Introduction

Obesity is a major health problem in the industrialized world, which has reached epidemic proportions globally. Its high prevalence is a result of changes in lifestyle, decreased physical activity and socioeconomic development, among other factors. Moreover, obesity is a complex multi-factorial, chronic disease, which is considered to be a risk factor for the genesis or development of various diseases which include hypertension, type 2 diabetes, coronary heart disease and respiratory complications (Barness 2007; Kopelman 2000). In this context, scientific research is constantly seeking to identify for new molecules that could be used as dietary functional ingredients in the fight against this disease and its co-morbidities. Among them, flavonoids represent a group of molecules of increasing interest.

Flavonoids belong to a group of natural substances, which have a variable phenolic structure and are found in fruit, vegetables, tea and wine. These natural foods were known for their beneficial effects on health long before flavonoids were isolated as the effective compounds. Flavonoids have a basic chemical structure of diphenylpropanes (C6-C3-C6) and are most often found attached to sugar (glycosides), but they can also be aglycones. Quercetin, which is found in abundance in onions, broccoli, tomatoes, apples and berries, is the most abundant flavonoid (Somerset and Johannot 2008).

It has been reported that quercetin exhibits a wide range of biological functions, including antioxidant, anticarcinogenic and anti-inflammatory activities (Bischoff 2008; Zhang et al. 2011; Chirumbolo 2010; Jung et al. 2013). More recently, beneficial effects on blood pressure and heart disease have been described (Perez-Vizcaino et al. 2009; Han et al. 2009; Jung et al. 2013). With regard to obesity, very little work has been carried out to date. As far as glycemic control is concerned, quercetin has been reported to improve diabetic status in animal models of either type 1 or type 2 diabetes (Aguirre et al. 2011).

The first aim of the present work was to gain more insight into the effects of quercetin on fat accumulation in adipose tissue and on glycemic control in rats fed an obesogenic diet, in order to establish whether this molecule can be useful in the prevention of obesity and insulin resistance related to it. A second aim was to determine the potential involvement of muscle fatty acid oxidation in the effect of quercetin on glycemic control.

Materials and methods

Diets and experimental design for the in vivo study

The study was conducted with eighteen 6-week-old male Wistar rats purchased from Harlan Ibérica (Barcelona, Spain), and took place in accordance with the institution’s guide for the care and use of laboratory animals (CUEID CEBA/30/2010).

Rats were individually housed in polycarbonate metabolic cages (Techniplast Gazzada, Guguggiate, Italy) and placed in an air-conditioned room (22 ± 2 °C) with a 12-h day-night rhythm. After a 6-day adaptation period, rats were randomly distributed in two groups (n = 9 per group): a control group and a quercetin group. Both groups were fed a commercial high-fat, high-sucrose diet (Harlan Ibérica; ref. TD. 06415) for 6 weeks. This diet was high in fat (225 g/kg) and sucrose (200 g/kg) and was either supplemented with quercetin (Sigma-Aldrich, St. Louis, MO, USA) or not supplemented. For dietary supplementation, quercetin was added to the diet daily in amounts that assured a dose of 30 mg/kg body weight/d (equivalent approximately to 0.045 % of quercetin in the diet). All animals had free access to food and water. Body weight and food intake were recorded on a daily basis.

At the end of the experimental period, animals were exsanguinated by cardiac puncture under anesthesia (chloral hydrate). Adipose tissue from different anatomical locations (epididymal, perirenal, mesenteric and subcutaneous) and gastrocnemius muscles were dissected, weighted, immediately frozen and stored at −80 °C for further analysis.

Glucose tolerance test

One week before killing, all rats were deprived of food, though not of water, 12 h before starting the experiment. Blood samples were obtained from the tail vein for the determination of basal glucose and insulin levels. Glucose load was injected intraperitoneally at the dose of 2 g/kg body weight, and glycemia was determined from the tail vein after 30, 60, 90 and 120 min. The area under the curve (AUC) was calculated by trapezoidal method (Tai 1994).

Serum analysis

Serum was obtained from blood samples after centrifugation (1,000g for 10 min at 4 °C). Commercial kits were employed to measure serum parameters: glucose (BioSystems, Barcelona, Spain), insulin (Linco, St. Charles, MO, USA), fructosamine (Spinreact, Sant Esteve de Bas, Spain) and free fatty acids (Roche, Penzberg, Germany).

The homeostatic model assessment for insulin resistance (HOMA-IR) was calculated from basal insulin and glucose values using Matthews’ formula (Matthews et al. 1985):

$${\text{HOMA-IR}} = {{\left[ {{\text{Fasting glucose }}\left( {{\text{mmol}}/{\text{L}}} \right) \times {\text{fasting insulin }}\left( {{\text{mU}}/{\text{L}}} \right)} \right]} \mathord{\left/ {\vphantom {{\left[ {{\text{Fasting glucose }}\left( {{\text{mmol}}/{\text{L}}} \right) \times {\text{fasting insulin }}\left( {{\text{mU}}/{\text{L}}} \right)} \right]} {22.5}}} \right. \kern-0pt} {22.5}}$$

Lipoprotein lipase and lipogenic activities in white adipose tissue

For heparin-releasable lipoprotein lipase (HR-LPL) activity determination, 400 mg of epididymal adipose tissue was incubated in 400 μL of KRP (Krebs–Ringer Phosphate) buffer, containing 2 μg/mL of heparine, at 37 °C during 45 min. Aliquots of this medium were incubated for 5 min at 37 °C with 1 mg dibutyryl fluorescein, 5 mL ethyleneglycol monoethyl ether, 3 mM NaH2PO4 and 50 mM Na2HPO4 with 2.5 M NaCl, or not, and then, the reaction was stopped in ice. Finally, fluorescence was measured. HR-LPL activity was calculated by subtracting non-LPL lipolytic activity in the presence of NaCl from the total lipolytic activity, determined without NaCl, and was expressed as nmol fluorescein released per minute per gram of tissue.

For lipogenic enzyme analysis purposes, 1 g of epididymal adipose tissue was homogenized in 3.0 mL of buffer (pH 7.6) containing 150 mM KCl, 1 mM MgCl2, 10 mM N-acetyl-cysteine and 0.5 mM dithiothreitol. After centrifugation at 100,000g for 40 min at 4 °C, the supernatant fraction was used for the quantification of enzyme activities. Fatty acid synthase (FAS), glucose-6-phosphate dehydrogenase (G6PDH) and malic enzyme (ME) activities were measured as previously described (Zabala et al. 2006). Enzyme activities were expressed as follows: nmol NADPH consumed per minute per g of tissue for FAS, and nmol NADPH produced per minute per g of tissue for G6PDH and ME.

Acetyl CoA carboxylase (ACC) activity was measured by using the ratio phosphorylated ACC/total ACC. The amounts of both ACC-phosphorylated and total ACC were measured by Western blot. To this end, 100 mg of epididymal adipose tissue was homogenated in 500 μL of cellular PBS (pH 7.4), containing nuclease inhibitors, 100 mM phenylmethylsulfonyl fluoride and 100 mM iodoacetamide. Homogenates were centrifuged at 500g for 10 min at 4 °C. Protein concentrations in homogenates were measured by using Bradford method (Bradford 1976) using bovine serum albumin as standard.

Immunoblot analyses were performed using 10 μg epididymal adipose tissue extracts separated by electrophoresis in a 10 % SDS–polyacrylamide gel and transferred to PVDF membranes. The membranes were then blocked with 5 % caseine PBS–Tween buffer for 2 h at room temperature. Subsequently, they were blotted with the appropriate antibodies overnight at 4 °C. ACC levels were detected via specific antibodies for total ACC (1:1,000), phosphorylated ACC (1:1,000) (Cell Signaling Technology, Danvers, MA, USA) and β-actin (1:5,000) (Sigma, St. Louis, MO, USA). Afterward, polyclonal mouse anti-β-actin and rabbit anti-ACC antibody (1:5,000) (Sigma, St. Louis, MO, USA) were incubated for 2 h at room temperature. First, total ACC was measured, and then phosphorylated ACC was determined by stripping and reprobing the blot. The bound antibodies were visualized by an ECL system (Thermo Fisher Scientific Inc., Rockford, IL, USA) and quantified by a ChemiDoc MP imaging system (Biorad, Hercules, Ca, USA). β-Actin was used as a loading control to normalize the results.

Triacylglycerols content in skeletal muscle

Total lipids were extracted from muscle samples according to Folch method (Folch et al. 1957). Lipid extract was dissolved in isopropanol. Triacylglycerol content was measured using a commercial kit (Spinreact, Sant Esteve de Bas, Spain).

Carnitine palmitoyltransferase-1b activity in skeletal muscle

The activity of carnitine palmitoyltransferase-1b (CPT-1b) was assessed in the mitochondrial/peroxisomal fraction. Tissue samples (1.5 g) were homogenized in 4.5 ml of buffer pH 7.4 containing 0.25 mol/L sucrose, 1 mmol/L EDTA and 10 mmol/L Tris–HCl. Homogenates were centrifuged (700g for 10 min at 4 °C), and the supernatant fluid was again centrifuged (12,000g for 15 min at 4 °C). Pellets were resuspended in 70 mmol/L sucrose, 220 mmol/L mannitol, 1 mmol/L EDTA, 2 mmol/L HEPES buffer, pH 7.4. CPT-1b activity was assayed by using the Bieber method (Bieber et al. 1972). The pellet protein content was determined by the Bradford method (Bradford 1976). CPT-1b activity was expressed as nmol CoA formed per minute per mg protein.

Citrate synthase activity in skeletal muscle

Citrate synthase (CS) activity was determined spectrophotometrically following the Srere method (Srere 1969), by measuring the appearance of free CoA. Briefly, muscle samples were homogenated in 10 vol (wt/vol) of 0.1 M Tris–HCl buffer (pH 8.0), and diluted by a factor of 200 in this buffer. Homogenates were incubated for 5 min at 30 °C with 0.1 M Tris–HCl buffer containing 0.1 mM DTNB, 0.25 % Triton X-100, 0.5 mM oxaloacetate and 0.31 mM acetyl CoA, and readings were taken at 412 nm. CS activity was expressed as nmol CoA formed per minute per mg of protein.

Extraction and analysis of RNA and semiquantification by reverse transcription-polymerase chain reaction (RT-PCR)

Total RNA was isolated from 100 mg of muscle using Trizol (Invitrogen, Carlsbad, CA, USA), according to the manufacturer’s instructions. RNA samples were then treated with DNA-free kit (Applied Biosystems, Austin, TX, USA) to remove any contamination with genomic DNA. The yield and quality of the RNA were assessed by measuring absorbance at 260, 270, 280 and 310 nm. A total of 1.5 μg of total RNA of each sample was reverse-transcribed to first-strand complementary DNA (cDNA) using iScript™ cDNA Synthesis Kit (Bio-Rad, Hercules, CA, USA). Acyl-coenzyme A oxidase (ACO), carnitine palmitoyl transferase-1b (CPT-1b), peroxisome proliferator-activated receptor gamma coactivator 1-α (PGC-1α), peroxisome proliferator-activated receptor α (PPAR-α), cluster of differentiation 36 (CD36), transcription factor A; mitochondrial (TFAM), cyclooxygenase-2 (COX-2), and uncoupling protein 3 (UCP3) genes were quantified, as well as 18S which served as the reference gene.

A 9.5-μL aliquot of each diluted cDNA sample was used for polymerase chain reaction amplification in a 25-μL reaction volume. The cDNA samples were amplified on an iCycler-MyiQ Real Time PCR Detection System (Bio-Rad, Hercules, CA, USA) in the presence of SYBRGreen master mix (Applied Biosystems, Austin, TX, USA) and a 300 nM concentration of each of the sense and antisense primers. Specific primers were synthesized commercially (Integrated DNA Technologies, Leuven Belgium), and the sequences are as described in Table 1. The PCR parameters were as follows: initial 2 min at 50 °C, denaturation at 95 °C for 10 min followed by 40 cycles of denaturation at 95 °C for 15 s, annealing at 60 °C for 30 s and extension at 60 °C for 30 s. In the case of PGC-1α and CD36, the annealing temperature was 63.9 °C and 66.4 °C, respectively.

Table 1 Primers for PCR amplification of each gene studied
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Gene expression analysis was performed using the comparative threshold cycle (Ct) method. Amplification of 18S sequence was performed in parallel and was used to normalize values obtained for target genes. The results were expressed as fold changes of threshold cycle (Ct) value relative to controls using the 2−ΔΔCt method (Livak and Schmittgen 2001).

Statistical analysis

Results are presented as mean ± SEM. Statistical analysis was performed using SPSS 17.0 (SPSS, Chicago, IL, USA). Normal distribution of data was confirmed by Shapiro–Wilks test. Therefore, data were analyzed by Student’s t test. Significance was assessed at the P < 0.05 level.

Results

Food intake, food efficiency, body weight and tissue weights

No significant differences were found between experimental groups in terms of food intake (g/d) (17.4 ± 0.4 in the control group vs. 16.7 ± 0.3 in the quercetin-treated group), or of final body weight (g) (393 ± 8 in the control group vs. 385 ± 3 and in the quercetin-treated group). Consequently, food efficiency calculated as increment of body weight/food intake remained unchanged (g/g) (0.28 ± 0.01 in the control group vs. 0.27 ± 0.01 in the quercetin-treated group).

With regard to fat accumulation in adipose tissue, the sum of epididymal, perirenal, mesenteric and subcutaneous adipose depots represented a 9.1 % reduction in the quercetin-treated group (55.8 ± 2.8 g in the control group vs. 50.7 ± 1.5 g in the quercetin-treated group), although this difference did not reach statistical significance. Moreover, no significant differences were found in gastrocnemius muscle weights (g) (2.56 ± 0.13 in the control group vs. 2.43 ± 0.10 in the quercetin-treated group).

Serum parameters and glucose tolerance test

Basal glucose and insulin were significantly reduced (P < 0.01) by quercetin. Consequently, HOMA-IR, an indirect index of insulin resistance, was also diminished (P < 0.01). Moreover, fructosamine concentration (an indicator of the average blood glucose concentration over a short-medium period) was significantly reduced by the addition of quercetin to the diet (P < 0.01). However, no significant differences were found in free fatty acid concentrations (Table 2).

Table 2 Serum parameters of rats from control and quercetin-treated groups
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In the glucose tolerance test, rats treated with quercetin showed significantly lower blood glucose values than control rats. Consequently, AUC in quercetin group was significantly reduced (−13 %, P < 0.01) (Fig. 1a, b).

Fig. 1
figure 1

Glycemic response in glucose tolerance test (a) and area under the curve (AUC) of glucose tolerance test (b) of rats from Control and Quercetin-treated groups (n = 9 per group). Values are mean ± SEM. Differences between groups were determined by Student’s t test. Statistical significance was set at the P < 0.05 level. *P < 0.05

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Enzyme activities in adipose tissue

Quercetin treatment did not modify the activity of lipogenic enzymes (G6PDH, ME and FAS) and HR-LPL in adipose tissue (Table 3). The phosphorylated ACC/total ACC protein ratio remained unchanged (2.37 ± 0.41 in the control group vs. 1.55 ± 0.41 in the quercetin-treated group), indicating that ACC activity was not modified by quercetin.

Table 3 Enzyme activities in adipose tissue and skeletal muscle of rats from control and quercetin-treated groups
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Skeletal muscle determinations

No significant differences were found in triacylglycerol content (mg/g) (11.3 ± 1.8 in the control group vs. 8.6 ± 0.8 in the quercetin-treated group). The amount of this lipid species in skeletal muscle depends to a great extent on fatty acid oxidation. Thus, the gene expression (Fig. 2) and the activity of CPT-1b, a rate-limiting enzyme for this metabolic pathway, and citrate synthase activity, a marker of mitochondrial density (Pajuelo et al. 2011), were assessed, and no significant differences were found between groups (Table 3).

Fig. 2
figure 2

Gene expressions in skeletal muscle of rats from Control and Quercetin-treated groups (n = 9 per group). Results are expressed as fold changes of threshold cycle (Ct) value relative to controls. Values are means ± positive and negative errors. Differences between groups were determined by Student’s t test. Statistical significance was set at the P < 0.05 level. No significant difference was found between both experimental groups. TFAM transcription factor A; mitochondrial; COX-2 cyclooxygenase-2; UCP 3 uncoupling protein 3; ACO acyl-coenzyme A oxidase; CPT-1b carnitine palmitoyl transferase-1b; PPAR-α peroxisome proliferator-activated receptor α; PGC-1α peroxisome proliferator-activated receptor gamma coactivator 1-α; CD36 cluster of differentiation 36

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Skeletal muscle was also used to measure the expression of CD36, a fatty acid transporter, as well of that of genes related to fatty acid oxidation, such as CPT-1b, ACO, PPAR-α, PGC-1α and UCP3. Finally, the expression of genes known as markers of mitochondria number, such as TFAM and COX-2, was analyzed. No effect on the expression of all these genes was observed (Fig. 2).

Discussion

Evidence supporting the health benefits of polyphenols has been increasing over the course of the past few years. In the field of obesity and related metabolic alterations, some of these polyphenols have shown a clear anti-obesity action in animal models. One of the most frequently studied molecules is resveratrol, which belongs to the group of stilbenes (Ahn et al. 2008a; Baile et al. 2011; Baur et al. 2006; Dal-Pan et al. 2010; Macarulla et al. 2009; Rivera et al. 2009; Szkudelska et al. 2009). With regard to flavonoids, and more specifically to quercetin, little is known of any potential role in obesity prevention or treatment.

In vitro studies have demonstrated that quercetin reduces triacylglycerol accumulation in cultured adipocytes (Kuppusamy and Das 1992; Hsu and Yen 2006; Ahn et al. 2008b). Data obtained in these studies are interesting and promising, but it is essential not to forget that important limitations exist in extrapolating these results to the in vivo situation. With regard to in vivo studies, some of these analyzed the effect of quercetin on body weight although body fat was not measured (Rivera et al. 2008; Kim et al. 2011). A small number of studies have analyzed the effect of this flavonoid on body fat. Stewart et al. (2008) found no changes in adiposity among mice fed on a high-fat diet supplemented with 0.8 % of quercetin (which led to a dose of approximately 30 mg/kg body weight/day) for 3 or 8 weeks. By contrast, Kobori et al. (2011) observed a significant decrease in visceral fat (−15.5 %) in mice fed a Western diet supplemented with 0.5 % quercetin for 20 weeks. More recently, Jung et al. (2013) have found a significant reduction in epididymal adipose tissue in mice fed a diet supplemented with 0.025 % for 9 weeks. With regard to experiments performed in rats, no changes in adipose tissue weight were observed in animals fed a high-fat diet supplemented with 0.03 % (25 mg diet/kg of body weight/day) for 4 weeks (Wein et al. 2010). By contrast, quercetin attenuated abdominal obesity (−37 %) in animals fed on a high-fat diet supplemented with 0.08 % quercetin for 8 weeks (Panchal et al. 2012).

As indicated in the previous paragraph, reported data from studies carried out in mice have been obtained by using a wide range of quercetin doses (0.025–0.8 % in the diet). Significant reductions in body fat have been observed in this range even with the lowest dose of 0.025 %. This suggests that high doses are not needed for this flavonoid to show anti-obesity effects. Another important factor to be considered is the length of the treatment period needed to cause a significant effect. Among the reported studies, those with experimental periods of 9 and 20 weeks reported significant reductions in body fat, and those with shorter experimental periods (3–8 weeks) did not. Thus, it can be hypothesized that quercetin may need at least 9 weeks to be effective as an anti-obesity molecule in mice. When data obtained in rats are analyzed, it can be observed that a dose of 0.3 % was effective in mice while ineffective in rats (Wein et al. 2010). This can support the hypothesis that short experimental periods are not enough for quercetin to reduce body fat because in that study, rats were treated for 4 weeks. Nevertheless, the possibility of a varying species-dependent threshold dose cannot be discarded.

In the present study, quercetin reduced by 9.1 % the fat accumulated in the four fat pads dissected and weighed (epididymal + perirenal + mesenteric + subcutaneous), but this reduction did not reach statistical significance. Taking into account the hypothesis provided in the previous paragraph, based on the results reported in the literature, the lack of a significant change could be attributable to the length of the experimental period. In this context, it is important to point out that in previous studies from this laboratory using exactly the same experimental design as the present study (polyphenol dose, treatment period length, diet, animals model), resveratrol induced a significant reduction in adipose tissue sizes (Alberdi et al. 2011), indicating that important differences exist in the potential anti-obesity action of polyphenols.

In order to gain more insight into the effect of quercetin on adipose tissue triacylglycerol metabolism, the activities of lipogenic enzymes (G6PDH, ME, FAS, ACC) and HR-LPL were analyzed. No changes were observed in any enzyme activity, which indicates that neither de novo lipogenesis nor the lipid uptake from circulating lipoproteins was affected by this flavonoid.

Taken together, these data do not lend support to an anti-obesity action of quercetin under the experimental conditions of dose and over the experimental period described here. When considering this conclusion, it is important to underline that the dose used in the present study (30 mg/kg/day), which is very similar to those used in other studies carried out in rodents, was equivalent to 4.86 mg/kg body weight/day in humans (340.5 mg for a person of 70 kg), calculated by using the formula reported by Reagan-Shaw et al. (2008), which is in the 200–400 mg/day range of average human consumption (Manach et al. 1998).

It is well known that a high-fat high-sucrose diet leads not only to increased body fat accumulation, but also to insulin resistance (Hegarty et al. 2003). In the present study, quercetin improved glycemic control, as shown by the HOMA-IR index, which in rats yields a good estimate of whole body insulin sensitivity (Cacho et al. 2008), glucose tolerance test and serum fructosamine concentration. This would appear to be a direct effect, independent of the fat accumulated in adipose tissues, since a significant reduction in this parameter was not observed. On the other hand, as previously mentioned, data in the literature suggest that treatment periods of <9-week duration are insufficient for quercetin to reduce fat but, according to the results showed in the present study, they allow this flavonoid to improve insulin action. This lends support to the hypothesis that the effect of quercetin on insulin action is independent of, and previous to, the effect on fat accumulation.

The present results are in good accordance with other published studies carried out in animal models showing insulin resistance or type 2 diabetes (Wein et al. 2010; Rivera et al. 2008; Kim et al. 2011; Jeong et al. 2012). Nevertheless, there is no general agreement concerning the effect of quercetin on glycemic control. For example, Stewart et al. (2008), whose experiment induced insulin resistance in rats by feeding animals on a high-fat diet, observed that quercetin, at a dose of 0.8 % in the diet, exacerbated diet-induced insulin resistance at 3 weeks.

The authors of those studies which found positive effects of quercetin on glycemic control proposed several mechanisms to explain the beneficial effect of this polyphenol: (a) the anti-oxidative protective action on the pancreatic islets (Coskun et al. 2005; Babujanarthanam et al. 2010; Jeong et al. 2012), (b) the increase in adiponectin circulating concentration (Wein et al. 2010), (c) the inhibition of small intestine glucosidase activity (Kim et al. 2011), (d) the reduction in the intestinal glucose absorption mediated by GLUT2 (Kwon et al. 2007), (e) the increase in glucokinase activity (Vessal et al. 2003) and (f) the increase in GLUT4 transporters in skeletal muscle (Jung et al. 2011; Shen et al. 2012; Anhê et al. 2012).

Recently, Shen et al. (2012) have proposed a new mechanism to explain the improvement in insulin resistance induced by pentamethylquercetin. These authors have shown that this flavonoid increases the expression of genes involved in fatty acid oxidation, such as PPAR-α, PGC-1α, CPT-1b and ACO, in C2C12 myotubes.

Skeletal muscle, the major peripheral tissue in which insulin-responsive glucose uptake and utilization take place, is one of the tissues negatively affected by insulin resistance. One of the proposed factors involved in the impairment of insulin function is increased skeletal muscle lipid deposition (Hulver and Dohm 2004). Under overfeeding conditions which lead to obesity, such as those of the present study, the influx of fatty acids to skeletal muscle is increased. This causes increased intramyocellular concentration of triacylglycerols and leads to insulin resistance by perturbing insulin signaling pathways (Eckardt et al. 2011).

The mechanism of action proposed by Shen et al. (2012) has not been demonstrated under in vivo conditions. Thus, in this context, the potential involvement of increased fatty acid oxidation in skeletal muscle in the reduction in insulin resistance induced by quercetin was assessed in the present study. Quercetin did not modify the expression of genes related to fatty acid oxidation, such as the transcription factor PPAR-α, its co-activator PGC-1α and two key enzymes CPT-1b and ACO regulated by PPAR-α. A similar situation was found when the expression of genes considered as markers of mitochondria number, such as TFAM and COX-2, was assessed. Finally, the expression UCP3, an uncoupling protein related to fatty acid oxidation (Senese et al. 2011) and CD36, a fatty acid transporter, remained unchanged after quercetin treatment. In good accordance with these data, quercetin did not modify the activity of CPT-1b and CS, a marker of mitochondrial density (Pajuelo et al. 2011), and did not show a delipidating effect in skeletal muscle. These results demonstrate that the increase in fatty acid oxidation reported under in vitro conditions in C2C12 myotubes did not take place in an animal model of insulin resistance, at least under the experimental conditions described here.

In conclusion, the present results suggest that quercetin seems to be more effective as an anti-diabetic than as an anti-obesity biomolecule, and that the improvement in insulin resistance induced by this flavonoid is not mediated by a delipidating effect in skeletal muscle.