From the Pennington Biomedical Research Center, Baton Rouge, Louisiana
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ABSTRACT |
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At the molecular and structural level, mitochondrial biogenesis and mitochondrial function are altered in diabetes, as well as in insulin-resistant relatives of type 2 diabetic subjects (1,2). At the ultra-structural level, a reduction in the number, location, and morphology of mitochondria is strongly associated with insulin resistance (1). Two recent microarray studies have shown that genes involved in oxidative phosphorylation (OXPHOS) exhibit reduced expression levels in the skeletal muscle of type 2 diabetic subjects and prediabetic subjects. These changes may be mediated by the peroxisome proliferatoractivated receptor coactivator-1 (PGC1) pathway. PGC1
- and PGC1ß-responsive OXPHOS genes show reduced expression in the muscle of patients with type 2 diabetes (3,4). In addition to the cellular energy sensor AMP kinase, the peroxisome proliferatoractivated receptor cofactors PGC1
(5,6,7) and possibly PGC1ß (8) activate mitochondrial biogenesis and increase OXPHOS gene expression by increasing the transcription, translation, and activation of the transcription factors necessary for mitochondrial DNA (mtDNA) replication. Similarly, PGC1
increases the transcription of enzymes necessary for substrate oxidation, electron transport, and ATP synthesis. Morphological and functional studies (1,9,10), combined with the recent microarray data, indicate that PGC1 is important in the development of type 2 diabetes.
Rates of ATP synthesis, measured in situ with magnetic resonance spectroscopy, are decreased in subjects with a family history of diabetes before the onset of impaired glucose tolerance (2,10). Based on these results, the prevailing view is that these defects have a genetic origin (2). One common feature of diverse insulin-resistant states is an elevation in nonesterified fatty acids (11). This gave rise to the concept of "lipotoxicity" and "ectopic fat" (12) and shifted attention toward the adipose tissue and increased free fatty acid concentrations as a potential foundation for insulin resistance (11).
Excess dietary fat has also been implicated in the development of obesity and diabetes (13). At energy balance, high-fat diets (HFDs) increase the flux of fatty acids through skeletal muscle for oxidation. The purpose of these experiments was to identify the transcriptional responses of skeletal muscle to an isoenergetic HFD in healthy young men using oligonucleotide microarrays. We found a HFD downregulated PGC1 and PGC1ß mRNA, as well as genes encoding proteins in complexes I, II, III, and IV of the electron transport chain. These changes were recapitulated and amplified in a murine model after a 3-week HFD, along with decreases in PGC1
and cytochrome C protein. These studies implicate increased dietary fat in the defects in OXPHOS genes observed in diabetes and the prediabetic/insulin-resistant state.
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RESEARCH DESIGN AND METHODS |
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Euglycemic-hyperinsulinemic clamp.
Insulin sensitivity was measured only at baseline (day 3) by euglycemic-hyperinsulinemic clamp (19) before HFD. After an overnight fast, glucose and insulin (80 mIU/m2 BSA) were administered. The glucose disposal rate (M value) was adjusted for kilograms of lean body mass.
Maximal aerobic capacity.
Maximal oxygen uptake was determined by a progressive treadmill test to exhaustion (20). The volume of O2 and CO2 was measured continuously using a metabolic cart (V-Max29 Series; SensorMedics, Yorba Linda, CA).
Body composition.
Body fat mass and lean body mass were measured on a Hologic Dual Energy X-ray Absorptiometer (QDR 4500; Hologic, Waltham, MA).
Indirect calorimetry.
Respiratory quotient and 24-h energy expenditure were determined in the whole-room calorimeter before and during 3 days of isocaloric HFD and confirmed an increase in fat oxidation (data not shown). Energy expenditure was set at 1.4 times the resting metabolic rate measured by metabolic cart and clamped across the 4-day chamber stay.
Animal study.
Male C57BL/6J mice were housed at room temperature with a 12-h-light/12-h-dark cycle for 5 weeks. Six mice consumed control diet ad libitum (D12450B [Research Diets, New Brunswick, NJ]: 10% of energy from fat, 20% of energy from protein, and 70% of energy from carbohydrate), and seven mice consumed HFD (D12451 [Research Diets]: 45% of energy from fat, 20% of energy from protein, and 35% of energy from carbohydrate). All animals ate the control diet ad libitum for 2 weeks, and seven were switched to HFD for 3 additional weeks. Gastrocnemius muscles were dissected and snap-frozen in liquid nitrogen.
RNA and DNA extraction.
Human and mouse total RNA from 50100 mg of vastus lateralis and gastrocnemius muscle, respectively, was isolated with Trizol reagent (Invitrogen, Carlsbad, CA). Gastrocnemius was digested overnight in proteinase K (FisherBiotech, Houston, TX) at 55°C. DNA was extracted with phenol-chloroform. The quantity and integrity of the RNA and DNA were confirmed by Agilent 2100 Bioanalyzer (Agilent Technologies, Palo Alto, CA).
Oligonucleotide microarrays.
RNA sample pairs (2 µg) from human subjects were labeled by reverse transcriptase with dCTP-Cy3 and dCTP-Cy5, respectively, and in inverse order (dye swap) using MICROMAX TSA Labeling and Detection kit (Perkin-Elmer, Wellesley, MA). Equal amounts of labeled cDNA probes were hybridized in duplicate to oligonucleotide slides containing 18,861 spots corresponding to 17,260 unique genes (Compugen, San Jose, CA) in hybridization chambers (GenomicSolutions, Ann Arbor, MI) for up to 72 h at 42°C. Detection and washing were performed at room temperature according to manufacturers protocol (Perkin-Elmer). Oligonucleotide chips were spotted on to poly-L-lysine slides using a GeneMachine OmniGrid microarrayer (GenomicSolutions) equipped with a Stealth SPH32 printhead and Stealth SMP4 Micro Spotting Pins (Telechem International, Sunnyvale, CA). Oligonucleotides were stored in 384-well plates in 45% DMSO. Microarray slides were scanned using a GSI Lumonics ScanArray 5,000 scanner (Perkin-Elmer) at high intensities (95% for Cy3,
75% for Cy5) and low intensities (
55% for Cy3,
35% for Cy5) applying ScanArray Express software and quantified using QuantArray (GenomicSolutions). All subsequent microarray analyses were performed using SAS version 8.2 (SAS, Cary, NC). A robust local regression procedure (LOWESS) was performed to remove the systematic variations in the measured gene expression levels so that differences in expression across the samples could be distinguished accurately and precisely (21). After normalization, gene shaving (22), bootstrapping (23), and cluster analysis were performed (24), and the slide effect, dye effect, variety effect, and duplicate design were taken into account in an ANOVA model (25). Resampling-based multiple pairwise comparison was used to identify the differentially expressed genes before versus after the HFD. Differentially expressed genes were identified based on a Bonferroni adjusted P < 0.01.
Real-time quantitative RT-PCR for RNA.
RNA sample pairs (1 µg) were reverse transcribed using iScript cDNA synthesis kit (BioRad, Hercules, CA). All primers and probes were designed using Primer Express version 2.1 (Applied Biosystems-Roche, Branchburg, NJ). Sequences of primers and probes are shown in Supplemental Table 1 (online appendix [available at http://diabetes.diabetesjournals.org]).
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Real-time PCR for mtDNA and genomic DNA copy number.
Taqman primers and probes were designed using Primer Express version 2.1 (Applied Biosystems-Roche). Real-time PCR was carried out in ABI PRISM 7900 sequence detector (Applied Biosystems) using the following parameters: one cycle of 50°C for 2 min, then 95°C for 10 min, followed by 40 cycles at 95°C for 15 s and 60°C for 1 min. Murine skeletal muscle genomic DNA copy number was measured at the UCP2 gene using a primer-probe set that amplifies genomic DNA. mtDNA copy number was measured from the cytochrome C oxidase II mtDNA gene. mtDNA copy number was calculated by taking the absolute value of Ct values between groups (control vs. HFD). Because amplification occurs exponentially (increasing twofold with each cycle of PCR), log base 2 of
Ct as the copy number for each sample (28).
Western immunoblotting.
Tissues were homogenized in buffer (50 mmol/l HEPES, pH 7.4, 2 mmol/l EDTA, 150 mmol/l NaCl, 30 mmol/l NaPPO4, 10 mmol/l NaF, 1% Triton X-100, 10 µl/ml protease inhibitor, 10 µl/ml phosphatase I inhibitor, 10 µl/ml phosphatase II inhibitor, and 1.5 mg/ml benzamidine HCl). The whole homogenates were centrifuged for 25 min at 15,000g, and supernatants were stored at 80°C before Western immunoblotting. Homogenates were run on a 10% PAGE, transferred to polyvinylidine fluoride membranes, incubated with the primary antibodies PGC1 (P3363; US Biological, Swampscott, MA) and cytochrome C (556433; BD Biosciences, San Jose, CA) and signal detected using the ECL detection system (Pierce, Rockford, IL). Glyceraldehyde-3-phosphate dehydrogenase (46999-555; Biogenesis, Kingston, NH) was used as an internal control, and brown adipose tissue was used as a positive control.
Skeletal muscle enzyme activities.
Skeletal muscle samples were diluted 20-fold and homogenized in extraction buffer (0.1 mol/l KH2PO4/Na2PHO4 and 2 mmol/l EDTA, pH 7.2). Citrate synthase, cytochrome C oxidase, and ß-hydroxyacyl-CoA dehydrogenase (BHAD) activities were determined spectrophotometrically as previously described (19). DNA was extracted from the same homogenate (total nucleic acid extraction; Epicenter, Madison, WI), and mtDNA was measured to adjust for differences in the content of mitochondria (29).
Statistical analysis.
Statistical analysis was performed using two-tailed paired Students t test for before versus after HFD (human) and unpaired Students t test for control versus HFD (mouse) to establish effects of the intervention. All values are presented in figures and tables as sample (raw) means ± SE. Population characteristics are represented as means ± SD. Type I error rate was set a priori at P < 0.05. Analysis was performed using GraphPad Prism version 4.0 (GraphPad Software, San Diego, CA).
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RESULTS |
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Expression of OXPHOS genes of complexes III and IV in human skeletal muscle.
As a subsequent step in elucidating effects of the diet intervention on expression of genes involved in mitochondrial function, we examined mRNA for genes in complexes III and IV using quantitative RT-PCR (Fig. 1A). Cytochrome C (complex III) and Surfeit one (complex IV) expression levels were reduced (1.13 ± 0.07 to 0.85 ± 0.05 AU, P < 0.01, and 1.10 ± 0.05 to 0.90 ± 0.05 AU, P < 0.01).
Reduced expression of transcription factors and transcriptional cofactors in human skeletal muscle after a short-term HFD.
Because expression levels of genes involved in the function of mitochondria decreased, we examined expression of genes known to be involved in mitochondrial biogenesis. We observed a 20% and a 25% reduction in mRNA levels in PGC1 and PGC1ß, respectively (Fig. 2A); PGC1
(1.44 ± 0.08 to 1.13 ± 0.06 AU, P < 0.01) and PGC1ß (2.12 ± 0.16 to 1.59 ± 0.18 AU, P < 0.05). Mitochondrial transcription factor A, TFAM, a key activator of mitochondrial transcription and its genome replication, was not significantly changed (2.00 ± 0.19 to 1.79 ± 0.19 AU, P = 0.3784), nor was nuclear respiratory factor 1, NRF1 (1.89 ± 0.13 to 1.56 ± 0.16 AU, P = 0.1398) (Fig. 2A).
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Reduced expression of genes involved in mitochondrial biogenesis in murine skeletal muscle after a 3-week HFD.
In parallel to the human experiment, we measured both PGC1 and PGC1ß mRNA in these same mice. A 90% reduction in mRNA levels was observed for both PGC1
and PGC1ß (Fig. 2B): PGC1
(34.63 ± 12.57 to 2.67 ± 0.31 AU, P < 0.01) and PGC1ß (25.75 ± 9.03 to 1.85 ± 0.30 AU, P < 0.01).
Measurement of mtDNA copy number in murine skeletal muscle after a 3-week HFD.
It has been shown that the half-life of a mitochondrion in mammalian cells can range from 3 to 10 days, depending on the measurement technique (30). Given that the expression of both PGC1 and PGC1ß were decreased, we hypothesized that skeletal muscle mtDNA copy number might be decreased by the HFD; however, we found no differences between animals fed a HFD when compared with controls (Fig. 2B): mtDNA in control animals, 1,166 ± 112.50, and in high-fat animals, 1,127 ± 70.28 AU, P = 0.76.
Protein content of PGC1 and cytochrome C and mitochondrial enzyme activity in murine skeletal muscle after a 3-week HFD.
PGC1 and cytochrome C protein expression levels were reduced by
40% in mice consuming a HFD (Fig. 2B): PGC1
(1.31 ± 0.19 to 0.84 ± 0.07 AU, P < 0.05) and cytochrome C (1.35 ± 0.17 to 0.76 ± 0.09 AU, P < 0.01).
Whole-tissue homogenates were analyzed for citrate synthase, cytochrome C oxidase, and BHAD activity in whole-tissue homogenates and normalized for mitochondrial content using quantitative PCR of mtDNA as described by Ritov et al. (29). Citrate synthase activity and mtDNA from the same homogenate were correlated (R2 = 0.51, P < 0.01). Animals fed a HFD had slightly, but not significantly, lower mitochondrial enzyme activity: citrate synthase, 0.18 ± 0.02 to 0.16 ± 0.01 AU, P = 0.26; cytochrome C oxidase, 0.41 ± 0.11 to 0.38 ± 0.10 AU, P = 0.86; and BHAD, 0.07 ± 0.01 to 0.06 ± 0.004 AU, P = 0.22.
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DISCUSSION |
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Through the combined use of microarray technology, advanced bioinformatics, and confirmation of microarray results with quantitative RT-PCR, we were able to identify subtle (2030%) changes in OXPHOS gene expression without a priori grouping of genes based on known function (3). The advantage of this approach is that genes that do not exhibit large changes in transcription but are clearly important in carbohydrate and energy metabolism (e.g., PGC1) may be identified. HFD elicits a coordinated downregulation of genes involved in OXPHOS within the electron transport chain.
Our results support the hypothesis that HFDs and/or high-fat flux through the mitochondria reduce the expression of nuclear genes encoding mitochondrial proteins and transcription factors involved in mitochondrial biogenesis. Both PGC1 and PGC1ß were decreased by
20% and accompanied by a 20% reduction in OXPHOS gene expression. Previous studies suggest a link between the downregulation of PGC1 and dysregulation of OXPHOS genes. Our results are consistent with this sequence of events, and three of our OXPHOS genes found by microarray analysis were also present in the analyses of Mootha et al. (3) and Patti et al. (4). Therefore, our findings expand the view beyond the relationship between PGC1 and OXPHOS genes. We move upstream to show that increased fatty acid flux through the mitochondria decreases PGC1 expression and associates with a downregulation of expression of OXPHOS genes. It remains unclear from this experimental data whether it is increased fatty acid mitochondrial oxidation per se or some other pathway triggered by fatty acids that is responsible for the effects on gene expression.
Puigserver and Spiegelman (5) demonstrated that PGC1 is a master regulator of mitochondrial biogenesis and OXPHOS gene expression (33). PGC1
co-activation of NRF1-mediated transcription leads to transcription and subsequent translocation of TFAM to the mitochondrion, thus increasing mtDNA transcription (34,35). In these studies, both coactivators PGC1
and PGC1ß were downregulated; however, we saw no significant change in two downstream targets, NRF1 and TFAM (Fig. 2A), suggesting alternate and compensatory regulation.
Although an increase in free fatty acid concentrations was not seen in this cohort, fatty acid flux through the muscle is by necessity increased in these subjects as demonstrated by a decrease in 24-h respiratory quotient (data not shown) to match fat intake in this experimental paradigm (14). Another explanation for the reduction in the expression of these genes is that HFD decreases insulin-stimulated gene expression. Fatty acids decrease insulin signaling both in vivo and in vitro. Recent microarray studies demonstrate an upregulation of OXPHOS genes after a short-term insulin infusion (36). A reduction in insulin signaling might reduce expression of these same genes. Our studies do not identify the exact mechanism of the reduction in PGC1, PGC1ß, or their downstream targets. Rather, these studies point toward dietary fat, or increased lipolysis, as a potential source of the previously reported reduction in mitochondrial OXPHOS and subsequent mitochondrial dysfunction.
Importantly, mice fed a HFD for 3 weeks showed a similar pattern of changes in gene expression as in the shorter human experiments. The magnitude of the changes in gene expression was much larger in mice than in man. In light of the fact that 3 days of HFD is not long enough to cause changes in mtDNA copy number as mitochondrial turnover is relatively slow (30), we next tested the hypothesis that the changes in the transcriptional cofactors (e.g., PGC1 and PGC1ß) would decrease mitochondrial number in mice fed a HFD for 3 weeks. We found large changes in PGC1
and PGC1ß mRNA, as well as decreases in both cytochrome C and PGC1
protein levels, whereas mtDNA content remained unchanged after 3 weeks of HFD in mice.
In some ways, our inability to find changes in mtDNA copy number are inconsistent with recent studies demonstrating a reduction in mitochondrial number in diabetes and insulin resistance (1,28) but similar to studies showing a decrease in OXPHOS gene expression (3,4). One possibility is that "chronic" versus "acute" effects of high-fat flux through mitochondria are different. In the prediabetic and diabetic states, increased lipid flux has been maintained for a longer period of time. Therefore, additional studies of mitochondrial number and function via electron microscopy will be needed to fully rule out subtle changes in mitochondrial number or function with chronic HFD.
Our studies reveal a key question: "why would increased fatty acid flux decrease the expression of genes needed to oxidize these same fatty acids?". Fasting is another "normal" physiological condition where fatty acid flux through skeletal muscle is increased. Surprisingly, fasting produces changes in gene expression that are strikingly similar to the pattern of fat-induced changes observed in our studies of HFDs. For example, Jagoe et al. (37) found that CASQ2 (calsequestrin 2), NDUFS1, glycogen synthase, and pyruvate dehydrogenase kinase isoenzyme 4, four genes found on our microarray "hit" list (Supplemental Table 2) and confirmed by quantitative RT-PCR (data not shown), were similarly regulated by fasting in rodents. This may explain the paradoxical decrease in systems needed to oxidize fatty acids (nuclear genes encoding mitochondrial proteins, PGC1) when fat flux is increased during a HFD. In other words, the parallel results between fasting and HFDs suggest that fat flux through the skeletal muscle might be interpreted as a signal of fasting/starvation by the muscle cell itself. Signaling systems normally reserved for responding to energy deprivation (fasting) may be co-opted when dietary fat is increased. This hypothesis is also consistent with observed changes in the transcription of genes involved in nonoxidative metabolism (e.g., glycolysis) found on our microarray "hit" list (Supplemental Table 2).
In conclusion, HFDs in both insulin-sensitive humans and mice were associated with reduction in the expression of genes involved in oxidative capacity (e.g., genes of the electron transport chain), nuclear genes encoding mitochondrial proteins (e.g., mitochondrial carrier proteins), and those involved in mitochondrial biogenesis (e.g., PGC1 and PGC1ß). These studies support the novel hypothesis that HFDs or high-fat flux explain the reduction in OXPHOS genes seen in aging, the prediabetic state, and in overt diabetes.
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ACKNOWLEDGMENTS |
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FOOTNOTES |
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Address correspondence and reprint requests to Steven R. Smith, Pennington Biomedical Research Center, 6400 Perkins Road, Baton Rouge, LA 70808. E-mail: smithsr{at}pbrc.edu
Received for publication December 10, 2004 and accepted in revised form April 4, 2005
BHAD, ß-hydroxyacyl-CoA dehydrogenase; HFD, high-fat diet; mtDNA, mitochondrial DNA; OXPHOS, oxidative phosphorylation; PGC1, peroxisome proliferatoractivated receptor coactivator-1
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REFERENCES |
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