
Guirimand et al. 2009).
RNA extraction and cDNA synthesis
After grounding of young leaves in liquid nitrogen, total
RNA was extracted using the NucleoSpin RNA Plant kit
(Macherey-Nalgel, France) according to the manufacturer’s
instructions. First-strand cDNA was synthesized from 5 lg
of total RNA using 500 ng of oligo(dT)18 primers and 15
units of Thermoscript reverse transcriptase (Invitrogen)
according to the manufacturer’s instructions. Following
retro-transcription, RNA complementary to cDNA was
removed by treatment with E. coli RNase H (Invitrogen)
during 20 min at 37 �C. For 50 RACE analysis, similar
reactions were carried out except that total RNA was sub-
sequently removed by treatment with RNase A (Sigma) and
the reaction product was purified using the NucleoSpin
Extract II kit. For real-time PCR, total RNA was extracted
with RNAeasy Plant mini kit (Qiagen) and treated (1.5 lg)
with RQ1 RNase-free DNase (Promega) before being used
for first-strand cDNA synthesis by priming with oligo (dT)17
(0.5 lM). Reverse transcription was carried out using
superscript III RT (Invitrogen) at 50 �C according to the
manufacturer’s instructions.
Cloning of the C. roseus cDNA encoding isopentyl
diphosphate isomerase 1
On the basis of the alignment of known plant IDI amino
acid sequences, a conserved region was identified and used
to design the degenerated primer IDIrev 1 (50-YTTRTGRA
TGSTYTTCATRCT-30). IDIrev1 was used in combination
with the M13 reverse universal primer to carry out PCR
amplifications on a kZAPII-oriented C. roseus cDNA
library using GoTaq DNA polymerase (Promega). A partial
cDNA encompassing the 50 end of a putative IDI coding
sequence was obtained and cloned into pGEM-T easy
vector (Promega) prior to sequencing. This sequence
allowed designing the ISOfor2 primer (50-TTGCTCTAA
TTCTACTACGCTTGC-30) used in combination with the
T7 universal primer to amplify the 30 end of the corre-
sponding cDNA using the C. roseus cDNA library as a
matrix. After sequencing of the resulting PCR product, the
two specific primers IPPfull-for (50-CCAACTCACTCATT
ACTACTCAAAAGCT-30) and IPPfull-rev (50-CTTAAAC
AGTGCACATCTAGAATACAGT-30) were then designed
to amplify a full-length open reading frame using Pfu DNA
polymerase (Promega). The resulting amplicon was cloned
into pSC-A vector (Stratagene) following A-tailing and
sequenced before deposition at NCBI under Genbank
accession number (EU135981).
Functional characterization of CrIDI1 and purification
of the recombinant enzyme
Based on ChloroP prediction (Table 1), a truncated cDNA
of CrIDI1 was amplified using primers pQE-IDI-Bam
(50-GCGGATCCATGGGTGCTGCCGTTACTGATTCC-30)and pQE-IDI-Hind (50-GCAAGCTTTTAAATCTTCTTGT
GAATGGTTTTCAT-30) to remove the 77 amino acid-
predicted transit peptide and to introduce BamHI and
HindIII restriction sites at the 50 and 30 end, respectively.
Amplification was performed using Pfu DNA polymerase
(Promega) and the corresponding PCR product was
cloned into pQE-30 (Qiagen, Courtaboeuf, France). After
sequencing, the plasmid expressing the pseudomature form
of CrIDI was used to carry out the functional character-
ization of IDI according to Phillips et al. (2008). The
recombinant protein was expressed in E. coli BL21 cells
cultivated at 37 �C in Luria–Bertani medium supplemented
with ampicillin (75 lg ml-1) under vigorous agitation
(250 rpm) until absorbance at 600 nm reached 0.6. After
addition of 1 mM isopropyl-b-D-thiogalactoside (IPTG),
cells were allowed to grow for 4 h under the same condi-
tions prior to protein purification with a Co2? column
according to the manufacturer’s protocol (Talon Resin
metal ion, Clontech). The quaternary structure of the pro-
tein was analyzed by migration in a native polyacrylamide
Plant Mol Biol (2012) 79:443–459 445
123
gel (PAGE) (12 %) following incubation with 10 mM
dithiothreitol (DTT) or water as previously described
(Takahashi et al. 1998).
Bioinformatic sequence analysis
The predictions of protein subcellular localization were
performed using PSORT (http://psort.ims.u-tokyo.ac.jp/),
Predotar (http://urgi.versailles.inra.fr/predotar/predotar.html),
ChloroP 1.1 (http://www.cbs.dtu.dk/services/ChloroP/), Mi-
toProt (http://ihg.gsf.de/ihg/mitoprot.html), TargetP 1.1 (http://
www.cbs.dtu.dk/services/TargetP/) and Target Signal Pre-
dictor (Target SP)—PTS1 binding sites (http://www.peroxiso
medb.org/diy_PTS1.html) softwares.
50 RACE analysis
A homopolymeric tail of cytosine was added at the 30 end
of the synthesized cDNA using terminal deoxinucleotidyl
transferase (Roche) according to the manufacturer’s
instructions. Unincorporated nucleotides and enzyme were
removed by purification using the NucleoSpin Extract II kit
and the purified cDNAs used as a matrix for nested PCR
using oligo(dG)18 primers and nested gene-specific primers
50 RACE-IDI2 (50-TGAACTCATCTACTGGGACATCTT
CAG-0) and 50 RACE-IDI3 (50-GATGGCTGCAGCATGT
GTTTGTC-30). 50 RACE PCR products were separated in a
2.5 % agarose gel, excised, purified and cloned into the
pGEM-T easy vector (Promega) prior to sequencing.
Gene expression measurements (real-time PCR
analysis)
The expression of the CrIDI1 (GenBank EU135981) and
RPS9 (GenBank AJ749993) genes was analyzed by real-
time PCR using primers qIDI-up (50-TGCTGCCGTTACT
GATTCCG-30), qIDI-down (50-ATACGCTGAAAGCCCT
GTGC-30), qRPS9-for (50-TTACAAGTCCCTTCGGTGG
T-30) and qRSP9-rev (50-TGCTTATTCTTCATCCTCTTC
ATC-30) on retro-transcribed RNA extracted from C.
roseus organs including roots, first internodes, young and
mature leaves, flower buds and flowers. Real-time PCR
was run on an ABI Prism 7000 SDS light cycler (Applied
Biosystems, Foster City, CA, USA) using the SYBR�
Green I technology. Each reaction was performed in a total
reaction volume of 25 ll containing 1 ll of a 1/3 dilution
of the first cDNA strand synthesis reaction, 0.2 lM for-
ward and reverse primers and 19 MESA GREEN qPCR
Master mix Plus buffer (Eurogentec, Angers, France). The
reaction was initiated by a denaturation step at 95 �C for
10 min, followed by 40 cycles at 95 �C for 15 s and 60 �C
for 1 min. CrRPS9 was used as a control gene to allow the
normalization of the gene copy numbers in each sample.
Each assay was performed in triplicate. Data correspond
to average values (n = 3) ± standard deviation (SD).
Relative transcripts levels in each sample are expressed as
a ratio of the abundance of the CrRPS9 transcripts and
normalized to the transcript level of young leaves that was
set to one for each gene separately.
In situ hybridization of C. roseus leaves
Full-length CrIDI1 cDNA cloned in pSC-A vector (Strat-
agene) was used for the synthesis of sense and anti-sense
RNA-probes as previously described (Mahroug et al.
2006). For CrG10H, a previously described plasmid was
used for the riboprobe transcription (Burlat et al. 2004).
Paraffin-embedded serial longitudinal sections of young
developing leaves were hybridized with digoxigenin-
labeled transcripts and localized with anti-digoxigenin-
alkaline phosphatase conjugates according to Mahroug
et al. (2006).
Constructs for subcellular localization studies
and bimolecular fluorescent complementation assays
The subcellular localization of CrIDI1 has been studied
by creating fluorescent fusion proteins using the pSCA-
Table 1 Predictions of CrIDI1 subcellular localization
Enzyme PSORT Predotar ChloroP MitoProt TargetP Target SP
CrIDI1 P (stroma) 0.928 P 0.89 Y (0.582)
77 residues
Y (0.922)
18 residues
cTP (0.779)
mTP (0.062)
0.8
HKLM (matrix) 0.595 M 0.11
P (thy mb) 0.595 E 0.10
For PSORT and Predotar predictions, the three most favorable localizations are reported with the corresponding score. For ChloroP, MitoProt
and TargetP predictions, the score of transit peptide presence and transit peptide length are given. For target signal predictor (Target SP)
prediction, the score and sequence of the peroxisome targeting sequence (PTS1) is given
cTP chloroplast transit peptide, E elsewhere, M mitochondria, mTP mitochondria transit peptide, P plastid, thy mb thylakoid membrane
446 Plant Mol Biol (2012) 79:443–459
123
cassette GFPi and pSCA-cassette YFPi plasmids (Guiri-
mand et al. 2009). Full-length ORF of CrIDI1 as well as
its truncated variants were amplified with Pfu DNA poly-
merase using the specific primers described in supple-
mental Table 1, designed to introduce BglII and/or SpeI
restriction sites at both cDNA extremities. After amplifi-
cation, these cDNA were sequenced and cloned in frame
with the 50 end of the GFP coding sequence to generate
CrIDI–GFP fusion protein for example. Details on primers
and constructs are given in supplemental Table 1. The
subcellular localization of AtIDI1 (At5g16440) and AtIDI2
(At3g02780) has been studied by a similar approach: the
AtIDI1 coding sequence has been amplified with primers
AtIDI1-Bgl (50-GTAGATCTGATGTCTACTGCTTCACT
ATTTAGCTTC-30) and AtIDI1-Spe (50-GTACTAGTGAG
CTTGTGAATGGTTTTCATGTCT-30) and cloned in the
BglII and SpeI restriction sites of the pSCA-cassette GFPi
plasmid; the AtIDI2 coding sequence has been amplified
with primers AtIDI2-for-Spe (50-GTACTAGTATGTCTG
CTTCTTCTTTATTTAATCTCCCATTG-30) and AtIDI2-
rev-Spe (50-GTACTAGTGAGTTTGTGGATGGTTTTCA
TGTCTATAGC-30) and cloned in the BglII restriction site
of the pSCA-cassette GFPi plasmid. For testing the effect
of the presence of an additional isoleucine residue located
downstream of the SKL PTS1 on the peroxisome import
efficiency, the YFP coding sequence of the pSCA-cassette
YFPi plasmid has been removed and replaced by an YFP
coding sequence coding for either YFP-SKL, amplified
with primers YFPfor2 (50-GAAGATCTGACTAGTATGG
TGAGCAAGGGCGAGGAGCTGTTCACC-30) and YF-
Prev-SKL-stop (50-GCGCTAGCTTACAGCTTCGAGCC
ACCGCCGCCGCCTCTAGATCCGGTGGATCTGAGTC
C-30) or YFP–SKLI, amplified with primers YFPfor2 (50-GAAGATCTGACTAGTATGGTGAGCAAGGGCGAGG
AGCTGTTCACC-30) and YFPrev-SKLI-stop (50-GCGCT
AGCTTAAATCAGCTTCGAGCCACCGCCGCCGCCTC
TAGATCCGGTGGATCTGAGTCC-30).The CrIDI1 self interactions have been characterized by
bimolecular fluorescence complementation (BiFC) assays
using the pSCA-SPYNE173 and pSCA-SPYCE(M) plas-
mids (Guirimand et al. 2010b) modified from original BiFC
plasmids (Waadt et al. 2008), which allow expressing
proteins fused to the N-terminal extremity of the two split-
YFP fragments (YFPN, residues 1–173 and YFPC, residues
156–239). Details on primers and cloning procedures are
given in supplemental Table 2. Negative control constructs
allowing the targeting of the split-YFP fragments to plas-
tids were generated by cloning the targeting peptide of IDI
(amplified with primers IDI–GFP–AS and pepATG4-rev)
at the 50 end of the coding sequence of the N-terminal
(YFPN, amino acids 1–173) and C-terminal (YFPC, amino
acids 156–239) fragments of YFP, in the BglII and SpeI
restriction sites of pSCA-SPYNE173 and pSCA-SPY-
CE(M). Interactions of the CrIDI1 long isoform have been
studied by the cloning of full length cDNA amplified with
primers IDI–GFP–S and IDI–GFP–AS, in the BglII and SpeI
restriction sites of pSCA-SPYNE173 and pSCA-SPY-
CE(M), to express tpIDI–YFPN and tpIDI–YFPC. Interac-
tions of the CrIDI short isoform have been studied by
creating internal split-YFP fusions within the CrIDI
sequence. For this purpose, the split-YFP coding sequence of
both pSCA-SPYNE173 and pSCA-SPYCE(M) has been
removed and replaced respectively by a split-YFPN and split-
YFPC coding sequence exhibiting the coding sequence of the
11 last residues of CrIDI1 at their 30 end. The coding
sequence of the CrIDI1 short isoform (devoid of the 11 last
residues) amplified with primers IDI-del3 and IDI-rev-del
was subsequently cloned in the BglII and SpeI restriction
sites of the resulting plasmids.
Biolistic transformation of C. roseus cells
and epifluorescence microscopy
Transient transformation of C. roseus cells by particle
bombardment and fluorescence imaging were performed
following the procedures described by Guirimand et al.
(2009, 2010b). Briefly, C. roseus plated cells were bom-
barded with DNA-coated gold particles (1 lm) and 1,100
psi rupture disc at a stopping-screen-to-target distance of
6 cm, using the Bio-Rad PDS1000/He system. Cells were
cultivated for 14 h to 38 h prior to being harvested, treated
and observed. The protein subcellular localization was
determined using an Olympus BX-51 epifluorescence
microscope equipped with an Olympus DP-71 digital
camera and a combination of YFP and CFP filters. The
pattern of localization presented in this work is represen-
tative of circa 50 observed cells.
Organelle markers and cell co-transformation
A set of organelle markers was used in co-transformation
experiments with the CrIDI–GFP constructs for identifi-
cation of the subcellular compartments accumulating
fusion proteins. The ‘‘plastid’’-mcherry (CD3–1,000) and
‘‘plastid’’-CFP (CD3–994) markers, ‘‘mitochondria’’-
mcherry (CD3–992) and ‘‘mitochondria’’-CFP (CD3–986)
markers, and the ‘‘peroxisome’’-CFP marker, described
by Nelson et al. (2007) were obtained from the ABRC
(http://www.arabidopsis.org). The mcherry-GUS cytosolic
marker and the mcherry nucleocytosolic marker were
described previously (Guirimand et al. 2011a). Plasmid
co-transformations were performed according to Guirimand
et al. (2009, 2011b) using 400 ng of each plasmid or 100 ng
for BiFC assays.
Plant Mol Biol (2012) 79:443–459 447
123
Results
Isolation of a C. roseus IDI (CrIDI1) full-length cDNA
A full-length cDNA sequence of a putative C. roseus IDI
(CrIDI1) was successively cloned from an oriented C.
roseus cells cDNA library. This amplified full-length
cDNA is 1,271-bp long and has been deposited at NCBI
under Genbank accession number (EU135981). Interest-
ingly, albeit degenerated primers were used for the first
rounds of amplification, no other sequences homologous to
CrIDI1 were amplified. In addition, Genbank EST database
screening only retrieved EST strictly homologous to CrIDI1
(supplemental Table 3) as well as in the 653,830 EST
sequences of the MAGPIE database (V. De Luca, personal
communication). However, contigs of a putative second
isoform (named CrIDI2) were identified in the Medicinal
Plant Genomics Resource (http://medicinalplantgenomics.
msu.edu/) but the associated transcriptomic data reveal
that CrIDI2 mRNAs are barely detectable as compared to
those of CrIDI1 (supplemental Table 4). Such EST/mRNA
distributions strongly suggest that CrIDI1 is the mainly
expressed isoform in C. roseus plants. As a consequence,
this work has been focused on the sole characterization of
this isoform.
The 936-bp open reading frame of CrIDI1 encodes a
311-residues long protein with an estimated mass of
35 kDa. Amino acid comparison highlights the high degree
of identity of CrIDI1 with plant orthologs (89 and 88 %
with AtIDI1 and AtIDI21, respectively) as well as with
bacterial and yeast ones (21 and 32 %, respectively)
(Fig. 1). In addition, this protein displays the fourteen
residues composing the conserved active site of IDIs as
well as a Nudix (Nucleoside Diphosphate linked to X)
motif of the Nudix hydrolase family, classically found in
phosphohydrolases and other IDIs (Fig. 1). CrIDI1 also
~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~~ CrIDI 1 MSSTLTTSYFQTILKRISVCSLPSSTSSSNSLYPILLKHKFSSFPSVSFSSSASSPC-------SNSTTLAAFSSIAAPS AtIDI1 1 --------------------------MSTASLFSFPSFHLRSLLPSLSSSSSSSSSRFAPPRLSPIRSPAPRTQLSVRAF AtIDI2 1 --------------------------MSASSLFNLPLIRLRSLALSSSFSSFRFAHR-------PLSSISPRKLPNFRAF EcIDI 1 -------------------------------------------------------------------------------- ScIDI 1 ------------------------MTADNNSMPHGAVSSYAKLVQNQTPEDILEEFP-------EIIPLQQRPNTRSSET
~~~ # # # # # #CrIDI 74 FSSMGAAVTDSAMDAVQRRLMFEDECILVDENDHVVGHDTKYNCHLMEKIESENLLHRAFSVFLFNSKFELLLQQRSATKAtIDI1 55 SAVTMTDSNDAGMDAVQRRLMFEDECILVDENDRVVGHDTKYNCHLMEKIEAENLLHRAFSVFLFNSKYELLLQQRSKTKAtIDI2 48 SGTAMTDTKDAGMDAVQRRLMFEDECILVDETDRVVGHDSKYNCHLMENIEAKNLLHRAFSVFLFNSKYELLLQQRSNTKEcIDI 1 --------------------MQTEHVILLNAQGVPTGTLEKYAAHT-----ADTRLHLAFSSWLFNAKGQLLVTRRALSKScIDI 50 SNDESGETCFSGHDEEQIKLMNEN-CIVLDWDDNAIGAGTKKVCHLMENIE-KGLLHRAFSVFIFNEQGELLLQQRATEK
# # # # # # # CrIDI 154 VTFPLVWTNTCCSHPLYRESELIE-----ENVLGVRNAAQRKLLDELGIVA-EDVPVDEFMPLGRMLYKAPSDGIWGEHEAtIDI1 135 VTFPLVWTNTCCSHPLYRESELIE-----ENVLGVRNAAQRKLFDELGIVA-EDVPVDEFTPLGRMLYKAPSDGKWGEHEAtIDI2 128 VTFPLVWTNTCCSHPLYRESELIQ-----DNALGVRNAAQRKLLDELGIVA-EDVPVDEFTPLGRMLYKAPSDGKWGEHEEcIDI 56 KAWPGVWTNSVCGHPQLGESNEDAVIRRC------RYELGVEITPPESIYP-DFRYRATDPSGIVENEVCPVFAARTTSA ScIDI 128 ITFPDLWTNTCCSHPLCIDDELGLKGKLDDKIKGAITAAVRKLDHELGIPEDETKTRGKFHFLNRIHYMAPSNEPWGEHE
# CrIDI 228 LDYLLFIVRDVKVN----PNPDEVADVKYMTRDDLKELLRKADAGEEGLKLSPWFRLVVDNFLFKWWDHVEKGTLLEAADAtIDI1 209 VDYLLFIVRDVKLQ----PNPDEVAEIKYVSREELKELVKKADAGDEAVKLSPWFRLVVDNFLMKWWDHVEKGTITEAADAtIDI2 202 LDYLLFIVRDVKVQ----PNPDEVAEIKYVSREELKELVKKADAGEEGLKLSPWFRLVVDNFLMKWWDHVEKGTLVEAIDEcIDI 129 LQINDDEVMDYQWC----DLADVLHGIDATPWAFSPWMVMQATNREARKRLSAFTQLK---------------------- ScIDI 208 IDYILFYKINAKENLTVNPNVNEVRDFKWVSPNDL-----KTMFADPSYKFTPWFKIICENYLFNWWEQLDDLSEVENDR
CrIDI 304 MKTIHKLI AtIDI1 285 MKTIHKL- AtIDI2 278 MKTIHKL- EcIDI -------- ScIDI 283 QIHRML--
* * *
mTP cTP
PTS1
Fig. 1 Multiple sequence alignment of type I IDIs. Amino acid
comparison of IDI from C. roseus (CrIDI1; GenPept ABW98669) with
A. thaliana long isoform 1 (AtIDI1, AGI accession number
At5g16440), A. thaliana long isoform 2 (AtIDI2, AGI accession
number At3g02780), E. coli (EcIDI, GenPept NP_417365) and
Saccharomyces cerevisiae (ScIDI; GenPept NP_015208). Identical
and similar residues are highlighted by dark and gray shading,
respectively. Asterisks indicate methionine residues conserved in IDI
from plant species and the horizontal bar represents the conserved
region of the N-terminal extension. #Designates the conserved catalytic
residues of IDI according to the NCBI conserved domain search.
Arrowheads delimitate the Nudix hydrolase conserved sequence
(PFAM00293). Putative type 1 peroxisome targeting sequence
(PTS1), mitochondrial (mTP) and chloroplast (cTP) target peptides
are shown
448 Plant Mol Biol (2012) 79:443–459
123
contains an N-terminal extension of 93 residues as com-
pared to E. coli IDI, which is moreover 18- and 25-residues
longer than the AtIDI1 and AtIDI2 extension, respectively
(Fig. 1). Such extension ends with a conserved region
containing three methionine residues conserved in plant
IDI that could be used for alternative initiation of transla-
tion (Cunningham and Gantt 2000; Phillips et al. 2008).
Since plant IDIs display a complex localization within
cells, the subcellular targeting features of CrIDI1 were
investigated with protein subcellular localization prediction
servers. As detailed in Table 1, most of the algorithms
predicted a plastidial localization based on the identifica-
tion of a putative plastid targeting peptide (TP) of 77 res-
idues (ChloroP prediction) located in the N-terminal
extension of CrIDI1. Interestingly, both PSORT and Mi-
toprot predicted a putative mitochondrial localization with
a high confidence for Mitoprot based on the identification
of a mitochondrial TP corresponding to the first 18-residues
of CrIDI1 (Fig. 1). Finally, the target signal predictor of the
peroxisome database also detected a potential type I per-
oxisome targeting sequence (PTS1) at the C-terminal end
of the protein (HKL, residues 308–310) as previously
observed in both Arabidopsis IDIs (Sapir-Mir et al. 2008)
albeit an additional isoleucine residue was present down-
stream of the PTS1 in CrIDI1 (Fig. 1).
Functional characterization of CrIDI1
To confirm that the cloned cDNA encodes a functional
IDI, the activity of the recombinant protein has been
evaluated by the measurement of the catalytic conversion
of IPP into DMAPP (Fig. 2). Since the N-terminal exten-
sions of plant IDIs are not required for enzyme activity
(Campbell et al. 1998), the recombinant protein was
expressed as a truncated protein (Fig. 2a), devoid of the
first 76 residues, after cloning the deleted coding sequence
in the pQE-30 plasmid (IDI–pQE). The amount of isom-
erized IPP was measured in protein extracts from IDI–pQE
transformed BL21 E. coli cells in comparison with protein
extracts from untransformed BL21 cells and boiled protein
extracts from IDI to pQE transformed BL21 cells (control
conditions). Extracts were obtained from cultures adjusted
to nearly identical cell densities. A significant IPP isom-
erization ([1.50 nmol h-1) was measured in the induced
protein extracts from IDI–pQE transformed cells with no
significant background in control conditions (Fig. 2b). IPP
isomerization (0.44 nmol h-1) was also obtained in the
uninduced protein extract from these cells, resulting
probably from uncontrolled expression from the plasmid
promoter as observed in Fig. 2a. On the basis of these
results and the high identity of CrIDI1 to previously
characterized plant IDIs, it could be assumed that CrIDI1
encodes a functional IDI.
Spatial distribution of CrIDI1-encoding transcripts
The distribution of the CrIDI1 transcripts was first ana-
lyzed by real-time PCR (qPCR) within distinct organs of
fully developed C. roseus plants. CrIDI1 mRNAs were
detectable in all the tested organs with two patterns of
expression (Fig. 3a). In roots, young leaves and flowers of
C. roseus, CrIDI1 transcript levels are circa twofold higher
than those measured in internodes, mature leaves and
flower buds in agreement with transcriptomic data (sup-
plemental Table 4). This represents an intermediate situa-
tion as compared to A. thaliana where the highest amount
of AtIDI1 and AtIDI2 gene products are mainly restricted to
flowers and roots, respectively (Okada et al. 2008; Phillips
et al. 2008).
The tissue-specific distribution of CrIDI1 transcripts was
subsequently investigated by RNA in situ hybridization
performed on serial sections of young developing C. roseus
leaves since these organs constitute the main site of CrIDI1
expression as revealed by qPCR analysis. As depicted on
Fig. 3b, labeling with the antisense probe allowed detecting
CrIDI1 transcripts in the adaxial part of the leaf vascular
Fig. 2 Functional characterization of CrIDI1. a SDS–PAGE of
protein crude extracts from E. coli cells harboring the pQE-30 empty
vector or the pQE-30-IDI vector after 0, 2 or 4 h following the
induction of protein expression. b The functional activity of
recombinant CrIDI1 was evaluated by the measurement of the IPP
to DMAPP catalytic conversion as described by Phillips et al. (2008)
Plant Mol Biol (2012) 79:443–459 449
123
region, corresponding to the internal phloem associated
parenchyma (IPAP) cells as confirmed by the colocalization
of CrG10H mRNA in this tissue (Fig. 3d; Burlat et al. 2004).
Transcripts were also detected in both the adaxial and
abaxial epidermis of leaves albeit the mRNA level was
dramatically lower than those measured in IPAP cells
(Fig. 3b). No significant background was observed using the
sense probes (Fig. 3c, e). On the basis of these results, it
could be hypothesized that the distribution of CrIDI1 tran-
scripts is restricted to the major sites of isoprenoid biosyn-
thesis within C. roseus leaves.
CrIDI1 is expressed as short and long transcripts
In A. thaliana, AtIDI1 and AtIDI2 are both expressed as
long and short isoforms that differ by the presence of either
a plastid (AtIDI1) or a mitochondrion (AtIDI2) TP at the
N-terminal end of the long isoform. This mechanism
directly influences the subcellular localization of the cor-
responding proteins since AtIDI1 long isoform is mostly
targeted to plastids and the AtIDI2 long isoform is mostly
targeted to mitochondria while both short isoforms are
sorted to peroxisomes via a type 1 PTS1 located at the
C-terminal end of the proteins (Okada et al. 2008; Phillips
et al. 2008; Sapir-Mir et al. 2008). To determine whether
this kind of alternative transcription also occurs for CrIDI1,
50 RACE was performed on RNA extracted from young C.
roseus leaves. Separation of amplification products by
electrophoresis allowed identifying cDNAs of two different
sizes (Fig. 4a). Sequence analysis revealed that the longer
50 RACE products originate from full-length transcripts
including the initiation codon of the putative plastid/
mitochondrion TP (Fig. 4b; Table 1). The shorter 50 RACE
products lack 145 bp at the 50 end and begin 37 bp
downstream of this initiation codon but contain three
internal Met codons that could initiate translation of a
shorter CrIDI1 isoform lacking the putative plastid/mito-
chondrion TP. These results demonstrate that similar pro-
cesses of alternative transcription exist for IDI genes in A.
thaliana and C. roseus yielding to the formation of long
and short isoforms of CrIDI1, bearing or not the N-terminal
transit TP.
CrIDI1 long isoform is dually targeted to plastids
and mitochondria
The presence of both long and short isoforms of CrIDI1
prompted us to study the localization of both types of
protein within C. roseus cells. The subcellular localization
of the long isoform was first investigated by GFP/YFP
tagging. The full length coding sequence of CrIDI1 was
fused to the N-terminal end of GFP and the corresponding
construct was transiently expressed in C. roseus cells
(Fig. 5a). The IDI–GFP fusion protein displayed a dual
pattern of fluorescence signal located in both plastids
including stromules, and mitochondria as confirmed by co-
localisation with specific markers of each compartment
(Fig. 5b–m). This dual targeting appears to occur at an
apparent similar efficiency as suggested by the high fluo-
rescence observed in plastids or mitochondria. Interest-
ingly, this differs from the situation described in A.
Fig. 3 Analysis of CrIDI1 transcript distribution in C. roseus.
a Analysis of CrIDI1 transcript levels as determined by real-time
RT–PCR analyses from different C. roseus organs. Total RNA was
extracted from organs and subjected to reverse transcription. Tran-
script levels for CrIDI1 and CrRPS9 were determined by real-time
PCR using gene-specific primers. CrIDI1 expression level was
normalized using CrRPS9. The transcript level of young leaves was
set to ‘‘1’’. b–e Cellular distribution of CrIDI1 transcripts in young
leaves analyzed by in situ RNA hybridization. Paraffin-embedded
serial sections of young leaves were hybridized with digoxigenin-
labelled transcripts, which were subsequently localized with anti-
digoxigenin-alkaline phosphatase conjugates followed by nitro blue
tetrazolium chloride (NBT)/5-bromo 4-chloro-3-indolyl phosphate
(BCIP) color development. Hybridization of the geraniol 10-hydrox-
ylase (CrG10H) transcripts was used as a positive control. The anti-
sense (AS) probes used for RNA labeling (b, d) and control
hybridization with sense (S) RNA probes (c, e) are mentioned on
the figure. Arrows and arrowheads show labeling within the internal
parenchyma associated phloem (IPAP) and both the adaxial and
abaxial epidermis, respectively. Bars 100 lm
450 Plant Mol Biol (2012) 79:443–459
123
thaliana in which a preferential localization to either
plastids or mitochondria has been described for AtIDI1 and
AtIDI2, respectively (Phillips et al. 2008) and confirmed in
C. roseus cells (Supplemental Fig. 1). To gain insight into
this dual localization, fusion/deletion experiments of the
predicted TP of CrIDI1 were also conducted. First, pre-
dicted TP of various lengths (from the first residue to
residues surrounding one of the three internal methionine
residues) were fused to YFP and transiently expressed in
C. roseus cells (Fig. 6a). Irrespective to the length of the
TP, a dual localization in plastids and mitochondria was
observed as exemplified for the shorter (pepATG1) and
longer (pepATG4) peptide, respectively (Fig. 6b–i). The
same dual localization was also observed for the two
additional constructs pepATG2 and pepATG3 (data not
shown). Similarly, gradually TP deleted versions of CrIDI1
were expressed as YFP-fused proteins initiated from each
of the three internal methionine residues (Fig. 6j). For the
three constructs, a similar nucleocytosolic localization was
observed as illustrated by the perfect overlapping of fluo-
rescence with the mcherry nucleocytosolic marker as
exemplified for the deletion of the first 76-residues (IDI-
del1, Fig. 6k–n). Taken together, these results show that
the first 76 residues of CrIDI1 encompass the minimal TP
of this enzyme and are solely responsible for the dual
mitochondria/plastids targeting. In addition, since the
extreme N-terminus of CrIDI1 has been predicted to allow
a mitochondrial targeting (Table 1), the first 18-residues
of the CrIDI1 TP were also fused to GFP (Fig. 7a). In C.
roseus transiently transformed cells, the corresponding
fusion protein displayed a specific localization in mito-
chondria as revealed by the merge of fluorescence with the
mito-mcherry marker (Fig. 7b–e). However, the remaining
part of the TP (including residues 19–76, Fig. 7f) was
unable to address the fusion protein to plastids or mito-
chondria (Fig. 7g–j). This suggests that the first 18 residues
of CrIDI1 TP allow the mitochondrial targeting but are also
required for the plastidial targeting in association with the
remaining part of the TP.
CrIDI1 short isoform is targeted to peroxisomes
Since short isoforms of AtIDI1 and AtIDI2 are addressed to
peroxisomes (Sapir-Mir et al. 2008), the potential targeting
of the CrIDI1 short isoform to this subcellular compart-
ment has been also investigated. For this purpose, YFP
internal fusions were constructed to maintain the accessi-
bility of the putative PTS1 (HKL) located at the C-terminal
extremity of CrIDI (Fig. 8). As previously mentioned by
Sapir-Mir et al. (2008), the sole addition of the predicted
PTS1 or the entire CrIDI1 short isoform to the C-terminal
end of YFP failed to target the fusion protein to peroxi-
somes. A similar result was also obtained for the YFP
internal fusion proteins engaging the last 11 residues of
CrIDI1 at the C-terminus of YFP and the remaining part of
the short isoform at the N-terminus of YFP (data not
shown). As a consequence, internal fusions within long and
short versions of CrIDI1 were performed with a modified
version of YFP flanked by 6 or 7 residues-long spacers
(Fig. 8a, f) as previously performed by Sapir-Mir et al.
(2008). In C. roseus transiently transformed cells, the
fusion protein engaging the CrIDI1 long isoform (tp-IDI–
YFP–PTS1, Fig. 8a) displayed a dual fluorescence signal
located in plastids and mitochondria as revealed by the
Fig. 4 The CrIDI1 gene displays two transcripts of different length.
a 50 RACE analysis was conducted on RNA extracted from young
C. roseus leaves allowing the amplification of long (a) and short
(b) products. b Nucleotidic and deduced amino-acid sequences of the
two RACE products. The initiation codon of the full length coding
sequence and the alternative internal initiation codon of short
transcripts are indicated by solid lines
Plant Mol Biol (2012) 79:443–459 451
123
overlapping with the fluorescence signal emitted by the
‘‘mito’’-CFP marker and by the comparison with plastid
morphology (Fig. 8b–e). By contrast, the localization
studies of the fusion protein engaging the CrIDI1 short
isoform (IDI–YFP–PTS1, Fig. 8f) resulted in a simple
punctuated fluorescence, which entirely overlaps the fluo-
rescence signal of the peroxisome-CFP marker (Fig. 8g–j).
This demonstrates that the CrIDI1 short isoform is targeted
to peroxisomes despite the presence of an additional iso-
leucine residue located downstream of the PTS1. The
absence of effect of this residue after a PTS1 has also been
confirmed by the peroxisomal targeting of both the YFP–
SKLI and YFP–SKL fusion proteins (Supplemental Fig. 2).
Taken together, these results show that the gene products of
CrIDI1 displayed a unique triple localization within cells
including a dual targeting to plastids and mitochondria for
the long isoforms and a peroxisome targeting for the short
isoforms.
Fig. 5 CrIDI1–GFP is targeted to the plastids and mitochondria. C.roseus cells were transiently co-transformed with plasmids expressing
the CrIDI1–GFP fusion proteins (a, b, f, j) and the ‘‘plastid’’-mcherry
(c, g) or ‘‘mitochondria’’-mcherry (k) markers. Co-localization of the
two signals appeared in yellow while merging the two individual
(green/red) color images (d, h, l). Cell morphology is observed with
differential interference contrast (DIC, e, i, m). Bars 10 lm
Fig. 6 N-terminus target peptides of different length from the CrIDI1
long isoform allow the dual targeting to plastids and mitochondria. C.roseus cells were transiently co-transformed with plasmids expressing
the truncated version of the transit peptide of CrIDI1 fused to GFP
including the 76 (pepATG1), 81 (pepATG2), 91 (pepATG3) or 97
(pepATG4) first residues (a, b, f) or transit peptide deleted version of
CrIDI1 (initiated at residue 77 for IDI-del1, 86 for IDI-del2 or 94 for IDI-
del3) fused to GFP (j, k) and the ‘‘plastid’’-mcherry (c), ‘‘mitochondria’’-
mcherry (g) or ‘‘nucleocytosolic’’-mcherry (l) markers. Co-localization
of the two signals appeared in yellow while merging the two individual
(green/red) color images (d, h, m). Cell morphology is observed with
differential interference contrast (DIC, e, i, n). Bars 10 lm
c
452 Plant Mol Biol (2012) 79:443–459
123
CrIDI1 is capable of self-interactions in plastids,
mitochondria and peroxisomes
Since systematic analysis of protein complexes strongly
suggested that type I IDIs are able of self-interactions in
yeast (Gavin et al. 2002), we performed BiFC assays in C.
roseus cells. The full coding sequence of CrIDI1 was
cloned in frame with the 50 end of the coding sequence of
the two split-YFP fragments (YFPN and YFPC) to generate
the IDI–YFPN and IDI–YFPC fusion proteins bearing an
accessible N-terminal TP. As a control, the two split-YFP
fragments were also fused to the sole TP of CrIDI1. This
allowed to target the two split-YFP fragments to plastids
and mitochondria as pseudo-mature non fused protein
(tpIDI–YFPN; tpIDI–YFPC) and to evaluate the spontane-
ous association of these proteins and the resulting non
specific fluorescence in cell organelles. As shown in
Fig. 9a–d, the transient expression of the two control pro-
teins in C. roseus cells did not result in the reformation of a
BiFC complex since no fluorescence was detected, dem-
onstrating that the two split-YFP fragments were unable
to interact in the absence of a protein partner under
our experimental conditions. By contrast, the transient
co-expression of IDI–YFPN and IDI–YFPC gave a fluo-
rescent signal in both plastids and mitochondria (Fig. 9e–k)
as previously observed for IDI–GFP (Fig. 5a–m). This
suggests that CrIDI1 is able of self-interaction in these two
types of organelles. In addition, since CrIDI1 is also tar-
geted to peroxisomes, the ability of the protein to self-
interact within this compartment was studied by the creation
of internal fusions with the split-YFP fragments on the basis
of those constructed for the analysis of the subcellular
localization of the CrIDI1 short isoform (Figs. 8f, 9l). Using
these constructs, we also observed the formation of a BiFC
complex within peroxisomes as revealed by the perfect
overlapping of the YFP signals and of the CFP peroxisome
marker (Fig. 9m–o), suggesting that CrIDI1 is also able of
self interaction within this subcellular compartment. Self-
interaction capacities were further confirmed using the
purified recombinant enzyme (Fig. 9p) following migration
on native PAGE (Fig. 9q). In this condition, the recombi-
nant enzyme displayed distinct levels of organization
including complexes of low and high molecular weights as
revealed by the presence of slow and fast migrating bands
on the gel. Following the incubation of the enzyme with
DTT, the slow migrating bands tempted to disappear to the
Fig. 7 The first 18-residues of the CrIDI1 long isoform transit
peptide allow the unique mitochondrial targeting. C. roseus cells were
transiently co-transformed with plasmids expressing the first 18-res-
idues of the CrIDI1 transit peptide fused to GFP (a pepIDI-mito) or
the remaining part of the transit peptide (residues 19–76) fused to
GFP (f, pepIDI-D) with the ‘‘mitochondria’’-mcherry (c) and ‘‘nucle-
ocytosolic’’-mcherry (h) markers, respectively. Co-localization of the
two signals appeared in yellow while merging the two individual
(green/red) color images (d, i). Cell morphology is observed with
differential interference contrast (DIC, e, j). Bars 10 lm
454 Plant Mol Biol (2012) 79:443–459
123
benefit of the fastest migrating band. This confirms that
CrIDI1 is able of self-interactions and suggests that the
formation of the higher molecular weight complexes also
requires disulfide bonds. However, DTT concentration had
virtually no effect on CrIDI1 activity in our in vitro assays,
suggesting that protein–protein interactions are not strictly
required for CrIDI1 activity.
Discussion
Isomerization of IPP into DMAPP is a crucial step for the
synthesis of isoprenoids of various lengths and nature. In
plant cells, this reaction is catalyzed by type 1 IDIs that
display a complex subcellular localization well character-
ized in A. thaliana (Okada et al. 2008; Phillips et al. 2008;
Sapir-Mir et al. 2008). To pursue this characterization in
plants producing high amount of specialized isoprenoids,
we have cloned and functionally validated a cDNA
encoding a type 1 IDI from C. roseus (CrIDI1), a plant
widely studied due to its capacity to synthesize valuable
MIA (Facchini and De Luca 2008). Albeit generally
encoded by at least two distinct genes (Campbell et al.
1998; Cunningham and Gantt 2000; Nakamura et al. 2001),
a single sequence was amplified during this work. Inter-
estingly, a search in C. roseus EST database preferentially
identify the CrIDI1 sequence (Supplemental Table 3)
suggesting that the other IDI putative gene(s) and espe-
cially CrIDI2 are expressed at very low level and/or under
specific conditions as confirmed by the transcriptomic data
obtained from the MPGR (supplemental Table 4). The
analysis of the mRNA organ distribution of the CrIDI1 by
qPCR also revealed that the corresponding transcripts
could be detected in all the tested organs with the highest
amount measured in roots, young leaves and flowers
(Fig. 3a). The organ-specific expression profile of CrIDI1
somehow corresponds to the addition of the expression
profiles of both Arabidopsis IDIs since the highest
expression of AtIDI1 and AtIDI2 has been detected in
flowers and roots, respectively (Phillips et al. 2008). This
Fig. 8 An accessible C-terminal peroxisomal targeting sequence-1
allows the peroxisomal targeting of the short CrIDI1 isoform. C.roseus cells were transiently co-transformed with plasmids expressing
internal YFP fusion of the long (a, b) and short (f, g) isoforms of
CrIDI1 with the ‘‘mitochondria’’-CFP (c) and ‘‘peroxisome’’-CFP
(h) markers, respectively. Glycine and alanine containing spacers
were added at both extremities of YFP as mentioned in italic on the
schematic representations of the constructs. Co-localization of the two
signals appeared in yellow while merging the two individual (green/
red) color images (d, i). Cell morphology is observed with differential
interference contrast (DIC, e, j). Bars 10 lm
Plant Mol Biol (2012) 79:443–459 455
123
correlates with the fact that a single coding sequence of IDI
seems to be highly expressed in C. roseus. At the cellular
level, we have established using RNA in situ hybridization
that CrIDI1 is mainly expressed in IPAP cells of young
developing leaves as previously described for MEP path-
way genes and G10H, the enzyme catalyzing the first
committed step in the formation of the monoterpenoid
precursor of MIA (Fig. 3b–e) (Burlat et al. 2004; Cour-
davault et al. 2005). This reinforces the identification of
IPAP as a prominent tissue in isoprenoid biosynthesis in
C. roseus. In addition, low amounts of transcripts were also
detected in both the adaxial and abaxial epidermis of leaves
in agreement with the identification of CrIDI1 EST within
the C. roseus leaf epidermis database (Murata et al. 2008)
and with the immunolocalization at low levels of a MEP
pathway enzyme within this tissue (Oudin et al. 2007). C.
roseus leaf epidermis has also been described as the main
site of the MVA pathway activity on the basis of the
selective gene expression profiles in this tissue (Murata
et al. 2008). Previous works in A. thaliana using mutant
analysis, radiolabelled precursor feeding and subcellular
localizations, have shown that the two IDI genes have
partially redundant functions, rendering difficult the
assignation of each isoform to either MVA or MEP path-
ways (Okada et al. 2008; Phillips et al. 2008). However, on
the basis of the cellular distribution of the CrIDI1 tran-
scripts and according to the relative abundance of CrIDI1
mRNA as compared to CrIDI2 mRNA (supplemental
Table 4), we could hypothesize that CrIDI1 isomerizes IPP
from the MEP and/or MVA pathways in a tissue-dependant
manner. Assuming that the MVA pathway is mainly
located in the epidermis of C. roseus leaves (Murata et al.
2008) and that the epidermis also houses low level of MEP
pathway enzymes (Oudin et al. 2007; Murata et al. 2008), it
could be hypothesized that CrIDI1 isomerizes IPP from
both pathways in this tissue allowing for instance the
synthesis of epidermal triterpenes from the MVA pathway.
By contrast, in IPAP cells that constitute the main site of
expression of MEP pathway genes and CrG10H, we could
reasonably think that the strong CrIDI1 expression should
be related to the isomerization of MEP-pathway derived
IPP needed for the synthesis of the monoterpenoid pre-
cursor of MIA in this tissue.
Fig. 9 CrIDI1 is able of self-interaction within plastids, mitochondria
and peroxisomes of C. roseus cells. Analysis of the CrIDI1 self
interactions was conducted by BiFC following co-transformation of
C. roseus cells using a combination of plasmids expressing the
negative control tpIDI-YFPN and tpIDI-YFPC (a–d), the CrIDI1 long
isoform fused to the split-YFP fragments IDI-YFPN and IDI-YFPC
(e–k) and internal fusions of the split-YFP fragments within the
CrIDI1 short isoform IDI-YFPN-PTS1 and IDI-YFPC-PTS1 (l–o). C.roseus cells were transiently co-transformed with each pair of
plasmids and either ‘‘plastid’’-CFP (g), ‘‘mitochondria’’-CFP (j) and
‘‘peroxisome’’-CFP (n) marker. The morphology was observed by
differential interference contrast (DIC) microscopy and combined
with the marker fluorescence signals (c, g, j, n). Superimpositions of
these combined images and of the YFP fluorescence signal emitted by
the BiFC complexes are provided on the merged images (h, k, o).
Bars 5 lm. p Purification profile of the recombinant CrIDI1 protein
analyzed by SDS–PAGE. M protein standards. q Native PAGE of the
purified enzyme incubated 10 min at room temperature in the
presence of water or 10 mM DTT. Arrowheads and stars indicate
fast and slow migrating bands on the gel, respectively
c
456 Plant Mol Biol (2012) 79:443–459
123
At the subcellular level, we have established using YFP/
GFP imaging that CrIDI1 exhibits a complex triple sub-
cellular localization based on the formation of transcripts
of various lengths as revealed by 50 RACE analysis
(Fig. 4). This phenomenon, previously described in
A. thaliana (Phillips et al. 2008), leads to the formation of
short and long isoforms of CrIDI1 that differ by the
absence/presence of the plastid (AtIDI1) or mitochondrion
(AtIDI2) TP at their N-terminal end. Thus, we showed that
the CrIDI1 short isoform lacking the N-terminal TP is
targeted to peroxisomes in agreement both with the pres-
ence of a PST1 at the C-terminus of the protein (Fig. 8f–j)
and with the results obtained for AtIDI1 and AtIDI2 (Sapir-
Mir et al. 2008). As mentioned by these authors, we noticed
that the peroxisomal targeting of IDI seems to be mediated
by particular mechanisms since both the N-terminal part
and the C-terminal end of pseudo-mature short protein
have to be accessible for proper peroxisome targeting
(Fig. 8f). The C-terminal end of CrIDI1 and its orthologs
from A. thaliana (AtIDI1 and AtIDI2) display the same
PTS1 (HKL) but differ by the presence of an additional
isoleucine residue located just after the PTS1 in CrIDI1
(Fig. 1). However, we showed that this supplemental resi-
due did not alter the efficiency of the CrIDI1 PTS1 as also
confirmed for the YFP-SKLI fusion protein (Supplemental
Fig. 2). At the physiological level, the peroxisomal locali-
zation of CrIDI1 is in direct correlation with the presence of
other isoprenoid biosynthetic enzymes acting upstream or
downstream of CrIDI1 within this compartment. These
include the 5-phosphomevalonate kinase (PMK) and the
mevalonate 5-diphosphate decarboxylase (MVD) catalyz-
ing the two last steps of the MVA pathway as well as a
farnesyl diphosphate synthase (Simkin et al. 2011; Thabet
et al. 2011; Guirimand et al. 2012). Therefore, the peroxi-
somal localization clearly suggests the involvement of short
CrIDI1 in the biosynthesis of isoprenoids derivated from the
MVA pathway and reinforces the description of peroxi-
somes as major organelles in isoprenoid biosynthesis.
The CrIDI1 long isoform exhibits a N-terminal TP that
targets the pseudo-mature protein to both mitochondria and
plastids including stromules at an apparent similar effi-
ciency (Fig. 5a–m). This constitutes the main difference
with A. thaliana in which the long isoforms are preferen-
tially addressed to either plastid (AtIDI1) or mitochondria
(AtIDI2), respectively (Sapir-Mir et al. 2008). These spe-
cific localizations have been confirmed under our experi-
mental conditions and in our plant system (Supplemental
Fig. 1) confirming that the dual localization of the CrIDI1
long isoform is dependant of the protein, per se and not
to the cell type. Fusion/deletion experiments of CrIDI1
revealed that the first 76 residues are sufficient to target
the protein to both mitochondria and plastids (Fig. 6a–n)
in agreement with bioinformatic predictions (Table 1).
Interestingly, we also noted that the first 18 residues of the
TP, corresponding to a specific part of the CrIDI1 TP as
compared to those of Arabidopsis orthologs (Fig. 1), are
solely responsible of the mitochondrial targeting (Fig. 7a–
e). By contrast, the remaining part of the CrIDI1 (residues
19–76) is unable to drive a fusion protein to plastids
(Fig. 7f–j), suggesting that the whole TP is required to
plastid targeting. Dual targeting to mitochondria and
plastid is a common feature, observed for an increasing
number of proteins (Mitschke et al. 2009). There are two
basic ways in which a single gene can provide a product
targeted to both organelles. It includes the ‘‘twin’’ targeting
sequences represented by a mitochondrial and a plastidial
targeting sequence positioned in tandem at the N-terminus
of the protein, and the ambiguous targeting sequence that is
recognized as an import signal by both organelles (Peeters
and Small 2001; Pujol et al. 2007; Mitschke et al. 2009).
The N-terminal TP of CrIDI1 constitutes an intermediate
situation since the first 18-residues are sufficient to mediate
import in mitochondria while the first 76-residues
(including the first 18-residues) are required to mediate
additional import into plastids. It could therefore allow a
dual targeting albeit a preferential targeting to either
plastids or mitochondria could also be hypothesized
depending on the TP phosphorylation status since it has
been described to increase the efficiency of plastid import
by several fold (Waegemann and Soll 1996; Martin et al.
2006). From a physiological point of view, the presence of
CrIDI1 in plastids could be linked to the synthesis of MEP
derived isoprenoid and its mitochondrial localization to the
production of other specific isoprenoids such as ubiqui-
none (Lutke-Brinkhaus et al. 1984). In addition, we can
hypothesize that the dual targeting of CrIDI1 to plastids
and mitochondria could be required to maintain IDI
activity and the associated isoprenoid biosynthesis in these
two organelles since the sole CrIDI1 gene seems to be
expressed at detectable level within C. roseus organs. Such
interpretation could also be extrapolated to the peroxisomal
localization of CrIDI1. Nevertheless, we cannot rule out
the existence of an organelle specific targeting for the
CrIDI1 long isoform that could depend on the cell type
housing the enzyme. For instance, in IPAP cells where the
MEP pathway is most active, a preferential targeting to
plastids could occur to allow the production of high amount
of the isoprenoid precursor of MIA. Finally, our combined
approaches of BiFC assays and migration of recombinant
protein in native PAGE allowed us to establish that CrIDI1
is capable of self-interaction within the three subcellular
compartment housing this enzyme, including plastids,
mitochondria and peroxisomes (Fig. 9a–q). Our results do
not fit with the hypothesis that IDIs mainly operate as
monomers based upon the elucidation of the crystal
structure of the E. coli type 1 IDIs and from the purification
Plant Mol Biol (2012) 79:443–459 457
123
of IDIs from Cinchona robusta cells (Ramos-Valdivia et al.
1997; Durbecq et al. 2001). However, our results corrob-
orate the analysis of the yeast proteome complexes dem-
onstrating the propensity of type 1 IDIs to self interact
in multi-protein complexes (Gavin et al. 2002). Albeit
apparently not required for the catalytic activity, the
CrIDI1 self-interactions could be required for the control of
the metabolic flux. All together, our results demonstrated
that two CrIDI1 isoforms encoded by a single gene display
a unique triple localization in plastids, mitochondria and
peroxisomes under self-interacting complexes suggesting
that distinct mechanisms of compartmentalization of the
isoprenoid biosynthetic pathways could occur within plants
synthesizing high amount of specialized isoprenoids (e.g.
C. roseus) and plants mainly accumulating’’housekeeping’’
levels of non-specialized isoprenoids and low amount of
specialized isoprenoids (e.g. A. thaliana).
Acknowledgments This work was financially supported by the
‘‘Ministere de l’Enseignement Superieur et de la Recherche’’ (MESR)
and by a grant from the University of Tours. Gregory Guirimand
and Anthony Guihur were financed by MESR fellowships. We thank
Pr. Jorg Kudla (University of Munster, Germany) for providing us the
BiFC plasmids. We also thank M. A. Marquet, M. F. Aury, E. Danos
and E. Marais for help in maintaining cell cultures.
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