|A PGC1-α-dependent myokine that drives brown-fat-like development of white fat and thermogenesis.|
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|PMID: 22237023 Owner: NLM Status: MEDLINE|
|Exercise benefits a variety of organ systems in mammals, and some of the best-recognized effects of exercise on muscle are mediated by the transcriptional co-activator PPAR-γ co-activator-1 α (PGC1-α). Here we show in mouse that PGC1-α expression in muscle stimulates an increase in expression of FNDC5, a membrane protein that is cleaved and secreted as a newly identified hormone, irisin. Irisin acts on white adipose cells in culture and in vivo to stimulate UCP1 expression and a broad program of brown-fat-like development. Irisin is induced with exercise in mice and humans, and mildly increased irisin levels in the blood cause an increase in energy expenditure in mice with no changes in movement or food intake. This results in improvements in obesity and glucose homeostasis. Irisin could be therapeutic for human metabolic disease and other disorders that are improved with exercise.|
|Pontus Boström; Jun Wu; Mark P Jedrychowski; Anisha Korde; Li Ye; James C Lo; Kyle A Rasbach; Elisabeth Almer Boström; Jang Hyun Choi; Jonathan Z Long; Shingo Kajimura; Maria Cristina Zingaretti; Birgitte F Vind; Hua Tu; Saverio Cinti; Kurt Højlund; Steven P Gygi; Bruce M Spiegelman|
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|Type: Journal Article; Research Support, N.I.H., Extramural; Research Support, Non-U.S. Gov't Date: 2012-01-11|
|Title: Nature Volume: 481 ISSN: 1476-4687 ISO Abbreviation: Nature Publication Date: 2012 Jan|
|Created Date: 2012-01-27 Completed Date: 2012-03-02 Revised Date: 2014-06-06|
Medline Journal Info:
|Nlm Unique ID: 0410462 Medline TA: Nature Country: England|
|Languages: eng Pagination: 463-8 Citation Subset: IM|
|APA/MLA Format Download EndNote Download BibTex|
Adipose Tissue, Brown / cytology*, drug effects, metabolism
Adipose Tissue, White / cytology*, drug effects, metabolism
Cell Respiration / drug effects
Culture Media, Conditioned / pharmacology
Energy Metabolism / drug effects, genetics, physiology
Exercise / physiology
Gene Expression Regulation / drug effects, genetics
Hormones / metabolism, secretion
Insulin Resistance / physiology
Intracellular Signaling Peptides and Proteins / genetics, metabolism
Ion Channels / metabolism
Mice, Inbred BALB C
Mitochondrial Proteins / metabolism
Muscle Cells / metabolism
Obesity / blood, chemically induced, prevention & control
Physical Conditioning, Animal / physiology
Plasma / chemistry
Subcutaneous Fat / cytology, drug effects, metabolism
Thermogenesis* / drug effects, genetics
Trans-Activators / deficiency, genetics, metabolism*, secretion
|DK31405/DK/NIDDK NIH HHS; DK54477/DK/NIDDK NIH HHS; K99 DK087853/DK/NIDDK NIH HHS; P30 DK057521/DK/NIDDK NIH HHS; R01 DK054477/DK/NIDDK NIH HHS; R01 DK061562/DK/NIDDK NIH HHS; R37 DK031405/DK/NIDDK NIH HHS|
|0/Culture Media, Conditioned; 0/Hormones; 0/Intracellular Signaling Peptides and Proteins; 0/Ion Channels; 0/Mitochondrial Proteins; 0/Ppargc1a protein, mouse; 0/Trans-Activators; 0/Transcription Factors; 0/mitochondrial uncoupling protein|
Nat Rev Endocrinol. 2012 Apr;8(4):195
Nature. 2012 Aug 30;488(7413):E9-10; discussion E10-1 [PMID: 22932392 ]
Nat Rev Drug Discov. 2012 Mar;11(3):189 [PMID: 22338642 ]
Cell Metab. 2012 Mar 7;15(3):277-8 [PMID: 22405065 ]
Journal ID (nlm-journal-id): 0410462
Journal ID (pubmed-jr-id): 6011
Journal ID (nlm-ta): Nature
Journal ID (iso-abbrev): Nature
nihms-submitted publication date: Day: 7 Month: 6 Year: 2012
Electronic publication date: Day: 11 Month: 1 Year: 2012
pmc-release publication date: Day: 14 Month: 12 Year: 2012
Volume: 481 Issue: 7382
First Page: 463 Last Page: 468
PubMed Id: 22237023
|A PGC1α-dependent myokine that drives browning of white fat and thermogenesis|
|Mark P. Jedrychowski2|
|James C. Lo1|
|Kyle A. Rasbach1|
|Elisabeth Almer Boström3|
|Jang Hyun Choi1|
|Jonathan Z. Long1|
|Maria Cristina Zingaretti5|
|Birgitte F. Vind6|
|Steven P. Gygi2|
|Bruce M. Spiegelman1*|
1Dana-Farber Cancer Institute and Harvard Medical School, 3 Blackfan Circle, CLS Building, floor 11, Boston, MA, 02115, USA
2Department of Cell Biology, Harvard Medical School, Boston, MA, 02115, USA
3Renal Division, Brigham and Women’s Hospital, Harvard Medical School
4UCSF Diabetes Center and Department of Cell and Tissue Biology, University of California, San Francisco
5Department of Experimental and Clinical Medicine, Università Politecnica delle Marche, Electron Microscopy Unit-Azienda Ospedali Riuniti, Ancona 60020, Italy
6Diabetes Research Center, Department of Endocrinology, Odense University Hospital, Denmark
7LakePharma, Inc. 530 Harbor Blvd, Belmont CA 94002
|Correspondence: Corresponding author: email@example.com, Tel: 617-632-3567
PGC1α (PPARγ coactivator-1 α) is a transcriptional coactivator that mediates many biological programs related to energy metabolism. Originally described as a coactivator of PPARγ that modulated expression of uncoupling protein 1 (UCP1) and thermogenesis in brown fat1, it has also been shown to control mitochondrial biogenesis and oxidative metabolism in many cell types. PGC1α is induced in muscle by exercise and stimulates many of the best known beneficial effects of exercise in muscle: mitochondrial biogenesis, angiogenesis and fiber-type switching2. It also provides resistance to muscular dystrophy and denervation-linked muscular atrophy 3. The healthful benefits of elevated muscle expression of PGC1α may go beyond the muscle tissue itself. Transgenic mice with mildly elevated muscle PGC1α are resistance to age-related obesity and diabetes and have a prolonged life-span4. This strongly suggests that PGC1α might stimulate the secretion of factors from skeletal muscle that affects the function of other tissues. In this paper, we show that PGC1α stimulates the expression of several muscle gene-products that are potentially secreted, including Fndc5. The Fndc5 gene encodes a type I membrane protein that is processed proteolytically to form a new hormone secreted into blood, termed irisin. Irisin is induced in exercise and activates profound changes in the subcutaneous adipose tissue, stimulating browning and UCP1 expression. Importantly, this causes a significant increase in total body energy expenditure and resistance to obesity-linked insulin-resistance. Thus, irisin action recapitulates some of the most important benefits of exercise and muscle activity.
Mice with transgenically increased PGC1α in muscle are resistant to age-related obesity and diabetes4, suggesting that these animals have a fundamental alteration in systemic energy balance. We therefore analyzed the adipose tissue of the PGC1α transgenic mice for expression of genes related to a thermogenic gene program and genes characteristic of brown fat development. There were no significant alterations in the expression of brown fat-selective genes in the interscapular brown adipose tissue or in the visceral (epididymal) white adipose tissue (Fig. 1a). However, the subcutaneous fat layer (inguinal), a white adipose tissue which is particularly prone to “browning” (i.e. formation of multilocular, UCP1 positive adipocytes), had significantly increased levels of UCP1 and Cidea mRNAs (Fig. 1b). We also observed increased UCP1 protein levels and more UCP1-positive stained multilocular cells in the transgenic mice, compared to controls (Fig. 1c and d). There are recent reports that exercise causes a mild increase in the expression of a thermogenic gene program in the visceral adipose tissue, a depot that has minimal expression of these genes5. Since it is the subcutaneous white adipose depot that has the greatest tendency to turn on a thermogenic gene program and alter the systemic energy balance of mice6, we re-investigated this with regard to browning of the white adipose tissues in two types of exercise. Similar to what has been reported5, a 2-fold increase in UCP1 mRNA expression was observed in the visceral, epididymal fat with three weeks of wheel running (Supplementary Fig. S1). However, a much larger change (approximately 25 fold) was seen in the same mice in the subcutaeneous inguinal fat depot. Similarly, a small increase in UCP1 mRNA expression was seen in the epididymal fat with repeated bouts of swimming in warm (32°C) water (Supplementary Fig. S1); however a very large increase (65 fold) was observed in the inguinal white depot (Supplementary Fig. S1). Thus, muscle-specific expression of PGC1α drives browning of subcutaneous white adipose tissue, possibly recapitulating part of the exercise program.
The effect on browning of the adipose tissues from PGC1α-expressing muscle could be due to either direct muscle-fat signaling or to another, indirect mechanism. To investigate this, we treated cultured primary subcutaneous adipocytes with serum-free media conditioned by myocytes expressing PGC1α or cells expressing GFP. As shown in Fig 1e, the media from cells expressing ectopic PGC1α increased the mRNA levels of several brown fat-specific genes (Fig. 1e). This suggested that PGC1α causes the muscle cells to secrete molecule(s) that can induce a thermogenic gene program in the cells.
We used a combination of Affymetrix-based gene expression arrays and an algorithm that predicts protein secretion to search for proteins that could mediate the browning of adipose tissues under the control of muscle PGC1α (Methods). Proteins with mitochondrial targeting sequences were excluded, and all candidates were validated in gain-of-function systems for PGC1α in vivo (Methods). Five proteins were identified as PGC1α target genes in muscle and likely to be secreted: IL-15, Fndc5, VEGFβ, Lrg1 and TIMP4 (Fig. 2a). Conversely, expression of these genes was reduced in mice with muscle-specific deletion of PGC1α (Supplementary Fig. S2). Furthermore, they were also found to be increased at the mRNA level in muscle from exercised mice (Fig. 2b). The expression of this same set of genes was also examined in muscle biopsies from human subjects before and after a controlled period of endurance exercise7 (Fig. 2c). Fndc5, VEGFβ and TIMP4 mRNAs were all significantly induced in humans with exercise. IL-15 has previously been reported as being secreted from muscle under the influence of exercise8, while the regulation of Fndc5, VEGFβ, Lrg1 and TIMP4 by exercise has not been described. Fndc5 mRNA and brown fat markers in subcutaneous fat were not regulated by acute exercise, and Fndc5 mRNA was not induced by exposure to cold (4° C) for 6 hours (Supplementary Fig. S2).
Several of the proteins encoded by these genes were commercially available, so they were applied directly to primary subcutaneous white adipocytes during differentiation. Factors such as IL-15 or VEGFβ had minimal effects on the expression of UCP1 and other brown fat genes at concentrations of 200 nM or higher. However, Fndc5 promoted a 7-fold induction of UCP1 mRNA at a concentration of 20 nM (Fig. 2d). The transcriptional changes induced by Fndc5 were addressed on a global scale using gene expression arrays (Supplementary Fig. S3). Strikingly, UCP1 and 3 other known brown fat genes, Elovl3, Cox7a and Otop1, were among the 8 most up-regulated genes (Supplementary Fig. S4). Conversely, genes characteristic of white fat development were down-regulated, such as leptin (Supplementary Fig. S3). These data strongly suggest that the activation of browning and thermogenic genes by Fndc5 is a major part of the action of this polypeptide on these cells.
The effects of Fndc5 treatment were remarkably robust; UCP1 mRNA was increased 7–500 fold in more than 10 experiment using Fndc5 at a concentration of 20 nM (Fig. 3a and Supplementary Fig. S5). Moreover, we could demonstrate a clear dose-dependence, with an effective range between 20 and 200 ng/ml (1.5 to 15 nM) (Fig. 3b). In contrast, BMP-7, reported as a potent inducer of browning9, had a much smaller effect (maximal of 2-fold) on the same cells at 3.3 μM (Fig. 3a).
We also utilized immunohistochemistry to study cells treated with Fndc5 and observed a robust increase in UCP1-positive adipocytes with multilocular lipid droplets (Supplementary Fig. S4). Electron microscopic analysis of Fndc5-treated cells showed a higher density of mitochondria compared to control cells, consistent with a brown fat-like phenotype and elevated mitochondrial gene expression (Supplementary Fig S5). The sizes of mitochondria, however, were similar between groups (Supplementary Fig. S4). Lastly, measurements of oxygen consumption provided functional evidence of increased energy expenditure with Fndc5 exposure. Total oxygen consumption was greatly increased (100%) by 20 nM of Fndc5, and the majority of this respiration was uncoupled (Fig. 3c). Thus, Fndc5 potently induces thermogenesis and a brown fat-like gene program in cultured adipocytes. In striking contrast, Fndc5 showed little or no effects on the classical brown fat cells isolated from the interscapular depot (Supplementary Figure S4).
We sought to define the time-frame during the differentiation process when Fndc5 was effective. Fndc5 was applied to cells in 2 day windows from day 0–6, and this was compared to cells where the protein was added during the entire 6 day differentiation process. As shown in Supplementary Figure S5, treatment during days 3–4 and 5–6 was effective at inducing UCP1 mRNA, though not as effective as when the Fndc5 was present throughout the differentiation process. Furthermore, treatment during the initial two days had no effect on UCP1 levels, suggesting that Fndc5 act mainly during the differentiation process of cells committed to the adipocytes lineage. Cyclic AMP (cAMP) is an important signaling pathway in thermogenesis, promoting the brown-fat gene program downstream of β–adrenergic stimulation. We therefore asked whether Fndc5 effects were additive or redundant with cAMP signaling. As shown in Fig. 3d, Fndc5-exposed cells increase UCP1 expression in an additive manner when exposed to forskolin, an adenyl cyclase activator. Two-way ANOVA tests demonstated that there was a significant (p<0.01) interaction between Fndc5 and forskolin treatment, indicating synergistic effects.
A key question is how Fndc5 is able to stimulate a thermogenic gene program. One potentially important transcription factor induced by Fndc5, identified using gene expression arrays, was PPARα This nuclear receptor has been shown to drive UCP1 expression and several other genes involved in browning of adipose cells10. PPARα is increased 3-fold at the mRNA level by Fndc5 treatment (Fig. 3e). Importantly, the Fndc5-mediated increase in UCP1 was significantly reduced when cells were simultaneously subjected to the selective PPARα antagonist GW6471 (Fig. 3f). The functional interaction between the Fndc5 and GW6471 treatments on UCP1 expression was confirmed using two-way ANOVA (p<0.05). Conversely, the PPARα antagonist normalized the reduction seen in white adipose genes leptin and adiponectin after Fndc5-treatment. Together, these data suggest that Fndc5 acts to induce UCP1 gene expression, at least in part, via PPARα.
Fndc5 / Frcp2, also known as PeP, was previously shown to have a signal peptide, two fibronectin domains and one hydrophobic domain that is likely to be membrane-inserted11–12 (Fig. 4a). Previous studies did not investigate whether part of this protein might be secreted11–12. With this structure in mind, we considered the possibility that Fndc5 might be synthesized as a type I membrane protein, followed by proteolytic cleavage, and release of the N-terminal part of the protein into the extracellular space. Thus, any C- or N-terminal tags would be lost during processing of the mature protein or interfere with localization. Indeed, expression of a C-terminally FLAG-tagged Fndc5 (Fig. 4a), did not result in any FLAG-immunoreactivity in the medium from cells expressing this construct (Fig. 4b). However, when we immunobloted the same samples with an antibody that recognizes the endogenous Fndc5 protein, we could easily detect substantial amounts of Fndc5 in the media at approximately 32 kD: this is slightly larger than the cellular Fndc5 (Fig. 4b). These data strongly suggests that Fndc5 is C-terminally cleaved, secreted and possibly further modified.
Western blot of media fractions with antibodies against wild-type Fndc5 showed multiple bands, suggestive of glycosylation, a common feature of secreted proteins. Treatment of supernatants from Fndc5-expressing cells with Peptide N-Glycosidase F (PNGase F) resulted in a significant size decrease as detected by SDS-gel electrophoresis, from 32 kD to 20 kD (Fig. 4c).
Mass spectrometry (MS) was used to determine the sequence of the Fndc5-derived polypeptide found in the media (methods). To do this, we fused the N-terminus of Fndc5 (without the signal peptide) to the C-terminus of the FC-domain of IgG. After purification and enzymatic deglycosylation of the secreted material, MS analyses indicated that secreted Fndc5 was truncated at glutamic acid 112 (not including the signal sequence), as shown in Figure 4e. The secreted portion of Fndc5 has remarkable conservation between species, with 100% identity between mice and humans (Supplementary Fig. S6). Since this distinct, secreted polypeptide has not been previously described and signals from muscle to other tissues (see above and below), we named it irisin, after Iris, the Greek messenger goddess.
The ability of the anti-Fndc5 antibodies to react with irisin allowed us to investigate the contribution made by irisin to the browning activity secreted by muscle cells expressing PGC1α. Media conditioned by muscle cells that had forced expression of PGC1α were incubated with control or anti-fndc5 antibodies before they were applied to the fat cell cultures. As shown in Supplementary Figure S6, the Fndc5 antibody caused a striking reduction in the ability of the PGC1α conditioned media to induce UCP1 and Cidea mRNA in the primary inguinal cells. This suggests that irisin accounts for a significant fraction of this activity secreted by muscle cells with forced PGC1α expression. We cannot, however, exclude the possibility that other factors might also contribute to this response.
We next analyzed levels of irisin in plasma from wild-type mice, using intravenous adenoviral delivery of full length Fndc5 as a positive control. This method results in strong forced expression from liver, and potential secretion to plasma, where we detected irisin using western blot after albumin/IgG-depletion and deglycosylation. As seen in Figure 5a, Fndc5-expressing virus resulted in a clear increase in an immunoreactive band at 22 kDa. Importantly, this was the only band altered on these blots. Using western blots of purified Fndc5 protein as a quantitative standard, irisin is present in the plasma of control mice at a concentration of approximately 40 nM. We also analyzed plasma of PGC1α muscle-specific knockout mice as a negative control, and the irisin band at 22 kDa was decreased by 72% in these animals (Fig. 5b). Furthermore, an immunoreactive band of identical electrophoretic mobility was found in plasma from healthy human subjects (Fig. 5c). This band was greatly diminished when the anti-Fndc5 antibody was neutralized with an excess of antigen (Supplementary Fig. S7).
We examined blood levels of irisin after exercise in mice and human subjects. Mice had significantly elevated (65%) plasma concentrations of irisin after they were subjected to three weeks of free wheel running (Fig. 5d). Similar analyses in healthy adult humans subjected to supervised endurance exercise training for 10 weeks revealed a 2-fold increase in the circulating irisin levels compared to the non-exercised state (Fig. 5e). Thus, irisin is present in mouse and human plasma, and is increased with exercise. The increase in circulating protein in both species is roughly proportional to the increases observed at the mRNA level in muscle (Fig. 2c).
We used adenoviral vectors to express full-length Fndc5 (or a control GFP) and examined its biological and therapeutic effects. This method resulted in a 15-fold increase in liver Fndc5 mRNA, though the liver expresses very low endogenous levels of this mRNA. Plasma levels of irisin were increased 3–4 fold (Fig. 5a). The mice did not display any adverse reaction, and upon gross pathological examination, there was no apparent toxicity in any major organ system. There was also no increase in plasma AST levels, and inflammatory genes were not significantly altered in the liver when the two groups were compared (Supplementary Fig. S8). Ten days after injection, UCP1 mRNA was increased by 13-fold in the subcutaneous depot relative to the same depot in mice receiving the virus expressing GFP (Fig 6a,b); Cidea was also significantly up-regulated (Fig. 6a). There were no changes in expression of UCP1 in the interscapular BAT, but we did observe a minor elevation in PRDM16 and PGC1α mRNA (Supplementary Fig. S8). The changes in gene expression in the subcutaneous adipose tissues were accompanied by a clear increase in the number of UCP1 positive, multilocular adipocytes (Fig. 6c). We did not, however, detect any change in body weight in the GFP vs. Fndc5 groups of animals. We observed similar results in young B/6 mice (Supplementary Fig. 9). Thus, moderate increases in circulating irisin can induce browning of white adipose tissues in vivo, including increased expression of UCP1.
Since activation of the classical brown fat or browning of white fat has been shown to improve obesity and glucose homeostasis in vivo6,13, we delivered Fndc5-expressing adenovirus to mice rendered obese and insulin-resistance by feeding a high fat diet. We chose C57Bl/6 mice for these experiments because they are highly prone to diet-induced obesity and diabetes. The expression of irisin increased UCP1 gene expression to the same degree as in lean mice (Supplementary fig 9). There was also an elevation in expression of several mitochondrial genes (Supplementary Fig. S8). Notably, these changes occurred with only moderately increased irisin blood levels, 3-fold, compared to the GFP-expressing mice. This effect was accompanied with a large increase in oxygen consumption (Fig 6d), consistent with the gene expression data, and body weights of the irisin expressing mice were slightly reduced after 10 days compared to GFP-expressing controls (Fig. 6e). These effects of irisin on mitochondrial gene expression in the fat were not seen in skeletal muscle in vivo or in cultured myocytes (Supplementary Fig. S10). Irisin expression in the high-fat fed mice caused a significant improvement in glucose tolerance when compared to the control mice expressing GFP. In addition, fasting insulin was also reduced (Fig. 6f–g). These data illustrate that even moderately increased levels of circulating irisin potently increases energy expenditure, reduces body weight and improves diet-induced insulin resistance.
Finally, we asked whether irisin is required for the exercise-induced effects on the subcutaneous white fat. Injection of anti-Fndc5 antibodies into mice prior to 10 days of swim training dramatically reduced the effect of this exercise on UCP1 and Cidea gene expression, compared injection of control antibodies (Fig. 6h). In contrast, PRDM16 mRNA levels were not increased with exercise and were also not affected by the anti-Fndc5 antibodies. Thus, irisin is required for a substantial part of the effect of exercise on these gene expression events in the browning of white fat.
Exercise has the capacity to improve metabolic status in obesity and type 2 diabetes via mechanisms that are poorly understood. Importantly, exercise increases whole body energy expenditure beyond the calories used in the actual work performed14. However, the relative contribution of the adipose tissues to this phenomenon has not been clarified. Since transgenic mice expressing PGC1α selectively in muscle showed a remarkable resistance to age-related obesity and diabetes4, we sought factors secreted from muscle under control of this coactivator that might increase whole body energy expenditure. This paper describes a new polypeptide hormone, irisin, which is regulated by PGC1α, secreted from muscle into blood and activates thermogenic function in adipose tissues. Irisin is remarkable in several respects. First, it has very powerful effects on the browning of certain white adipose tissues, both in culture and in vivo. Nanomolar levels of this protein increase UCP1 in cultures of primary white fat cells by 50 fold or more, resulting increased respiration. Perhaps more remarkable, viral delivery of irisin that causes only a moderate increase (~3 fold) in circulating levels stimulates a 10–20 fold increase in UCP1, increased energy expenditure and an improvement in glucose tolerance of high fat fed mice. Since this is in the range of increases seen with exercise in mouse and man, it is likely that irisin is responsible for at least some of the beneficial effects of exercise on the browning of adipose tissues and increases in energy expenditure. It is important to note that the evidence provided here does not exclude a role for other tissues besides muscle in the biological regulation and secretion of irisin.
Second, the cleaved and secreted portion of Fndc5, the hormone irisin, is highly conserved in all mammalian species sequenced. Mouse and human irisin are 100% identical, compared to 85% identity for insulin, 90% for glucagon and 83% identity for leptin. This certainly implies a highly conserved function that is likely to be mediated by a cell surface receptor. The identity of such a receptor is not yet known.
Based on the gene structure of Fndc5, with a signal peptide that was evidently missed in the studies of Ferrer-Martinez, et al, we considered that Fndc5 might be a secreted protein. Indeed, we have observed that the signal peptide is removed, and the mature protein is further proteolytically cleaved and glycosylated, to release the 112 aa polypeptide irisin. The cleavage and secretion of irisin is similar to the release/shedding of other transmembrane polypeptide hormones and hormone-like molecules such as the epidermal growth factor (EGF) and transforming growth factor alpha (TGF-α).
Since the conservation of calories would likely provide an overall survival advantage for mammals, it appears paradoxical that exercise would stimulate the secretion of a polypeptide hormone that increases thermogenesis and energy expenditure. One explanation for the increased irisin expression with exercise in mouse and man may have evolved as a consequence of muscle contraction during shivering. Muscle secretion of a hormone that activates adipose thermogenesis during this process might provide a broader, more robust defense against hypothermia.
The therapeutic potential of irisin is obvious. Exogenously administered irisin induces the browning of subcutaneous fat and thermogenesis, and it presumably could be prepared and delivered as an injectable polypeptide. Increased formation of brown or beige/brite fat has been shown to have anti-obesity, anti-diabetic effects in multiple murine models6, and adult humans have significant deposits of UCP1-positive brown fat15. Data presented here shows that even relatively short treatments of obese mice with irisin improves glucose homeostasis and causes a small weight loss. Whether longer treatments with irisin and/or higher doses would cause more weight loss remains to be determined. The worldwide, explosive increase in obesity and diabetes strongly suggests exploring the clinical utility of irisin in these and related disorders.
Another potentially important aspect of this work relates to other beneficial effects of exercise, especially in some diseases for which no effective treatments exist. The clinical data linking exercise with health benefits in many other diseases suggests that irisin could also have significant effects in these disorders.
Primary mouse stromal-vascular fractions from adipose tissues were differentiated as described6. Fndc5/irisin were purchased from ABNOVA (GST-fused), or produced from Syd Laboratories (GST-fused) or LakePharma (FC-fusions). Hydrodynamic injections were performed as described in Bell et. al,16. Electron microscopy was performed as described in Cinti et. al.17. Treadmil running was performed as in Wu et. al,18. Unless otherwise stated, bar graph data is presented as mean +/− SEM, and * p<0.05 compared to control group. Students T-test was used for single comparisons and one-way ANOVA for multiple.
Antibodies against UCP1, tubulin and Fndc5 were from Abcam. Forskolin, insulin, dexamethasone, rosliglitazone, GW6471 and antibody against flag were from Sigma. Primers for all qPCR experiments are listed in supplemental table I. Recombinant Fndc5, Lrg1, IL-15, VEGFβ and TIMP4 were from ABNOVA (Taiwan). Coomassie staining kit and Lipofectamine 2000 was from Invitrogen.
All PGC1α-induced genes as judged from gene expression analysis in MCK-PGC1α muscle with a fold change of at least 2 and p<0.05 were subjected to the following analysis. The protein sequence of the longest transcript were analyzed in the SignalP-software19 (http://www.cbs.dtu.dk/services/SignalP/). Sequences with positive S, C, Y and D-score were considered positive for a signal sequence. All positive proteins were then screened for mitochondrial target sequences (http://www.cbs.dtu.dk/services/TargetP/) whereas positive sequences were removed. All remaining hit proteins were then analyzed using qPCR in muscle from MCK-PGC1α mice and myocytes over expressing PGC1α.
The SVF from inguinal fat depots of 8–12 week old BALB/C mice were prepared and differentiated for 6 days as described in 20. Rosiglitazone was used at the two first days of differentiation. For all experiments, unless otherwise indicated, recombinant Fndc5 was added to the culture media at a concentration of 1μg/ml the last 4 days of differentiation. Primary myoblasts were cultured and differentiated as described in21.
293HEK or primary myocytes were transfected by standard methods or transduced with adenovirus at a MOI of 20 as indicated. 24 hours after transfection, media was removed, and cells were washed in large volumes of PBS five times, followed by incubation in Freestyle serum-free media (GIBCO) for 24 hours. The cells and media were then collected separately, and media centrifuged ×3 at 3000rpm to pellet debris. Thereafter, ¼ volume of ice-cold TCA was added and precipitated protein was pelleted at 14000 rpm and washed ×3 in acetone. Pellet was then dried and resuspended in SDS-containing lysis buffer. Protein concentration was measured in both cell and media fraction and adjusted either by protein or volume as indicated.
QPCR was carried out after Trizol-based RNA extraction using RNAeasy (Invitrogen) and thereafter SYBR green. All data was normalized to TBP, 18S or indicted in-house gene and quantitative measures obtained using the delta-delta-CT method.
Protein amounts from all samples were assessed using the BCA-kit (Thermo Scientific) followed by protein concentration normalization prior to all western blot experiments. Western blot was carried out following standard procedure and final band intensity (QL-BG) was quantified using BioPix iQ22. All data was normalized to background and loading controls.
CLARK electrode measurements, energy expenditure in vivo, IGTT and immunohistochemistry against UCP1 were performed as described in6, with the exception that CLARK output was normalized to total cell protein. FC-fusion construction and protein purification was performed by LakePharma (Ca).
C57/Bl6J mice were fed a high fat (60% Kcal) diet (D12492, Research Diets) for 20 weeks, starting at 6 weeks of age. Mice were then injected with indicated doses of adenovirus expressing GFP or Fndc5, and Comprehensive Lab Animal Monitoring Systems (CLAMS, Columbia instruments)-cage analysis was performed as described in Seale, 2011. Briefly, mice were acclimated in metabolic chambers for 2 days prior to analysis in order to minimize stress. C02 and 02 levels were then collected every 36 minutes for a period of 3 days. Data on activity, heat generation and food intake were measured on more frequent intervals. Circadian rhythm was observed for most parameters Data was not normalized to body weights unless otherwise stated.
Gel bands were digested with sequencing grade trypsin (Promega) or ASP-N(Sigma-Aldrich) as per manufactures’ instructions. Extracted in-gel protein digests were resuspended in 8 μL 5% formic acid/5% acetonitrile, and 4 μL were analyzed by microcapillary liquid chromatography electrospray ionization tandem mass spectrometry (LC-MS/MS). Analyses were done on a LTQ Orbitrap Velos mass spectrometer (Thermo Fisher Scientific, Germany) equipped with a Thermo Fisher Scientific nanospray source, an Agilent 1100 Series binary HPLC pump, and a Famos autosampler. Peptides were separated on a 100 μm × 16 cm fused silica microcapillary column with an in-house made needle tip. The column was packed with MagicC18AQ C18 reversed-phase resin (particle size, 5 μm; pore size, 200 Å; Michrom Bioresources). Separation was achieved through applying a 30 min gradient from 0 to 28% acetonitrile in 0.125% formic acid. The mass spectrometer was operated in a data dependent mode essentially as described previously23 with a full MS scan acquired with the Orbitrap, followed by up to 10 LTQ MS/MS spectra on the most abundant ions detected in the MS scan. Mass spectrometer settings were: full MS (AGC, 1×106; resolution, 6×104; m/z range, 375–1500; maximum ion time, 1000 ms); MS/MS (AGC, 5x103; maximum ion time, 120 ms; minimum signal threshold, 4×103; isolation width, 2 Da; dynamic exclusion time setting, 30 sec). Following mass spectrometry data acquisition, RAW files were converted into mzXML format and processed using a suite of software tools developed in-house for analysis. All precursors selected for MS/MS fragmentation were confirmed using algorithms to detect and correct errors in monoisotopic peak assignment and refine precursor ion mass measurements. All MS/MS spectra were then exported as individual DTA files and searched with no enzyme using the Sequest algorithm. These spectra were then searched against a database containing sequence of mouse Fndc5 in both forward and reversed orientations. The following parameters were selected to identify Fndc5: 10 ppm precursor mass tolerance, 0.8 Da product ion mass tolerance, fully tryptic or ASP-N digestion, and up to two missed cleavages. Variable modifications were set for methionine (+15.994915). In addition, a fixed modification for the carbamidomethylation for cysteine (+57.021464) was used as well. C-terminal fragment for Fndc5 was identified (KDEVTMKE) by trypsin digestion and reconfirmed by a separate ASP-N digestion.
35 μl of mouse or human plasma was precleared for albumin/IgG using the ProteoExtract-kit (CalBiochem) as recommended by the manufacturer. Samples were then concentration to approximately 100μl and >8μg/μl, followed by deglycosylation of 150μg using PNGase F (New England Biolabs). Totally 80μl were then prepared containing 1X sample buffer with reducing agent and 1,7μg/μl protein, sonicated, boiled and analyzed using western blot against Fndc5 or indicated antibody.
The Fndc5 expression vector was purchased with a C-terminal FLAG-tag from OriGene. The QuickChange Multi Site XL Directed Mutagenesis Kit (Aligent Technologies) was used to introduce a FLAG tag downstream of the signal sequence and to mutate the c-terminal flag tag, thus resulting in the NTF-Fndc5 construct (Fig. 5a). The NTF and CTF Fndc5 constructs were then subcloned into the pENTR1a vector (Invitrogen) and recombined into the pAd-CMV-DEST-V5 vector (Invitrogen) and adenovirus was produced using the virapower system (Invitrogen), including three rounds of amplification. Thereafter, virus was concentrated using the Vivapure adenopack 100 (Sartorius Stedim Biotech) and buffer exchanges to saline reaching a concentration of 9–10 ifu/μl. A GFP-containing adenovirus previously used was prepared in parallel.
The MCK-PGC1α transgenic and muscle-specific PGC1α knockout mice have been described previously24.
Blood samples and skeletal muscle biopsies were obtained from 8 male non-diabetic individuals before and after 10 weeks of aerobic training as described previously7. In brief, the exercise-training program consisted of cycling on stationary bikes with 4–5 sessions of 20–35 min per week at an average intensity of ~65% of maximal oxygen consumption. Informed consent was obtained from all volunteers before participation. The study was approved by the Local Ethics Committee and was performed in accordance with the Helsinki Declaration.
PB and BMS planned the majority of experiments and wrote the paper, while PB executed most of the experiments. JW performed a subset of cultured cell experiments and contributed valuble materials. MPJ and SPG performed the peptide fingerprinting identification of irisin cleavage. AK contributed with technical assistance and LY and SK performed the CLARK electrode experiments. EAB assisted with the hydrodynamic injections. JCL assisted with IV injections and KAR with bioinformatics. JZL and JHC performed in vitro experiments. PB and HT and LakePharma designed and provided FC-fusion proteins. KH and BFV performed the human cohort study, and MCZ and SC performed the electron microscopy studies.
FN3Reprints and permissions information is available at www.nature.com/reprints.
FN4The authors have no financial interest to disclose.
FN5Supplementary Information is linked to the online version of the paper at www.nature.com/nature
This study was supported by NIH grant DK54477, DK31405, DK61562 to BMS. PB and EAB were supported by the Wenner-Gren Foundation, Swedish Heart and Lung Foundation and SSMF. JW was supported by a postdoctoral fellowship from the American Heart Association (Founders Affiliate #09POST2010078). The animal procedures were in accordance with IAUCC-protocols 110-2008 and 056-2009. The authors thank Drs. Susan Loffredo and Marc Kirschner for helpful discussions and suggestions on the manuscript.
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