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Electrophoresis 2009, 30, 1329–1341
Emanuele Loro1
Elisabetta Gianazza2
Silvia Cazzola1
Adriana Malena1
Robin Wait3
Shajna Begum3
Carmen Brizio4
Federica Dabbeni-Sala5
Lodovica Vergani1
1
Dipartimento di Neuroscienze,
Facoltà di Medicina, Università
degli Studi, Padova, Italy
2
Gruppo di Studio per la
Proteomica e la Struttura delle
Proteine, Dipartimento di
Scienze Farmacologiche,
Università degli Studi, Milano,
Italy
3
Kennedy Institute of
Rheumatology Division, Faculty
of Medicine, Imperial College
London, Hammersmith, London,
UK
4
Dipartimento di Biochimica e
Biologia Molecolare, Università
degli Studi, Bari, Italy
5
Dipartimento di Farmacologia,
Facoltà di Medicina, Università
degli Studi, Padova, Italy
Received September 5, 2008
Revised October 24, 2008
Accepted October 30, 2008
Research Article
Development and characterization of
polyspecific anti-mitochondrion antibodies
for proteomics studies on in toto tissue
homogenates
We describe the characterization of polyclonal antibodies directed against the whole
mitochondrial subproteome, as obtained by hyperimmunization of rabbits with an
organelle fraction purified from human skeletal muscle and lysed by sonication. After
2-DE separations with either blue native electrophoresis or IPG as first dimension and
blotting, the polyspecific antibodies detect 113 proteins in human muscle mitochondria,
representative of all major biochemical pathways and oxidative phosphorylation
(OXPHOS) complexes, and cross-react with 28 proteins in rat heart mitochondria. Using
as sample cryosections of human muscle biopsies lysed in urea/thiourea/CHAPS, the
mitochondrial subproteome can be detected against the background of contractile
proteins. When comparing with controls samples from mitochondrial encephalomyopathy with lactic acidosis and stroke-like episodes patients, immunoblotting shows in the
latter a drastic reduction for the subunits of OXPHOS complex I as well as an increase of
several enzymes, including ATP synthase. This finding is the first evidence at the
proteomic level of massive up-regulation in a number of metabolic pathways by which
the affected tissues try to compensate for the deficit in the OXPHOS machinery.
Keywords:
Antibodies / Mitochondria / Proteomics
1 Introduction
Immunological detection in an unpurified sample is an
expedient alternative to general protein detection after
purification. Specific recognition of a single antigen with
Correspondence: Dr. Elisabetta Gianazza, Gruppo di Studio per
la Proteomica e la Struttura delle Proteine, Dipartimento di
Scienze Farmacologiche, Università degli Studi, via G. Balzaretti
9, I-20133 Milano, Italy
E-mail: elisabetta.gianazza@unimi.it
Fax: +39-0250318284
Abbreviations: ACADV, acyl-CoA dehydrogenase, verylong-chain specific; ACON, aconitate hydratase; ADT,
ADP/ATP translocase; AL4A1, D-1-pyrroline-5-carboxylate
dehydrogenase; BN, blue native; CISY, citrate synthase;
COX, cytochrome c oxidase; ETF, electron transfer
flavoprotein;
G3P,
glyceraldehyde-3-phosphate
dehydrogenase; IDHP, isocitrate dehydrogenase; KCRS,
creatine kinase; MDHM, malate dehydrogenase; MELAS,
mitochondrial encephalomyopathy with lactic acidosis and
stroke-like
episodes;
NDUFA,
NADH-ubiquinone
oxidoreductase; OXPHOS, oxidative phosphorylation; SDH,
succinate dehydrogenase (ubiquinone); VDAC, voltagedependent anion-selective channel protein
& 2009 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim
DOI 10.1002/elps.200800576
monospecific antibodies is most often the focus not only in
quantifications on unprocessed biological samples but also
in immunoblotting procedures after electrophoretic separations. Nonetheless, the use of polyspecific antisera proves
useful in some instances. In routine clinical laboratory
methods as well as in experimental protocols aiming at
recognizing disease markers (e.g. [1–3]), patient’s sera are
analyzed as containing antibodies against either ‘‘self’’
(normal or pathological tissue) or ‘‘not-self’’ antigens
(infectious agents, parasites, allergens). Polyspecific antisera
raised through experimental hyperimmunization are used
in diagnostic immunoelectrophoresis [4, 5] and in microbiology/parasitology methods (for isolate subtyping and for
characterization of immunodominant antigens/protective
antibodies [6–10]) but also in biochemical investigations
(isolation of cDNA clones encoding proteins of complex
structures [11]). With the use of commercial anti-rat serum
antibodies we could detect in 2-DE blots of whole-brain
tissue homogenates a sharp increase of serum proteins in
the affected versus the unaffected hemisphere of post-stroke
rats [12].
The first aim of the present investigation is then to
develop and characterize polyspecific antibodies directed
against the whole mitochondrion subproteome. The main
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1330
E. Loro et al.
use of such an immunological reagent would be in the
specific detection of at least the most abundant mitochondrial proteins in crude tissue extracts. A relevant application
could be with biochemical investigations either on needle
biopsies from muscles of patients reporting myopathy
symptoms or on cell cultures, when only minute amounts
of samples are available. A panel of antisera of various
specificity against mitochondrial proteins and protein
complexes is commercially available (see at http://
www.mitosciences.com/immunocytochemistry.html)
but
no product fits the requirements of polyspecificity inherent
to the approach we mean to take. The occurrence in human
patients of anti-mitochondrial autoantibodies [13] suggests
human muscle mitochondrial proteins may act as highly
immunogenic heteroantigens in rabbits.
As a second step, the polyspecific antibodies are applied
to the evaluation of the mitochondrial subproteome in
muscle specimens from patients with mitochondrial encephalomyopathy with lactic acidosis and stroke-like episodes
(MELAS), a rare type of myopathy secondary to an A-to-G
transition mutation at nucleotide pair 3, 243 in the dihydrouridine loop of mitochondrial tRNA(Leu)(UUR) [14]. No
such sample has ever been investigated before with
proteomic procedures.
Electrophoresis 2009, 30, 1329–1341
natants were pooled and centrifuged at 7000g for 10 min at
41C. The mitochondria in the final pellet were suspended in
3 mL of 5 mM MOPS, pH 7.4, containing 220 mM mannitol, 70 mM sucrose, 1 mM EDTA, 2 mM b-mercaptoethanol
(MSEM) and centrifuged at 9000g for 10 min at 41C. The
washed mitochondria were immediately frozen and stored
in liquid nitrogen.
2.2 Antibody production
Procedures involving animals and their care were conducted
at Dipartimento di Neuroscienze, Università degli Studi di
Padova, in conformity with the institution’s guidelines,
which are in compliance with national and international
rules and policies.
Two milligrams of mitochondria from human
skeletal muscle, suspended in 0.1 M NaCl at a final
concentration of 0.5 mg/mL, were sonicated four times at
60 W for 5 s and added volume-to-volume with incomplete
Freund’s adjuvant. This mixture was injected, in five
immunizations at 2 wk intervals, in each of two male New
Zealand white rabbits (Charles River, Calco, CO). Polyclonal
polyspecific antisera were collected 5 months after the last
injection.
2 Materials and methods
2.3 Antibody purification
2.1 Preparation of muscle homogenates and mitochondria
Control samples of human skeletal muscle (quadriceps)
were obtained by open biopsies from subjects undergoing
orthopedic surgery, after informed consent of the patients.
Pathological muscles were from two Italian male MELAS
patients [15]. Patient 1, already described in [16], was 42
years old and had 70% mutant mtDNA in muscle; patient 2
was 20 years old and had 80% mutant mtDNA. Both
presented MELAS symptoms and bilateral hearing loss,
vomiting, diarrhea and abdominal pain [15].
All muscle samples were frozen in liquid nitrogen and
stored at 801C until use.
Muscle homogenates were prepared using a glass
pestle in a glass potter, with a buffer containing 20 mM
HEPES, pH 7.4, 100 mM KCl, 1 mM EDTA, 2 mM
b-mercaptoethanol (buffer A) [17]. For some experiments,
cryosections, 10 mm thick, prepared from vastus lateralis
biopsies, were solubilized in urea/thiourea/CHAPS and
protein concentration was evaluated with 2-D Quanta Kit
(GE-Amersham).
Human muscle mitochondria were isolated from fresh
muscle specimens as described in [17]. Tissue was minced,
washed free of blood cells and homogenized in cold buffer
A. The homogenate was centrifuged at 800g for 10 min at
41C. The resulting supernatant was filtered through gauze
to remove fat while the pellet was resuspended in buffer A,
further homogenized and centrifuged. The filtered super& 2009 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim
Antibodies were purified from rabbit sera as described in
[18]. The antiserum was adjusted to pH 8.5 with
0.1 N NaOH. An aliquot of 2 mL, in continuous stirring,
was added dropwise with 7 mL of 0.4% rivanol (2-ethoxy
6,9-diaminoacridine lactate) solution. The supernatant,
containing the immunoglobulins, was decanted, centrifuged
to remove sediments and decolorized with activated
charcoal (approx. 100 mg, eventually removed by filtration
trough a paper disc). IgG, precipitated by incubation
overnight at 41C with an equal volume (5 mL) of saturated
ammonium sulfate, were collected by centrifugation at
4000g for 20 min at 41C and finally resuspended in a
volume of saline equivalent to half the volume
of the starting antiserum (1 mL). Sulfate residues were
removed by chromatography on a Sephadex G-25
column (PD10 from GE-Amersham). The purified immunoglobulin concentration was determined by Lowry’s
assay [19].
2.4 SDS-PAGE and electroblotting
Total proteins from human muscle homogenates and
purified mitochondria were separated by SDS-PAGE on a
7.5–17.5%T PAA gradient in the discontinuous buffer
system of Laemmli [20]. The protein pattern was either
revealed by CBB staining or electroblotted to nitrocellulose
(NC) membrane [21].
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Electrophoresis 2009, 30, 1329–1341
2.5 Analysis of oxidative phosphorylation complexes by blue native-PAGE
Oxidative phosphorylation (OXPHOS) complexes were
extracted as described in [22, 23]. Aliquots of 2 mg of
mitochondria were suspended in 2 mL of 400 mM sucrose,
1 mM EDTA, 0.2 mM PMSF and 0.2 M MOPS, pH 7.2, and
centrifuged at 32 000g for 30 min at 41C. The pellet was
resuspended in 200 mL of 1 M aminocaproic acid, 50 mM
Bis-Tris/HCl pH 7.0 (buffer B) and added with 37.5 mL of
freshly prepared 10% w/v lauryl maltoside. After 10 min
incubation, the samples were centrifuged at 128 000g for
30 min at 41C. The supernatants, containing solubilized
OXPHOS complexes, were collected and their protein
content was determined by Bradford assay [24]. Samples
were then frozen in liquid nitrogen and stored at 801C up
to several months.
Blue native (BN)-PAGE was performed using a minigel
apparatus (Miniprotean Bio-Rad) as described in [17].
Different amounts of proteins (from 7.5 to 50 mg), in a
loading buffer containing 7% v/v of a 5% w/v solution of
Serva Blue G in 1 M aminohexanoic acid and 1% glycerol,
were run on a 5–13%T gradient gel (Bio-Rad) and processed
as described in [23]. Aliquots of 5 mg of rat heart mitochondrial complexes and of 7.5 mg of human skeletal muscle
complexes were loaded for native separation followed by ingel activity assays (Section 2.6.) or native electroblotting
(Section 2.7). Aliquots of 50 mg of proteins were run in first
dimension for 2-DE separation BN-PAGE–SDS-PAGE
(Section 2.8).
Proteomics and 2-DE
1331
dilution (a gift of Prof. F. Dabbeni-Sala, Padova, Italy), and
polyclonal antibodies against FAD covalently bound to the
flavoprotein subunit of complex II, used at 1:500 dilution
(a gift of Prof. R. Brandsch, Freiburg, Germany). Incubation
lasted 4 h. Test polyspecific antibodies raised in rabbits in
our laboratories (Section 2.3.) were used at a concentration
of 0.6 mg/mL; incubation lasted overnight. The secondary
antibodies (GE-Amersham), tagged with HRP, were used at
a 1:2500 dilution; peroxidase zymography was visualized by
enhanced chemiluminescence (ECL, GE-Pharmacia).
2.8 2-DE BN-PAGE–SDS-PAGE
Single subunits of OXPHOS complexes, separated in 1-DBN-PAGE, were resolved by SDS-PAGE on a 7.5–17.5%T
PAA gradient in the discontinuous buffer system of
Laemmli [20] similar to the protocol in [23]. Equilibration
between first and second dimensions was obtained by
incubation for 30 min at 371C, in 2 mL of 10 mM Tris/
acetate, pH 8.2, containing 4% w/v SDS, 0.3% v/v
b-mercaptoethanol, 20% v/v glycerol and 1% v/v Pyronin
Red. Individual 1-DE lanes were overlaid to each SDS-PAGE
slab; the 2-DE gels were run at 50 V until the tracking dye
passed the stacking gel, then at 150 V. A pair of gels was
always processed in parallel: one to be stained with CBB, the
other to be blotted into NC membrane for immunodetection
with rabbit polyspecific antibodies. Both 2-DE patterns were
then scanned and analyzed with commercial software.
All the CBB-stained spots positive to immunodetection
were excised for identification through trypsinolysis and
ESI-MS/MS.
2.6 In-gel activity assay
Immediately after the electrophoretic run, enzymatic colorimetric reactions were performed on the BN-PAGE gel,
according to the protocols described in [17]. Aliquots of 5 mg
of rat heart mitochondrial complexes and of 7.5 mg of
human skeletal muscle complexes were loaded for native
separation. Single lanes were incubated for the zymograms
for NADH-ubiquinone oxidoreductase (NDUFA) (EC
1.6.5.3); for ATPase (ATP synthase) (EC 3.6.3.14); for
cytochrome c oxidase (COX); and for succinate dehydrogenase (ubiquinone) (SDH) (EC 1.3.5.1). Enzymatic reactions
were visible after 1 h of incubation at room temperature
with rat heart and after 2–3 h with human skeletal muscle
samples. A reference lane was stained with CBB.
2.7 Immunodetection
Reference antibodies were complex-specific: commercial
monoclonal antibodies directed against complexes I and IV
(Molecular Probes) used at 1:500 and 1:750 dilution,
respectively; polyclonal antibodies against complex III, used
at 1:200 dilution (a gift of Dr. R. Bisson, Padova, Italy);
polyclonal antibodies against complex V, used at 1:10 000
& 2009 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim
2.9 2-DE IEF–SDS-PAGE
First dimension was run on 4–10 NL IPG [25], second
dimension on a 7.5–17.5%T PAA gradient in the discontinuous buffer system of Laemmli [20]. With IPG, two
procedures were tried: (i) polymerization of an anodic IP
plateau [26], reswelling in 8 M urea, on-gel anodic sample
application and run ‘‘upside up’’ in a Multiphor chamber
[27] of 8 cm-long, 7 mm-wide strips; (ii) polymerization of
both anodic and cathodic, 2 cm long, IP plateaus [26], in-gel
rehydration with 7 M urea, 2 M thiourea and 4% w/v
CHAPS and run ‘‘upside down’’ in a Protean IEF cell [28]
of 12 cm-long and 3.5 mm-wide strips. Equilibration
between first and second dimensions was according to
standard protocols [29]. Second dimension was run in a
MiniVE chamber (GE-Amersham), with slab size
85 70 1.5 mm3. Typical sample loads were 50–100 mg
of mitochondrial proteins and 50–400 mg of either cryosection lysate or muscle homogenate. The latter contains a very
high concentration of BSA from the extraction buffer
(Section 2.1.); hence the total protein load in the experiments was proportionally higher. All detection procedures
after 2-DE were as in Section 2.8.
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E. Loro et al.
2.10 MS
In-gel digestion with trypsin was performed according to
published methods [30–32] modified for use with a robotic
digestion system (Genomic Solutions, Huntington, UK)
[33]. Cysteine residues were reduced with DTT and
derivatized by treatment with iodoacetamide. The gel pieces
were dehydrated with acetonitrile and dried at 501C, prior to
addition of modified trypsin (Promega, Madison, WI; 10 mL
at 6.5 ng/mL in 25 mM ammonium hydrogen carbonate).
After incubation at 371C for 8 h, peptides were sequentially
extracted with 25 mM ammonium hydrogen carbonate, 5%
formic acid and acetonitrile.
Tandem electrospray mass spectra were recorded using
a Q-Tof hybrid quadrupole/orthogonal acceleration time of
flight spectrometer (Micromass, Manchester, UK) interfaced
to a Micromass CapLC capillary chromatograph. Samples
were dissolved in 0.1% aqueous formic acid, injected onto a
Pepmap C18 column (300 mm 0.5 cm; LC Packings,
Amsterdam, NL), and eluted into the mass spectrometer
with an acetonitrile/0.1% formic acid gradient (5–70%
acetonitrile over 20 min). The capillary voltage was set to
3500 V.
A survey scan over the m/z range 400–1300 was used to
identify protonated peptides with charge states of 2, 3 or 4,
which were automatically selected for data-dependent MS/
MS analysis, and fragmented by collision with argon. The
resulting product ion spectra were transformed onto a singly
charged m/z axis using a maximum entropy method
(MaxEnt3, Micromass) and proteins were identified by
correlation of uninterpreted spectra to entries in Swiss-Prot/
TrEMBL, using ProteinLynx Global Server (Version 1.1,
Micromass). The database was created by merging the
FASTA format files of Swiss-Prot, TrEMBL and their associated splice variants (1 768 175 entries at the time of writing). No taxonomic, or protein mass and pI constraints were
applied. One missed cleavage per peptide was allowed, and
the fragment ion mass tolerance window was set to
100 ppm. For confirmation of identifications spectra were
also searched against the NCBI nr database using MASCOT.
Hits that rested on a single matching peptide were
confirmed by manual interpretation of sequence specific
fragment ions using the MassLynx program PepSeq
(Micromass).
3 Results
To evaluate the diverse immunological responses induced
by mitochondrial proteins in the two hyperimmunized
rabbits, proteins from whole human skeletal muscle
homogenate and from purified skeletal muscle mitochondria were resolved in gradient SDS-PAGE, electroblotted
and probed with immunoglobulins purified from the two
polyspecific antisera. ECL development of HRP zymography
had identical duration for all NC membranes. Figure 1A
shows how the antibodies produced by the two rabbits (left
and middle panels) recognize different specific mitochondrial proteins with different affinity, both when in a purified
sample and in whole muscle homogenate. On the basis of
Figure
1. Immunodetection
of
mitochondrial
proteins with polyspecific
antibodies raised in rabbits
after 1-DE or 2-DE and
electroblotting. A 5 1-DE of
varying
amounts,
as
marked, of mitochondria
purified from human skeletal muscle and of whole
human skeletal muscle
homogenates. Primary antibody from rabbit-1 in the
blot to the left, from rabbit2 in the middle, from both
rabbits to the right. Rightmost, Mr listing of protein
standards.
B 5 2-DE
of
mitochondria, left (same as
in Fig. 3), and of muscle
homogenate, right (same
as in Fig. 6). The extra spots
detected in muscle homogenate versus purified
mitochondria are marked
with their names.
& 2009 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim
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Electrophoresis 2009, 30, 1329–1341
Proteomics and 2-DE
1333
whole muscle homogenate and not in mitochondria
(Fig. 1A) and due to cross-reactivity with serum albumin
(see Tables S1 and S2 in Supporting Information). When
comparing the immunostaining of the two types of samples
after 2-D (IEF–SDS-PAGE) (Fig. 1B) two more peculiar
spots were present in whole muscle homogenate (right) but
not in purified mitochondria (left): (i) one at high molecular
weight, due to cross-reactivity with myosin and (ii) the other
at pI 7–29 kDa, identified as carbonic anhydrase, a protein
that accounts for 8% of total muscle proteins (see Tables S1
and S2 in Supporting Information).
BN-PAGE, developed to investigate membrane-bound
protein complexes and designed for the mitochondrial
OXPHOS system [22], was used to evaluate which
complexes, and which of their constituent subunits, were
recognized by the rabbit polyspecific antibodies. Figure 2A
illustrates the 1-DE run on a 5–13%T PAA gradient gel of
7.5 mg of human skeletal muscle mitochondrial complexes
isolated by a one-step protocol [23]. The separation of the
individual complexes, on the basis of their size, is visualized
both by CBB staining and by in-gel activity assays specific
for the different complexes: complex II or SDH (EC1.3.5.1),
complex IV or cytochrome c oxidase (EC 3.6.3.14) (COX),
complex V or ATPase (EC 3.6.3.14) and complex I or NADH
dehydrogenase (EC1.6.5.3) (NDUFA).
We also analyzed the relative presence of the different
complexes by native electroblotting and immunodetection
with all available monospecific antibodies, lane ‘‘blot
(mono-)’’ (a composite picture from five independent
experiments). These signals are to be compared with the
banding obtained with the rabbit polyspecific antibodies,
lane ‘‘blot (poly-)’’. The polyspecific antibodies recognize all
the complexes in a specific way, but with different affinity.
In fact complexes I, V, III and IV develop bands of similar
intensity to blot (mono-), indicating a high antigenic activity
of these four complexes; on the contrary complex II gives
3 Figure 2. Detection of mitochondrial complexes purified from
this evidence, in all of the following experiments a balanced
pool of the immunoglobulins from the two antisera was
used for immunodetection (right panel).
The pattern of 1-D immunodetection presented a single
discrepancy between purified mitochondria and whole cell
extract – a band, about 66 kDa in size, detected only in
& 2009 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim
human muscle mitochondria: (A) 5 after 1-DE (BN-PAGE); (B and
C) 5 after 2-DE (BN-PAGE–SDS-PAGE). (A) The strips, bottom up,
correspond to CBB staining; to immunodetection with polyspecific antibodies raised in rabbits (blot poly-); to a composite
picture of the immunodetections of individual complexes
(banding as marked) with already available monospecific
antibodies (blot mono-); to the zymogram for NDUFA (EC
1.6.5.3); to the zymogram for ATPase (ATP synthase F0) (EC
3.6.3.14); to the zymogram for COX; to the zymogram for SDH
(EC 1.3.5.1). Protein load 5 7.5 mg. (B) The maps correspond to
CBB staining (bottom) and to immunodetection with polyspecific antibodies raised in rabbits after electroblotting (top).
Protein load as marked. The spots detected by the polyclonal
antisera were excised from the CBB gel and processed for
protein identification through trypsinolysis and ESI-MS/MS.
Each of these spots is marked with a number, the same as
associated to the matching entry in the alphabetical list of
identified proteins in Table S1. (C) The identified spots are
labeled by function, in order to highlight supramolecular
assemblies. I–V 5 OXPHOS complexes I–V; downwards triangles 5 enzymes of carbohydrate and amino acid metabolism;
upwards triangles 5 enzymes of lipid metabolism; squares 5 PDH subunit; pentagon 5 prohibitin; circle 5 transport.
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E. Loro et al.
a weaker signal when probed with the polyspecific than with
the monospecific antibodies.
To further dissect the properties of the rabbit polyspecific antibodies raised in our laboratories, the single
subunits of the native complexes were separated in second
dimension by SDS-PAGE, as also shown in Fig. 2. One gel
was stained with CBB (Fig. 2B, bottom); another blotted and
probed with the polyspecific antibodies (Fig. 2B, top). All the
spots that were positive both to immunodetection and to
CBB staining were excised, trypsin-digested and analyzed by
ESI-MS/MS. The identified proteins are listed, in alphabetical order, in Supporting Information Table 1S, each entry
being identified by a number that also marks the corresponding spot in Fig. 2B (CBB stain panel). Table 2S in
Supporting Information provides the full list of matching
peptide sequences for each spot. In panel 2C the proteins
are labeled on the basis of their biochemical function or of
the metabolic pathway they take part into. In several
instances we observe the comigration of subunits of different OXPHOS complexes, and/or the comigration of
OXPHOS subunits with various matrix or membrane
proteins. This finding supports the concept of supramolecular interactions among enzymes resulting in the organization of a ‘‘metabolon’’, defined as a functional complex of
enzymes sequential in a metabolic pathway and bound to a
cell structural element.
A similar procedure was performed in another set of
experiments, in which 50 mg of human skeletal muscle
mitochondrial proteins were resolved by IEF on IPG,
followed by SDS-PAGE in the second dimension. Figure 3
compares the protein patterns after immunoblotting and
after CBB staining. The MS-identified proteins are listed in
Supporting Information Table 1S, while matching sequences are listed in Table 2S of Supporting Information.
Cross-immunoreactivity towards related antigens, namely
mitochondrial complexes from a different species, the rat, and
a different type of muscular tissue, the heart, was then tested,
as illustrated in Fig. 4. Resolution of rat heart OXPHOS by
2-DE separation BN-PAGE–SDS-PAGE was performed as
described in Fig. 2B. As shown in the list of Table 1S, many of
the rat proteins are detected by the polyspecific antibodies
raised against the corresponding human proteins.
To test whether the use of the polyspecific antibodies
could detect differences between control and pathological
samples, we thoroughly characterized mitochondria
from MELAS patients. As shown in Fig. 5A by the densitometric evaluation of the zymograms developed after BNPAGE, enzymatic activity of ATPase and of SDH are unaffected by the pathology. Conversely, the activity of COX is
strongly reduced and the activity of NDUFA is virtually abolished. Figure 5B is the 2-DE (BN-PAGE–SDS-PAGE) of the
mitochondrial complexes from a MELAS sample as immunodetected after electroblotting; the arrowheads mark changes
in spot intensity versus a matched control. A decrease in the
intensity of complex I subunits is evident together with an
increase of ADP/ATP translocase (ADT) and of ATP synthase
subunits (B, D, O, g and f subunits).
& 2009 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim
Electrophoresis 2009, 30, 1329–1341
Figure 3. Detection of mitochondrial proteins purified from
human skeletal muscle after 2-DE (IEF–SDS-PAGE). CBB staining
(bottom) and immunodetection with polyspecific antibodies
raised in rabbits after electroblotting (top). Protein load as
marked. Spots analysis and map labeling were as in Fig. 2.
Finally, the applicability of rabbit polyspecific antisera
was tested towards a high background of unrelated antigens
such as in total skeletal muscle. In a first step (Fig. 6A, top)
the patterns of MELAS muscle lysates (right; N 5 2) were
compared to control samples after SDS-PAGE and immunoblotting; Fig. 6B plots the ratio between the integrated
optical densities of the stained bands, MELAS versus controls,
when normalized for the b-actin signal in each lane (Fig. 6A,
bottom). Band intensity is higher in pathological samples at
Mr ca. 80 and 40 kDa, much higher at Mr ca. 30 kDa. Then, as
shown in Fig. 6C, 300 mg of whole proteins from normal and
MELAS skeletal muscle were resolved by 2-DE through
IEF–SDS-PAGE. Even at this high concentration, the most
prominent spots detected by Ponceau staining are only
slightly positive to immunodetection. In this 2-DE procedure
alternative protocols for sample preparation and IPG run had
been compared (data not shown). Direct solubilization of
muscle cryosections in urea/thiourea/CHAPS and anodic ongel loading afforded both highest sample loading and least
streaking. As a further advantage, the use of cryosections
requires the lowest total amount of material with virtually no
waste and is thus compatible with biopsy processing.
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Proteomics and 2-DE
Electrophoresis 2009, 30, 1329–1341
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Figure 5. Characterization of mitochondrial proteome in MELAS.
(A) Ratios between the densitometric data for enzyme activities
after BN-PAGE in control and MELAS samples; abbreviations for
protein names are as in Fig. 2A. (B) Immunoblotting after 2-DE
(BN-PAGE–SDS-PAGE) on mitochondrial complexes. The
upwards and downwards arrowheads stand for increase or
decrease of spot intensity versus control.
Figure 4. Detection of mitochondrial complexes purified from
rat heart mitochondria after 2-DE (BN-PAGE–SDS-PAGE). CBB
staining (middle) and immunodetection with polyspecific antibodies raised in rabbits after electroblotting (top). Protein load
as marked. Spots analysis and map labeling were as in Fig. 2.
Bottom panel: same as in Fig. 2C.
Figure 6C shows a clearly increased abundance of a
number of immunoreactive components in the total MELAS
muscle lysate in comparison with a matched control sample.
This difference may be observed in the middle panels
(blotting and detection with polyspecific antibodies). Specifically the areas of increased immunological reactivity
correspond to the regions where, in Fig. 3, the following
proteins are found to migrate: ACADV (acyl-CoA dehydrogenase, very-long-chain specific), AL4A1 (D-1-pyrroline-5carboxylate dehydrogenase), aconitate hydratase (ACON), ATP
synthase a and b (ATPA and ATPB), citrate synthase (CISY),
glyceraldehyde-3-phosphate dehydrogenase (G3P), isocitrate
& 2009 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim
dehydrogenase (IDHP), KCRS (creatine kinase), MDHM
(malate dehydrogenase) and VDAC1 (voltage-dependent
anion-selective channel protein 1; synonym: porin).
4 Discussion
Given the importance of mitochondria in human diseases [15],
protocols that permit the analysis of the mitochondrial
subproteome from small amounts of biopsy tissue and even
cell culture material would have great diagnostic utility. In this
report we describe the possibility to develop polyspecific
antibodies directed against the whole human mitochondrial
subproteome by rabbit hyperimmunization with purified
skeletal muscle mitochondria, and the application of these
antibodies in protocols using small amounts of human muscle.
Such a strategy overcomes the limitations of the protocols
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E. Loro et al.
Electrophoresis 2009, 30, 1329–1341
Figure 6. Detection of
mitochondrial proteins
in whole human skeletal muscle from control
and MELAS patients.
(A) Comparison of the
SDS-PAGE pattern for
five controls (left) and
two
MELAS
(right)
muscles after immunoblotting using polyclonal anti-mitochondrion
antibodies (top) and
after reprobing the NC
membrane
with
commercial anti-actin
antibodies
(bottom).
(B) Results from densitometric evaluations of
the SDS-PAGE patterns
in panel A, plotted as
ratios between MELAS
and control samples.
(C) 2-DE (IEF–SDSPAGE) and electroblotting of lysed cryosections from control and
MELAS
muscle:
Ponceau Red staining
(left), immunodetection
with polyspecific antibodies raised in rabbits
(right). Experimental:
muscle
cryosections
directly lysed in urea/
thiourea/CHAPS,
loaded on gel near the
anode. The upwards
and downwards arrowheads
stand
for
increase or decrease of
spot intensity versus
control.
described thus far to obtain purified mitochondria from gram
amounts of muscle as starting material – a requirement hardly
met with human specimens.
4.1 Characterization of the polyspecific
anti-mitochondrion antibodies
Specificity of antibodies rests primarily on the purity
of the antigen. The mitochondria used to produce the
polyclonal antibodies belong to the same batch already
used to define the reference 2-DE map of human
muscle mitochondria [28]. In this preparation MS procedures identified only a negligible number of non-mitochondrial proteins [28], which has been confirmed by the new
MS data listed in Tables 1S and 2S of Supporting
Information.
& 2009 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim
The characterization of polyspecific antibodies specificity was performed against human muscle mitochondria
and rat heart mitochondria. About 200 gel features from
2-DE, either BN-PAGE–SDS-PAGE or IEF–SDS-PAGE,
were recognized, and analyzed with ESI-MS/MS. The antibodies detected (Table 1S) 20 homologous proteins both in
human and in rat samples, 85 proteins only in human
muscles and 8 proteins only in rat heart. This high degree of
cross-reactivity may be explained by the high sequence
identity between mammalian mitochondrial proteomes as it
had already been reported for humans, mice and cows
(Mitomap [34, 35]).
On the basis of Entrez Gene [36], the Human Protein
Reference Database [37] and MitoP [38], 113 proteins were
functionally categorized; no function could be assigned to 21
polypeptides listed in TrEMBL [39]. The distribution
of the functionally classified proteins is shown in Fig. 7 and
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Electrophoresis 2009, 30, 1329–1341
Figure 7. Distribution of the 113 functionally classified proteins
detected by polyspecific antibodies. Assignments to functional
classes were made on the basis of (i) classifications provided in
the MITOP database and (ii) information provided at National
Center for Biotechnology Information’s Entrez Gene website
(http://www.ncbi.nih.gov/entrez/query.fcgi?db 5 gene) and Human
Protein Reference Database (http://www.hprd.org).
their localization in enzymatic pathways is visualized in
Fig. 8.
Depending on the electrophoretic procedure in first
dimension, the proteins recognized by the polyspecific
antibodies in the 2-DE maps are mostly proteins embedded
in, or connected to, the mitochondrial membranes when
resolved by BN-PAGE (Figs. 2 and 4) and mostly proteins
from the mitochondrial matrix space when resolved by IEF
(Fig. 3). As an example, the ADT1 is a very hydrophobic and
basic inner-membrane carrier, and one of the principal
proteins in mitochondrial preparations [40]. ADT1 was
not observed in IEF–SDS-PAGE but was found in
BN-PAGE–SDS-PAGE (Figs. 2B and 4).
4.1.1 OXPHOS
Subunits of the five complexes that constitute the OXPHOS
machinery represent the main group, amounting to 48% of the
functionally classified mitochondrial proteins recognized by the
antibodies (Fig. 7). This includes 14/45 complex I subunits, 2/4
complex II subunits (plus 2 complex II-related subunits), 7/11
complex III subunits, 4/13 complex IV subunits and 11/16
complex V subunits.
4.1.2 Metabolism
The enzymes of the TCA cycle (plus pyruvate dehydrogenase) are represented by 11 distinct proteins
(enzymes or enzyme subunits) whereas lipid metabolism
is represented by 16 proteins – an indication of the primary
role of fatty acid oxydation as energy source in skeletal
muscle.
4.1.3 Enzyme association
The protocol BN-PAGE–SDS-PAGE allows the isolation of
active OXPHOS enzymes without loss of subunits, as shown
& 2009 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim
Proteomics and 2-DE
1337
by in-gel activities in Fig. 2A. As apparent in Figs. 2B and 4,
and confirmed by MS analysis, the second dimension
electrophoresis resolves from the position where each
OXPHOS complex has migrated in first dimension not
only the specific complex subunits but also significant
amounts of other mitochondrial membrane proteins
together with unexpected proteins known to be localized
in the matrix (bottom panels in Figs. 2 and 4). Some of these
proteins are involved in metabolic processes (TCA cycle,
amino acid and lipid metabolism), some take part in protein
folding (prohibitin) or are transport proteins (VDAC and
ADT1). These impurities might be due to simple contamination; however it appears that the concentration of
detergent we used (1.5% lauryl maltoside, chosen to
minimally disrupt complexes and to maintain their activity
according to Zerbetto et al. [17]) may be too low to weaken
native contacts with OXPHOS complexes. This hypothesis is
confirmed by several reports that, using different technical
approaches, described physical interactions between
OXPHOS complexes and proteins of b-oxidation and TCA
cycle, resulting in enzyme assemblies of high functional
efficiency [41–45].
The in-gel activity assay for complex I (Fig. 2A) recognizes a sharp band at 1 MDa and a lighter band at 200 kDa.
Consistently we observe the presence of two complex I
subunits (NADH B22 subunit, NADH 39 kDa subunit)
intermixed with complex IV subunits after second dimension migration (Fig. 2B). Comigration of mixed elements of
complex I, three subunits of complex III (core subunits 1
and 2, subunit 14 kDa) and complex IV isolated in active
state (Fig. 2A) seems to indicate an interaction preserved by
a mild solubilization protocol and made evident by polyspecific antibodies.
These findings are in line with previous evidences
showing that complexes I, III and IV assemble into so-called
‘‘supercomplexes’’ leading to the formation of supramolecular structures called ‘‘respirasomes’’ (first described in [46]
and reviewed in [47, 48]), which seem to be of great functional importance [47, 48].
Recent structural analyses revealed the association of
ATP synthase with the phosphate carrier and ADT1 into the
functional metabolon called ‘‘ATP synthasome’’ [49, 50]. In
the human skeletal sample, ADT runs in association with
complex I, V–III, IV–II (Fig. 2C) and with VDAC, consistent
with the described associations in ATP synthasome [49, 50]
and in VDAC–ADT interaction complexes [51].
Subunits of complex V, running in association with
subunits of complexes I, III and IV (subunits 2 and 4), may
indicate that, under our experimental conditions, a small
amount of complex V was retained in supercomplexes of
OXPHOS machinery, as previously observed in experiments
of immunocapture of functionally active human heart
complex V [42] and complex I [43].
Subunits of complex I of muscle mitochondria run also
in association with prohibitin 2 and mitofilin (Fig. 2C and
Supporting Information Table 1S). Mitofilin is a mitochondrial inner membrane protein controlling mitochonwww.electrophoresis-journal.com
1338
E. Loro et al.
Electrophoresis 2009, 30, 1329–1341
Figure 8. Mapping of the proteins detected by the polyspecific anti-mitochondrion antibodies on a simplified chart of the main metabolic
pathways. Names of the relevant enzymes are boxed, according to the following graphical code: light grey filling for all identified
enzymes; dark grey filling for the enzymes (or enzyme subunits) up-regulated in MELAS patients; black filling for the enzymes (or
enzyme subunits) decreased in MELAS patients; framing with both a continuous and a dashed thick line for enzymes (or enzyme
subunits) recognized in both human skeletal muscle and rat heart samples; framing with a thick dashed line for enzymes recognized only
in rat heart samples; framing with a thin continuous line and white filling for enzymes not identified in the present investigation.
Abbreviations were as in the caption to Fig. 1 of [28], except: AATC: aspartate aminotransferase, cytoplasmic; AATM: aspartate
aminotransferase, mitochondrial; ACSM: medium-chain acyl-Coa synthetase; ADT1: ADP/ATP translocase 1; AL4A1:D-1-pyrroline-5carboxylate dehydrogenase; ALDH2: aldehyde dehydrogenase; CMC1: calcium-binding mitochondrial carrier protein Aralar1
(mitochondrial aspartate glutamate carrier 1); DECR: 2,4-dienoyl-CoA reductase; IDHP: isocitrate dehydrogenase (NADP); KCRS: creatine
kinase, sarcomeric; M2OM: mitochondrial 2-oxoglutarate/malate carrier protein; MDHC: malate dehydrogenase, cytoplasmic; MDHM:
malate dehydrogenase, mitochondrial; MPC: mitochondrial pyruvate carrier (unidentified); NNTM: NAD(P) transhydrogenase; PRDX3:
thioredoxin-dependent peroxide reductase; SODM: superoxide dismutase (Mn); THIOM: thioredoxin; TRXR2: thioredoxin reductase 2;
VDAC1: voltage-dependent anion-selective channel protein 1; VDAC2: voltage-dependent anion-selective channel protein 2.
drial cristae morphology that assembles into large multimeric complexes, for which a close cosedimentation with
complex I has been previously demonstrated [45]. Prohibitins are a family of proteins with low molecular weight,
which assemble into large structures in the mitochondrial
inner membrane and act as membrane-bound chaperones
for the stabilization of newly synthesized mitochondrial
translation products [52]. In particular, a role in the
assembly or degradation of mitochondrial complex I has
been suggested [53]. We found that prohibitins comigrate
with complex I at 1 MDa (Fig. 2C), in agreement with
previous findings [54].
In rat heart, SDH flavoprotein subunits comigrate with
electron transfer flavoprotein (ETF) a subunit, IDHP and
ADT (Fig. 4, bottom). Similarly, in human muscle, SDH
flavoprotein comigrates with medium chain acyl-CoA
& 2009 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim
dehydrogenase, CISY, IDHP and ADT, whereas NADH
dehydrogenase
subunit
75 kDa
comigrates
with
the a subunit of trifunctional enzyme (Fig. 2, bottom).
Existence of functional assemblies between enzymes of the
b-oxidation pathway and OXPHOS (specifically, complexes I
and II) had been previously reported [55, 56] with the
suggestion of a functional channeling of NADH and CoA/
acetylCoA by a b-oxidation metabolon [55].
In a similar way we interpret the presence of different
matrix soluble enzymes such as CISY-IDHP and transenoylCoA isomerase (Fig. 2B) at a position (200 kDa)
corresponding to activity and presence of complex IV in first
dimension as supportive evidence of interactions between
inner membrane and matrix. Previous reports [57, 58] had
already shown interactions among TCA cycle enzymes as
well as interactions between these enzymes and the cis
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Electrophoresis 2009, 30, 1329–1341
surface of the inner mitochondrial membrane. It was
proposed that these multiple interactions could result in a
supramolecular protein–membrane complex defined as the
TCA cycle metabolon [58].
4.1.4 Non-mitochondrial proteins
Four distinct cytoplasmic proteins – the glycolytic enzyme
G3P, carbonic anhydrase 3, and the structural proteins actin
and myosin – have been recognized by the polyspecific antimitochondrion antibodies. These may represent either
minor contaminants, proteins that have physical associations with the mitochondria or proteins/protein isoforms
that are also present inside the mitochondria. It is
noteworthy that the recognized isoform of G3P exhibits
basic pI value and may electrostatically associate with the
mitochondrial outer membrane, as it has been previously
reported [40, 59]. Actin and myosin may represent artifacts
of the isolation procedure, but may also reflect the
cytoskeletal architecture with which mitochondria are
intimately associated. In a recent report 2-DE (BN–SDSPAGE) of OXPHOS from five rat organs resulted in the
identification of 92 non-redundant soluble and membraneembedded non-OXPHOS proteins including 36 proteins
known or presumed to be localized to non-mitochondrial
compartments [60].
4.1.5 Undetected proteins
Since the antibodies identify only about 10% of the known
mitochondrial proteins, it is likely that the list is underestimated. We did not observe antibodies against proteases,
such as mitochondrial processing peptidase, against proteins
involved in cell death, such as Smac and AIF, in protein
targeting, such as components of the protein translocation
machinery, and in RNA–DNA–protein synthesis, such as
mitochondrial ribosomal proteins or DNA polymerase.
Although we have assembled a list of physico-chemically and
functionally diverse proteins recognized by our polyspecific
antibodies, our choice of methodology may not be optimal for
certain proteins. For example, in the case of OXPHOS
complexes our antibodies did not identify very hydrophobic
proteins (for example ATPase subunit C, the proteolipid
anchor of complex V). Similarly the absence of other proteins
may reflect either a low abundance or physical properties/
chemistries unfavorable to detection by our analytical strategies
(BN-PAGE, IEF). Therefore, additional investigations and
strategies, such as immunoprecipitation, may further extend
the list of the mitochondrial proteins identified by these
polyspecific antibodies.
4.2 Analysis of lysates from whole muscle of MELAS
patients
No proteomic data on specimens from MELAS patients are
currently available in the literature. After a transcriptomic
& 2009 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim
Proteomics and 2-DE
1339
investigation, in 1999 Heddie et al. [61] reported on the
‘‘coordinate induction of energy gene expression in tissues
of mitochondrial disease patients’’, including a MELAS
subject. Our data, based on the results of electrophoretic
separations plus immunoblotting using the polysepcific antimitochondrion antibodies, fully confirm their data and
extend the list of the affected proteins specific to the
mitochondrial compartment.
BN-PAGE-based procedures focus information on
proteins of mitochondrial membranes. The lack of complex
I activity when MELAS samples are assayed in-gel after 1-DE
separation (Fig. 5A) is in agreement with the finding of a
strongly reduced presence of both CBB stained (data not
shown) and immunoreactive material migrating at the
position typical for NDUFA subunits after 2-DE separation
(BN-PAGE–SDS-PAGE) (Fig. 5B). The reduction of activity
for complex IV (Fig. 5A) has no obvious counterpart in a
quantitative alteration in 2-DE pattern (either CBB- or
immunostained, Fig. 5B). However, a qualitative alteration
of the pattern is observed, featuring a minor shift in BNPAGE mobility, which could be caused by ROS-mediated
oxidation, as it has been previously suggested [62]. The
normal ATPase activity is consistent with previous observations of milder bioenergetic defect in cells harboring 3243
MELAS mutation in comparison with other mtDNA point
mutations [63, 64] Conversely, after 1-DE with SDS-PAGE
(Fig. 6A-B), the use of polyclonal antibodies on MELAS
whole muscle samples shows an overall increase in the
amount of immunoreactive material in comparison with
whole control muscle. This finding is likely connected with
the distinctive proliferation of mitochondria in the tissues of
mitochondrial disease patients. Indeed, a hallmark of
MELAS muscles is the histological evidence of an increased
number of subsarcolemmar mitochondria made evident by
the trichromic staining [15]. However, the percent increase
of protein content in MELAS versus control is different in
different molecular size ranges, and is maximal for lower
molecular weight species. With a more detailed investigation through 2-DE protocols (IEF–SDS-PAGE), specific
energy pathways are found to be affected: ADT1 is found
increased in 2-DE with BN-PAGE as first dimension,
ACADV, AL4A1, ACON, CISY, G3P, IDHP, KCRS, MDHM
and VDAC in 2-DE with IEF as first dimension, ATP
synthase subunits with both types of 2-DE experiments.
The increase in the number of mitochondria as well as
in the amount of specific enzymes is most likely a
compensatory phenomenon in response to energy deprivation. Our data are thus consistent with the transcriptomics
findings reported by Heddi et al. [61] who observed
increased levels of transcripts for mtDNA as well as for
nuclear OXPHOS genes. Specifically, among the 16 genes
tested for, they reported up-regulated transcription for
ATPB, ADT and KCRS, for which we find an increase in
protein levels. Their observations and ours thus suggest that
muscle tissue attempts to counteract OXPHOS defects
associated with mtDNA mutations by stimulating mitochondrial biogenesis and by boosting the metabolic pathwww.electrophoresis-journal.com
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E. Loro et al.
ways that may circumvent the absence of OXPHOS complex
I as well as the reduction in activity of complex IV.
In the metabolic map of Fig. 8 most of the affected
enzymes are seen to cluster as closely linked to one another.
Four enzymes sequential in the Krebs cycle – MDHM,
CISY, ACON and IDHP – are involved. Complex II directly
acts on Krebs cycle intermediates by converting succinate to
fumarate and complex III accepts reducing equivalents from
FADH2 through ETF and UQ. FADH2 is mainly produced
by fatty acid catabolism, and ACADV, another of the upregulated enzymes in MELAS, catalyzes one of the ratelimiting steps of this process. The practical relevance
of the up-regulation of the Krebs cycle may be highlighted
by the report of a case of successful treatment with
succinate of an uncontrolled convulsive MELAS patient
[65].
Increasing evidence supports the notion that G3P is a
housekeeping gene with multiple functions linked to
various intracellular localizations [66]. The role of G3P in
mitochondria and its up-regulation in MELAS are worth
notice on the basis of G3Ps novel connection with cellular
survival [67] and deserve further investigation. Similarly, the
up-regulation in MELAS of AL4A1 might be the result of a
stress response [68]. AL4A1 catalyzes a necessary step
in the proline-NO homeostasis. Proline oxidase, a
mitochondrial enzyme that oxidizes proline to form
pyrroline-5-carboxylate, the substrate of AL4A1, is inhibited
by lactate [69], and lactic acidosis is one of the most typical
features of MELAS. Reduction in mitochondrial production
of pyrroline-5-carboxylate secondary to lactate inhibition was
hypothesized as the most likely cause of hypocitrullinemia,
recorded in MELAS patients, and consequent altered NO
homeostasis [70]. Hypocitrullinemia may be exacerbated by
the up-regulation of AL4A1, further unbalancing these
metabolic pathways.
This work was supported by grants from AFM (Grant
11643, Call 2005), MIUR (FIRB, Grant RBNE03B8KK, Call
2003) and from Università degli Studi di Milano (FIRST 2006)
to Dr. Elisabetta Gianazza; from AFM (Grant 11032, Call
2005) to Lodovica Vergani. C.B. was supported by a postdoctoral research fellowship (Giovani Ricercatori) financed by
FIRB (Grant RBNE03B8KK, Call 2003).
The authors have declared no conflict of interest.
6 References
[1] Bernatsky, S., Ramsey-Goldman, R., Clarke, A., Curr.
Opin. Rheumatol. 2006, 18, 129–134.
[2] Fernandez Madrid, F., Cancer lett. 2005, 230, 187–198.
[3] Saif, M. W., Zalonis, A., Syrigos, K., Expert Opin. Biol.
Ther. 2007, 7, 493–507.
[4] Grabar, P., Williams, C. A., Biochim. Biophys. Acta 1953,
10, 193–194.
[5] Clarke, H. G., Freeman, T., Clin. Sci. 1968, 35, 403–413.
[6] Needham, G. R., Jaworski, D. C., Simmen, F. A.,
Sherif, N., Muller, M. T., Exp. Appl. Acarol. 1989, 7,
21–32.
[7] Petersen, C., Gut, J., Leech, J. H., Nelson, R. G., Infect.
Immun. 1992, 60, 2343–2348.
[8] Sambri, V., Armati, S., Cevenini, R., FEMS Immunol.
Med. Microbiol. 1993, 7, 67–71.
[9] Fallon, P. G., Doenhoff, M. J., Parasite Immunol. 1995,
17, 261–268.
[10] Dumke, R., Catrein, I., Pirkil, E., Herrmann, R.,
Jacobs, E., Int. J. Med. Microbiol. 2003, 292, 513–525.
[11] Birkett, C. R., Parma, A. E., Gerke-Bonet, R., Woodward,
R., Gull, K., Gene 1992, 110, 65–70.
[12] Sironi, L., Guerrini, U., Tremoli, E., Miller, I. , Gelosa, P.,
Lascialfari, A., Zucca, I. et al., J. Neurosci. Res. 2004, 78,
115–122.
5 Concluding remarks
[13] Bogdanos, D. P., Baum, H., Vergani, D., Clin. Liver Dis.
2003, 7, 759–777, vi.
In conclusion in the present report we described that
polyspecific anti-mitochondrion antibodies may be used to
detect informative features on the main components of
mitochondrial subproteome from small amount of human
muscle of patients, processed through 1-D and 2-D
electrophoresis. The same may be expected to apply also
to cell cultures. For the latter, it may then be possible to test
in parallel the effects of a number of treatments either
aiming at a more detailed definition of the underlying
biochemical defects or mimicking a possible therapeutic
intervention while using a limited amount of material and
avoiding lengthy fractionation procedures. In addition to the
qualitative and quantitative information on individual
proteins, such as post-translational modifications and/or
mass reduction, we deem that this new tool could help shed
further light on the supramolecular organization of
mitochondrial enzymes and on their association with nonmitochondrial proteins.
[14] Goto, Y., Nonaka, I., Horai, S., Nature 1990, 348,
651–653.
& 2009 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim
[15] McFarland, R., Taylor, R. W., Turnbull, D. M., Curr. Top.
Dev. Biol. 2007, 77, 113–155.
[16] Vergani, L., Malena, A., Sabatelli, P., Loro, E., Cavallini, L.,
Magalhaes, P., Valente, L. et al., Brain 2007, 130,
2715–2724.
[17] Zerbetto, E., Vergani, L., Dabbeni-Sala, F., Electrophoresis 1997, 18, 2059–2064.
[18] Hurn, B. A. L., Chantler, S. M., Methods Enzymol. 1980,
70, 104–141.
[19] Lowry, O. H., Rosebrough, N. J., Farr, A. L., Randall,
R. J., J. Biol. Chem. 1951, 193, 265–275.
[20] Laemmli, U. K., Nature 1970, 227, 680–685.
[21] Towbin, H., Staehelin, T., Gordon, J., Proc. Natl. Acad.
Sci. USA 1979, 76, 4350–4354.
[22] Schägger, H., von Jagow, G., Anal. Biochem. 1991, 199,
223–231.
www.electrophoresis-journal.com
Electrophoresis 2009, 30, 1329–1341
[23] Schägger, H., Cramer, W. A., von Jagow, G., Anal.
Biochem. 1994, 217, 220–230.
[24] Bradford, M. M., Anal. Biochem. 1976, 72, 248–254.
[25] Gianazza, E., Giacon, P., Sahlin, B., Righetti, P. G.,
Electrophoresis 1985, 6, 53–56.
[26] Gianazza, E., Guerini Rocco, A., Marchetto, A., Vergani,
L., Electrophoresis 2007, 28, 2953–2956.
[27] Fratelli, M., Demol, H., Puype, M., Casagrande, S.,
Eberini, I., Salmona, M., Bonetto, V. et al., Proc. Natl.
Acad. Sci. USA. 2002, 99, 3505–3510.
[28] Gianazza, E., Vergani, L., Wait, R., Brizio, C., Brambilla, D.,
Begum, S., Giancaspero, T. A. et al., Electrophoresis
2006, 27, 1182–1198.
[29] Görg, A., Postel, W., Weser, J., Günther, S., Strahler,
S. R., Hanash, S. M., Somerlot, L., Electrophoresis 1987,
8, 122–124.
[30] Jeno, P., Mini, T., Moes, S., Hintermann, E., Horst, M.,
Anal. Biochem. 1995, 224, 75–82.
[31] Wilm, M., Shevchenko, A., Houthaeve, T., Breit, S.,
Schweigerer, L., Fotsis, T., Mann, M., Nature 1996, 379,
466–469.
[32] Shevchenko, A., Wilm, M., Vorm, O., Mann, M., Anal.
Chem. 1996, 68, 850–858.
[33] Wait, R., Gianazza, E., Eberini, I., Sironi, L., Dunn, M. J.,
Gemeiner, M., Miller, I., Electrophoresis 2001, 22,
3043–3052.
[34] Kogelnik, A. M., Lott, M. T., Brown, M. D.,
Navathe, S. B., Wallace, D. C., Nucleic Acids Res. 1996,
24, 177–179.
[35] Schilling, B., Murray, J., Yoo, C. B., Row, R. H., Cusack,
M. P., Capaldi, R. A., Gibson, B. W., Biochim. Biophys.
Acta 2006, 1762, 213–222.
[36] Maglott, D., Ostell, J., Pruitt, K. D., Tatusova, T., Nucleic
Acids Res. 2007, 35, D26–D31.
[37] Peri, S., Navarro, J. D., Amanchy, R., Kristiansen, T. Z.,
Jonnalagadda, C. K., Surendranath, V., Niranjan, V.
et al., Genome Res. 2003, 13, 2363–2371.
[38] Cotter, D., Guda, P., Fahy, E., Subramaniam, S., Nucleic
Acids Res. 2004, 32, D463–D467.
[39] Bairoch, A., Apweiler, R., Nucleic Acids Res. 1996, 24,
21–25.
[40] Hartmann, C. M., Gehring, H., Christen, P., Eur.
J. Biochem. 1993, 218, 905–910.
[41] Sumegi, B., Srere, P. A., J. Biol. Chem. 1984, 259,
15040–15045.
[42] Aggeler, R., Coons, J., Taylor, S. W., Ghosh, S. S.,
Garcia, J. J., Capaldi, R. A., Marusich, M. F. J. Biol.
Chem. 2002, 277, 33906–33912.
[43] Murray, J., Zhang, B., Taylor, S. W., Oglesbee, D., Fahy, E.,
Marusich, M. F., Ghosh, S. S. et al., J. Biol. Chem. 2003,
278, 13619–13622.
Proteomics and 2-DE
1341
[46] Schagger, H., Pfeiffer, K., EMBO J. 2000, 19, 1777–1783.
[47] Boekema, E. J., Braun, H. P., J. Biol. Chem. 2007, 282, 1–4.
[48] Lenaz, G., Genova, M. L., Am. J. Physiol. Cell Physiol.
2007, 292, C1221–C1239.
[49] Ko, Y. H., Delannoy, M., Hullihen, J., Chiu, W., Pedersen,
P. L., J. Biol. Chem. 2003, 278, 12305–12309.
[50] Chen, C., Ko, Y., Delannoy, M., Ludtke, S. J., Chiu, W.,
Pedersen, P. L., J. Biol. Chem. 2004, 279, 31761–31768.
[51] Vyssokikh, M. Y., Brdiczka, D., Acta Biochim. Pol. 2003,
50, 389–404.
[52] Nijtmans, L. G., de Jong, L., Artal Sanz, M., Coates, P. J.,
Berden, J. A., Back, J. W., Muijsers, A. O. et al. EMBO J.
2000, 19, 2444–2451.
[53] Bourges, I., Ramus, C., Mousson de Camaret, B.,
Beugnot, R., Remacle, C., Cardol, P., Hofhaus, G. et al.,
Biochem. J. 2004, 383, 491–499.
[54] Nijtmans, L. G., Artal, S. M., Grivell, L. A., Coates, P. J.,
Cell. Mol. Life Sci. 2002, 59, 143–155.
[55] Eaton, S., Middleton, B., Sherratt, H. S., Pourfarzam, M.,
Quant, P. A., Bartlett, K., Adv. Exp. Med. Biol. 1999, 466,
145–154.
[56] Parker, A., Engel, P. C., Biochem. J. 2000, 345, 429–435.
[57] Porpaczy, Z., Sumegi, B., Alkonyi, I., Biochim. Biophys.
Acta 1983, 749, 172–179.
[58] Robinson, J. B., Jr., Srere, P. A., J. Biol. Chem. 1985,
260, 10800–10805.
[59] Taylor, S. W., Fahy, E., Zhang, B., Glenn, G. M.,
Warnock, D. E., Wiley, S., Murphy, A. N. et al., Nat.
Biotechnol. 2003, 21, 281–286.
[60] Reifschneider, N. H., Goto, S., Nakamoto, H., Takahashi, R.,
Sugawa, M., Dencher, N. A., Krause, F., J. Proteome Res.
2006, 5, 1117–1132.
[61] Heddi, A., Stepien, G., Benke, P. J., Wallace, D. C.,
J. Biol. Chem. 1999, 274, 22968–22976.
[62] Lenaz, G., Baracca, A., Carelli, V., D’Aurelio, M., Sgarbi, G.,
Solaini, G., Biochim. Biophys. Acta 2004, 1658, 89–94.
[63] James, A. M., Wei, Y. H., Pang, C. Y., Murphy, M. P.,
Biochem. J. 1996, 318, 401–407.
[64] Pallotti, F., Baracca, A., Hernandez-Rosa, E., Walker,
W. F., Solaini, G., Lenaz, G., Melzi D’Er.il, G. V. et al.,
Biochem. J. 2004, 384, 287–293.
[65] Oguro, H., Iijima, K., Takahashi, K., Nagai, A., Bokura, H.,
Yamaguchi, S., Kobayashi, S., Intern. Med. 2004, 43,
427–431.
[66] Sirover, M. A., J. Cell. Biochem. 2005, 95, 45–52.
[67] Colell, A., Ricci, J. E., Tait, S., Milasta, S. , Maurer, U.,
Bouchier-Hayes, L., Fitzgerald, P. et al., Cell 2007, 129,
983–997.
[68] Yoon, K. A., Nakamura, Y., Arakawa, H., J. Hum. Genet.
2004, 49, 134–140.
[44] Schägger, H., de Coo, R., Bauer, M. F., Hofmann, S.,
Godinot, C., Brandt, U., J. Biol. Chem. 2004, 279,
36349–36353.
[69] Dillon, E. L., Knabe, D. A., Wu, G., Am. J. Physiol. 1999,
276, G1079–G1086.
[45] John, G. B., Shang, Y., Li, L., Renken, C., Mannella, C. A.,
Selker, J. M., Rangell, L. et al., Mol. Biol. Cell 2005, 16,
1543–1554.
[70] Naini, A., Kaufmann, P., Shanske, S., Engelstad, K., De
Vivo, D. C., Schon, E. A., J. Neurol. Sci. 2005, 229– 230,
187–193.
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