Diabetologia

, Volume 57, Issue 10, pp 2155–2164 | Cite as

Exosomes participate in the alteration of muscle homeostasis during lipid-induced insulin resistance in mice

  • Hala Aswad
  • Alexis Forterre
  • Oscar P. B. Wiklander
  • Guillaume Vial
  • Emmanuelle Danty-Berger
  • Audrey Jalabert
  • Antonin Lamazière
  • Emmanuelle Meugnier
  • Sandra Pesenti
  • Catherine Ott
  • Karim Chikh
  • Samir El-Andaloussi
  • Hubert Vidal
  • Etienne Lefai
  • Jennifer Rieusset
  • Sophie Rome
Open Access
Article

Abstract

Aims/hypothesis

Exosomes released from cells can transfer both functional proteins and RNAs between cells. In this study we tested the hypothesis that muscle cells might transmit specific signals during lipid-induced insulin resistance through the exosomal route.

Methods

Exosomes were collected from quadriceps muscles of C57Bl/6 mice fed for 16 weeks with either a standard chow diet (SD) or an SD enriched with 20% palm oil (HP) and from C2C12 cells exposed to 0.5 mmol/l palmitate (EXO-Post Palm), oleate (EXO-Post Oleate) or BSA (EXO-Post BSA).

Results

HP-fed mice were obese and insulin resistant and had altered insulin-induced Akt phosphorylation in skeletal muscle (SkM). They also had reduced expression of Myod1 and Myog and increased levels of Ccnd1 mRNA, indicating that palm oil had a deep impact on SkM homeostasis in addition to insulin resistance. HP-fed mouse SkM secreted more exosomes than SD-fed mouse SkM. This was reproduced in-vitro using C2C12 cells pre-treated with palmitate, the most abundant saturated fatty acid of palm oil. Exosomes from HP-fed mice, EXO-Post Palm and EXO-Post Oleate induced myoblast proliferation and modified the expressions of genes involved in the cell cycle and muscle differentiation but did not alter insulin-induced Akt phosphorylation. Lipidomic analyses showed that exosomes from palmitate-treated cells were enriched in palmitate, indicating that exosomes likely transfer the deleterious effect of palm oil between muscle cells by transferring lipids. Muscle exosomes were incorporated into various tissues in vivo, including the pancreas and liver, suggesting that SkM could transfer specific signals through the exosomal route to key metabolic tissues.

Conclusions/interpretation

Exosomes act as ‘paracrine-like’ signals and modify muscle homeostasis during high-fat diets.

Keywords

Exosomes High-fat diet Insulin resistance Muscle Palmitate 

Abbreviations

adeno-GFP

Adenoviruses expressing GFP

CM

Conditioned medium

FAME

Fatty acid methyl ester

GFP

Green fluorescent protein

HP

SD enriched with 20% palm oil

IR

Insulin resistance

miRNA

MicroRNA

MVB

Multivesicular body

qRT-PCR

Quantitative real-time PCR

SD

Standard chow diet

SkM

Skeletal muscle

Introduction

Skeletal muscle (SkM)-secreted proteins have important roles in intercellular communications. Among them, a large number of soluble peptide hormones and cytokines (myokines) are capable of triggering adaptations of homeostasis in other peripheral organs or are involved in the process of myogenesis [1]. Studies during the last 10 years have demonstrated that cells also release bioactive nanovesicles. A particularly important class of extracellular vesicle is the exosomes, which represent a discrete population of 50–120 nanometre-sized vesicles [2]. Exosomes are formed in endocytic compartments called multivesicular bodies (MVBs) during endosome maturation, by inward budding of their limiting membrane. They are released from the cell into the microenvironment following the fusion of MVBs with the plasma membrane. Exosomes can transfer both functional protein and RNA species from one cell to another whereby an array of biological processes, including cell proliferation and differentiation, can be affected [3]. It is believed that exosomes could have a much more potent influence on the physiology of the cells they encounter than single-molecule mediators because the numerous proteic, lipidic and nucleic acid components they carry can affect multiple signalling pathways inside target cells. Exosomes can modulate immune-regulatory processes, set up tumour escape mechanisms and mediate regenerative or degenerative processes [4].

All insulin-sensitive tissues release exosomes [5, 6, 7, 8]. In this context, it has been demonstrated that adipose tissue-released exosomes in leptin-deficient (ob/ob) mice are taken up by peripheral blood monocytes and can stimulate the differentiation of monocytes into activated macrophages with increased secretion of TNF-α and IL-6 [9]. This finding suggests that exosomes released from adipose tissue of obese animals could act as a mode of communication with macrophages. Moreover, when administered to wild-type mice, adipose tissue-released exosomes from ob/ob mice contributed to the development of insulin resistance (IR) [9]. Other studies have shown that adipocyte-derived exosomes are involved in the control of lipid storage and cell size between adipocytes [10] and they have been described as mediators of angiogenesis [11].

Although communication between SkM and other tissues appears to be important in the relationship between obesity and diabetes [12], the possibility that SkM-derived exosomes act as a mode of systemic communication has hitherto never been discussed. Until now, the roles of exosomes in the development of metabolic syndrome and IR are poorly understood and little is known about the connection between lipid exposure and exosome secretion from muscle cells.

Therefore, we investigated whether SkM cells might transmit specific signals via exosomes during lipid-induced IR. Especially, we examined whether exosomes from palmitate-treated myotubes could transfer the deleterious action of palmitate between muscle cells. In addition, we analysed in mice the biodistribution of labelled exosomes from control- or palmitate-exposed myotubes. We provide evidence that exosomes from muscle cells act both as ‘paracrine-like’ signals by locally perturbing muscle homeostasis during lipid-induced IR and as ‘endocrine-like’ signals by targeting other insulin-sensitive tissues in vivo.

Methods

Cell culture

C2C12 myoblasts [13] were maintained in DMEM (4.5 g/l glucose, 10% heat-inactivated FBS, 1,000 U/ml penicillin, 1,000 U/ml streptomycin, 2 mmol/l l-glutamine; PAA laboratories; Vélizy-Villacoublay, France) at 37°C under 5% CO2 atmosphere. Cell differentiation was induced by replacing FBS with 2% horse serum.

Mouse model

Male C57BL/6 mice (Harlan Laboratories, Gannat, France) were housed in a common animal centre (PBES - Lyon Sud, Lyon, France). Animal experiments were approved by the Lyon Local Board for Laboratory Animals (No. 2010-008). At 4 weeks, mice were divided into two groups and fed either a standard chow diet (SD; 57% carbohydrate, 5% fat and 18% protein) or an SD diet enriched with 20% palm oil (HP; palmitic acid 44.5%, oleic acid 38.5%). After 16 weeks, blood was withdrawn into heparinised microcapillary tubes from the orbital sinus of anaesthetised mice in a fed state. The mice were then killed by cervical dislocation. Quadriceps and gastrocnemius muscles were excised and used, respectively, for exosome purification or gene and protein expression analyses.

Palmitate and oleate preparation and C2C12 treatment

Palmitate or sodium oleate (P-0500 and Fluka-75165, respectively; Sigma-Aldrich, Saint-Quentin Fallavier, France) were pre-complexed with 10% (wt/vol.) fatty acid-free BSA (Roche Diagnostic, Grenoble, France) in DMEM at 50°C for 2 h to prepare stock solutions of 8 mmol/l. The stock solutions were filtered and diluted in serum-free culture medium to a final concentration of 0.5 mmol/l, as lower concentrations of palmitate or oleate did not affect insulin-induced Akt phosphorylation (see electronic supplementary material [ESM] Fig. 1). The concentration of glucose in the medium (4.5 g/l vs 1 g/l) did not modify alteration of insulin-induced Akt phosphorylation induced by palmitate. For the analysis of insulin signalling, treated myotubes were incubated with or without 10−7 mol/l of insulin for 20 min.

Isolation of muscle exosomes

Exosomes were purified from conditioned media (CM) either from C2C12 cells [14, 15] or from quadriceps cut into small pieces in serum-free DMEM (24 h). Cell debris and organelles were eliminated by centrifugation at 2,000 g for 20 min. The supernatant fraction was further centrifuged at 10,000 g for 30 min and then filtered through a 0.22 μm filter. Exosomes were pelleted at 100,000 g for 70 min at 4°C (Optima L-80-XP ultracentrifuge, type 50-2Ti rotor; Beckman-Coulter, Villepinte, France). Pellets from a single sample were pooled, resuspended in 25 ml PBS and again centrifuged at 100,000 g for 70 min. Finally, the exosome pellet was resuspended in 100 μl PBS. Exosomal proteins were quantified using a Bradford protein assay. A NanoSight (Malvern Instruments, Orsay, France) was employed to measure the size of particles [16]. The number of particles and their movement were recorded for 1 × 60 s and analysed using the NS500 software. Exosomes were visualised by transmission electron microscopy as previously described [15] (ESM Fig. 2).

Production of C2C12 exosomes containing green fluorescent protein

Non-replicative adenoviruses expressing the green fluorescent protein (adeno-GFP) were generated as previously described [17]. Differentiated C2C12 cells were infected with adeno-GFP for 24 h in differentiation medium. Twenty-four hours later all myotubes had green fluorescence in the cytoplasm indicating that all cells had been infected. Myotubes were washed with PBS to remove both non-integrated adenovirus and exosomes from FBS and then were incubated for another 48 h in exosome-depleted DMEM. GFP-containing exosomes accumulated in CM for 48 h were extracted.

Differentiated C2C12 myotubes were incubated with 2 μg GFP-containing exosomes depleted of viral particles (EXO-GFP) per ml of medium [14, 15]. Forty-eight hours later cells were visualised with a Zeiss Axiovert 200 M Fluorescence/Live cell Imaging microscope equipped with Axiovision software (Carl Zeiss, Marly le Roi, France).

Microarray data analysis

C2C12 RNA profiling was performed using the Mouse GE 4*44K v2 Microarray kit (Agilent Technologies, Les Ulis, France). Briefly, 100 ng of RNA was labelled with Cy-3 using the Low Input Quick Amp Labeling kit (Agilent Technologies) and microarrays were hybridised and scanned following the manufacturer’s instructions. Microarray analyses were performed with R environment using Agi4x44PreProcess and Limma packages from BioConductor [18]. The dataset is available from the GEO database GSE52048 (www.ncbi.nlm.nih.gov/gds/).

Quantitative real-time PCR

Quantitative real-time PCR (qRT-PCR) was performed using ABsolute QPCR SYBR Green ROX Mix (Abgene, Courtaboeuf, France) with a Rotor-Gene 6000 system (Corbett Life Science, Qiagen, France). Results were normalised with a reference gene encoding TBP (TATA box binding protein) [19]. PCR primers are listed in ESM Table 1.

Western blotting

Cells were lysed in RIPA lysis buffer (PBS, 0.1% SDS, 0.5% sodium deoxycholate, 1% Nonidet NP40, 5 mmol/l EDTA, 1 mmol/l Na3VO4, 20 mmol/l NaF, 1 mmol/l dithiothreitol, protease inhibitors). Proteins were denatured and migrated on 12% SDS-PAGE gels and transferred onto nitrocellulose PVDF (polyvinylidene difluoride) membranes. Membranes were incubated with anti-rabbit antibodies (ESM Table 1). Signals were revealed with Immuno detection kit ECL Luminata Classico (Merck-Millipore, Guyancourt, France) and imager Molecular Image ChemiDocXRS+ (Bio-Rad, Marnes-la-Coquette, France). Protein quantification was achieved using ImageLab 3.0 (Bio-Rad).

Biodistribution of C2C12 exosomes

Exosomes were pelleted in the presence of 1 μmol/l fluorescent lipophilic tracer DiR (1,1-dioctadecyl-3,3,3,3-tetramethylindotricarbocyanine iodide) (D12731; Invitrogen Life Technologie, Cergy Pontoise, France) by ultracentrifugation (110,000 g, 90 min). DiR dye has been used previously for both cell and exosomal tracking in vivo [20]. A washing step was performed by re-suspending the pellet in 25 ml PBS and ultracentrifuging (110,000 g, 90 min). The pellet was resuspended in 210 μl PBS. Particle analysis was performed with a NanoSight (Malvern Instruments [16]) to measure the particle size distribution of post re-pelleting with DiR. DiR-labelled exosomes were injected through the tail vein of female C57BL/6 mice (16 g/body weight) for 24 h to obtain the highest amount of fluorescence in each tissue. As a control we injected with mock-PBS-DiR, and performed the same procedures as for the labelling of exosomes but without exosomes (ESM Fig. 3). Mice were then killed and the organs were carefully harvested and imaged for 2 s (exCitation 710 nm, emission 760 nm) using a high-sensitivity CCD camera IVIS Spectrum (PerklinElmer, Sverige, Sweden). As shown in ESM Fig. 3, the free DiR showed a signal, with a total tissue signal about 14–15% that of C2C12-DiR-EXO.

Animal experiments were approved by the Swedish Local Board for Laboratory Animals and performed in accordance with ethical permission and designed to minimise animal suffering and pain.

Exosome lipidomic analysis

The fatty acid profile of total exosome lipids was determined by fatty acid methyl ester (FAME) analysis. Total lipid extract was trans-esterified in 2 ml of methanol H2SO4 2% at 70°C for 1 h. FAMEs were analysed by GC-MS on an Agilent 5975 in series with GC (Hewlett Packard 6890 series) (Agilent Technologies). Quantification was achieved by normalisation with an internal standard of nonadecanoic acid methyl ester and the response factors for the various fatty acids were calculated with weighted methyl ester calibrators FAME mix (Restek, Lisses, France) [21].

Impedance measurement with the xCELLigence RTCA DP Instrument

The effect of exosomes on C2C12 myoblast proliferative capacities was monitored with the xCELLigence live cell analysis System (Life Science Roche, Meylan, France), which offers dynamic live cell monitoring [22]. One day post-plating, cells were grown in serum-free DMEM and 4.5 g/l glucose supplemented with exosomes, and monitored every 15 min for 24 h [15]. At the end of the experiment, cells were trypsinised, counted and their sizes were determined by using the Scepter 2.0 handheld automated cell counter from Millipore (Guyancourt, France).

Statistical analysis

All results were expressed as mean ± SEM. A parametric Student’s t test was used for mean comparison. A p value < 0.05 was considered significant.

Results

Lipids modified muscle exosome release

Mice fed with HP for 16 weeks were obese, hyperinsulinaemic and hyperglycaemic (ESM Fig. 4) compared with SD-fed mice. Insulin-induced Akt phosphorylation was altered ex vivo in gastrocnemius muscles of HP-fed mice (Fig. 1a). Muscles of HP- and SD-fed mice were incubated ex vivo for 24 h in serum-free medium and exosomes released into the CM during this time period were extracted by filtration and ultracentrifugation [5, 14, 23] (ESM Fig. 2). The vesicle size distribution displayed a bell-shaped curve (ESM Fig. 2) in agreement with the reported size of exosomes [2, 24]. As shown on Fig. 1b, muscles from HP-fed mice secreted more exosomes than the muscles from SD-fed mice. This result was reproduced in-vitro when C2C12 cells were incubated for 18 h in serum-free medium with palmitic acid only (C16:0), the most abundant saturated fatty acid of palm oil (Fig. 1c, d). This tendency was still observed 9 h post-palmitate incubation compared with cells pre-treated with BSA (Fig. 1e, f). Reducing the concentration of palmitate in the C2C12 medium from 0.5 mmol/l to 0.1 mmol/l led to a decrease in exosomes released (80 μg of exosomes are released from C2C12 treated with 0.5 mmol/l palmitate compared with 30 μg when cells are treated with 0.1 mmol/l palmitate).
Fig. 1

(a, c, e) Phospho-Akt and Akt quantified by western blot in gastrocnemius muscle of SD- and HP-fed mice incubated ex vivo with 10−7 mol/l insulin for 15 min (a), in C2C12 cells treated with 0.5 mmol/l palmitate (Palm) for 18 h (c) and in C2C12 cells 9 h post palmitate treatment (e). Data are unitless (phospho-Akt/total Akt intensities). *p < 0.05; **p < 0.01, for indicated comparisons. (b, d, f) Quantities of exosomes released from quadriceps of SD- and HP-fed mice (b), from C2C12 cells treated with 0.5 mmol/l palmitate for 18 h (d) or from C2C12 cells 9 h post palmitate treatment (f). White bars and black bars represent incubation without and with insulin, respectively. *p < 0.05

Exosomes can transfer proteins between C2C12 myotubes

As we recently demonstrated that exosomes could transfer microRNAs (miRNAs) and proteins between muscle cells [14, 15] we aimed to determine whether myotubes could use the exosomal route to transfer proteins. Myotubes were infected with adeno-GFP protein (Fig. 2a) in order to collect EXO-GFP. Fresh C2C12 myotubes were incubated with EXO-GFP and fluorescence in their cytoplasm was monitored. Forty-eight hours post-incubation, myotubes with fluorescent cytoplasm were detected (Fig. 2b) indicating that exosomes had transferred their GFP contents into recipient myotubes (Fig. 2c). This data suggested that increased release of exosomes from muscle cells incubated with palmitic acid might modify the crosstalk between muscle cells and thus perturb muscle homeostasis
Fig. 2

(a) C2C12 myotubes (MT) infected with adeno-GFP (magnification × 10). (b) MT incubated for 48 h with EXO-GFP released from infected MTs described in (a) (magnification × 20). (c) Western blot detection of GFP in infected MTs (1 μg) or in their released EXO-GFP (1 μg) or in MTs incubated with EXO-GFP (50 μg); Exo-MT, exosomes from myotubes

EXO-Post Palm increased the Akt content of recipient muscle cells

To determine whether palmitate treatment affected the biological properties of muscle-released exosomes, differentiated myotubes were incubated with exosomes from cells pre-treated with BSA or palmitate [14, 15]. To ensure that exosomes were not contaminated with cell-free palmitate we used exosomes collected 9 h after palmitate removal from the medium (EXO-Post Palm). As shown in Fig. 1e, insulin-induced Akt phosphorylation was still altered during this time period, indicating that the effect of palmitate was not lost. Results indicated that incubation with EXO-Post Palm, compared with EXO-Post BSA, induced an increase in the total Akt content of the recipient myotubes (Fig. 3a). An increase in the Akt level was also found when examining quadriceps-released exosomes from HP-fed mice (EXO-HP) vs SD-fed mice (EXO-SD) (Fig. 3b). By contrast, EXO-Post Palm and EXO-HP did not significantly affect insulin-stimulated Akt phosphorylation (data not shown), indicating that they did not transfer lipid-induced insulin-resistance between muscle cells.
Fig. 3

Akt quantified by western blot. Actin was used as loading control. Data are unitless (total Akt/actin intensities). (a, b) C2C12 myotubes incubated with C2C12-released exosomes collected from cells pre-treated with EXO-Post Palm vs EXO-Post BSA (a) or with quadriceps-released exosomes from HP-fed mice vs SD-fed mice (b). (c, d) C2C12 myotubes incubated with CM of cells pre-treated with palmitate (CM-Post Palm) (c) or with CM-Post Palm depleted of exosomes (CM-DE) (d)

To determine the specific effects of exosomes compared with the global medium from palmitate-treated C2C12 cells, conditioned medium (CM-Post Palm) was divided during exosome extraction. Although not significant, CM-Post Palm induced an increase in the total Akt level (Fig. 3c) as did the exosomal fraction alone. CM-Post Palm depleted of exosomes had no effect on Akt level (Fig. 3d), indicating that exosomes likely participated in the effect of CM on total Akt in C2C12 cells.

EXO-Post Palm modified expression of genes involved in cell cycle and muscle differentiation in recipient myotubes

Myotubes were incubated either with EXO-Post BSA or EXO-Post Palm in serum-free medium for 24 h and their transcriptomes were analysed by microarrays. mRNA levels of 240 genes were significantly modified in response to EXO-Post Palm (163 genes were upregulated and 77 were downregulated) compared with EXO-Post BSA (ESM Table 2). Functional enrichment analyses (Babelomics 4.3), comparing the 163 upregulated genes with the 77 downregulated genes, revealed that ‘cell cycle’, ‘mitosis’ and ‘DNA metabolic process’ genes were significantly enriched in the upregulated genes (Fig. 4). The 77 significantly downregulated genes were involved in ‘cell adhesion’, ‘cell differentiation’, ‘development’ and ‘protein metabolic process’ (Fig. 4). Microarray data were confirmed by measuring Ccnd1, Il-6 and Slc2a4 (Glut4) mRNA levels (ESM Table 2 and Fig. 5a). In addition, we found a downregulation of Myog and Myod1, two markers of muscle cell terminal differentiation, in cells treated with EXO-Post Palm (Fig. 5a).
Fig. 4

Gene ontology (GO) pathways (levels from 3 to 9) significantly enriched in genes differentially regulated in C2C12 cells treated with EXO-Post Palm vs EXO-Post BSA (p < 0.05). White bars, upregulated genes; grey bars, downregulated genes

Fig. 5

Expression levels of Ccnd1, Il-6, Slc2a4, Myod1 and Myog quantified by qRT-PCR. (a) C2C12 cells pre-treated with EXO-Post BSA (white bars), EXO-Post Palmitate (black bars) or EXO-Post Oleate (grey bars). (b) C2C12 cells pre-treated with palmitate (black bars) or BSA (white bars). (c) mRNA expressions in gastrocnemius muscle of SD (white bars) or HP (black bars) mice. All data are unitless (mRNA/Tbp mRNA level). n = 4 biological replicates; *p < 0.05, **p < 0.01 vs EXO-Post BSA, BSA or SD

EXO-Post Palm affected C2C12 proliferation

As the biological effect of exosomes was studied on unproliferative C2C12 myotubes, we wondered whether the increase in Ccnd1 mRNA level involved in the regulation of cell cycle resulted from a residual myoblast population. Myoblasts were grown in serum-free medium complemented with EXO-Post BSA or EXO-Post Palm. The cell growth curves were automatically recorded every 15 min for 48 h. As shown in Fig. 6a, b, EXO-Post Palm induced myoblast proliferation compared with EXO-Post BSA. These effects were not associated with modification of mean cell sizes (Fig. 6c–e).
Fig. 6

C2C12 myoblasts (n = 8) were incubated with serum-free DMEM supplemented with EXO-Post Palm or EXO-Post Oleate. (a, b) Impedance measurement with the xCELLigence System. (a) The presence of the cells on top of the electrodes will affect the local ionic environment at the electrode/solution interface, leading to an increase in the electrode impedance. The more cells attached to the electrodes, the larger the increase in electrode impedance. (b) Data is graphed as ‘Delta Cell Index’, which is the change in impedance from the time point immediately after cells were added (*p < 0.05 vs EXO-Post BSA). (ce) Myoblast sizes determined by the Scepter 2.0 handheld automated cell counter after 48 h proliferation. (c) Serum-free DMEM (grey line) or EXO-Post BSA (black line). (d) EXO-Post BSA (grey line) or EXO-Post Palm (black line). (e) EXO-Post BSA (grey line) or EXO-Post Oleate (grey line)

Exosomes transferred lipids between muscle cells

We observed that Slc2a4, Myod1, Myog, Ccnd1 and Il-6 mRNA levels were altered in the same direction both in muscle cells used to collect exosomes (muscle cells of HP-fed mice vs SD-fed mice; C2C12 cells treated with palmitate vs BSA) (Fig. 5b, c) and in the recipient C2C12 cells treated with those exosomes (Fig. 5a). From these data we suspected that exosomes from palmitate-treated cells could potentially transfer the effect of palmitate by transferring lipid messengers between cells. We performed a lipidomic analysis to determine whether treatment with palmitate had modified the exosome composition. Exosomes released from cells treated with palmitate were enriched in palmitate compared with exosomes from cells treated with BSA (Fig. 7), suggesting that EXO-Post Palm could transfer palmitate between muscle cells. To determine whether such transfer might occur with other fatty acids, we incubated C2C12 myotubes with exosomes collected from cells pre-treated with oleate (EXO-Post Oleate), the most abundant unsaturated fatty acid of palm oil. In contrast with palmitate, oleate did not alter insulin-stimulated Akt phosphorylation in muscle cells (ESM Fig. 1). However, compared with EXO-Post BSA, EXO-Post Oleate altered the expression of Ccnd1, Il-6, Slc2a4, Myod1 and Myog in C2C12 myotubes in a similar manner to EXO-Post Palm (Fig. 5a). EXO-Post Oleate also induced myoblast proliferation (Fig. 6).
Fig. 7

Quantification of fatty acids in exosomes. EXO-Palm (black bars) and EXO-BSA (white bars) from C2C12 treated for 18 h with BSA or palmitate

Biodistribution of exosomes from muscle cells

EXO-Post Palmitate or EXO-Post BSA labelled with fluorescent lipophilic dye DiR were injected into the tail vein of mice. Twenty-four hours post-injection, the mice were killed and fluorescence was monitored in various tissues. Figure 8 shows that most of the exosomes went to the liver, spleen and lungs but fluorescence was detected in all analysed tissues. Both types of exosome (BSA vs palmitate) targeted the same tissue.
Fig. 8

Biodistribution of C2C12 exosomes. EXO-Post BSA (6.02 × 1010 particles/ml; white bars) and EXO-Post palmitate (3.44 × 1010 particles/ml; black bars) were used for tail injection in C57Bl/6 mice. (a) Quantification of fluorescent signals for each organ, normalised to background. (b) Organs targeted by C2C12 DiR exosomes; 1 = brain, 2 = liver, 3 = heart, 4 = lungs, 5 = gastrointestinal tract, 6 = spleen, 7 = pancreas, 8 = quadriceps, 9 = kidney

Discussion

Palmitic acid is the most abundant systemic saturated NEFA of palm oil and has received considerable attention in investigations of metabolic consequences of dietary lipids since it is suspected to participate in the onset of IR in SkM [25, 26]. In this context it has been demonstrated that palmitate-induced IR in C2C12 myotubes is associated with impaired expression of myokines (i.e. irisin, CTRP15 [family with sequence similarity 132, member B] and FGF21 [fibroblast growth factor 21]) known for their potential beneficial roles in metabolic diseases [27]. In agreement, irisin in plasma is reduced in type 2 diabetes by 50% [28]. These data indicated that under chronic elevation of plasma NEFA SkM may secrete specific signals that would act either as ‘paracrine-like’ signals by locally perturbing muscle homeostasis or as ‘endocrine-like’ signals by targeting other insulin-sensitive tissues. In this study, HP-fed mice consuming a standard diet enriched with 20% palm oil for 16 weeks presented marked obesity, hyperinsulinaemia and hyperglycaemia compared with SD-fed mice. Moreover, they displayed altered Akt phosphorylation in response to insulin and reduced expression of Slc2a4 mRNA in SkM. Interestingly, HP-fed mice were also found to have reduced mRNA levels of Myod1 and Myog, two markers of muscle differentiation, and increased mRNA level of Ccnd1, indicating that palm oil had a deep impact on muscle homeostasis in addition to IR.

The first finding of our study is that feeding mice with palm oil modified the rate of exosome secretion from SkM ex vivo. This was confirmed in vitro by showing that increasing the amount of palmitate in the medium of C2C12 cells induced an increase in exosome release. It is possible that de novo synthesis of ceramides from palmitate could contribute to an increase in intracellular exosome formation as exosome membranes are enriched in ceramides and intracellular ceramide levels are involved in exosome secretion by permitting the inward budding of MVBs [29, 30]. Here, we did not quantify ceramides in exosomes but we found a marked enrichment in palmitic acid after treatment of C2C12 cells indicating that there was a modification of the lipid composition of exosomes. In addition, palmitate-induced exosome release could also occur through the palmitoylation of proteins involved in invagination of endosomal membranes (i.e. proteins involved in the ESCRT [endosomal sorting complex required for transport] machinery [31]), possibly leading to modifications of the proteins’ subcellular localisation, stability, trafficking, translocation to lipid rafts, aggregation and interactions with new effectors [32].

Although palmitate treatment does not reproduce exactly the in vivo situation where a mixture of fatty acids exists provided by the diet, these results support the notion that excessive concentration of circulating saturated fatty acids might modify exosome secretion from SkM in vivo.

We have previously shown that muscle-released exosomes are involved in the process of myogenesis, being able to transfer proteins and miRNAs from differentiated myotubes to proliferating myoblasts [14, 15]. In this study we further demonstrated that exosomes can also transfer their protein contents between differentiated muscle cells. Thus we postulated that in response to palm oil, muscle cells might secrete exosomes able to transfer part of the deleterious effect of palm oil to neighbouring cells. Our data showed that palmitate-induced IR is not transferred between muscle cells through the exosomal route. However, EXO-Post Palm, as well as EXO-HP, was able to perturb the myotube phenotype (i.e. decrease in Myog and Myod1 mRNA levels) and to induce myoblast proliferation (i.e. increase in Akt protein and Ccnd1 mRNA levels). Interestingly, these alterations in genes expressions were similar to those observed in vivo in muscles of HP-fed mice or in palmitate-treated C2C12 cells. These results indicate, therefore, that muscle-released exosomes can likely transfer the deleterious effect of palm oil between muscle cells by transferring lipids and thus may participate in vivo in the alterations of muscle homeostasis in high-fat diets.

EXO-Post Palm or EXO-HP modified the expression of genes encoding 20 secreted proteins in recipient myotubes (ESM Table 2). Among them, Cxcl1 and Cxcl5 have been found to be altered in the serum of patients with type 2 diabetes [33, 34]. We validated the upregulation of Il-6, the gene encoding IL-6, one of the several pro-inflammatory cytokines associated with IR and type 2 diabetes [35]. In vitro studies have suggested that IL-6 plays a part in myogenesis and muscle atrophy [36, 37]. Thus these data support the concept that in addition to altering muscle homeostasis, muscle-exosomes are able to modulate the expression of several myokines, hence suggesting a potential role for these extracellular vesicles in whole-body homeostasis during lipid-induced IR.

Until now the mechanism of exosome uptake by target cells has been poorly understood. Integrins and tetraspanins [38], as well as cell-surface heparan sulfate proteoglycans, have been implicated in exosome uptake and internalisation [39]. However, despite the fact that exosomes can be used for the delivery of small RNAs and anti-inflammatory agents to target cells in vivo [40, 41] it is not known whether exosomes have restricted tissue specificities. Indeed, in these previous studies exosomes were modified in order to target tissues of interest. We have shown recently that, in vitro, myotube-released exosomes can transfer siRNA and miRNA to myoblasts [14]. Importantly, we found in the present study that fluorescently labelled muscle-released exosomes intravenously injected into mice were incorporated into various tissues in addition to SkM. Incorporation into the pancreas and liver might suggest that SkM could transfer specific signals through the exosomal route to key metabolic tissues in vivo. Alterations in this signalling system during a high-fat diet may eventually contribute to the development of IR and type 2 diabetes. Further studies are now required to demonstrate whether exosomes from insulin-resistant SkM can reach the blood circulation and regulate the homeostasis of the other insulin-sensitive tissues and to decipher the affected functions in these target tissues.

Notes

Acknowledgements

We thank E. Errazuriz (Centre Commun d’Imagerie de Laënnec, SFR Santé Lyon-Est, University of Lyon, France) for transmission electron microscopy images.

Funding

This work was supported by grants from Fondation pour la Recherche Médicale (FRM-2010), Association Française de Diabétologie (SDF/Rochediagnostics France) and INRA specific grant (ANSSD-2010). The funders had no role in study design, data collection and analysis, decision to publish or preparation of the manuscript.

Duality of interest

The authors declare that there is no duality of interest associated with this manuscript.

Contribution statement

All the authors provided substantial contributions to the conception and design of this study and to aquisition and analysis of the data. All the authors participated in drafting the article and approved the version to be published. SR is responsible for the integrity of the work as a whole.

Supplementary material

125_2014_3337_MOESM1_ESM.pdf (229 kb)
ESM Fig. 1(PDF 228 kb)
125_2014_3337_MOESM2_ESM.pdf (14.7 mb)
ESM Fig. 2(PDF 15051 kb)
125_2014_3337_MOESM3_ESM.pdf (49 kb)
ESM Fig. 3(PDF 49 kb)
125_2014_3337_MOESM4_ESM.pdf (76 kb)
ESM Fig. 4(PDF 76 kb)
125_2014_3337_MOESM5_ESM.pdf (15 kb)
ESM Table 1(PDF 14 kb)
125_2014_3337_MOESM6_ESM.xls (85 kb)
ESM Table 2(XLS 85 kb)

References

  1. 1.
    Pedersen BK, Febbraio MA (2012) Muscles, exercise and obesity: skeletal muscle as a secretory organ. Nat Rev 8:457–465Google Scholar
  2. 2.
    Thery C, Boussac M, Veron P et al (2001) Proteomic analysis of dendritic cell-derived exosomes: a secreted subcellular compartment distinct from apoptotic vesicles. J Immunol 166:7309–7318PubMedCrossRefGoogle Scholar
  3. 3.
    Mathivanan S, Ji H, Simpson RJ (2010) Exosomes: extracellular organelles important in intercellular communication. J Proteome 73:1907–1920CrossRefGoogle Scholar
  4. 4.
    Lopez-Verrilli MA, Court FA (2013) Exosomes: mediators of communication in eukaryotes. Biol Res 46:5–11PubMedCrossRefGoogle Scholar
  5. 5.
    Guescini M, Guidolin D, Vallorani L et al (2010) C2C12 myoblasts release micro-vesicles containing mtDNA and proteins involved in signal transduction. Exp Cell Res 316:1977–1984PubMedCrossRefGoogle Scholar
  6. 6.
    Aoki N, Jin-no S, Nakagawa Y et al (2007) Identification and characterization of microvesicles secreted by 3T3-L1 adipocytes: redox- and hormone-dependent induction of milk fat globule-epidermal growth factor 8-associated microvesicles. Endocrinology 148:3850–3862PubMedCrossRefGoogle Scholar
  7. 7.
    Conde-Vancells J, Rodriguez-Suarez E, Embade N et al (2008) Characterization and comprehensive proteome profiling of exosomes secreted by hepatocytes. J Proteome Res 7:5157–5166PubMedCentralPubMedCrossRefGoogle Scholar
  8. 8.
    Lee HS, Jeong J, Lee KJ (2009) Characterization of vesicles secreted from insulinoma NIT-1 cells. J Proteome Res 8:2851–2862PubMedCrossRefGoogle Scholar
  9. 9.
    Deng ZB, Poliakov A, Hardy RW et al (2009) Adipose tissue exosome-like vesicles mediate activation of macrophage-induced insulin resistance. Diabetes 58:2498–2505PubMedCentralPubMedCrossRefGoogle Scholar
  10. 10.
    Muller G, Schneider M, Biemer-Daub G, Wied S (2011) Upregulation of lipid synthesis in small rat adipocytes by microvesicle-associated CD73 from large adipocytes. Obesity (Silver Spring MD) 19:1531–1544CrossRefGoogle Scholar
  11. 11.
    Aoki N, Yokoyama R, Asai N et al (2011) Adipocyte-derived microvesicles are associated with multiple angiogenic factors and induce angiogenesis in vivo and in vitro. Endocrinology 151:2567–2576CrossRefGoogle Scholar
  12. 12.
    DeFronzo RA, Tripathy D (2009) Skeletal muscle insulin resistance is the primary defect in type 2 diabetes. Diabetes Care 32(Suppl 2):S157–S163PubMedCentralPubMedCrossRefGoogle Scholar
  13. 13.
    Yaffe D, Saxel O (1977) Serial passaging and differentiation of myogenic cells isolated from dystrophic mouse muscle. Nature 270:725–727PubMedCrossRefGoogle Scholar
  14. 14.
    Forterre A, Jalabert A, Berger E et al (2014) Proteomic analysis of C2C12 myoblast and myotube exosome-like vesicles: a new paradigm for myoblast-myotube cross talk? PLoS One 9:e84153PubMedCentralPubMedCrossRefGoogle Scholar
  15. 15.
    Forterre A, Jalabert A, Chikh et al (2014) Myotube-derived exosomal miRNAs downregulate Sirtuin1 in myoblasts during muscle cell differentiation. Cell Cycle 13:78–89PubMedCrossRefGoogle Scholar
  16. 16.
    Dragovic RA, Gardiner C, Brooks AS et al (2011) Sizing and phenotyping of cellular vesicles using Nanoparticle Tracking Analysis. Nanomedicine 7:780–788PubMedCentralPubMedCrossRefGoogle Scholar
  17. 17.
    Dif N, Euthine V, Gonnet E, Laville M, Vidal H, Lefai E (2006) Insulin activates human sterol-regulatory-element-binding protein-1c (SREBP-1c) promoter through SRE motifs. Biochem J 400:179–188PubMedCentralPubMedCrossRefGoogle Scholar
  18. 18.
    Smyth GK (2004) Linear models and empirical bayes methods for assessing differential expression in microarray experiments. Stat Appl Genet Mol Biol 3: Article 3Google Scholar
  19. 19.
    Stern-Straeter J, Bonaterra GA, Hormann K, Kinscherf R, Goessler UR (2009) Identification of valid reference genes during the differentiation of human myoblasts. BMC Mol Biol 10:66PubMedCentralPubMedCrossRefGoogle Scholar
  20. 20.
    Ohno S, Takanashi M, Sudo K et al (2012) Systemically injected exosomes targeted to EGFR deliver antitumor microRNA to breast cancer cells. Mol Ther 21:185–191PubMedCentralPubMedCrossRefGoogle Scholar
  21. 21.
    Lamaziere A, Richard D, Barbe U et al (2013) Differential distribution of DHA-phospholipids in rat brain after feeding: a lipidomic approach. Prostaglandins Leukot Essent Fat Acids 84:7–11CrossRefGoogle Scholar
  22. 22.
    Ke N, Wang X, Xu X, Abassi YA (2011) The xCELLigence system for real-time and label-free monitoring of cell viability. Methods Mol Biol 740:33–43PubMedCrossRefGoogle Scholar
  23. 23.
    Thery C, Amigorena S, Raposo G, Clayton A (2006) Isolation and characterization of exosomes from cell culture supernatants and biological fluids. Curr Protoc Cell Biol: Chapter 3: Unit 3.22Google Scholar
  24. 24.
    Atay S, Gercel-Taylor C, Kesimer M, Taylor DD (2011) Morphologic and proteomic characterization of exosomes released by cultured extravillous trophoblast cells. Exp Cell Res 317:1192–1202PubMedCrossRefGoogle Scholar
  25. 25.
    Randle PJ (1998) Regulatory interactions between lipids and carbohydrates: the glucose fatty acid cycle after 35 years. Diabetes Metab Rev 14:263–283PubMedCrossRefGoogle Scholar
  26. 26.
    Roden M, Price TB, Perseghin G et al (1996) Mechanism of free fatty acid-induced insulin resistance in humans. J Clin Invest 97:2859–2865PubMedCentralPubMedCrossRefGoogle Scholar
  27. 27.
    Yang M, Wei D, Mo C et al (2013) Saturated fatty acid palmitate-induced insulin resistance is accompanied with myotube loss and the impaired expression of health benefit myokine genes in C2C12 myotubes. Lipids Health Dis 12:104PubMedCentralPubMedCrossRefGoogle Scholar
  28. 28.
    Yan B, Shi X, Zhang H et al (2014) Association of serum irisin with metabolic syndrome in obese Chinese adults. PLoS One 9:e94235PubMedCentralPubMedCrossRefGoogle Scholar
  29. 29.
    Trajkovic K, Hsu C, Chiantia S et al (2008) Ceramide triggers budding of exosome vesicles into multivesicular endosomes. Science (New York, N.Y.) 319:1244–1247Google Scholar
  30. 30.
    Wang G, Dinkins M, He Q et al (2012) Astrocytes secrete exosomes enriched with proapoptotic ceramide and prostate apoptosis response 4 (PAR-4): potential mechanism of apoptosis induction in Alzheimer disease (AD). J Biol Chem 287:21384–21395PubMedCentralPubMedCrossRefGoogle Scholar
  31. 31.
    Raiborg C, Stenmark H (2009) The ESCRT machinery in endosomal sorting of ubiquitylated membrane proteins. Nature 458:445–452PubMedCrossRefGoogle Scholar
  32. 32.
    Aicart-Ramos C, Valero RA, Rodriguez-Crespo I (2011) Protein palmitoylation and subcellular trafficking. Biochim Biophys Acta 1808:2981–2994PubMedCrossRefGoogle Scholar
  33. 33.
    Sajadi SM, Khoramdelazad H, Hassanshahi G et al (2013) Plasma levels of CXCL1 (GRO-alpha) and CXCL10 (IP-10) are elevated in type 2 diabetic patients: evidence for the involvement of inflammation and angiogenesis/angiostasis in this disease state. Clin Lab 59:133–137PubMedGoogle Scholar
  34. 34.
    Chavey C, Fajas L (2009) CXCL5 drives obesity to diabetes, and further. Aging 1:674–677PubMedCentralPubMedGoogle Scholar
  35. 35.
    Pickup JC, Chusney GD, Thomas SM, Burt D (2000) Plasma interleukin-6, tumour necrosis factor alpha and blood cytokine production in type 2 diabetes. Life Sci 67:291–300PubMedCrossRefGoogle Scholar
  36. 36.
    Hoene M, Runge H, Haring HU, Schleicher ED, Weigert C (2013) Interleukin-6 promotes myogenic differentiation of mouse skeletal muscle cells: role of the STAT3 pathway. Am J Physiol Cell Physiol 304:C128–C136PubMedCrossRefGoogle Scholar
  37. 37.
    Haddad F, Zaldivar F, Cooper DM, Adams GR (2005) IL-6-induced skeletal muscle atrophy. J Appl Physiol 98:911–917PubMedCrossRefGoogle Scholar
  38. 38.
    Rana S, Yue S, Stadel D, Zoller M (2012) Toward tailored exosomes: the exosomal tetraspanin web contributes to target cell selection. Int J Biochem Cell Biol 44:1574–1584PubMedCrossRefGoogle Scholar
  39. 39.
    Christianson HC, Svensson KJ, van Kuppevelt TH, Li JP, Belting M (2013) Cancer cell exosomes depend on cell-surface heparan sulfate proteoglycans for their internalization and functional activity. Proc Natl Acad Sci U S A 110:17380–17385PubMedCentralPubMedCrossRefGoogle Scholar
  40. 40.
    Alvarez-Erviti L, Seow Y, Yin H, Betts C, Lakhal S, Wood MJ (2011) Delivery of siRNA to the mouse brain by systemic injection of targeted exosomes. Nat Biotechnol 29:341–345PubMedCrossRefGoogle Scholar
  41. 41.
    Zhuang X, Xiang X, Grizzle W et al (2011) Treatment of brain inflammatory diseases by delivering exosome encapsulated anti-inflammatory drugs from the nasal region to the brain. Mol Ther 19:1769–1779PubMedCentralPubMedCrossRefGoogle Scholar

Copyright information

© The Author(s) 2014

Open Access This article is distributed under the terms of the Creative Commons Attribution License which permits any use, distribution, and reproduction in any medium, provided the original author(s) and the source are credited.

Authors and Affiliations

  • Hala Aswad
    • 1
  • Alexis Forterre
    • 1
  • Oscar P. B. Wiklander
    • 2
  • Guillaume Vial
    • 1
  • Emmanuelle Danty-Berger
    • 1
  • Audrey Jalabert
    • 1
  • Antonin Lamazière
    • 3
  • Emmanuelle Meugnier
    • 1
  • Sandra Pesenti
    • 1
  • Catherine Ott
    • 4
  • Karim Chikh
    • 1
  • Samir El-Andaloussi
    • 2
    • 5
  • Hubert Vidal
    • 1
  • Etienne Lefai
    • 1
  • Jennifer Rieusset
    • 1
  • Sophie Rome
    • 1
    • 6
  1. 1.CarMeN Laboratory (Inserm 1060, INRA 1397, INSA)University of Lyon, Faculté de Médecine Lyon-SudOullinsFrance
  2. 2.Department of Laboratory Medicine, Clinical Research Center, Karolinska InstitutetKarolinska University Hospital HuddingeHuddingeSweden
  3. 3.Laboratory of Mass Spectrometry, Inserm ERL 1157, CNRS UMR 7203 LBMSorbonne UniversitésParisFrance
  4. 4.Laboratoire Commun de Recherche HCL-bioMérieux Lyon-SudOullinsFrance
  5. 5.Department of Physiology, Anatomy and GeneticsUniversity of OxfordOxfordUK
  6. 6.CarMeN Laboratory (Inserm 1060, INRA 1397, INSA)University of Lyon, Faculté de Médecine Lyon-SudOullinsFrance

Personalised recommendations