Increased triacylglycerol - Fatty acid substrate cycling in human skeletal muscle cells exposed to eicosapentaenoic acid.

It has previously been shown that pretreatment of differentiated human skeletal muscle cells (myotubes) with eicosapentaenoic acid (EPA) promoted increased uptake of fatty acids and increased triacylglycerol accumulation, compared to pretreatment with oleic acid (OA) and palmitic acid (PA). The aim of the present study was to examine whether EPA could affect substrate cycling in human skeletal muscle cells by altering lipolysis rate of intracellular TAG and re-esterification of fatty acids. Fatty acid metabolism was studied in human myotubes using a mixture of fatty acids, consisting of radiolabelled oleic acid as tracer (14C-OA) together with EPA or PA. Co-incubation of myotubes with EPA increased cell-accumulation and incomplete fatty acid oxidation of 14C-OA compared to co-incubation with PA. Lipid distribution showed higher incorporation of 14C-OA into all cellular lipids after co-incubation with EPA relative to PA, with most markedly increases (3 to 4-fold) for diacylglycerol and triacylglycerol. Further, the increases in cellular lipids after co-incubation with EPA were accompanied by higher lipolysis and fatty acid re-esterification rate. Correspondingly, basal respiration, proton leak and maximal respiration were significantly increased in cells exposed to EPA compared to PA. Microarray and Gene Ontology (GO) enrichment analysis showed that EPA, related to PA, significantly changed i.e. the GO terms "Neutral lipid metabolic process" and "Regulation of lipid storage". Finally, an inhibitor of diacylglycerol acyltransferase 1 decreased the effect of EPA to promote fatty acid accumulation. In conclusion, incubation of human myotubes with EPA, compared to PA, increased processes of fatty acid turnover and oxidation suggesting that EPA may activate futile substrate cycling of fatty acids in human myotubes. Increased TAG-FA cycling may be involved in the potentially favourable effects of long-chain polyunsaturated n-3 fatty acids on skeletal muscle and whole-body energy metabolism.

Introduction

<pan class="Chemical">span class="Chemical">Fatty acidsn>n> (FA) have many diverse functions ranging from being structurally the main component in cellular membranes, to play a central role in metabolic processes and acting as signaling molecules [1]. <spapan>n class="Chemical">Long-chain <span class="Chemical">n-3 polyunsaturated fatty acids (n-3 FA), such as eicosapentaenoic acid (EPA, 20:5n-3) has been given much attention during recent decades for their potentially beneficial effects on human health and diseases [2]. Among other things, n-3 FA exerts favourable effects on energy metabolism, including improvements in lipid metabolism and increased thermogenesis, and prevention of obesity [3-6].

In the <pan class="Chemical">span class="Species">mammaliann>n> cell there are certain processes that are entirely uncoupled,”futile”, and therefore thermogenic or energy consuming. It is well known that brown adipose tissue is a highly thermogenic organ wherein <spapan>n class="Gene">uncoupling protein 1 play a central role [7]. In comparison, skeletal muscle mass in <span class="Species">human is much greater and potential futile cycling or uncoupling mechanisms in muscle could therefore have a substantially effect on regulating energy homeostasis as well as muscle function [7]. The energy lost by triacylglycerol—fatty acid (TAG—FA) cycling is an example of a substrate cycle in which esterification of TAG is followed by hydrolysis, leading to heat expenditure [8]. For instance, it has been observed that TAG—FA cycling plays an important role in controlling lipid metabolism in vivo in humans during and after exercise [9]. This cycle is also present in vitro in cells such as isolated human white adipocytes [10, 11], 3T3-L1 mice adipocytes [12] and C2C12 myotubes [13]. Further, it has been observed that a combined intervention using n-3 FA (docosahexaenoic acid (DHA) and EPA) and mild calorie restriction exerted synergism in the prevention of obesity in mice fed a high-fat diet. This was associated with strong hypolipidemic and insulin-sensitizing effects involving a futile substrate cycle in white adipose tissue based on lipolysis of intracellular TAG and re-esterification of fatty acids, in association with induction of mitochondrial oxidative phosphorylation capacity, fatty acid β-oxidation and increased energy expenditure [6, 14]. Thus, there are some mechanistic animal studies that suggest futile TAG—FA cycling induced by feeding n-3 FA/EPA, and that this might also occur in human skeletal muscle. We have previously observed that pretreatment of human skeletal muscle cells (myotubes) with EPA promoted uptake of FA, increased TAG accumulation and fatty acid β-oxidation while also stimulating glucose uptake and oxidation without changing insulin action [15, 16]. EPA was also shown to increase FA accumulation compared to palmitic acid (PA) and oleic acid (OA), to positively influence energy metabolism and metabolic switching of myotubes [15-17]. In addition, we have observed in human myotubes that the differences between OA and PA on their cellular accumulation and lipolysis were eliminated when co-incubated with EPA [18]. However, in that study we did not focus on the possibility of EPA to increase cellular TAG—FA cycling.

In the present study our focus was therefore to simultaneously examine the effect of pan class="Chemical">EPA compan>red to PA on real-time <span class="Chemical">fatty acid accumulation, lipolysis and re-esterification and on <span>n>n>n class="Chemical">fatty acid oxidation and mitochondrial function to further explore if an increased TAG—FA turnover, e.g. futile substrate cycling, may be present in skeletal muscle and possibly be involved in the favourable effects caused by EPA on cellular energy metabolism.

Materials and methods

Materials

Dulbecco´s modified Eagles medium (<pan class="Chemical">span class="Chemical">DMEM-Glutamaxn>n>), <spapan>n class="Chemical">DMEM without <span class="Chemical">phenol red, minimum essential media (αMEM), heat-inactivated fetal calf serum (FCS) and horse serum, and penicillin-streptomycin-amphotericin B were purchased from Gibco Invitrogen (Gibco, Life Technologies, Paisley, UK). Ultroser G was purchased from PALL Life Science (Port Washington, NY, US), insulin (Actrapid) from NovoNordisk (Bagsvaerd, Denmark), BSA (bovine serum albumin) (essentially fatty acid-free), Dulbecco’s phosphate-buffered saline (DPBS with Mg2+ and Ca2+), eicosapentaenoic acid (EPA, 20:5n-3), palmitic acid (PA, 16:0), oleic acid (OA, 18:1n-9), linoleic acid (LA, 18:2n-6), extracellular matrix gel, HEPES, A922500 (DGAT1 inhibitor) were all obtained from Sigma (St. Louis, MO, US).

<pan class="Chemical">span class="Chemical">[1-14C]oleic acidn>n> (58.2 mCi/mmol) was from PerkinElmer NEN (Boston, MA, US). Corning CellBIND tissue culture 96-well plates were obtained from Corning Life-Sciences (Schiphol-Rijk, The N<spapan>n class="Chemical">etherlands). Biocoat 25 cm2 cell flasks were from BD Biosciences (Franklin Lakes, NJ, US) and 12-well plates from Corning Life-Sciences (Lowell, MA, US). Ecoscint A scintillation solution was from National diagnostics (Hessle, England, UK). OptiPhase Supermix, UniFilter-96 GF/B, ScintiPlate-96 TC plates and all liquid scintillation was performed by 2450 MicroBeta2 scintillation counter, were obtained from PerkinElmer (Shelton, CT, US). Thin layer chromatography plates were purchased from Merck (Darmstadt, Germany). NuGO human Genechip arrays were obtained from Affymetrix (Santa Clara, CA, US). Seahorse XF96e analyzer, XF Base medium and XF Cell Mito Stress Test Kit were from Agilent (Wilmington, DE, US).

Methods

Cell culture

Satellite cells were isolated as previously described [19] from the <pan class="Chemical">span class="Species">m. obliquusn>n> internus abdominis, m. vastus lateralis or mm. interspinales of 9 healthy <spapan>n class="Species">donors. <span class="Species">Donors were both male (4) and female (5), 38 ± 5 years old, had a body mass index of 22.5 ± 1.1 kg/m2 and fasting glucose 5.3 ± 0.3 mM. The biopsies were obtained with informed consent and approved by the National Committee for Research Ethics, Norway (S-04133 REK sør, 2011/2007 REK sør-øst B, 2015/124 REK sør-øst B). Clonetics human myoblasts isolated from two healthy female donors were used for measurement of oxygen consumtion rate (Lonza, Cologne, Germany). Skeletal muscle cells from each donor (at passage 2–4) were cultured on 12- or 96-well plates or 25 cm2 flasks in DMEM-Glutamax (5.5 mM glucose), 2% fetal calf serum (FCS), 2% Ultroser G, 25 IU pencillin, 25 μg/ml streptomycin, and 1.25 μg/ml amphotericin B. At 70–80% confluence, the growth medium was replaced by DMEM-Glutamax supplemented with 2% FCS, 25 IU penicillin, 25 μg/ml streptomycin, 1.25 μg/ml amphotericin B, and 25 pM insulin to induce differentiation of myoblasts to form multinucleated myotubes. Experiments were performed after 6–7 days of differentiation. The cells were cultured in humidified 5% CO2 atmosphere at 37°C, and the media were changed every 2–3 days. Each experiment were performed with different donors, however not all donors were used in all experiments. For the oxygen consumption rate measurements, skeletal muscle cells cultured and differentiation into myotubes were initiated by replacing the growth medium by αMEM containing 2% horse serum.

Scintillation proximity assay (SPA)

Radiolabeled substpan class="Species">rates taken up and accumulated by adherent cells will be concentrated close to the scintillator embedded in the plastic bottom of each well (ScintiPlate-96 TC, PerkinElmer) and provide a stronger signal than the radiolabel dissolved in the medium alone [20]. Myotubes were cultured in 96-well ScintiPlate as described above with a mixture of 100 μM <span class="Chemical">fatty acids. Measurements of <span class="Chemical">fatty acids present in the cell by scintillation proximity assay (SPA) were performed in medium without phenol red with [1-14C]OA (0.5 μCi/ml, 9 μM) and non-labeled PA (16:0) and EPA (20:5, n-3) and were monitored for 0, 1, 2, 4, 6 and 24 h during the incubation. Thereafter, the media were changed to DPBS with 10 mM HEPES, 0.5% BSA, and 0.1 mM glucose and liquid scintillation measurements were monitored at 0, 1, 2, 4 and 6 h. The decline in [1-14C]OA present in the cells in the absence and presence of triacsin C (10 μM) was then studied. Triacsin C inhibits long-chain fatty acyl-CoA synthetase and will therefore inhibit, among other pathways, fatty acid re-esterification. Earlier reports in human skeletal myotubes have shown that TAG synthesis is efficiently blocked with incubation of 10 μM triacsin C (an inhibitor of fatty acid re-esterification and oxidation) for 3 h [21]. Re-esterification can be estimated as fatty acid present in the cells, calculating the difference with and without triacsin C present, as previously reported by Bezaire et al. [22]. The amount of radioactivity in the cells was related to total cell protein content measured according to Bradford [23].

Lipid distribution

Myotubes were treated with a mixture of 100 μM <pan class="Chemical">span class="Chemical">fatty acidsn>n> for 24 h. The mixture was trace amounts of [1-<spapan>n class="Chemical">14C]OA (0.5 μCi/ml, 9 μM) and non-labeled PA (16:0) and EPA (20:5, n-3). After incubation the myotubes were washed twice with PBS and harvested with two additions of 125 μl distilled <span class="Chemical">water. Cellular lipids were extracted as previously described [24] by extraction of homogenized cell fraction, separation of lipids by thin layer chromatography and quantification by liquid scintillation. A non-polar solvent mixture of hexane:ether:acetic acid (65:35:1) was used to separate the lipids. The amount of neutral lipids was related to total cell protein content.

Acid soluble metabolites

Myotubes were treated with a mixture of 100 μM <pan class="Chemical">span class="Chemical">fatty acidsn>n> for 24 h. The mixture was trace amounts of [1-<spapan>n class="Chemical">14C]OA (0.5 μCi/ml, 9 μM) and non-labeled PA (16:0) and EPA (20:5, n-3). Measurement of acid soluble metabolites (ASMs) was performed using a method modified from Skrede et al. [25]. Incubation media (100 μl) were transferred to Eppendorf tube, precipitated with 300 μl <span class="Chemical">HClO4 (1 M) and 30 μl BSA (6%), and centrifuged at 10.000 rpm (9600×g) for 10 min at 4°C. Then, 200 μl of the supernatant was counted by liquid scintillation. ASMs consist mainly of tricarboxylic acid cycle metabolites and reflect incomplete fatty acid oxidation, and were related to total cell protein content.

Substrate oxidation assay

Myotubes were cultured on 96-well CellBIND microplates. The cells were preincubated with 100 μM PA or pan class="Chemical">EPA for 24 h. Then [1-<span class="Chemical">14C]OA (0.5 μCi/ml, 100 μM) was given to the cells in <span>n>n>n class="Chemical">DPBS (with Mg2+ and Ca2+, Gibco) with 10 mM HEPES and 1 mM L-carnitine during the 4 h CO2 oxidation assessment. OA was bound to BSA at a ratio of 2.5:1. A 96-well UNIFILTER microplate (PerkinElmer) was mounted on top of the CellBIND plate as previously described [20], and the cells were incubated at 37°C for 4 h. The [14C]CO2 trapped in the filter was counted by liquid scintillation, and the result reflects CO2 production. The remaining cell-associated radioactivity (substrate accumulated) was also assessed by liquid scintillation, and both CO2 and cell-associated were related to total cell protein content.

Measurement of oxygen consumption rate

<pan class="Chemical">span class="Chemical">Oxygenn>n> consumption rates (OCR) were recorded in primary <spapan>n class="Species">human skeletal muscle cells from two different <span class="Species">donors (Lonza) on a Seahorse XF96e analyzer. One hour before the start of the recordings, the medium was changed to Seahorse XF Base medium, supplemented with 5 mM glucose, 2 mM glutamine, 1 mM sodium pyruvate and 0.5 mM HEPES, pH 7.4. Then, OCR was recorded three times at 6 min intervals at baseline, and following injections with 5 μM oligomycin, 3 μM FCCP and 4 μM rotenone/antimycin A (XF Cell Mito Stress Test Kit), respectively. Determinant of mitochondrial function (basal respiration, proton leak, maximal respiration, spare respiratory capacity, non-mitochondrial oxygen consumption and ATP production) were calculated by the Seahorse XF Mito Stress Test Report Generator using the following formulaes: basal respiration = last rate measurement before first injection–non-mitochondrial respiration rate; proton leak = minimum rate measurement after oligomycin injection–non-mitochondrial respiration; maximal respiration = maximum rate measurement after FCCP injection–non-mitochondrial respiration); spare respiratory capacity = maximal respiration–basal respiration; non-mitochondrial oxygen consumption = minimum rate measurement after rotenon/antimycin A injection; ATP production = last rate measurement before oligomycin injection–minimum rate measurement after oligomycin injection.

Gene expression and bioinformatics analysis

Previously performed array was submitted to Gene Expression Omnibus (accession number: GSE18589). In short, <pan class="Chemical">span class="Species">humann>n> myotubes from three <spapan>n class="Species">donors were cultured in 25 cm2 flasks and preincubated with 100 μM PA or EPA for 24 h. Thereafter the cells were harvested, RNA isolated and Affymetrix <span class="Species">human NuGO GeneChip arrays was run [17]. Here log2-transformed values were imported into Partek Genomics Suite 6.6. software for analysis, corrected for donor differences and 2-way ANOVA was performed. Genes with a p<0.05 for EPA vs PA were used for GO enrichment analysis.

Presentation of data and statistics

All values are reported as means ± SEM. The value n usually represents the number of different <pan class="Chemical">span class="Species">donorn>n>s used each with at least triplicate samples. Linear mixed models (LMM) (SPSS version 20 (IBM SPSS Statistics, Armonk, NY, US) were used to compare effects of different <spapan>n class="Chemical">fatty acids over time when SPA was used in accumulation, lipolysis and re-esterification experiments. A p-value <0.05 was considered significant. Student´s t-test was also used for comparison of EPA vs PA for single data points. Data underlying the findings are presented in S1 File.

Results

Fatty acid accumulation was increased in myotubes during co-incubation with eicosapentaenoic acid

Myotubes were treated with mixtures of 100 μM <pan class="Chemical">span class="Chemical">fatty acidsn>n> for 24 h and cell-associated radioactivity was measured during 24 h by scintillation proximity assay (SPA). By using non-labelled PA or EPA it was necessary to use a different <spapan>n class="Chemical">fatty acid as tracer, like [<span class="Chemical">14C]OA, to study the effect the two fatty acids had on lipid metabolism. The FA mixtures were trace amounts of [14C]OA (9 μM) and non-labeled PA (16:0) or EPA (20:5n-3). Co-incubation of human myotubes with eicosapentaenoic acid (EPA) markedly increased real-time accumulation of labeled OA as compared to co-incubation with PA at all time points measured (Fig 1A). The difference in accumulation between EPA and PA was established already after 1 h of co-incubation. For co-incubation experiments with [14C]OA and LA (18:2n-6) the effect on fatty acid accumulation was similar to the effect of PA (S1 Fig). Moreover, also when using [14C]PA as substrate EPA showed increased accumulation during co-incubation compared to OA and LA (S1 Fig).

Fig 1

Accumulation and distribution of oleic acid in myotubes when co-incubated with fatty acids.

Human myotubes were grown and differentiated in 96-well ScintiPlate or 12-well tissue culture plates. On day 6 of differentiation the myotubes were treated with a mixture of 100 μM fatty acids for 24 h. The mixture was trace amounts of [14C]OA (9 μM) and non-labeled PA (16:0) or EPA (20:5, n-3) (91 μM). (A) Cell-associated radioactivity was measured during 24 h by SPA. Real-time accumulation of radiolabel was monitored as described in Methods. Results represent mean ± SEM (nmol/mg protein) for n = 3 donors. Significant increase for EPA vs. PA (all-over effect). p<0.05 for EPA vs. PA, LMM statistical test (SPSS). (B-C) Lipids were separated by thin layer chromatography and quantified by liquid scintillation. Results are shown as mean ± SEM for absolute values, nmol/mg protein (B) and related to PA, % (C) from 4 individual experiments. *p<0.05 for EPA vs. PA (t-test). EPA, eicosapentaenoic acid; PA, palmitic acid; SPA, scintillation proximity assay; LMM, linear mixed model; FFA, free fatty acid; DAG, diacylglycerol; TAG, triacylglycerol; CE, cholesteryl ester; PL, phospholipids.

<pan class="Chemical">span class="Species">Humann>n> myotubes were grown and differentiated in 96-well ScintiPlate or 12-well tissue culture plates. On day 6 of differentiation the myotubes were treated with a mixture of 100 μM <spapan>n class="Chemical">fatty acids for 24 h. The mixture was trace amounts of [<span class="Chemical">14C]OA (9 μM) and non-labeled PA (16:0) or EPA (20:5, n-3) (91 μM). (A) Cell-associated radioactivity was measured during 24 h by SPA. Real-time accumulation of radiolabel was monitored as described in Methods. Results represent mean ± SEM (nmol/mg protein) for n = 3 donors. Significant increase for EPA vs. PA (all-over effect). p<0.05 for EPA vs. PA, LMM statistical test (SPSS). (B-C) Lipids were separated by thin layer chromatography and quantified by liquid scintillation. Results are shown as mean ± SEM for absolute values, nmol/mg protein (B) and related to PA, % (C) from 4 individual experiments. *p<0.05 for EPA vs. PA (t-test). EPA, eicosapentaenoic acid; PA, palmitic acid; SPA, scintillation proximity assay; LMM, linear mixed model; FFA, free fatty acid; DAG, diacylglycerol; TAG, triacylglycerol; CE, cholesteryl ester; PL, phospholipids.

Lipid distribution was changed after co-incubation with eicosapentaenoic acid

Myotubes were treated with the two mixtures of 100 μM <pan class="Chemical">span class="Chemical">fatty acidsn>n> as described above for 24 h and <spapan>n class="Chemical">lipid distribution was measured. EPA caused a significantly higher incorporation of labeled OA into <span class="Chemical">diacylglycerol (DAG) and triacylglycerol (TAG) in comparison with PA (Fig 1B). When relating the data to PA, EPA significantly increased the incorporation of labeled OA into all lipid classes (total cellular lipids, free fatty acids, phospholipids, DAG, TAG and cholesteryl ester) (Fig 1C). The greatest difference between EPA and PA was observed with a 3.9-fold increase for TAG and 3-fold for DAG, respectively. The level of unesterified oleic acid in the cells was also higher for EPA compared to PA (Fig 1C).

Lipolysis and fatty acid re-esterification was increased after co-incubation with eicosapentaenoic acid

After 24 h co-incubation with PA or pan class="Chemical">EPA and [<span class="Chemical">14C]OA total lipolysis (lipolysis in presence of <span>n>n>n class="Chemical">triacsin C) was measured by SPA at 0, 1, 2, 4 and 6 h. Total lipolysis was markedly increased by EPA compared to PA for all time points measured (Fig 2A). The relative decline in cell-associated [14C]OA after 24 h co-incubation was also significantly higher for EPA compared to PA indicating that lipolysis of [14C]OA was increased also when adjusting for increased accumulation of labeled OA in the presence of EPA (Fig 2B). After 24 h co-incubation with PA or EPA, re-esterification of [14C]OA was also increased by EPA during 2–6 h compared to PA (Fig 2C).

Fig 2

Lipolysis and re-esterification of oleic acid in myotubes after co-incubation with fatty acids.

Human myotubes were grown and differentiated in 96-well ScintiPlate tissue culture plates. On day 6 of differentiation the myotubes were treated with a mixture of 100 μM fatty acids for 24 h. The mixture was trace amounts of [14C]OA (9 μM) and non-labeled PA or EPA (20:5, n-3) (91 μM). (A) Total lipolysis (lipolysis measured in presence triacsin C, 10 μM) of cell-associated [14C]OA at 1, 2, 4, and 6 h after 24 h pretreatment. (B) Total lipolysis presented as relative decline (i.e. data normalized to cell-associated radioactivity at zero time) in cell-associated [14C]OA at 1, 2, 4, and 6 h after 24 h pretreatment. (C) Re-esterification of [14C]OA, calculated as the difference between lipolysis measured at 1, 2, 4, and 6 h by SPA in the presence or absence of triacsin C (10 μM). Results represent mean ± SEM as nmol/mg protein (A, C) and relative decline in cell-associated radioactivity (B) for n = 3 donors. Significant increased lipolysis, decline and re-esterification for EPA vs. PA. p<0.05 for EPA vs. PA (all-over effect), LMM statistical test (SPSS). EPA, eicosapentaenoic acid; PA, palmitic acid; SPA, scintillation proximity assay; LMM, linear mixed model.

<pan class="Chemical">span class="Species">Humann>n> myotubes were grown and differentiated in 96-well ScintiPlate tissue culture plates. On day 6 of differentiation the myotubes were treated with a mixture of 100 μM <spapan>n class="Chemical">fatty acids for 24 h. The mixture was trace amounts of [<span class="Chemical">14C]OA (9 μM) and non-labeled PA or EPA (20:5, n-3) (91 μM). (A) Total lipolysis (lipolysis measured in presence triacsin C, 10 μM) of cell-associated [14C]OA at 1, 2, 4, and 6 h after 24 h pretreatment. (B) Total lipolysis presented as relative decline (i.e. data normalized to cell-associated radioactivity at zero time) in cell-associated [14C]OA at 1, 2, 4, and 6 h after 24 h pretreatment. (C) Re-esterification of [14C]OA, calculated as the difference between lipolysis measured at 1, 2, 4, and 6 h by SPA in the presence or absence of triacsin C (10 μM). Results represent mean ± SEM as nmol/mg protein (A, C) and relative decline in cell-associated radioactivity (B) for n = 3 donors. Significant increased lipolysis, decline and re-esterification for EPA vs. PA. p<0.05 for EPA vs. PA (all-over effect), LMM statistical test (SPSS). EPA, eicosapentaenoic acid; PA, palmitic acid; SPA, scintillation proximity assay; LMM, linear mixed model.

Fatty acid beta-oxidation was increased during co-incubation with eicosapentaenoic acid

Myotubes were co-incubated with the same mixtures of <pan class="Chemical">span class="Chemical">fatty acidsn>n> as above. Cell culture medium was collected at 24 h and <spapan>n class="Chemical">fatty acid oxidation measured as acid-soluble metabolites (ASMs), which give an indication of <span class="Chemical">fatty acid β-oxidation. There was a 60% increase in formation of ASM in the presence of EPA when compared to PA (Fig 3A).

Fig 3

Oleic acid accumulation and oxidation after preincubation with fatty acids.

(A) OA β-oxidation during co-incubation with fatty acids. Human myotubes were grown and differentiated in 12-well tissue culture plates. On day 6 of differentiation the myotubes were treated with a mixture of 100 μM fatty acids for 24 h. The mixture was trace amounts of [14C]OA (9 μM) and non-labeled PA (16:0) or EPA (20:5, n-3) (91 μM). Figure shows formation of acid-soluble metabolites (ASMs) in myotubes after 24 h. Results are shown as mean ± SEM (related to PA, %) from 4 individual experiments. Absolute values (mean ± SEM); PA: 24.5 ± 4.8; EPA: 41.3 ± 8.7 nmol/mg cell protein. (B) OA accumulation and complete oxidation after preincubation with fatty acids. Human myotubes were treated with fatty acids (100 μM EPA or PA) for 24 h. Thereafter, accumulation (cell-associated) and complete oxidation (CO2 production) from added [14C]OA (100 μM) was measured for 4 h. Results represent mean ± SEM, n = 3. Absolute values (mean ± SEM) for PA; CO2: 15.9 ± 2.3; Cell-associated: 49.9 ± 10.9 nmol/mg cell protein. *p<0.05 for EPA vs. PA (t-test). CA, cell-associated; EPA, eicosapentaenoic acid; PA, palmitic acid.

(A) OA β-oxidation during co-incubation with <pan class="Chemical">span class="Chemical">fatty acidsn>n>. <spapan>n class="Species">Human myotubes were grown and differentiated in 12-well tissue culture plates. On day 6 of differentiation the myotubes were treated with a mixture of 100 μM <span class="Chemical">fatty acids for 24 h. The mixture was trace amounts of [14C]OA (9 μM) and non-labeled PA (16:0) or EPA (20:5, n-3) (91 μM). Figure shows formation of acid-soluble metabolites (ASMs) in myotubes after 24 h. Results are shown as mean ± SEM (related to PA, %) from 4 individual experiments. Absolute values (mean ± SEM); PA: 24.5 ± 4.8; EPA: 41.3 ± 8.7 nmol/mg cell protein. (B) OA accumulation and complete oxidation after preincubation with fatty acids. Human myotubes were treated with fatty acids (100 μM EPA or PA) for 24 h. Thereafter, accumulation (cell-associated) and complete oxidation (CO2 production) from added [14C]OA (100 μM) was measured for 4 h. Results represent mean ± SEM, n = 3. Absolute values (mean ± SEM) for PA; CO2: 15.9 ± 2.3; Cell-associated: 49.9 ± 10.9 nmol/mg cell protein. *p<0.05 for EPA vs. PA (t-test). CA, cell-associated; EPA, eicosapentaenoic acid; PA, palmitic acid.

Cell-associated fatty acid and complete fatty acid oxidation were increased in myotubes after incubation with eicosapentaenoic acid

<pan class="Chemical">span class="Chemical">Oleic acidn>n> metabolism was also examined after exposure to 100 μM EPA or PA for 24 h (Fig 3B). Cell-associated and oxidation to <spapan>n class="Chemical">carbondioxide (<span class="Chemical">CO2) after 4 h incubation with [14C]OA was increased by 70% and 48% after pretreatment with EPA in comparison with PA.

Mitochondrial respiration was increased after incubation with eicosapentaenoic acid

<pan class="Chemical">span class="Species">Miton>n>chondrial respiration was determined in <spapan>n class="Species">human skeletal muscle cells using an extracellular flux analyzer (Fig 4A). Basal respiration, proton leak and maximal respiration were significantly increased (by means 30, 30 and 19%, respectively) in cells exposed for 24 h to 100 μM EPA compared to PA (Fig 4B), while <span class="Chemical">ATP production tended to increase (mean increase 43%, p = 0.055).

Fig 4

Mitochondrial function after preincubation with fatty acids.

Human skeletal muscle cells were grown in 96-well Seahorse tissue culture plates, and treated with 100 μM of PA or EPA for 24 h, before measurement of oxygen consumption rate (OCR) with the Seahorse XF96e analyzer. (A) OCR time curve from an experiment with one of two donors. (B) OCR parameter calculations by the Seahorse XF Mito Stress Test Report Generator from experiments with two different donors (n = 8). Results represent mean ± SEM. *p<0.05 for EPA vs. PA (t-test). EPA, eicosapentaenoic acid; PA, palmitic acid; Oligo, oligomycin; FCCP, carbonyl cyanide-p-trifluoromethoxyphenylhydrazone; Rot, rotenone, AA, antimycin A.

<pan class="Chemical">span class="Species">Humann>n> skeletal muscle cells were grown in 96-well Sea<spapan>n class="Species">horse tissue culture plates, and treated with 100 μM of PA or EPA for 24 h, before measurement of <span class="Chemical">oxygen consumption rate (OCR) with the Seahorse XF96e analyzer. (A) OCR time curve from an experiment with one of two donors. (B) OCR parameter calculations by the Seahorse XF Mito Stress Test Report Generator from experiments with two different donors (n = 8). Results represent mean ± SEM. *p<0.05 for EPA vs. PA (t-test). EPA, eicosapentaenoic acid; PA, palmitic acid; Oligo, oligomycin; FCCP, carbonyl cyanide-p-trifluoromethoxyphenylhydrazone; Rot, rotenone, AA, antimycin A.

Microarray analysis of gene expression

Microarray analysis was performed to examine wh<pan class="Chemical">span class="Chemical">ethern>n> treatment for 24 h with 100 μM EPA regulated gene expression differently in the myotubes compared to 100 μM PA. Gene Ontology (GO) enrichment analysis revealed that, among others, the GO terms”Neutral <spapan>n class="Chemical">lipid metabolic process” (GO:0006638) and”Regulation of <span class="Chemical">lipid storage” (GO:0010883) were significantly changed (p<0.05) by EPA compared to PA (Fig 5). Genes involved in the GO terms in Fig 5 are listed in S1 Table. All genes that were differently regulated (EPA vs. PA) are listed in S2 Table.

Fig 5

GO enrichment analysis.

Myotubes were incubated with PA or EPA (100 μM) for 24 h and then harvested for RNA isolation. Affymetrix human NuGO GeneChip arrays was used to measure gene expression and analysis performed in Partek Genomics Suite 6.6 software. GO enrichment analysis revealed that the GO terms”Neutral lipid metabolic process” (GO:0006638, upper 3) and”Regulation of lipid storage” (GO:0010883, lower 4) were changed significantly (p<0.05) by EPA vs. PA. They are presented with % of genes up- or down-regulated in each child GO term and genes are presented in S1 Table. EPA, eicosapentaenoic acid; PA, palmitic acid.

Myotubes were incubated with PA or pan class="Chemical">EPA (100 μM) for 24 h and then harvested for RNA isolation. Affymetrix <span class="Species">human NuGO GeneChip arrays was used to measure gene expression and analysis performed in Partek Genomics Suite 6.6 software. GO enrichment analysis revealed that the GO terms”Neutral <span>n>n>n class="Chemical">lipid metabolic process” (GO:0006638, upper 3) and”Regulation of lipid storage” (GO:0010883, lower 4) were changed significantly (p<0.05) by EPA vs. PA. They are presented with % of genes up- or down-regulated in each child GO term and genes are presented in S1 Table. EPA, eicosapentaenoic acid; PA, palmitic acid.

Diacylglycerol acyltransferase 1 inhibition reduced the effect of eicosapentaenoic acid to promote lipid accumulation

To further look into mechanisms for increased TAG accumulation by pan class="Chemical">EPA compan>red to PA we studied how the effect of a specific inhibitor of <span class="Gene">diacylglycerol acyltransferase 1 (A922500 [26]) affected <span>n>n>n class="Chemical">lipid accumulation and turnover for 4 h (Fig 6A) or 24 h (Fig 6B). Diacylglycerol acyltransferase (DGAT) catalyse the last and dedicated step in TAG synthesis, the esterification of fatty acyl-CoA to DAG [27]. By using an inhibitor of DGAT we could determine if the effect of EPA on skeletal muscle cells was mechanistically linked to TAG accumulation and turnover. This inhibitor has previously been used in experiments with human myotubes showing 90% decrease in incorporation of [14C]OA into TAG [18]. DGAT1 inhibition significantly reduced cell-associated [14C]OA in myotubes both after preincubation with EPA (Fig 6A) and during co-incubation with EPA (Fig 6B), whereas there was no effect when cells were treated with PA.

Fig 6

Effect of DGAT1 inhibitor on cell-associated and accumulated oleic acid.

(A) Human myotubes were treated with fatty acids (100 μM EPA or PA) for 24 h. Cell-associated [14C]OA (100 μM) was measured after 4 h with and without DGAT1 inhibitor (D1i, A922500, 1 μM). Results represent mean ± SEM, from experiments with 4 different donors and 4–8 parallels (n = 26). Cell-associated PA (100%): 53.8 ± 4.0 nmol/mg cell protein. (B) Human myotubes were grown and differentiated in 96-well ScintiPlate tissue culture plates. On day 6 of differentiation the myotubes were treated with a mixture of 100 μM fatty acids for 24 h and cell-associated radioactivity was measured during 24 h by SPA. The mixture was trace amounts of [14C]OA (9 μM) and non-labeled PA or EPA (91 μM). DGAT1 inhibitor was also added for 24 h. Results represent mean ± SEM from experiments with 3 different donors and 8 parallels (n = 24). Accumulated PA (100%): 156 ± 13.8 nmol/mg cell protein. #p<0.05 for D1i inhibitor vs. control in EPA-treated cells (t-test). EPA, eicosapentaenoic acid; PA, palmitic acid; D1i, diacylglycerol acyltransferase 1 inhibitor.

(A) <pan class="Chemical">span class="Species">Humann>n> myotubes were treated with <spapan>n class="Chemical">fatty acids (100 μM EPA or PA) for 24 h. Cell-associated [<span class="Chemical">14C]OA (100 μM) was measured after 4 h with and without DGAT1 inhibitor (D1i, A922500, 1 μM). Results represent mean ± SEM, from experiments with 4 different donors and 4–8 parallels (n = 26). Cell-associated PA (100%): 53.8 ± 4.0 nmol/mg cell protein. (B) Human myotubes were grown and differentiated in 96-well ScintiPlate tissue culture plates. On day 6 of differentiation the myotubes were treated with a mixture of 100 μM fatty acids for 24 h and cell-associated radioactivity was measured during 24 h by SPA. The mixture was trace amounts of [14C]OA (9 μM) and non-labeled PA or EPA (91 μM). DGAT1 inhibitor was also added for 24 h. Results represent mean ± SEM from experiments with 3 different donors and 8 parallels (n = 24). Accumulated PA (100%): 156 ± 13.8 nmol/mg cell protein. #p<0.05 for D1i inhibitor vs. control in EPA-treated cells (t-test). EPA, eicosapentaenoic acid; PA, palmitic acid; D1i, diacylglycerol acyltransferase 1 inhibitor.

Discussion

In the present study our focus was to study the effects of <pan class="Chemical">span class="Chemical">fatty acidsn>n> to modify cellular TAG—FA cycling in <spapan>n class="Species">human skeletal muscle cells. Based on previous studies with different <span class="Chemical">fatty acids we decided to examine the effect of eicosapentaenoic acid (EPA) compared to palmitic acid (PA) on real-time fatty acid accumulation, lipolysis, re-esterification and β-oxidation during co-incubation with trace amounts of labeled oleic acid (OA) in myotubes. We observed an enhanced accumulation, lipolysis and re-esterification of [14C]OA by co-incubation with EPA when compared to PA. Lipid distribution showed that EPA promoted increased incorporation of [14C]OA into various lipid classes, especially into DAG and TAG, and the level of unesterified [14C]OA in the cells was also higher in presence of EPA compared to PA. Furthermore, an increased fatty acid β-oxidation was seen after co-incubation with EPA. Preincubation of myotubes with EPA also increased basal and maximal mitochondrial respiration and proton leak, as well as complete oxidation of [14C]OA. Gene expression studies indicated that EPA, compared to PA, did alter the expression of genes involved in neutral lipid metabolism and lipid storage. Finally, the effect of EPA to promote fatty acid accumulation was reduced by inhibition of diacylglycerol acytransferase 1 (DGAT1), which catalyzes the conversion of DAG and fatty acyl-CoA to TAG.

The effect of pan class="Chemical">EPA to increase uptake of <span class="Chemical">fatty acids acutely (during 4 h) after pretreatment, as well as during co-incubation is in accordance with our previous observations that EPA promoted accumulation of labeled <span>n>n>n class="Chemical">fatty acids such as OA and PA [15, 16, 18]. In the present study this effect was established already after 1 h of co-incubation. Previously, we have seen that chronic incubation of human myotubes with EPA for 24 h or 4 days, respectively, promoted uptake of both labeled OA and PA, increased TAG accumulation and fatty acid β-oxidation and reduced the levels of acyl-CoA [16]. Consistent with this, treatment with EPA increased the number of lipid droplets compared to PA in another study on human myotubes [17]. Furthermore, we have also observed that the differences between OA and PA on their cellular accumulation and lipolysis were eliminated in human myotubes when co-incubated with EPA [18].

Here we in addition observed indications of an increased TAG—FA cycling after pan class="Chemical">EPA exposure in myotubes. The observation that n>n class="Chemical">EPA increased lipolysis and re-esterification might be a result of a higher accumulation of TAG. However, EPA also caused increased lipolysis compared to PA when adjusting for the amount of accumulated <span class="Chemical">fatty acid in the cells. Moreover, <span class="Chemical">fatty acid re-esterification was simultaneously increased by EPA. Combined with co-incubation data this indicates a higher enrichment in TAG as well as increased turnover of labeled fatty acids in the presence of EPA when compared to PA, but also during co-incubation with other fatty acids such as LA and OA. It was shown in vivo in mice that n-3 FA supplementation to a high-fat saturated diet modulated metabolic pathways of TAG synthesis, lipolysis, fatty acid oxidation and thermogenesis in skeletal muscle at mRNA and protein levels suggesting activation of TAG—FA substrate cycling [28]. To study TAG accumulation and turnover in more detail we blocked the final step in the synthesis of TAG using an inhibitor of DGAT1. Our data showed that DGAT1 inhibition counteracted EPA´s effect to promote OA accumulation, indicating that the effect of EPA on fatty acid metabolism and lipid turnover may be dependent of TAG synthesis and possibly be mediated through increased TAG—FA cycling. Accordingly, there was no effect of DGAT1 inhibition on OA accumulation after co-incubation with PA. In another study, increased fatty acid uptake was shown to increase futile cycling of fatty acids into TAG in C2C12 mice skeletal muscle cells [13]. They observed that cycling of fatty acids was important for maintaining a low TAG content and insulin responsiveness of the cells [13]. Futile cycling of TAG has been described in adipocytes by induction of glycerol kinase and glycerogenesis mediated by PGC-1 alpha and PPARs activation [11, 12, 29]. It is known that n-3 fatty acids activates PPAR isoforms [30-32], although their affinity for the receptors may vary. However, we have previously observed that various fatty acids (PA, OA, LA and EPA) increase mRNA expressions of PPAR-regulated genes in skeletal muscle cells compared to a fatty acid-free control [17]. This is likely because both saturated and unsaturated fatty acids are ligands for PPAR activation [33], which further might explain why there was only small effects on PPAR-regulated genes in our microarray gene expression analysis when EPA was compared with PA.

In the present study <pan class="Chemical">span class="Species">miton>n>chondrial respiration and proton leak was increased in myotubes after exposure to EPA for 24 h. We have previously observed that pretreatment of <spapan>n class="Species">human myotubes with EPA promoted <span class="Chemical">fatty acid β-oxidation, while also stimulating glucose transport and oxidation compared to OA [15, 16]. There are also in vivo studies that suggest increased skeletal muscle mitochondrial function after n-3 FA supplementation [28, 34]. Ten weeks of EPA supplementation in aging mice improved mitochondrial oxidative capacity and bioenergetic efficiency in skeletal muscle, however supplementation of another n-3 FA, docosahexaenoic acid (DHA), had no effect [34]. In a study in older human adults, 16 weeks of n-3 PUFA supplementation did not change skeletal muscle mitochondrial respiration, but reduced mitochondrial ROS production [35], neither did supplementation of EPA plus DHA for 6 months change muscle mitochondrial function in insulin-resistent non-diabetic humans [36]. However, in young, healthy adults 12 weeks of EPA plus DHA supplementation improved mitochondrial membrane composition and ADP kinetics in skeletal muscle [37].

In our study, we compared expression of genes induced by pan class="Chemical">EPA related to PA, and the fold changes found (S2 table) are in general small (e.g. carnitine pal<span class="Species">mitoyltransferase 1A (CPT1A), perilipin 2 (PLIN2) and monoglyceride lipase (MGLL) with fold change 1.2–1.4) or opposite of expected (e.g. cluster of differentiation 36/<span>n>n>n class="Chemical">fatty acid translocase (CD36) fold change -1.33). Therefore, GO enrichment analysis from the microarray mRNA expression analysis was exerted to get a more overall picture of the biological processes that may be modified differently by the two fatty acids. GO enrichment analysis revealed that EPA compared to PA enhanced only some biological processes involved in neutral lipid biosynthesis and catabolic processes. Among GO terms under “Regulation of lipid storage”, “Regulation of sequestering of triglyceride” was increased and “Negative regulation of lipid storage” was decreased by EPA. Among GO terms under “Neutral lipid metabolic process”, both “Neutral lipid biosynthetic process” and “Neutral lipid catabolic process” were increased by EPA. This, as well as the acute effect of EPA to promote fatty acid accumulation during co-incubation, suggest that the effects of EPA on lipid turnover and oxidation in part may be mediated by changes in gene expression and that non-genomic mechanisms also may be involved [38, 39]

Skeletal muscle is the largest organ and a major contributor to basal metabolic pan class="Species">rate. Increasing energy expenditure in muscle through non-shivering thermogenic mechanisms such as TAG—FA cycling could substantially affect whole body metabolism and body <span class="Disease">weight gain [40, 41]. Although heat production from muscle has long been recognized as a thermogenic mechanism, wh<span>n>n>n class="Chemical">ether muscle can produce heat independently of contraction remains controversial. Thus, current evidence does not indicate a clear role of skeletal muscle in non-shivering thermogenesis, which may be due to lack of methods allowing measurement of these processes separately from other muscle thermogenic processes [40]. We believe our cell model is a valuble tool to study some of these procesess in more detail.

In conclusion, findings from this study suggest an increased TAG—FA turnover i.e. futile substpan class="Species">rate cycling in <span class="Species">human myotubes induced by EPA, combined with increased <span>n>n>n class="Chemical">fatty acid oxidation and mitochondrial function. Our data indicate that enhancing these processes could be of importance for the potential favourable effects of long-chain n-3 fatty acids on skeletal muscle as well as whole-body energy metabolism.

Data underlying the findings.

Absolute data from each experiment.

(XLSX)

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Real time fatty acid accumulation in myotubes when co-incubated with various fatty acids.

<pan class="Chemical">span class="Species">Humann>n> myotubes were grown and differentiated in 96-well ScintiPlate. On day 6 of differentiation the myotubes were treated with a mixture of 100 μM <spapan>n class="Chemical">fatty acids for 24 h and cell-associated (CA) radioactivity was measured during 24 h by SPA. The mixture was trace amounts of [<span class="Chemical">14C]OA (9 μM) and non-labeled PA (16:0) and LA (18:2, n-6) (A), or or trace amounts of [14C]PA (9 μM) and non-labeled OA (18:1, n-9), LA (18:2, n-6) and EPA (20:5, n-3) (B). Results represent mean ± SEM for n = 5–7 donors related to PA or OA at 24 h in percent (70 ± 17 nmol/mg for PA (A) and 107 ± 54 nmol/mg for OA (B)). Significant increase for EPA vs. OA/LA (all-over effect). p<0.05 for EPA vs. OA/LA, LMM statistical test (SPSS). EPA, eicosapentaenoic acid; LA, linoleic acid; OA, oleic acid; PA, palmitic acid; SPA, scintillation proximity assay; LMM, linear mixed model.

(TIF)

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Genes changed by EPA vs. PA in myotubes.

Genes in the GO terms”Neutral <pan class="Chemical">span class="Chemical">lipidn>n> metabolic process” (GO:0006638) and”Regulation of <spapan>n class="Chemical">lipid storage” (GO:0010883) that is changed (p<0.05) for EPA vs. PA are presented. Myotubes from three <span class="Species">donors were incubated with PA or EPA (100 μM) for 24 h and then harvested for RNA isolation. Gene expression was measured by Affymetrix human NuGO GeneChip arrays and analysis performed in Partek Genomics Suite 6.6. software. EPA, eicosapentaenoic acid; PA, palmitic acid.

(DOCX)

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Genes that is changed (p<0.05) for pan class="Chemical">EPA vs. PA are presented. Myotubes from three <span class="Species">donors were incubated with PA or EPA (100 μM) for 24 h and then harvested for RNA isolation. Gene expression was measured by Affymetrix <span>n>n>n class="Species">human NuGO GeneChip arrays and analysis performed in Partek Genomics Suite 6.6. software. EPA, eicosapentaenoic acid; PA, palmitic acid.

(XLSX)

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