FEBS Letters 582 (2008) 3359–3366
Pyruvate uptake is inhibited by valproic acid and metabolites
in mitochondrial membranes
Cátia C.P. Airesa, Graça Soveralb, Paula B.M. Luı́sa, Herman J. ten Brinkc,
Isabel Tavares de Almeidaa, Marinus Durand, Ronald J.A. Wandersd, Margarida F.B. Silvaa,*
a
iMED.UL, Centro de Patogénese Molecular, Faculdade de Farmácia da Universidade de Lisboa, Av. Prof. Gama Pinto, 1649-003 Lisboa, Portugal
b
REQUIMTE, Departamento de Quı́mica, FCT, Universidade Nova de Lisboa, 2829-516 Caparica, Portugal
c
Department of Clinical Chemistry, Free University Medical Center, De Boelelaan 1117, 1081 HV Amsterdam, The Netherlands
d
Laboratory Genetic Metabolic Diseases, Department of Clinical Chemistry and Pediatrics, Academic Medical Centre, University of Amsterdam,
Meibergdreef 9, 1105 AZ Amsterdam, The Netherlands
Received 28 May 2008; revised 6 August 2008; accepted 22 August 2008
Available online 5 September 2008
Edited by Judit Ovádi
Abstract The pyruvate uptake rate in inverted submitochondrial vesicles prepared from rat liver was optimized and further
characterized; the potential inhibitory effects of the anticonvulsive drug valproic acid or 2-n-propyl-pentanoic acid (VPA),
D4-valproic acid or 2-n-propyl-4-pentenoic acid and the respective coenzyme A (CoA) conjugates were studied in the presence
of a proton gradient. All tested VPA metabolites inhibited the
pyruvate uptake, but the CoA esters were stronger inhibitors
(40% and 60% inhibition, respectively, for valproyl-CoA and
D4-valproyl-CoA, at 1 mM). At the same concentration, the specific inhibitor 2-cyano-4-hydroxycinnamate decreased the pyruvate uptake rate by 70%. The reported inhibition of the
mitochondrial pyruvate uptake may explain the significant
impairment of the pyruvate-driven oxidative phosphorylation induced by VPA.
2008 Federation of European Biochemical Societies. Published
by Elsevier B.V. All rights reserved.
Keywords: Valproic acid; D4-Valproic acid; Mitochondrial
pyruvate uptake; Pyruvate transport; Drug metabolism;
Inverted submitochondrial membranes
1. Introduction
The oxidative metabolism of pyruvate in mitochondria is a
highly regulated process which depends on the import and/or
diffusion of this 2-oxoacid from the cytosolic compartment.
Any xenobiotic that may interfere with this transport will compromise mitochondrial functioning and thus energy metabolism. Valproic acid (VPA, 2-n-propyl-pentanoic acid) is a
powerful antiepileptic drug, with specific indications for many
forms of epilepsy and many types of seizures, affecting children
or adults.
*
Corresponding author. Fax: +351 21 794 64 91.
E-mail address: mbsilva@ff.ul.pt (M.F.B. Silva).
Abbreviations: VPA, valproic acid or 2-n-propyl-pentanoic acid; D4VPA, D4-valproic acid or 2-n-propyl-4-pentenoic acid; CoA, coenzyme
A; VP-CoA, valproyl-CoA; D4-VP-CoA, D4-valproyl-CoA; ISMV,
inverted submitochondrial vesicles; IMM, inner mitochondrial membrane; UCP, uncoupling protein; CHC, 2-cyano-4-hydroxycinnamate;
SEM buffer, sucrose/EGTA/MOPS buffer; MES, 2-[N-morpholino]ethanesulfonic acid; HEPES, N-(2-hydroxyethyl)piperazine-N 0 -(2-ethanesulfonic acid); DCIP, 2,6-dichloroindophenol
Previous in vitro studies from our group showed that VPA
and its metabolites induce a striking decrease in the pyruvate-driven mitochondrial oxygen consumption and ATP synthesis [1]. One hypothesis raised by these results was the
putative interference of VPA or its biotransformation products
with the mitochondrial pyruvate uptake. Besides its complete
oxidation, the transport of pyruvate across mitochondrial
membranes is an essential process for many other metabolic
pathways, such as glucose oxidation, lipogenesis, gluconeogenesis and amino acid metabolism [2].
Since the early 1970s, many proteins that transport metabolites, nucleotides and co-factors across the inner mitochondrial
membrane (IMM) have been identified [3]. The mitochondrial
ADP/ATP carrier, the uncoupling proteins (UCPs), the phosphate, oxoglutarate/malate, citrate and carnitine/acylcarnitine
carriers among many others, have been identified, purified
and characterized [3,4].
The transport of pyruvate was first described by Papa et al.
in 1971, in rat liver mitochondria, and it was shown that this
process is coupled to proton symport [5]. Later, in 1974, Halestrap and Denton identified a potent and specific inhibitor of
pyruvate transport, i.e. 2-cyano-4-hydroxycinnamate (CHC)
suggesting the existence of a specific carrier involved in the
pyruvate transport across the IMM [6–10].
The transport of pyruvate in bovine heart mitochondria was
also characterized [11] and the transport assays were performed using a reconstituted system of solubilized submitochondrial particles incorporated into liposomes [11,12].
Using this system, the CHC-sensitive pyruvate-exchange reaction had substrate and inhibitor characteristics similar to
those observed in mitochondria. A 34 kDa protein was described as being responsible for the pyruvate uptake both in
bovine heart [11] and rat liver mitochondria [13]. In yeast,
the pyruvate carrier was identified in a fraction containing
two polypeptides of apparent molecular mass of 26 and
50 kDa [14].
In 2003, Hildyard et al. identified the mitochondrial pyruvate carrier in Saccharomyces cerevisiae, by measuring the
inhibitor-sensitive pyruvate uptake in isolated mitochondria
from mutant yeast strains in which the genes coding for each
of the members of the mitochondrial carrier family, were disrupted one-by-one [2,15]. Mitochondria isolated from the yeast
mutant YIL006w exhibited a specific loss of pyruvate uptake.
However, the gene product of YIL006w, named Ndt1p, was
0014-5793/$34.00 2008 Federation of European Biochemical Societies. Published by Elsevier B.V. All rights reserved.
doi:10.1016/j.febslet.2008.08.028
3360
later shown to transport NAD+ instead of pyruvate [16] which
casts doubt about the function of this protein as a mitochondrial pyruvate carrier in yeast.
In plants, several biochemical and molecular studies have
suggested the presence of a specific carrier in the IMM which
mediates the electroneutral uptake of pyruvate, driven by a
pH gradient. This protein was found to be inhibited by CHC
and other molecules, giving support to the fact that (1) plant
pyruvate transport has biochemical features similar to mammalian pyruvate transport and that (2) it involves a carrier
rather than pyruvate entering by means of diffusion [17].
The UCPs are also specialized transporters located in the
IMM. They allow passive proton transport through the
IMM, reducing the proton electrochemical gradient built up
by the respiratory chain [18,19]. Different isoforms of these
proteins have been identified in mammals (UCP1 present in
brown adipocytes, UCP2 in several tissues, UCP3 in brown
adipose tissue and muscle, UCP4 and UCP5 in brain) [19].
Moreover, it has been reported that UCP1 exhibits the widest
substrate specificity among the other homologous anion transporters, being also able to transport pyruvate [20]. The liver is
the organ in which expression of UCPs is the lowest, at least
under basal conditions [21]. Only a low level of expression of
UCP2 was detected in the adult rat liver [21], as other UCP
genes are silent in this tissue.
The hypothesis that the mitochondrial pyruvate uptake
could be affected by VPA, has been proposed in one single
study, using brain mitochondria [22] where a competitive inhibition mechanism was reported. Nevertheless, under in vivo
conditions VPA will probably undergo rapid activation to its
coenzyme A (CoA)-ester and will also be metabolized. This
prompted the study described in this paper, in which we studied the effect of VPA and the respective CoA-ester [23,24], as
well as D4-valproic acid or 2-n-propyl-4-pentenoic acid (D4VPA), its main microsomal product [25], and D4-valproylCoA (D4-VP-CoA) [26]. The results presented herein provide
evidence that VPA, and in particular some specific metabolites
that are most probably more abundant in cytosol and/or mitochondria than the parent molecule [24], inhibit the uptake of
pyruvate in inverted submitochondrial vesicles (ISMV),
accounting for the mitochondrial dysfunction that has been
associated with valproate.
2. Materials and methods
2.1. Materials
Sucrose, BSA, CHC, valinomycin, L-lactate, VPA and other chemicals were obtained from SIGMA Aldrich. The sodium salt of [1-14C]pyruvic acid (250 lCi, specific activity 27 mCi/mmol, 243 lCi/mg,
M = 111 g/mol) was obtained from Amersham Biosciences. UltimaGold liquid scintillation solution was purchased from Packard.
2.2. Synthesis of valproyl-CoA (VP-CoA), D4-VPA and D4-VP-CoA
VP-CoA and D4-VP-CoA were synthesized according to published
procedures [24] from VPA and D4-VPA, respectively. D4-VPA was obtained by chemical synthesis following a reported procedure [27]. VPCoA and D4-VP-CoA were purified by solid phase extraction, and its
purity checked using HPLC with diode array detection (>95%).
2.3. Isolation of rat liver mitochondria
The study was conducted according to the National Guidelines for
the care and use of laboratory animals (Faculty of Pharmacy animalsÕ
laboratory).
C.C.P. Aires et al. / FEBS Letters 582 (2008) 3359–3366
Adult male Wistar rats (200–300 g) were starved for 18–20 h. After
cervical displacement, the livers were immediately removed and rinsed
into ice-cold homogenization medium containing 250 mM sucrose,
0.5 mM ethylene glycol-bis(b-aminoethyl ether)-N,N,N 0 ,N 0 -tetraacetic
acid, 5 mM 3-[N-morpholino]propanesulfonic acid, pH 7.4 (sucrose/
EGTA/MOPS buffer, SEM buffer). Rat liver mitochondria were prepared according to a published procedure [24]. Briefly, after mincing
and 2–3 washings with SEM buffer (at 4 C), the chopped liver was
homogenized in a precooled Teflon pestle glass homogenizer. From
here onwards the whole process was conducted at 4 C. The homogenate was centrifuged at 600 · g (10 min) and the obtained post-nuclear
supernatant was further centrifuged at 3600 · g (10 min). The obtained
pellet was suspended in SEM buffer and after one last round of centrifugation at 2700 · g (10 min), the mitochondria were finally resuspended in the homogenization medium (25–50 mg/ml).
2.4. Preparation of ISMV
ISMV were obtained from the above prepared rat liver mitochondria according to a published procedure [28] with minor modifications.
Mitochondria were resuspended in 0.25 M sucrose and 1 g/l BSA keeping the temperature at 4 C. The suspension was gently homogenized
with a dounce tissue grinder (6–7 strokes) and centrifuged at
27 000 · g (15 min). The obtained pellet was resuspended in 5 ml of
sonication medium (225 mM sucrose, 10 mM NaH2PO4, 1 g/l BSA,
pH 7.4) and sonicated 3 · 30 s. The obtained vesicle suspension was diluted in 25 ml of sonication medium and centrifuged at 23 500 · g
(10 min). The supernatant was further centrifuged at 44 000 · g
(60 min). The ISMV were obtained after resuspending the final pellet
in 2 ml of a medium containing 225 mM sucrose, 10 mM Tris–HCl,
1 mM EDTA and 1 g/l BSA (pH 7.4) and passing it through a 21 g needle. Protein was measured using the Bradford method [29], with BSA
as a reference substance. This sonication technique provides an homogeneously oriented vesicle preparation with a percentage of inversion
ranging from 90% to 96% [28,30].
2.5. Characterization of ISMV preparations
2.5.1. Succinate dehydrogenase activity. The purity of the membrane vesicle preparation was assessed by the measurement of succinate dehydrogenase activity as described elsewhere [31]. The reaction
mixture contained 50 mM KPi, 0.015% 2,6-dichloroindophenol
(DCIP), 2 mM KCN and 15 mM sodium succinate. Reactions were
started by adding 50 ll of sample (approx. 40 lg of protein) and the
decrease in absorbance was measured at 600 nm (total volume 1 ml).
The enzyme activity was calculated using eDCIP 600 nm = 21 mM 1 cm 1.
2.5.2. Vesicle size determination. Vesicle size of all prepared batches
was determined by quasi-elastic light scatter (QELS) using a particle
sizer (BI-90 Brookhaven Instruments). An application of this technique in the determination of vesicular sizes has been published [32].
2.5.3. Osmotic response by stopped-flow light-scatter. In order to assure the sealing and leakiness of the membrane vesicles, the osmotic response of ISMV (swelling and shrinking) was assessed by stopped-flow
light scattering in which aliquots of ISMV were subjected to hypo- and
hyperosmotic shocks. Experiments were performed on a HI-TECH
Scientific PQ/SF-53 stopped-flow apparatus, which has a 2 ms dead
time, interfaced with an IBM PC/AT compatible 80386 microcomputer, at a controlled temperature. ISMV in the isotonic resuspension
buffer (0.1 ml, 0.4 mg/ml protein) were mixed with an equal amount of
hypo-, iso- or hyper-osmotic mannitol solutions at 23 C to reach different inwardly or outwardly directed gradients of solute (swelling and
shrinking; osmotic gradients 62.5, 0, 125 and 375 mosM). The timecourse of 90 scattered light intensity at 400 nm was followed until a
stable light-scattered signal was obtained. The change in light scatter
intensity (I) of the ISMV preparation after an osmotic shock
(DI = I0 I1) is related to their vesicular volume change [33] and thus,
it can be used as a tool to assure vesicle integrity. The osmolarities of
all solutions were measured using a cryometric automatic semi-micro
osmometer (Knauer, Germany).
2.6. Pyruvate uptake measurements
The rate of the radiolabeled substrate [1-14C]-pyruvate uptake by
ISMV was measured in the presence or absence of an inwardly directed
proton gradient. Prior to the uptake, the ISMV were equilibrated in
100 mM KCl, 20 mM N-(2-hydroxyethyl)piperazine-N 0 -(2-ethanesulfonic acid) (HEPES), pH 7.4, by passing the vesicle preparation
3361
C.C.P. Aires et al. / FEBS Letters 582 (2008) 3359–3366
through a 21 g needle. The mitochondrial proton driven pyruvate uptake was measured at 4 C after incubation of the ISMV suspension
(final concentration range: 0.1–5.7 mg/ml, pH 7.4) with 5 ll of
240 mM 2-[N-morpholino]ethanesulfonic acid (MES) containing
0.066 lCi of [1-14C]-pyruvate and 10 lM valinomycin, resulting in an
extravesicular pH of 5.5 and a final concentration of 0.02–0.67 mM
pyruvate (final volume: 30 ll). The reaction was stopped by diluting
the sample with ice-cold stop solution (84 mM KCl, 17 mM HEPES,
40 mM MES, 1 mM CHC, pH 5.5) at appropriate times (0–60 s), followed by rapid filtration in a vacuum assembly through Osmonics filters (0.45 lm pore size), and 2–3 washing steps with the same cold stop
solution [34]. The filters were dried at room temperature, and the vesicle-associated radioactivity in the filters was determined by liquid scintillation counting in a Packard Tri-Carb 2100 TR Liquid Scintillation
Analyzer. The non-specific binding of the isotope to the surface of the
vesicles as well as to the filters was determined by a similar pyruvate
uptake experiment but without incubation. An average value was obtained from triplicate measurements (blanks), which was subtracted in
further corresponding experiments.
Pyruvate exchange in the absence of a proton gradient was assayed
under similar experimental conditions, replacing the incubation medium by 100 mM KCl, 20 mM HEPES containing [1-14C]pyruvate
and 10 lM valinomycin, resulting in an extravesicular pH of 7.4.
The stop solution consisted of 100 mM KCl, 20 mM HEPES and
1 mM CHC, final pH 7.4, and the subsequent steps were performed
accordingly.
a powerful and specific inhibitor of the mitochondrial pyruvate carrier
[8], was used as a positive control. The effect of lactate was also studied
using a similar concentration range. The subsequent pyruvate uptake
measurement driven by an inwardly directed proton gradient was assayed as described above, incubating the vesicles for 5 s with [1-14C]pyruvate at various concentrations (0.07, 0.17 and 0.67 mM final concentrations).
2.8. Data analysis
The kinetic parameters of the mitochondrial pyruvate transport
activity were determined by non-linear regression analysis using the
SigmaPlot 9.0 Technical Graphing Software.
3. Results
3.1. Characterization of the inner ISMV
Purified ISMV were prepared from mitochondria isolated
from rat liver homogenates by differential centrifugation.
The activity of the marker enzyme succinate dehydrogenase,
an enzymatic complex bound to the IMM that participates
in both the citric acid and the mitochondrial electron transport
chain (complex II), was measured. The obtained values were
0.013 ± 0.002 U/mg protein and 0.023 ± 0.01 U/mg protein,
respectively, determined in the initial mitochondrial homogenates and in the ISMV suspension, indicating a two-fold vesicle enrichment after purification.
The size distribution of ISMV preparations determined by
quasi-elastic light scattering is shown in Fig. 1A. A mean diameter
2.7. Pyruvate uptake measurements in the presence of inhibitors
The effect of VPA, VP-CoA, D4-VPA and D4-VP-CoA on the mitochondrial pyruvate uptake was assessed by pre-incubating the ISMV
(2 mg/ml) with purified solutions of these compounds at various concentrations (0.5–2 mM), for 3 min, prior to the uptake assay. CHC,
A
B
100
Mean Diameter: 293 nm
Osmotic Gradient
(mosM)
Scattered light intensity
(arbitrary units)
% ISMV’s
80
60
40
20
-62.5
0
125
375
0
10
100
1000
0
0.1
0.2
Diameter (nm)
0.3
0.4
0.5
Time (sec)
∆I
C 0.8
0.7
0.6
0.5
0.4
0.3
0.2
0.1
0
-0.1
-0.2
-100
0
100
200
300
400
Osmotic Gradient (mosM)
Fig. 1. (A) ISMV size determination by quasi-elastic light scattering (QELS). Vesicles in the resuspension buffer were homogeneous in size with a
mean diameter of 293 ± 12 nm (n = 10). (B) Record of a typical stopped-flow experiment where the light scatter intensity from an ISMV suspension
was suddenly exposed to different osmotic shocks ( 62.5, 0, 125 and 375 mosM). The time course of volume change was followed for 0.5 s. (C)
Dependence of the total change in light scatter (DI = I0 I1), related to the total volume change of the ISMV vesicles, for a specific applied osmotic
gradient (mosM).
3362
value of 293 ± 12 nm was obtained in the prepared batches
(n = 10) and as depicted, a unimodal distribution was achieved,
demonstrating that the vesicles were homogeneous in size.
Fig. 1B shows the recordings of a typical stopped-flow
experiment where the light scatter intensity from an ISMV suspension suddenly exposed to different solutions (iso-, hyperand hypo-osmotic) was monitored for 0.5 s. A remarkable
increase in scattered light was observed when vesicles were subjected to hyper-osmotic gradients of 125 and 375 mosM, in
contrast to the light scatter decrease for the hypo-osmotic gradient 62.5 mosM, in agreement with vesicle shrinking and
swelling. No change in scattered light was observed when vesicles were mixed with iso-osmotic buffer (absence of osmotic
gradient). The dependence of the total change in light scatter
(DI) for a given osmotic gradient applied (mosM) is shown
in Fig. 1C and demonstrates that the vesicles behaved like
osmometers for the chosen osmolarity range, therefore assuring vesicle integrity.
3.2. Pyruvate uptake measurements in ISMV
3.2.1. Time course and substrate dependence. Pyruvate uptake was assayed in vitro using purified ISMV by measuring
the uptake of [1-14C]-pyruvate by these vesicles. The rate of labelled substrate accumulation inside the vesicles was measured
through a rapid filtration technique and isotope scintillation
counting.
As shown in Fig. 2, a time-dependent uptake of radiolabeled
pyruvate was observed in ISMV, in the presence of an inwardly directed proton gradient (pHout 5.5 < pHin 7.4) suggesting apparent first order kinetics. Moreover, virtually no
pyruvate uptake was observed in the absence of a proton gradient (pHout = pHin 7.4). The rate of pyruvate uptake in the
prepared vesicles was linearly dependent on the protein content (0–6 mg/ml, data not shown). Considering the above results, a reaction time of 5 s and a protein content of 2 mg/ml
were selected for all subsequent studies.
The concentration dependence of pyruvate uptake was also
studied in ISMV, in the presence and absence of a driving proton gradient. Fig. 3 shows the uptake rate as function of the
pyruvate concentration. From a double reciprocal plot and
[14C]-pyruvate uptake (nmol/mg)
1.4
pHout < pHin
1.2
pHout = pHin
1.0
0.8
0.6
0.4
0.2
0.0
0
5
10 15 20 25 30 35 40 45 50 55 60 65
[14C]-pyruvate uptake (nmol/mg.s)
C.C.P. Aires et al. / FEBS Letters 582 (2008) 3359–3366
0.014
pHout < pHin
0.012
pHout = pHin
0.010
0.008
0.006
0.004
0.002
0.000
0.0
0.1
0.2
0.3
0.4
0.5
0.6
0.7
0.8
[14C]-pyruvate (mM)
Fig. 3. Effect of the proton gradient in the pyruvate uptake in ISMV as
function of increasing substrate concentration. The uptake was driven
by an inwardly directed proton gradient (pHout < pHin) (closed circles
d), and without proton gradient (pHout = pHin) (opened circles s).
The data shown are mean ± S.D. of triplicates of two independent
experiments.
from a non-linear regression analysis using the SigmaPlot
9.0 Technical Graphing Software, values of Km and Vmax were
obtained and are presented in Table 1. In the presence of a proton gradient, an approximate Km of 0.48 mM was calculated, a
value much lower than the value of 1.40 mM obtained in the
absence of a proton gradient. These values suggest an increase
in substrate affinity of the mediated pyruvate transport when a
proton force is driving the uptake. The Vmax was 5.5% higher
in the presence of a proton gradient.
3.2.2. Inhibitory effect of different VPA metabolites on the
uptake of [14C]-pyruvate. Fig. 4 shows the [14C]-pyruvate uptake in ISMV in the presence of CHC, VPA, D4-VPA and the
respective CoA esters (VP-CoA and D4-VP-CoA).
The parent drug, VPA, and its unsaturated metabolite, D4VPA (both at 1 mM), had only a mild to insignificant effect
on the mitochondrial uptake of pyruvate (22.0% and 15.7%
inhibition, respectively). However, at a higher concentration
(2 mM) only D4-VPA induced a significant inhibition of the
pyruvate uptake rate (76.2% inhibition), as shown in Fig. 4A.
Furthermore, the uptake of pyruvate was also found to be
inhibited by both D4-VP-CoA (73.1% inhibition) and VPCoA (50.1% inhibition), in parallel with an increase of Km values for the pyruvate transport (Fig. 4B and Table 1).
Our results confirm, by comparing all the tested compounds
at 1 mM, that CHC was in fact an effective inhibitor of the
pyruvate uptake in ISMV (71.6% inhibition), as shown in
Fig. 4B and C.
Lactate, a substrate that potentially competes with pyruvate,
also inhibited this ketoacid uptake in ISMV (42.1% inhibition)
as depicted in Fig. 4A and C.
Table 1 summarises the kinetic parameters values of the
pyruvate uptake, calculated in the presence of the tested
VPA metabolites, CHC and lactate, as well as the obtained
inhibition (%) of control uptake values.
Time (s)
Fig. 2. Uptake of [14C]-pyruvate by ISMV driven by an inwardly
directed proton gradient (pHout < pHin) (closed circles d), and without
proton gradient (pHout = pHin) (opened circles s). The data shown
correspond to mean of triplicates (S.D. < 0.03) obtained in two
independent experiments.
4. Discussion
The transport of pyruvate across membranes plays a central
role in cellular metabolism and metabolic communication be-
3363
C.C.P. Aires et al. / FEBS Letters 582 (2008) 3359–3366
Table 1
Effect of different inhibitors on the mitochondrial pyruvate uptake in ISMV
Kinetic parametersa
pHout = pHin
pHout < pHin
Control
Control
VPAb
VP-CoAc
D4-VPAc
D 4-VP-CoAc
CHCb
Lactateb
Km
K app
m
Vmax
app
V max
1.40
–
17.90
–
0.48
–
18.88
–
–
0.47
–
17.89
–
0.64
–
22.29
–
0.95
–
16.29
–
1.02
–
22.82
–
–
–
–
–
–
–
–
Inhibition (%)
–
–
22.0
50.1
76.2
73.1
71.6
42.1
(K app
m
app
max )
and V
and the average value of maximum inhibition (%) of the pyruvate uptake (100
The values represent the apparent kinetic parameters
minus % of control) in the presence of the respective inhibitors. Data shown are mean ± S.D. of triplicates of at least two independent experiments.
a
Values of Km and Vmax are, respectively, expressed in mM and pmol/mg s.
b
[Inhibitor] = 1 mM.
c
[Inhibitor] = 2 mM.
B
120
VPA
4
∆ -VPA
Lactate
100
80
60
40
20
0
0.0
0.5
1.0
1.5
2.0
2.5
[14C]-pyruvate uptake (% of control)
[14C]-pyruvate uptake (% of control)
A
120
Valproyl-CoA
∆4-valproyl-CoA
CHC
100
80
60
40
20
0
0.0
0.5
Concentration (mM)
[14C]-pyruvate uptake (% of control)
C
1.0
1.5
2.0
2.5
Concentration (mM)
120
100
80
60
40
20
0
M
trol
mM
mM
mM
mM e 1mM
1m
A2
A2
A2
C1
tat
CH
VPA yl-Co ∆4 -VP
l-Co
y
Lac
o
o
pr
pr
4 -val
Val
∆
Con
Fig. 4. [14C]-pyruvate uptake in ISMV using a proton gradient, in the presence of (A) valproic acid (VPA), D4-VPA and lactate and (B) valproylCoA, D4-valproyl-CoA and 2-ciano-4-hydroxycinnamate (CHC). (C) Maximum inhibition of the pyruvate uptake obtained with the different VPA
metabolites, compared with the control (100% of pyruvate uptake obtained in the absence of inhibitors) and the specific pyruvate carrier inhibitor
CHC (28% of pyruvate uptake). Data shown are mean ± S.D. of triplicates of at least two independent experiments.
tween subcellular compartments and tissues [15,35,36]. Many
cells rely on the end product of glycolysis, i.e. pyruvate, to produce most of their ATP. This pathway occurs in the cell cytosol, and thus the transport of pyruvate into the mitochondria
for further oxidation, is essential to fuel the citric acid cycle
after being converted into acetyl-CoA by pyruvate dehydrogenase [35,36]. For this purpose, the mitochondrial pyruvate carrier activity is critical for energy homeostasis.
3364
The transport of monocarboxylates, such as pyruvate and
lactate across the plasma membrane is well-characterized and
catalysed by a recently identified family of proton-linked
monocarboxylate transporters [36]. In mitochondria, the mammalian pyruvate carrier has not yet been cloned, sequenced
and fully characterized, however, it has been considered as a
member of the six-transmembrane-helix mitochondrial carrier
family [15].
After the identification of CHC as a specific and potent
inhibitor of the putative mitochondrial pyruvate carrier [6,9],
the existence of such protein has gained support by many studies and recently new highly potent inhibitors have been identified [15,35,36].
The scope of this paper is primarily focused on functional
studies using a simple experimental model to test the direct effect of a specific drug and/or its metabolites on the mitochondrial uptake of pyruvate. This study was performed using
ISMV, which allowed a strict control of the driving force of
pyruvate uptake, by regulating both internal and external
pH. Furthermore, the approach was strictly focused on the
proton-dependent transport of pyruvate and no other internal
substrates were added, excluding other putative pyruvate
translocators. The former uptake experiments using intact
mitochondria and labelled pyruvate could not avoid the subsequent metabolism of the substrate inside the organelle, a fact
that would certainly affect the pH and the osmolarity in the
matrix. The obtained homogeneity of the prepared ISMV
either in size or orientation, accounts for reproducible kinetic
measurements, at controlled conditions of pH.
Using this model, the results presented in this paper show
that pyruvate uptake decreases in ISMV in the absence of a
driving proton gradient, suggesting that the mitochondrial
transport of pyruvate is protein-mediated and coupled with a
proton-symport, as already proposed [2,36]. In addition,
CHC significantly inhibited the uptake of this monocarboxylate in the prepared vesicles, supporting the previous hypothesis. Furthermore, the uptake of pyruvate was inhibited in the
presence of lactate, suggesting that this compound may compete with pyruvate into these vesicles.
In the present study, VPA and D4-VPA were found to clearly
inhibit the uptake of pyruvate in ISMV (as indicated by the
observed increase on the Km for pyruvate uptake). In addition,
our results suggest that the respective CoA esters of VPA and
D4-VPA are stronger inhibitors of the mitochondrial pyruvate
uptake than the parent drug (VPA). Both free acids were recently found to be activated to the respective CoA esters not
only at the mitochondrial matrix, where the free acids are
prone to be metabolized by b-oxidation in the form of CoA esters, but also in the extra-mitochondrial compartment [26].
The extra-mitochondrial formation of VP-CoA and D4-VPCoA may affect numerous cellular functions, such as fatty-acid
elongation, peroxisomal metabolism, gluconeogenesis, ureagenesis and many other pathways involving cytosolic reactions. A targeted effect of these CoA conjugates on the
mitochondrial pyruvate uptake is the hypothesis clearly supported by the present results.
Previous studies of our group have shown that oxygen consumption and ATP synthesis driven by pyruvate was severely
decreased by VPA [1]. In addition, we recently reported that
VPA and D4-VPA also inhibit both 2-oxoglutarate and glutamate-driven oxidation and ATP synthesis [37] although not so
strikingly as with pyruvate. The reported data suggest that the
C.C.P. Aires et al. / FEBS Letters 582 (2008) 3359–3366
observed inhibitory effects of VPA and metabolites on mitochondrial ATP synthesis and oxidation of pyruvate, 2-oxoglutarate and glutamate are likely due to an inhibitory effect on
dihydrolipoamide dehydrogenase (DLDH, E3 subunit), the
common component of the multi-enzyme complexes 2-oxoglutarate dehydrogenase, pyruvate dehydrogenase and branchedchain 2-oxoacid dehydrogenase [37]. However, a specific effect
on the transport systems in the mitochondrial inner membrane
could not be excluded. Thus, the defective import of pyruvate
into this organelle suggested by the present results mainly induced by the respective CoA-esters (VP-CoA and D4-VPCoA), would be additive to the reported DLDH inhibition.
Being structurally related, those CoA esters do not diffuse in
membranes, due to their larger size and presence of double
bounds, and thereby they can potentially affect pyruvate uptake by interfering with the substrate binding-site or by modifying the protein transporter properties. Considering the free
acids, the data presented in this work suggest that the monocarboxylate anions, valproate and D4-valproate might enter
into the mitochondrial matrix by a symport process with H+,
competing with pyruvate for the same proton-linked transporter. However, further studies are required in order to elucidate the mechanisms of the reported inhibition on the
mitochondrial uptake of pyruvate.
The present data do clearly support an inhibition of the
mitochondrial CHC-sensitive pyruvate/H+ symporter by
VPA and its derivatives. However, the efficacy of other potential pyruvate uptake mechanisms, such as UCP1 and/or other
CHC-insensitive antiporter mechanisms [38–40] which may (or
may not) be inhibited by this drug, can possibly obviate a net
reduction in pyruvate transport in vivo.
The conversion of pyruvate to glucose, involving firstly its
uptake into mitochondria, is a crucial pathway in liver metabolism and a clear inhibition of gluconeogenesis from both lactate and pyruvate by VPA and D4-VPA has long been
recognized [41,42]. The influence of VPA on carbohydrate
metabolism is undisputed, since a significant weight-gain is
the most frequently reported adverse effect of a long-term
VPA treatment [43,44], potentially associated with hyperinsulinemia and steatosis. In addition, the effects of the drug on
fatty acid oxidation are well-documented [45] but their consequences to the imbalance of glucose homeostasis are far from
being elucidated, considering the reciprocally linked mechanisms of lipid and carbohydrate regulation in vivo.
Taken together, the present results may account for the limited oxidation of pyruvate previously observed, and thus to the
compromised energy production driven by this substrate induced by VPA and/or metabolites.
Acknowledgments: This work was financially supported by Fundação
para a Ciência e a Tecnologia (FCT), Lisboa, Portugal (POCTI/
FCB/48800/2002 with partial funding of FEDER and SFRH/BD/
22420/2005).
References
[1] Silva, M.F.B., Ruiter, J.P.N., IJlst, L., Jakobs, C., Duran, M., de
Almeida, I. Tavares and Wanders, R.J.A. (1997) Valproate
inhibits the mitochondrial pyruvate-driven oxidative phosphorylation in vitro. J. Inherit. Metab. Dis. 20, 397–400.
[2] Hildyard, J.C.W. and Halestrap, A.P. (2003) Identification of the
mitochondrial pyruvate carrier in Saccharomyces cerevisiae.
Biochem. J. 374, 607–611.
3365
C.C.P. Aires et al. / FEBS Letters 582 (2008) 3359–3366
[3] Palmieri, F., Agrimi, G., Blanco, E., Castegna, A., Di Noia,
M.A., Iacobazzi, V., Lasorsa, F.M., Morobbio, C.M.T., Palmieri,
L., Scarcia, P., Todisco, S., Vozza, A. and Walker, J. (2006)
Identification of mitochondrial carriers in Saccharomyces cerevisiae by transport assay of reconstituted recombinant proteins.
Biochim. Biophys. Acta 1757, 1249–1262.
[4] Palmieri, F., Bisaccia, F., Capobianco, L., Dolce, V., Fiermonte,
G., Iacobazzi, V., Indiveri, C. and Palmieri, L. (1996) Mitochondrial metabolite transporters. Biochim. Biophys. Acta 1275, 127–
132.
[5] Papa, S., Francavilla, A., Paradies, G. and Meduri, B. (1971) The
transport of pyruvate in rat liver mitochondria. FEBS Lett. 12 (5),
285–288.
[6] Halestrap, A.P. and Denton, R.M. (1974) Specific inhibition of
pyruvate transport in rat liver mitochondria and human erythrocytes by a-cyano-4-hydroxycinnamate. Biochem. J. 138, 313–316.
[7] Halestrap, A.P. (1975) The mitochondrial pyruvate carrier:
kinetics and specificity for substrates and inhibitors. Biochem. J.
148, 85–96.
[8] Halestrap, A.P. and Denton, R.M. (1975) The specificity and
metabolic implications of the inhibition of pyruvate transport in
isolated mitochondria and intact tissue preparations by a-cyano4-hydroxycinnamate and related compounds. Biochem. J. 148,
97–106.
[9] Halestrap, A.P. (1976) The mechanism of the inhibition of the
mitochondrial pyruvate transporter by a-cyanocinnamate derivates. Biochem. J. 156, 181–183.
[10] Halestrap, A.P. (1978) Pyruvate and ketone-body transport
across the mitochondrial membrane: exchange properties, pH
dependence and mechanism of the carrier. Biochem. J. 172, 377–
387.
[11] Nalecz, K.A., Bolli, R., Wojtczak, L. and Azzi, A. (1986) The
monocarboxylate carrier from bovine heart mitochondria: partial
purification and its substrate-transporting properties in a reconstituted system. Biochim. Biophys. Acta 851, 29–37.
[12] Bolli, R., Nalecz, K.A. and Azzi, A. (1989) Monocarboxylate and
a-ketoglutarate carriers from bovine heart mitochondria. J. Biol.
Chem. 264 (30), 18024–18030.
[13] Capuano, F., Paola, M.D., Azzi, A. and Papa, S. (1990) The
monocarboxylate carrier from rat liver mitochondria: purification
and kinetic characterization in a reconstituted system. FEBS Lett.
261 (1), 39–42.
[14] Nalecz, M.J., Nalecz, K.A. and Azzi, A. (1991) Purification and
functional characterisation of the pyruvate (monocarboxylate)
carrier from bakerÕs yeast mitochondria (Saccharomyces cerevisiae). Biochim. Biophys. Acta 1079, 87–95.
[15] Sugden, M.C. and Holness, M.J. (2003) Trials, tribulations and
finally, a transporter: the identification of the mitochondrial
pyruvate transporter. Biochem. J., 374, 10.1042/BJ20031105.
[16] Todisco, S., Agrimi, G., Castegna, A. and Palmieri, F. (2006)
Identification of the mitochondrial NAD+ transporter in Saccharomyces cerevisiae. J. Biol. Chem. 281 (3), 1524–1531.
[17] Laloi, M. (1999) Plant mitochondrial carriers: an overview. Cell.
Mol. Life Sci. 56, 918–944.
[18] Criscuolo, F., Mozo, J., Hurtaud, C., Nubel, T. and Bouillaud, F.
(2006) UCP2, UCP3, avUCP, what do they do when proton
transport is not stimulated? Possible relevance to pyruvate and
glutamine metabolism. Biochim. Biophys. Acta 1757, 1284–1291.
[19] Sluse, F.E., Jarmuszkiewicz, W., Navet, R., Douette, P., Mathy,
G. and Sluse-Goffart, C.M. (2006) Mitochondrial UCPs: new
insights into regulation and impact. Biochim. Biophys. Acta 1757,
480–485.
[20] Jezek, P. and Borecky, J. (1998) Mitochondrial uncoupling
protein may participate in futile cycling of pyruvate and other
monocarboxylates. Am. J. Physiol. Cell Physiol. 275, 496–504.
[21] Villarroya, F., Iglesias, R. and Giralt, M. (2007) PPARs in the
control of uncoupling proteins gene expression. PPAR Res. 2007,
74364.
[22] Benavides, J., Martin, A., Ugarte, M. and Valdivieso, F. (1982)
Inhibition by valproic acid of pyruvate uptake by brain mitochondria. Biochem. Pharmacol. 31 (8), 1633–1636.
[23] Silva, M.F.B., Ruiter, J.P.N., Overmars, H., Bootsma, A.H., van
Gennip, A.H., Jakobs, C., Duran, M., de Almeida, I. Tavares and
Wanders, R.J.A. (2002) Complete b-oxidation of valproate:
[24]
[25]
[26]
[27]
[28]
[29]
[30]
[31]
[32]
[33]
[34]
[35]
[36]
[37]
[38]
[39]
[40]
[41]
cleavage of 3-oxovalproyl-CoA by a mitochondrial 3-oxoacylCoA thiolase. Biochem. J. 362, 755–760.
Silva, M.F.B., Ruiter, J.P.N., IJlst, L., Allers, P., ten Brink, H.J.,
Jakobs, C., Duran, M., de Almeida, I. Tavares and Wanders,
R.J.A. (2001) Synthesis and intramitochondrial levels of valproylCoenzyme A metabolites. Anal. Biochem. 290, 60–67.
Abbott, F.S. and Anari, M.R. (1999) Chemistry and biotransformation in: Milestones in Drug Therapy-Valproate (Löscher, W.,
Ed.), pp. 47–75, Birkhäuser Verlag, Basel.
Aires, C.C.P., Ruiter, J.P.N., Luı́s, P.B.M., ten Brink, H.J., IJlst,
L., de Almeida, I. Tavares, Duran, M., Wanders, R.J.A. and
Silva, M.F.B. (2007) Studies on the extra-mitochondrial CoAester formation of valproic and 4-valproic acids. Biochim.
Biophys. Acta 1771, 533–543.
Rettenmeyer, A.W., Prickett, K.S., Gordon, W.P., Bjorge, S.M.,
Chang, S.-L., Levy, R.H. and Baillie, T.A. (1985) Studies on the
biotransformation in the perfused rat liver of 2-n-propyl-4pentenoic acid, a metabolite of the antiepileptic drug valproic
acid. Evidence for the formation of chemically reactive intermediates. Drug Metab. Dispos. 13, 81–96.
Hautecler, J.J., Sluse-Goffart, C.M., Evens, A., Duyckaerts, C.
and Sluse, F.E. (1994) Effect of aspartate and glutamate on the
oxoglutarate carrier investigated in rat heart mitochondria and
inverted submitochondrial vesicles. Biochim. Biophys. Acta 1185,
153–159.
Bradford, M.M. (1976) A rapid and sensitive method for
the quantification of microgram quantities of protein utilizing
the principle of protein-dye binding. Anal. Biochem. 72, 248–
254.
Harmon, H.J. (1982) Isolation of totally inverted submitochondrial particles by sonication of beef heart mitochondria. J.
Bioenerg. Biomembr. 14, 377–386.
King, T.E. (1967) Preparation of succinate dehydrogenase and
reconstitution of succinate oxidase. Method Enzymol. 10, 322–
331.
Perevucnik, G., Schurtenberger, P., Lasic, D.D. and Hauser, H.
(1985) Size analysis of biological membrane vesicles by gel
filtration, dynamic light scattering and electron microscopy.
Biochim. Biophys. Acta 821 (1), 169–173.
Soveral, G., Macey, R.I. and Moura, T.F. (1997) Water permeability of brush border membrane vesicles from kidney proximal
tubule. J. Membr. Biol. 158 (3), 219–228.
Havelaar, A.C., Mancini, G.M.S., Beerens, C.E.M.T., Souren,
R.M.A. and Verheijen, F.W. (1998) Purification of the lysosomal
sialic acid transporter. J. Biol. Chem. 273 (51), 34568–34574.
Hildyard, J.C.W., Ammala, C., Dukes, I.D., Thomson, S.A. and
Halestrap, A.P. (2005) Identification and characterization of a
new class of highly specific and potent inhibitors of the
mitochondrial pyruvate carrier. Biochim. Biophys. Acta 1707,
221–230.
Halestrap, A.P. and Price, N.T. (1999) The proton-linked
monocarboxylate transporter (MCT) family: structure, function
and regulation. Biochem. J. 343, 281–299.
Luı́s, P.B.M., Ruiter, J.P.N., Aires, C.C.P., Soveral, G., de
Almeida, I. Tavares, Duran, M., Wanders, R.J.A. and Silva,
M.F.B. (2007) Valproic acid metabolites inhibit dihydrolipoyl
dehydrogenase activity leading to impaired 2-oxoglutarate-driven
oxidative phosphorylation. Biochim. Biophys. Acta 1767, 1126–
1133.
Valenti, D., de Bari, L., Atlante, A. and Passarella, S. (2002) L Lactate transport into rat heart mitochondria and reconstruction
of the L -lactate/pyruvate shuttle. Biochem. J. 364 (Pt 1), 101–
104.
Passarella, S., Atlante, A., Valenti, D. and de Bari, L. (2003) The
role of mitochondrial transport in energy metabolism. Mitochondrion 2, 319–343.
De Bari, L., Atlante, A., Valenti, D. and Passarella, S. (2004)
Partial reconstruction of in vitro gluconeogenesis arising from
mitochondrial L -lactate uptake/metabolism and oxaloacetate
export via novel L -lactate translocators. Biochem. J. 380 (Pt. 1),
231–242.
Becker, C.M. and Harris, R.A. (1983) Influence of valproic acid
on hepatic carbohydrate and lipid metabolism. Arch. Biochem.
Biophys. 223, 381–392.
3366
[42] Rogiers, V., Vandenberghe, Y. and Vercruysse, A. (1985) Inhibition of gluconeogenesis by sodium valproate and its metabolites
in isolated rat hepatocytes. Xenobiotica 15, 759–765.
[43] Schmidt, D. (1999) Adverse effects and interactions with other
drugs in: Milestones in Drug Therapy-Valproate (Löscher, W.,
Ed.), pp. 223–264, Birkhäuser Verlag, Basel.
[44] El-Khatib, F., Rauchenzauner, M., Lechleitner, M., Hoppichler,
F., Naser, A., Waldmann, M., Trinka, E., Unterberger, I., Bauer,
C.C.P. Aires et al. / FEBS Letters 582 (2008) 3359–3366
G. and Luef, G.J. (2007) Valproate, weight gain and carbohydrate
craving: a gender study. Seizure 16, 226–232.
[45] Silva, M.F.B., Aires, C.C.P., Luis, P.B.M., Ruiter, J.P.N., IJlst,
L., Duran, M., Wanders, R.J.A. and de Almeida, I. Tavares
(2008) Valproic acid metabolism and its effects on mitochondrial
fatty acid oxidation: a review. J. Inherit. Metab. Dis. 31, 205–
216.