Specific shifts in the endocannabinoid system in
hibernating brown bears

Christian Boyer, Laura Cussonneau, Charlotte Brun, Christiane Deval,
Jean-Paul Pais de Barros, Stéphanie Chanon, Nathalie Bernoud-Hubac,
Patricia Daira, Alina Evans, Jon Arnemo, et al.

<figure><img src="image_1.png" /></figure>

To cite this version:

Christian Boyer, Laura Cussonneau, Charlotte Brun, Christiane Deval, Jean-Paul Pais de Barros, et al. Specific shifts in the endocannabinoid system in hibernating brown bears. Frontiers in Zoology, 2020, 17, pp.35. 10.1186/s12983-020-00380-y. hal-03054587

HAL Id: hal-03054587

https://hal.science/hal-03054587

Submitted on 31 Mar 2021

**HAL** is a multi-disciplinary open access
archive for the deposit and dissemination of sci-
entific research documents, whether they are pub-
lished or not. The documents may come from
teaching and research institutions in France or
abroad, or from public or private research centers.

L'archive ouverte pluridisciplinaire **HAL**, est
destinée au dépôt et à la diffusion de documents
scientifiques de niveau recherche, publiés ou non,
émanant des établissements d'enseignement et de
recherche français ou étrangers, des laboratoires
publics ou privés.

<figure><img src="image_2.png" /></figure>
RESEARCH

Open Access

<figure><img src="image_3.png" /></figure>

Check for
updates

# Specific shifts in the endocannabinoid system in hibernating brown bears

Christian Boyer<fnref n="1" />, Laura Cussonneau<fnref n="1" />, Charlotte Brun², Christiane Deval<fnref n="1" />, Jean-Paul Pais de Barros³,
Stéphanie Chanon⁴, Nathalie Bernoud-Hubac⁴, Patricia Daira⁴, Alina L. Evans⁵, Jon M. Arnemo⁵,⁶, Jon E. Swenson⁷,
Guillemette Gauquelin-Koch⁸, Chantal Simon⁴, Stéphane Blanc², Lydie Combaret<fnref n="1" />, Fabrice Bertile²† and
Etienne Lefai<fnref n="1" />*† ID

**Abstract**

In small hibernators, global downregulation of the endocannabinoid system (ECS), which is involved in modulating neuronal signaling, feeding behavior, energy metabolism, and circannual rhythms, has been reported to possibly drive physiological adaptation to the hibernating state. In hibernating brown bears (*Ursus arctos*), we hypothesized that beyond an overall suppression of the ECS, seasonal shift in endocannabinoids compounds could be linked to bear's peculiar features that include hibernation without arousal episodes and capacity to react to external disturbance. We explored circulating lipids in serum and the ECS in plasma and metabolically active tissues in free-ranging subadult Scandinavian brown bears when both active and hibernating. In winter bear serum, in addition to a 2-fold increase in total fatty acid concentration, we found significant changes in relative proportions of circulating fatty acids, such as a 2-fold increase in docosahexaenoic acid C22:6 n-3 and a decrease in arachidonic acid C20:4 n-6. In adipose and muscle tissues of hibernating bears, we found significant lower concentrations of 2-arachidonoylglycerol (2-AG), a major ligand of cannabinoid receptors 1 (CB1) and 2 (CB2). Lower mRNA level for genes encoding CB1 and CB2 were also found in winter muscle and adipose tissue, respectively. The observed reduction in ECS tone may promote fatty acid mobilization from body fat stores, and favor carbohydrate metabolism in skeletal muscle of hibernating bears. Additionally, high circulating level of the endocannabinoid-like compound N-oleoylethanolamide (OEA) in winter could favor lipolysis and fatty acid oxidation in peripheral tissues. We also speculated on a role of OEA in the conservation of an anorexigenic signal and in the maintenance of torpor during hibernation, while sustaining the capacity of bears to sense stimuli from the environment.

**Keywords:** Hibernation, Brown bear, Metabolism, Lipidomic, Docosahexaenoic acid, Endocannabinoid system, Cannabinoid receptor 1, Cannabinoid receptor 2, 2-arachidonoylglycerol, Anandamide, N-oleoylethanolamide

**Background**

To deal with seasonal cold and food shortage during winter, hibernating mammals show a combination of behavioral and physiological changes. To save energy during hibernation, hibernating animals use periods of torpor characterized by decreased metabolic rate and body

temperature, reduction in respiratory and heart rates, and physical inactivity [1, 2]. Brown bears (*Ursus arctos*) exhibit unique features, as they hibermate at mild hypothermia (32–35 °C) and can stay inside their dens for up to 7 months, without drinking, eating, defecating or urinating, and with no arousal episodes [3–6]. While denning, they reduce their metabolic rate by about 75% [7], and rely primarily on mobilization of fat stores, which is reflected by increased circulating fatty acid concentration and body fat store depletion during winter [8–10].

<footnote>* Correspondence: etienne.lefai@inrae.fr</footnote>

<footnote>†Fabrice Bertile and Etienne Lefai contributed equally to this work.</footnote>

<footnote n="1">¹Université Clermont Auvergne, INRAE, UNH, Clermont-Ferrand, France
Full list of author information is available at the end of the article</footnote>
Beyond energy substrates, lipids also have pleiotropic actions in the regulation of metabolism, and changes in membrane fatty acid composition have already been described in hibernating animals [11–14], including the brown bear [9]. Membrane phospholipids can also provide long-chain fatty acids for the synthesis of bioactive lipid mediators, such as endocannabinoids [15–17]. The endocannabinoid system (ECS) was originally described as being composed of G-protein coupled receptors (CB1 and CB2) and their endogenous ligands, of which the main ones are derived from arachidonic acid 20:4n-6 (AA) esterified into phospholipids, and called 2-arachidonoyl glycerol (2-AG) and anandamide (AEA) [15–20]. These two well-characterized compounds clearly show varying affinity for CB1 and CB2 receptors. Indeed, AEA is considered as a high affinity CB1-partial agonist (and weak CB2 agonist), whereas 2-AG is described as a low-to-moderate affinity CB1 and CB2 full agonist [21, 22]. 2-AG and AEA belong to the large family of 2-acylglycerols (2-AcGs) and N-acylethanolamines (NAEs), respectively [17, 19]. N-acyl-phosphatidylethanolamine-hydrolyzing phospholipase D (NAPEPLD) and sn-1-specific diacylglycerol lipase-α and β (DAGLA and DAGLB) are the main enzymes involved in the biosynthesis of NAEs and 2-AcGs, respectively [17, 19]. Fatty acid amide hydrolase (FAAH) is responsible for NAEs catabolism (and to a lesser extend for 2-AG) [23], and monoacylglycerol lipase (MGLL) specifically catabolizes 2-AcGs [17, 19]. eCBs can also be metabolized by lipoxygenases (LOXs) and by cyclooxygenase-2 (COX-2), an alternative pathway for eCBs catabolism [17].

The ECS includes structurally related compounds like N-oleoylethanolamine (OEA), called «endocannabinoids-like compounds» (eCBs-like). The latter are metabolized by the same biosynthetic and catabolic enzymes as eCBs [17]. Although eCBs-like compounds are not able to bind to CB1 and CB2 receptors, they can bind to other G-protein coupled receptors (e.g. GPR119 and GPR55) or nuclear receptors, like peroxisome proliferator-activated receptor α (PPARA) [17].

Endogenous cannabinoids are involved in the regulation of many physiological processes, including neuronal signaling [24], stress response [25], metabolism [25–27], feeding behavior and energy storage [25, 28]. Evidences support the fact that the ECS could be involved in sleep cycles [29], circadian and potentially circannual rhythms [30]. At the central level (e.g. hypothalamus), CB1 is able to promote food intake and reduce energy expenditure [25, 31]. In addition, CB1 activation in adipose tissue leads to fatty acid and glucose uptake, and to upregulation of lipogenesis [25]. In liver, CB1 signaling leads to increased expression of genes involved in the synthesis of fatty acids [32], and in skeletal muscle tissue, CB1 activation triggers a decrease in glucose uptake and insulin sensitivity [25]. The CB2 receptor is well known to be widespread over immune cells and

to have numerous immunomodulatory roles [33]. CB2 has also been detected in metabolic tissues, like adipose tissue and skeletal muscle [34, 35] and CB2 pharmacological or genetic inactivation in murine obesity models promote insulin-mediated glucose uptake in skeletal muscles, reduce adipose tissue inflammation, and thus improves insulin sensitivity [36, 37]. Finally, the eCB-like OEA promotes lipolysis, fatty acid oxidation in skeletal muscle and liver, and triggers an anorexigenic signal, notably through the nuclear receptor PPARA [38, 39]. Considering the pleiotropic roles of ECS in neuronal signaling, regulation of feeding behavior, energy metabolism and circannual rhythms, important changes are expected during hibernation. Several ECS circulating compounds have been quantified in hibernating black bears, during and around the torpor phase [40], with no major changes observed except a slight increase in 2-AG in the period of metabolic drop before torpor. Although a decrease in ECS tone has been observed in hibernating marmots (Marmota monax and flaviviventris) and ground squirrels (Spermophilus richardsonii) [30, 41, 42], we hypothesize that a similar decrease should occur in hibernating bears, not excluding specific changes due to their unique features during hibernation (mild hypothermia, no periodic arousal, and maintenance of alertness). Therefore, we explored here seasonal variations in fatty acid composition and ECS tone, in both circulating compartment and in muscle and adipose tissues, in winter-hibernating and summer-active brown bears.

## Results

### Seasonal differences in serum lipids

We explored the fatty acid (FA) composition of winter-hibernating (WBS) and summer-active (SBS) bear serum (see supplementary Table S1). From the lipidomic data, we compared both the summer and winter concentrations and proportions of fatty acids (see supplementary Table S2 and S3 for detailed lipidomic results). As shown in Fig. 1a, the total concentration of FAs was about twofold higher in WBS relative to SBS (28.82 ± 1.71 vs. 15.99 ± 1.09 mmol/L). All but two quantified lipid species were higher in concentration in hibernating bears, i.e. saturated fatty acids (SFAs), monounsaturated fatty acids (MUFAs), and n-6 polyunsaturated fatty acids (PUFAs) (Supplementary Table S2). Only concentrations of alpha-linolenic acid C18:3 n-3 (ALA) (0.49 -fold, non-significant) and eicosa-pentaenoic acid C20:5 n-3 (EPA) (0.26-fold) were lower in WBS (Supplementary Table S2).

Meanwhile, the molar percent of total n-6 species were found to be lower in WBS compared to SBS (Fig. 1b). Lipid species with the highest molar percent are presented in Fig. 1c (see Supplementary Table S3). Among SFAs, palmitic acid C16:0 (PA) was found in higher proportion, whereas stearic acid C18:0 (SA) was in lower proportion in winter serum. Similar proportions of oleic acid 18:1n-9 (OA),
<figure><img src="image_4.png" /><figcaption>Fig. 1 (See legend on next page.)</figcaption></figure>
(See figure on previous page.)

**Fig. 1** Lipidomic from summer and winter brown bear serum. The winter and summer bear serum mixes were prepared as described (Supplementary Table S1), a: Total fatty acid (FA) concentration. b: Total n-6 and n-3 FA relative proportions of total lipids. c: Highest molar percent lipid species D: Molar percent of the n-3 family lipid species. e: Molar ratios of DHA/AA in summer and winter serum. Detailed lipidomic results are presented in Supplementary Tables S2 and S3. Data are expressed in mmol/L for total FAs concentration, or molar percentage of total lipids and are represented as mean ± SEM of separate extractions and quantifications from the twelve mixes (six summer and six winter serum mixes, except for EPA with data from only three summer and three winter mixes). Paired Student t-test were used to compare wummer and winter data and Benjamini-Hochberg correction was applied for multiple comparisons. * indicates BH adjusted *p* value < 0.05 when comparing seasons, ** for *p* < 0.01, *** for *p* < 0.001, NS: non significant. AA:arachidonic acid, ALA: alpha-linolenic acid, DHA: docosahexaenoic acid, DPA: docosapentaenoic acid, EPA: eicosapentaenoic acid, LA: linoleic acid, OA: oleic acid, PA: palmitic acid, SA: stearic acid, SBS: summer bear serum, WBS: winter bear serum

belonging to the n-9 MUFAs, were found in winter and summer bear serum. Concerning n-6 PUFAs, the proportion of arachidonic acid C20:4 n-6 (AA) was lower during winter, whereas proportion of linoleic acid C18:2 n-6 (LA) remained unchanged (Fig. 1c). For individual species of the n-3 family (Fig. 1d and Supplementary Table S3), docosapentaenoic acid C22:5 n-3 (DPA, 1.5-fold) and docosahexaenoic acid C22:6 n-3 (DHA, 2.2-fold) were found in higher proportions.

The proportion of C20:5 n-3 (EPA) was found much lower (0.15-fold) in winter serum, as well as the alpha-linolenic acid C18:3 n-3 (ALA, 0.27-fold), a precursor of the EPA, DPA and DHA species.

From molar percent values, the DHA/AA ratio was 3.2-fold higher in winter (Fig. 1e).

## Changes in plasma endocannabinoids and endocannabinoids-like compounds

We next assessed circulating eCBs and eCBs-like in bear plasma. Paired samples were collected in winter and in summer from eight bears (Supplementary Table S1) and quantification of AEA, 2-AG and OEA are presented in Fig. 2 and supplementary Table S5. Lower concentrations were observed for AEA (0.63-fold) in winter compared to summer, whereas the reverse was observed for OEA (3.3-fold). No difference was found for 2-AG plasma concentration.

## Changes in endocannabinoid concentrations in muscle and adipose tissues

Quantification of endocannabinoids was then performed in bear muscle and adipose tissues. Paired tissues samples were collected from bears in winter and in summer (Supplementary Table S1) and quantification of AEA, 2-AG and OEA are presented in Fig. 3 and supplementary Table S5. AEA concentration was lower in both muscle and adipose tissues during winter versus summer, close to the statistical threshold (*p* = 0.064 and *p* = 0.069, respectively). 2-AG concentration was significantly lower in muscle and adipose tissues samples during winter, by about 1.6- and 9-fold, respectively. By contrast, no seasonal changes were found in OEA concentrations in both muscle and adipose tissues.

## Changes in endocannabinoid pathway-related gene expressions in muscle and adipose tissues

To explore tissue metabolism of endocannabinoids, we quantified gene expression in muscle and adipose tissue of the eCBs membrane receptors CB1 and CB2, and several enzymes involved in the synthesis and catabolism of eCBs. For muscle tissue, paired samples were from 8 bears at the two time points, while for adipose tissue, data are coming from 5 bears in summer and 13 bears

<figure><img src="image_5.png" /></figure>

**Fig. 2** Circulating endocannabinoids concentration in brown bear plasma. Concentration of three major endocannabinoids compounds in bear plasma. Plasma were collected from bears at both winter-hibernating and summer-active time points (Supplementary Table S1). Data are expressed in ng/mL and are represented as mean ± SEM of separate extractions and quantifications (n = 8). Paired Student t-test were used to compare wummer and winter data. * indicates *p* value < 0.05 when comparing seasons, *** for *p* < 0.001, NS: non significant. AEA: anandamide, 2-AG: 2-arachidonoylglycérol, eCBs: endocannabinoids, OEA: N-oleoylethanolamine, SBP: summer bear plasma, WBP: winter bear plasma
<figure><img src="image_6.png" /><figcaption>**Fig. 3** Endocannabinoids concentration in brown bear muscle and adipose tissue. Concentration of three major endocannabinoids compounds in bear muscle and adipose tissue. Tissues were collected from bears at both winter-hibernating and summer-active time points (Supplementary Table S1). Data are expressed in pg/mg and are represented as mean ± SEM of separate extractions and quantifications (n = 5 for muscle tissue and n = 6 for adipose tissue). Paired Student t-test were used to compare wummer and winter data. *** indicates p value < 0.0001 when comparing seasons, NS: non significant. AEA: anandamide, 2-AG: 2-arachidonoylglycérol, OEA: N-oleylethanolamine, SBA: summer bear adipose tissue, SBM: summer bear muscle, WBA: winter bear adipose tissue, WBM: winter bear muscle</figcaption></figure>

in winter (Supplementary Table S1). Data are presented in Fig. 4 and Supplementary Table S5.

For genes that encode the membrane receptors CB1 and CB2 in muscle tissue, CNR1 mRNA level, but not CNR2, was decreased (0.63-fold) in winter (Fig. 4). Concerning enzymes that catabolize AEA and 2-AG, mRNA level of FAAH was induced (2.3-fold) in winter, but MGLL gene expression did not change. For genes encoding enzymes of the biosynthetic pathway, DAGLA mRNA level was strongly reduced in muscle tissue during winter (0.40-fold), whereas DAGLB mRNA level was increased (1.53-fold). Finally, gene expression of NAPEPLD did not change in muscle (Fig. 4).

Conversely, in adipose tissue (Fig. 5), no significant changes in CNR1 gene expression were reported whereas CNR2 expression was strongly decreased in winter (0.42-fold). For gene expression of catabolic enzymes (FAAH and MGLL), did not change in adipose tissue between seasons. Finally, for genes encoding biosynthetic enzymes, mRNA levels of DAGLB and NAPELD were respectively found higher (1.44-fold) and lower (0.75-fold) in winter.

Discussion

Thanks to repeated capture sessions, we were able to gather samples of serum, plasma and tissues from high number of

free-living brown bears (*Ursus arctos*). From the 28 bears included in this study, samples were collected both in February during winter hibernation and in June during summer active period. Due to limited amount of available biological material, the analyses were performed on samples coming from different subsets of the 28 bears. In all but adipose tissue, analyses were performed on winter and summer paired samples (Supplementary Table S1). We examined circulating lipid and ECS compounds in both summer-active and winter-hibernating brown bears to explore the extent to which regulation of the ECS reflects bear hibernation peculiarities, including survival due to lipid oxidation, maintenance of muscle glycolysis, and maintained alertness during dormancy. The seasonal shift we highlighted in serum FAs composition, together with a decrease in tissue AEA and 2-AG, and a three-fold increase in circulating OEA during winter, could contribute to the behavioral and metabolic changes that occur in hibernating bears.

Hibernators experience extended periods of food shortage during hibernation and primarily rely on mobilization of fat stores from white adipose tissue [1]. Accordingly, we found that the concentration of total circulating fatty acids was elevated in hibernating bears, a finding in line with previous studies [5, 43]. Considering both the amount and
<figure><img src="image_7.png" /><figcaption>**Fig. 4** Fold change in gene expression of target genes involved in endocannabinoids biosynthesis and catabolism in brown bear muscle tissue. Muscle tissues were collected from bears at both winter-hibernating and summer-active time points (Supplementary Table S1), total RNA was extracted and expression levels were measured by RT-qPCR. Data are normalized against TBP mRNA levels and expressed as a fold change relative to the summer condition, represented as mean ± SEM of separate extractions and quantifications (n = 8). Paired Student t-test were used to compare wummer and winter data. \* indicates p value < 0.05 when comparing seasons, NS: non significant. CNR1: cannabinoid receptor 1, CNR2: cannabinoid receptor 2, DAGLA: diacylglycerol lipase alpha, DAGLB: diacylglycerol lipase beta, FAAH: fatty acid amide hydrolase, MGLL: monoacylglycerol lipase, NAPEPLD: N-acyl phosphatidylethanolamine phospholipase D, SBM: summer bear muscle, WBM: winter bear muscle</figcaption></figure>

relative proportions of circulating lipids, our results are consistent with changes in serum and plasma lipid profiles during hibernation that have been previously published [5, 9, 10], notably an enrichment in DHA C22:6 n-3 and depletions in ALA C18:3 n-3 and EPA C20:5 n-3, during winter compared to summer. Whether the depletion in the ALA and EPA precursor species could be directly linked to the observed DHA increase remains to be elucidated.

Here, the DHA serum enrichment that we observed in hibernating bears is actually not coming from dietary FAs intake but rather due to lipid stores mobilization. The health benefits that have been attributed to n-3 PUFAs (e.g. DHA), essentially triggered by DHA dietary intervention studies, could potentially be transposed in the context of hibernation. Indeed, it has already been hypothesized that DHA could be involved in the bear's resistance to muscle atrophy during hibernation [10]. DHA appears to prevent muscle atrophy in fasting mice, and increases muscle glycogen stores [44]. Strikingly, in parallel to DHA serum enrichment, hibernating bears have more than a 3-fold higher glycogen muscle content compared to summer-active animals [10]. In addition to its anti-inflammatory effects, DHA

is also known to exert a positive effect on protein balance by decreasing expression of factors involved in protein breakdown [45] and enhancing protein synthesis, notably by promoting mammalian Target Of Rapamycin (mTOR) activation [46].

Concomitantly to serum DHA enrichment, we observed a drop in AA proportion, thus leading to a sharp increase in the DHA/AA ratio. Omega-3/omega-6 ratio is known to have an impact on global health [47], and the balance of this ratio could also impact the endocannabinoid system [48], notably because AA is a precursor of the two main eCBs 2-AG and AEA. Indeed, n-6 PUFAs-enriched diets have been shown to increase the level of 2-AG or AEA in the brain, plasma, and peripheral tissues in non-hibernating animal models [49–52]. It is noteworthy to mention that, in response to DHA supplementation, an enrichment of this fatty acid in phospholipids of cell membranes occurs in parallel with a decrease in AA content [38, 49, 53, 54]. By remodeling the amount of AA-containing phospholipids, DHA is able to reduce the synthesis of AEA and 2-AG [49, 54]. Further studies on bears, focusing on fatty acid membrane composition in tissues at different time points, will be helpful to characterize the
<figure><img src="image_8.png" /><figcaption>**Fig. 5** Fold change in gene expression of target genes involved in endocannabinoids biosynthesis and catabolism in brown bear adipose tissue. Adipose tissues were collected from bears at both winter-hibernating and summer-active time points (Supplementary Table S1), total RNA was extracted and expression levels were measured by RT-qPCR. Data are normalized against TBP mRNA levels and expressed as a fold change relative to the summer condition, represented as mean ± SEM of separate extractions and quantifications (n = 5 for summer and n = 13 for winter samples). Unpaired Student t-test were used to compare summer and winter data.* indicates *p* value < 0.05 when comparing seasons. CNR1: cannabinoid receptor 1, CNR2: cannabinoid receptor 2, DAGLA: diacylglycerol lipase alpha, DAGLB: diacylglycerol lipase beta, FAAH: fatty acid amide hydrolase, MGLL: monoacylglycerol lipase, NAPEPLD: N-acyl phosphatidylethanolamine phospholipase D, SBA: summer bear adipose tissue, WBA: winter bear adipose tissue</figcaption></figure>

remodeling of membrane lipids that could affect the avail-
ability of FAs precursors for eCBs biosynthesis. Data on
eCBs compounds from experimental short fasting in non-
hibernating mammals are very divergent, depending on
the tissue considered (e.g. brain or peripheral tissues) and
the duration of food deprivation, but tissue levels of eCBs
are mainly regulated by the availability of their membrane
phospholipid precursors and by the activity of biosynthetic
and catabolic enzymes [28, 49, 55, 56].

We hypothesized that drastic reduction in metabolic activity, lack of intake of dietary PUFAs, significant increase in the serum DHA/AA ratio, and perhaps reduction in tissue AA-phospholipids concentration, could lead to a global reduction in ECS tone during the hibernation period. The reduction in ECS tone has already been documented in hibernating marmots [30, 41], but not confirmed in large-bodied hibernators.

Comparing active and hibernation states in brown
bears, we reported here a decrease in plasma concentra-
tion of AEA, and an unexpected 3-fold increase in OEA
circulating levels in hibernating bears. In both muscle
and adipose tissues, 2-AG and AEA (close to statistical
threshold) were found lower in winter, while OEA did
not change. Quantification of winter serum eCBs was

previously reported in black bears during and around
the topor phase, but summer active bears were not in-
vestigated [40]. Nutritional status of the captured ani-
mals and diet were not specified. These elements
strongly limit comparison between the two studies.

Taken together, our data allowed us to make several hy-
potheses about possible mechanisms by which ECS could
contribute to the metabolic and behavioral changes that
occur in bears during hibernation. First, considering that
AEA and 2-AG CB1 agonists favor food intake and stimu-
late lipogenesis [25], CB1 signaling is expected to be upreg-
ulated during the active summer period in order to
promote energy storage, and downregulated during winter
hibernation to stimulate lipolysis and FAs oxidation. The
tissue concentration drops in 2-AG and AEA observed
during winter could be due to a decrease in tissue AA-
phospholipids concentration, as we hypothesized above.
The degradation of AEA could also be increased in muscle
tissue during hibernation, as reflected in the higher mRNA
levels of FAAH, the main hydrolase that degrades AEA [19,
23]. In adipose tissue, lower NAPEPLD mRNA level con-
tent during hibernation may support a decrease in AEA
synthesis, and ultimately content. The tissue content in 2-
AG is decreased in winter with no changes in mRNA levels
of the catabolic enzyme MGLL. Furthermore, opposite
changes in DAGLA and DAGLB gene expression do not
allow to speculate on the biosynthetic/degradation balance.
One limitation of our study is that gene expression could
not reflect biological activity. Moreover, we only focused
on main biosynthetic and catabolic enzymes involved in
eCBs metabolism, and investigation on alternative degrad-
ation route as endocannabinoid oxygenation by cyclooxy-
genases and lipoxygenases would bring new insights.

During hibernation, lower 2-AG (and AEA close to stat-
istical threshold) tissue content and the reduction of
CNR1 and CNR2 mRNA levels in muscle and adipose tis-
sue, respectively, strongly support reduced ECS tone in
both tissues. In non-hibernating mammals, pharmaco-
logical inhibition of CB1 leads to a decrease in PDK4 ex-
pression [25, 57]. PDK4 is a major negative regulator of
PDH activity, that in turn regulates the whole body oxida-
tive carbohydrate metabolism. In hibernating bear muscle,
recent studies have shown that PDK4 is upregulated com-
pared to summer active state [10, 58] and expression of
PDK4 during hibernation appear thus to be disconnected
from direct regulation by CB1. CB1 receptor antagonism
also leads to an increased uptake of glucose in muscle via
PI3K signaling [59], and glycolysis appears preserved in
bear skeletal muscle during hibernation, as suggested by
an overall increase in the protein abundance of all glyco-
lytic enzymes [10]. As proposed by Chazarin et al. and
Vella et al., bears still oxidize glucose and produce lactate
in skeletal muscle during hibernation [10, 60].

Overactivation of the ECS is a hallmark of obesity [61, 62], and 2-AG is predominantly found in higher concentration in tissues of obese people [61, 63]. Interestingly, in murine models of obesity, gain of adipose tissue often leads to increased fat inflammation [36, 37]. Genetic or pharmacological inactivation of CB2 receptor contribute to reduce adipose tissue inflammation, increase insulin sensitivity and skeletal muscle glucose uptake [36, 37]. Strikingly, insulin resistance has been described in hibernating bears adipocytes [64]. As bears don't experience health consequences of circannual high body fat storage [65], a reduced CB2 signaling in adipose tissue could dampen adipose tissue inflammation. Lower amounts of 2-AG and AEA could also reduced CB1 signaling in adipose tissue, thus limiting lipogenesis and promoting lipolysis during hibernation in bears, as also suggested for hibernating marmots [30].

OEA is a high-affinity agonist for peroxisome
proliferator-activated receptor α (PPARA), regulating food
intake and stimulating fat catabolism [38, 39, 53, 66, 67].
The eCB-like OEA is generally synthesized in response to
dietary oleic acid intake by enterocytes of the small intes-
tine [49, 54], and inhibits food intake. It has already been
shown in rodents that food deprivation inhibits OEA syn-
thesis in the small intestine, but stimulates its synthesis in

liver [38, 53, 68, 69]. Therefore, during bear hibernation,
circulating OEA could originate from tissue synthesis
(probably hepatic) and be released in the blood flow. The
high OEA level that we found in hibernating bears, not trig-
gered by food intake, could participate in a sustained an-
orexigenic signal during the hibernation state.

Consequences of high levels of circulating OEA have
been studied in non-hibernating rodents. Intraperitoneal
OEA administration in rats notably impairs locomotor ac-
tivity, which is supported by a decrease in ambulation, an
increase of the time spent in inactivity, and the presence of
signs of catalepsy [66, 70]. We thus can hypothesize that a
higher amount of plasma OEA during bear hibernation can
participate in the maintenance of prolonged physical in-
activity. It has also been shown that intracerebroventricular
injections of OEA promote alertness, with the observation
of enhanced dopamine and c-Fos expressions in wake-
related brain areas [71]. Bears are known to stay sensitive
to disturbance during hibernation [72–74]. High circulating
amounts of OEA might thus participate in alertness to
external stimuli from the environment in hibernating bears.
OEA during winter possibly also favors body fat
mobilization for energy needs, with stimulation of FA and
glycerol release from adipocytes [38, 39]. Finally, a potential
role for OEA in the promotion of fasting-induced ketogen-
esis during hibernation could also be considered, as OEA
has been demonstrated to increase 3-hydroxybutyrate pro-
duction in in vivo rodent models [38, 39].

Conclusions

In conclusion, our results show a reduction in ECS tone
in hibernating bears and suggest a coordinated downreg-
ulation of CB1 and CB2 signaling in skeletal muscle and
adipose tissue. As summarized in Fig. 6, these features
could favor energy mobilization through lipolysis, and
optimization of glucose uptake by skeletal muscles.
Despite high fat stores in winter, bears do not exhibit
features of ECS overactivation, and decrease in CB2 sig-
naling could dampen adipose tissue inflammation. The
observed increase in circulating OEA level may partici-
pate in the behavioral and physiological adaptations dur-
ing bear hibernation state, like maintenance of an
anorexigenic signaling pathway, and promotion of lipoly-
sis and fatty acid β-oxidation. We also speculated about
OEA involvement in torpor maintenance and in motor
activity reduction, as well as a role in conservation of
alertness at the level of central nervous system.

Methods

Bear sample collection

A total of 28 free ranging subadult brown bears (*Ursus arctos*) from Dalarna and Gävleborg counties, Sweden, were included in this study, including 4 bears captured two consecutive years. All samples and data were collected
<figure><img src="image_9.png" /><figcaption>**Fig. 6** Hypothetical consequences of changes in circulating lipids and endocannabinoid system tone during hibernation in brown bear. Black arrows represent possible behavior and metabolic outcomes</figcaption></figure>

under protocols approved by the Swedish Ethical Committee on Animal Experiment (applications Dnr C3/2016 and Dnr C18/2015), the Swedish Environmental Protection Agency (NV-00741-18), and the Swedish Board of Agriculture (Dnr 5.2.18–3060/17). All procedures complied with Swedish laws and regulations.

As described previously [10, 75], blood, subcutaneous adipose tissue, and muscle tissue (vastus lateralis) samples were collected at two time points, in February during winter hibernation (W) and in June during summer-active period (S). Blood samples were collected from the jugular vein into 8 ml dry tubes for serum (Vacuette® Z serum Sep Clot Activator, Greiner Bio-One GmbH, Kremsmünster, Austria) or into 10 ml EDTA-coated tubes (BD Vacutainer®, FisherScientific, Illkirch, France) for plasma.

The analyses were performed on samples coming from different subsets of bears as described in Supplementary Table S1.

## Lipid extraction and analysis

To perform serum lipidomic analysis, serum mixes were prepared as followed: for a given year, 50 µl of summer serum from each bear of the year was pooled to obtain the summer mix. In parallel, 50 µl of winter serum from the same bears was pooled to obtain the winter mix. A total of 6 summer and winter paired mixes were obtained (Supplementary Table S1). Lipids were extracted and analyzed

as previously described [76]. After addition of an internal standard (tri-17:0 triacylglycerol), total lipids were extracted twice from bear serum mixes with ethanol/chloroform (1:2, v/v). The organic phases were dried under nitrogen and lipids were transmethylated. Briefly, samples were treated with toluene-methanol (1:1, v/v) and boron trifluoride in methanol (14%). Transmethylation was carried out at 100 °C for 90 min in screw-capped tubes. Then 1.5 mL K₂CO₃ in 10% water was added and the resulting fatty acid methyl esters were extracted by 2 mL of isooctane and analyzed by gas chromatography (GC) with a HP6890 instrument equipped with a fused silica capillary BPX70 SGE column (60 × 0.25 mm). The vector gas was hydrogen. Temperatures of the Ross injector and the flame ionization detector were set to 230 °C and 250 °C, respectively. Data were expressed in mmol/L for total or individual fatty acids (FAs) concentration or molar percentage of total lipids for individual FAs. Detailed lipidomic results are presented in supplementary Table S2 (serum fatty acid concentrations) and S3 (serum fatty acid relative proportions).

## Endocannabinoid quantification

For quantification of circulating endocannabinoids, analysis was performed on 500 µl of plasma collected at the two time points (S and W) from 8 individual animals (see supplementary Table S1). Standard endocannabinoids
(eCBs), i.e.- PEA, PEA-d5, OEA, OEA-d4, AEA, AEA-d4, 2AG, and 2AG-d5, were purchased from Cayman (Bertin BioReagent, Saint-Quentin en Yvelines, France). Mass spectrometry quality grade solvents were purchased from Fischer Scientific (Illkirch, France). Tissue samples (adipose and muscle tissues); c.a 100 mg) were crushed in an Omni Bead Ruptor 24 apparatus (Omni International, Kennesaw, USA) with circa twenty 1.4 mm OD zirconium oxide beads (S = 6.95 m/s, T = 30s, C = 3; D = 10s) and 900 µl of methanol/Tris-buffer (50 mM, pH = 8) 1/1 containing 20 ng of PEA-d5, 2 ng OEA-d4, 10 ng AEA-d4, and 20 ng 2AG-d5. Then, each homogenate was added with 2 mL of CHCl<sub>3</sub>/MeOH (1:1, v/v) and 500 µL of Tris (50 mM, pH = 8), vortexed and centrifuged 10 min at 3000 g. The organic layer was recovered and the upper aqueous phase was extracted twice with chloroform (1 mL). Finally, organic phases were pooled and evaporated under vacuum.

Plasma (500 µL) were mixed with 500 µL cold methanol containing 11 ng AEA. After protein precipitation at – 20 °C for 2 h, endocannabinoids were extracted with methanol/chloroform (1:1, v/v) (5 ml) and saline (1.25 mL). The organic phase was recovered and the aqueous phase was extracted twice with chloroform (3 mL). Organic phases were finally pooled and evaporated under vacuum.

Dried extracts were solubilized with methanol (200 µL) and centrifuged for 5 min at 20,000 g. Four microliters of the supernatant were injected into a 1200 LC system coupled to a 6460-QqQ MS/MS system equipped with an ESI source (Agilent technologies). Separation was achieved on Zorbax SB-C18 2.1 × 50 mm, 1.8 µm column (Agilent technologies) at a flow rate of 0.4 mL/min, 40 °C, with a linear gradient of (solvent A) water containing 0.1% formic acid and (solvent B) methanol containing 0.1% formic acid as follows: 10% of B for 1 min, up to 85% of B in 8 min, and then 100% B for 4.5 min. Acquisition was performed in positive Selected Reaction Monitoring (SRM) mode (source temperature: 350 °C, nebulizer gas flow rate: 10 L/min, 40 psi, sheath gas flow 10 L/min, sheath gas temperature 350 °C, capillary 4000 V, nozzle 1000 V).

Transitions used were: 2AG-d5 384.3 → 91.1 (frag 120 V, CE 62 V), 2AG 379.1 → 91 (frag 120 V, CE 62 V), AEA-d4 352.2 → 66.1 (frag 115 V, CE 14 V), AEA 348.2 → 62 (frag 120 V, CE 14 V), OEA-d4 330.2 → 66.1 (frag 120 V, CE 14 V), OEA 326.2 → 62 (frag 115 V, CE 14 V), PEA-d5 305.2 → 62 (frag 124 V, CE 14 V), and PEA 300.2 → 62 (frag 124 V, CE 14 V).

Endocannabinoids quantification in tissues was performed on tissue samples collected at the two time points (S and W) from 5 (muscle tissue) and 6 (adipose tissue) bears (Supplementary Table S1). eCBs from tissues were quantitated according to the isotope dilution method. Results are expressed as pg per mg of wet weight of tissue. eCBs from plasma were quantitated using calibration curves obtained with authentic standards extracted by the

same method used for plasma samples. Linear regression was applied for calculations. Results are expressed as ng of endocannabinoid per mL of plasma.

## Quantification of mRNAs by real-time RT-PCR

For mRNA quantification using RT-qPCR, total RNAs were obtained from muscle and adipose tissues collected at the two time points (S and W). For the muscle tissue, RNAs were extracted from 8 bears in summer and winter, while for adipose tissue, RNAs were extracted from 5 bears in summer and 13 bears in winter (Supplementary Table S1).

Muscle and adipose tissue total RNA was isolated using the TRIzol reagent (Invitrogen, Courtaboeuf, France) according to the manufacturer's instructions. First-strand cDNAs were synthesized from 1 µg of total RNA using the PrimeScript RT kit (Ozyme, Saint quentin en Yveline, France) with a mixture of random hexamers and oligo(dT) primers, and treated with 60 units of RnaseH (Ozyme). Real-time PCR assays were performed with Rotor-Gene 6000 (Qiagen, Courtaboeuf, France). The primers and real-time PCR assay conditions are listed in supplementary Table S4. The results were normalized by using TBP (TATA box binding protein) mRNA concentration, measured as reference gene in each sample.

## Statistical analysis

Statistical analysis was performed using the R software environment v3.0.2 [77]. For each set of values, distribution of the data was tested using the Shapiro-Wilk normality test, and using the *p* = 0.01 threshold normal distribution was considered in all cases. Differences between summer and winter data were tested using paired Student t-test for lipidomic, endocannabinoid quantification in plasma and tissues, and mRNA level in muscle tissue. For mRNA level in adipose tissue, differences between summer and winter data were tested using unpaired Student t-test. For multiple comparison (lipidomic data), the Benjamini-Hochberg correction using the p-adjust function (Package *stats* version 4.0.0 of R studio) was applied. Data are presented as means ± SEM and individual values are plotted as grey and black dots for respectively summer and winter values. Means, SEM, fold change and associated *p*-values are reported in supplementary Tables S2 to S5. Statistical significance was considered with *p* values or adjusted *p* values lower than 0.05.

## Supplementary Information

The online version contains supplementary material available at https://doi.org/10.1186/s12983-020-00380-y.

**Additional file 1 Table S1.** Characteristics of brown bears included in the study. **Table S2.** Serum fatty acid concentrations (mmol/L) in winter hibernating (WBS) and summer active (SBS) bears. **Table S3.** Serum fatty acid relative proportions (mol %) in winter hibernating (WBS) and summer active (SBS) bears. **Table S4.** List of primers used for RT-qPCR.
<caption>**Table S5:** Endocannabinoids (eCBs) and mRNA quantification in plasma and tissues in winter hibernating (W) and summer active (S) bears.</caption>

**Abbreviations**

AA: Arachidonic acid; 2-AcG: 2-acylglycerol; AEA: Anandamide; 2-AG: 2-arachidonylglycerol; ALA: Alpha-linolenic acid; AMPK: AMP-activated protein kinase; CNR1: Cannabinoid receptor 1 (gene); CB1: Cannabinoid receptor 1; CNR2: Cannabinoid receptor 2 (gene); CB2: Cannabinoid receptor 2; DAGLA: Diacylglycerol lipase α; DAGLB: Dicacylglycerol lipase β; DPA: Docosapentaenoic acid; DHA: Docosahexaenoic acid; eCB: Endocannabinoid; eCB-like: Endocannabinoid-like compound; ECS: Endocannabinoid system; EPA: Eicosapentaenoic acid; FA: Fatty acid; FAAH: Fatty acid amide hydrolase; GPR55: G protein-coupled receptor 55; GPR119: G protein-coupled receptor 119; LA: Linoleic acid; MGLL: Monoacylglycerol lipase; mTOR: Mammalian target of rapamycin; MUFA: Monounsaturated fatty acid; NAE: N-acyl-phosphatidylethanolamine; NAPEPLD: N-acyl-phosphatidylethanolamine-hydrolyzing phospholipase D; OA: Oleic acid; OEA: N-oleoylethanolamide; PA: Palmitic acid; PDH: Pyruvate dehydrogenase; PDK4: Pyruvate dehydrogenase kinase 4; PPARA: Peroxisome proliferator-activated receptor α; PUFA: Polyunsaturated fatty acid; SA: Stearic acid; SBA: Summer bear adipose tissue; SBM: Summer bear muscle; SBP: Summer bear plasma; SBS: Summer bear serum; SFA: Saturated fatty acid; WBA: Winter bear adipose tissue; WBM: Winter bear muscle; WBP: Winter bear plasma; WBS: Winter bear serum

**Acknowledgments**

The authors wish to thank the field capture team (D Ahlqvist, A Friebe, H Nordin, H Blomgren, S Persson), and are grateful to Hélène Choubley and Victoria Bergas from the lipidomic platform of the university of Bourgogne-Franche-Comté for their valuable technical assistance.
This is scientific paper no. 296 from the SBBRP.

**Authors' contributions**

EL, and FB conceived the study; CBo, CBr, LCu, CD, JBP, IC, NBH, PD, AE, JMA, SB, EL, and FB performed the experiments and analyzed the data; CBr, FB and EL wrote the original draft; LCu, GG-K, CS, JS, FB, and EL reviewed and edited the manuscript. All authors read and approved the final manuscript.

**Funding**

This work was supported by the French Space Agency (CNES), iSITE Challenge 3 Mobility program (UCA), CNRS and Strasbourg University (H2E project; MyoBears project of the PEPS ExoMod program), French Proteomic Infrastructure (ProFI; ANR-10-INSB-08-03, and MetaHUB (French infrastructure in metabolomics & fluxomics; ANR-11-INBS- 0010). CBo was supported by a grant from the MESRI, LCu by grants from the INRAE and Clermont Metro-pole and CBr by a grant from French space agency (CNES). The long-term funding of Scandinavian Brown Bear Research Project (SBBRP) has come pri-marily from the Swedish Environmental Protection Agency, the Norwegian Environment Agency, the Austrian Science Fund, and the Swedish Associ-ation for Hunting and Wildlife Management.

**Availability of data and materials**

The datasets generated during and/or analyzed during the current study available from the corresponding author on reasonable request.

**Ethics approval**

All samples and data were collected under protocols approved by the Swedish Ethical Committee on Animal Experiment (applications Dnr C3/2016 and Dnr C18/2015), the Swedish Environmental Protection Agency (NV-00741-18), and the Swedish Board of Agriculture (Dnr 5.2.18–3060/17). All procedures complied with Swedish laws and regulations.

**Competing interests**

The authors declare no competing interests.

**Author details**

Plateform, Lyon, France. ⁵Department of Forestry and Wildlife Management, Inland Norway University of Applied Sciences, Campus Evenstad, NO-2480 Koppang, Norway. ⁶Department of Wildlife, Fish, and Environmental Studies, Swedish University of Agricultural Sciences, SE-901 83 Umeå, Sweden.
⁷Faculty of Environmental Sciences and Natural Resource Management, Norwegian University of Life Sciences, NO-1432 Ås, Norway. ⁸Centre National d'Etudes Spatiales, CNES, F-75001 Paris, France.

Received: 16 May 2020 Accepted: 20 October 2020

Published online: 23 November 2020

**References**

1. Carey HV, Andrews MT, Martin SL. Mammalian hibernation: cellular and molecular responses to depressed metabolism and low temperature. Physiol Rev. 2003;83:1153-81.

2. Geiser F. Hibernation. Curr Biol. 2013;23:R188-93.

3. Folk GE, Hunt JM, Folk MA. Further evidence for hibernation of bears. Bears Their Biol Manag. 1980;4:43.

4. Hellgren EC. Physiology of hibernation in bears. Ursus. 1998;10:467-77.

5. Hissa R, Hohtola E, Tuomala-Saramaki T, Laine T, Kallio H. Seasonal changes in fatty acids and leptin contents in the plasma of the European brown bear (Ursus arctos arctos). Ann Zool Fenn. 1998;35:215-24.

6. Manchi S, Swenson JE. Denning behaviour of Scandinavian brown bears Ursus arctos. Wildl Biol. 2005;11:123-32.

7. Toien O, Blake J, Edgar DM, Grahn DA, Heller HC, Barnes BM. Hibernation in black bears: independence of metabolic suppression from body temperature. Science. 2011;331:906-9.

8. LeBlanc PJ, Obbard M, Battersby BJ, Felskie AK, Brown L, Wright PA, et al. Correlations of plasma lipid metabolites with hibernation and lactation in wild black bears Ursus americanus. J Comp Physiol B. 2001;171:327-34.

9. Giroud S, Chery I, Bertile F, Bertrand-Michel J, Tascher G, Gauquelin-Koch G, et al. Lipidomics reveal seasonal shifts in large-bodied hibernator, the brown bear. Front Physiol. 2019;10:389.

10. Chazarin B, Storey KB, Ziemiianin A, Chanon S, Plumel M, Chery I, et al. Metabolic reprogramming involving glycolysis in the hibernating brown bear skeletal muscle. Front Zool. 2019;16:12.

11. Aloia RC, Raison JK. Membrane function in mammalian hibernation. Biochim Biophys Acta BBA - Rev Biomembr. 1989;988:123-46.

12. Munro D, Thomas DW. The role of polyunsaturated fatty acids in the expression of torpor by mammals: a review. Zool Jena. 2004;107:29-48.

13. Ruf T, Arnold W. Effects of polyunsaturated fatty acids on hibernation and torpor: a review and hypothesis. Am J Physiol-Regul Integr comp Physiol. American Physiological Society. 2008;294:R1044-52.

14. Arnold W, Ruf T, Frey-Roos F, Bruns U. Diet-Independent Remodeling of Cellular Membranes Precedes Seasonally Changing Body Temperature in a Hibernator. PLOS ONE. Public Libr Sci. 2011;6:e18641.

15. Battista N, Di Tommaso M, Bari M, Maccarrone M. The endocannabinoid system: an overview. Front Behav Neurosci. 2012;14:6-9.

16. De Petrocellis L, Di Marzo V. An introduction to the endocannabinoid system: from the early to the latest concepts. Best Pract Res Clin Endocrinol Metab. 2009;23:1-15.

17. Fezza F, Bari M, Florio R, Talamonti E, Feole M, Maccarrone M. Endocannabinoids, related compounds and their metabolic routes. Mol Basel Switz. 2014;19:17078-106.

18. Aizpurua-Olaizola O, Elezgarai I, Rico-Barrio I, Zarandona I, Etxebarria N, Usobiaga A. Targeting the endocannabinoid system: future therapeutic strategies. Drug Discov Today. 2017;22:105-10.

19. Di Marzo V. New approaches and challenges to targeting the endocannabinoid system. Nat Rev Drug Discov. 2018;17:623-39.

20. Ligresti A, Petrosino S, Di Marzo V. From endocannabinoid profiling to 'endocannabinoid therapeutics.' Curr Opin Chem Biol 2009;13:321-331.

21. Zou S, Kumar U. Cannabinoid receptors and the Endocannabinoid system: signaling and function in the central nervous system. Int J Mol Sci. 2018;19:833.

22. Di Marzo V, De Petrocellis L. Why do cannabinoid receptors have more than one endogenous ligand? Philos Trans R Soc B Biol Sci. 2012;367:3216-28.

23. Di Marzo V, Maccarrone M. FAAH and anandamide: is 2-AG really the odd one out? Trends Pharmacol Sci. 2008;29:229-33.

24. Wilson RI, Nicoll RA. Endocannabinoid signaling in the brain. Science. 2002; 296:678-82.

25. Piazza PV, Cota D, Marsicano G. The CB1 receptor as the cornerstone of exostosis. Neuron. 2017;93:1252-74.

<footnote n="1">¹Université Clermont Auvergne, INRAE, UNH, Clermont-Ferrand, France.</footnote>

<footnote n="2">²Université de Strasbourg, CNRS, IPHC UMR 7178, Strasbourg, France.</footnote>

<footnote n="3">³Plateforme de Lipidomique, INSERM UMR1231, Université de Bourgogne, Dijon, France. ⁴Université de Lyon, INSERM, INRAE, INSA, Functional Lipidomic</footnote>
26. Shrestha N, Cuffe JSM, Hutchinson DS, Headrick JP, Perkins AV, McAinch AJ, et al. Peripheral modulation of the endocannabinoid system in metabolic disease. Drug Discov Today. 2018;23:592-604.

27. Silvestri C, Di Marzo V. The Endocannabinoid system in energy homeostasis and the Etiopathology of metabolic disorders. Cell Metab. 2013;17:475-90.

28. Matias I, Bisogno T, Marzo VD. Endogenous cannabinoids in the brain and peripheral tissues: regulation of their levels and control of food intake. Int J Obes Nature Publishing Group. 2006;30:57-12.

29. Prospéro-García O, Amancio-Belmont O, Becerril Meléndez AL, Ruiz-Contreras AE, Méndez-Díaz M. Endocannabinoids and sleep. Neurosci Biobehav Rev. 2016;71:671-9.

30. Vaughn LK, Denning G, Stuhr KL, de Wit H, Hill MN, Hillard CJ. Endocannabinoid signalling: has it got rhythm? Br J Pharmacol. 2010;160:530-43.

31. Cardinal P, Bellocchio L, Clark S, Cannich A, Klugmann M, Lutz B, et al. Hypothalamic CB1 cannabinoid receptors regulate energy balance in mice. Endocrinology. 2012;153:4136-43.

32. Osei-Hyiaman D, DePetrillo M, Pacher P, Liu J, Radaeva S, Bátkai S, et al. Endocannabinoid activation at hepatic CB1 receptors stimulates fatty acid synthesis and contributes to diet-induced obesity. J Clin Invest. 2005;115: 1298-305.

33. Turcotte C, Blanchet M-R, Laviolette M, Flamand N. The CB2 receptor and its role as a regulator of inflammation. Cell Mol Life Sci. 2016;73:4449-70.

34. Cavuoto P, McAinch AJ, Hatzinikolas G, Janovská A, Game P, Wittert GA. The expression of receptors for endocannabinoids in human and rodent skeletal muscle. Biochem Biophys Res Commun. 2007;364:105-10.

35. Starowicz KM, Cristino L, Matias I, Capasso R, Racioppi A, Izzo AA, et al. Endocannabinoid Dysregulation in the pancreas and adipose tissue of mice fed with a high-fat diet. Obesity. 2008;16:553-65.

36. Agudo J, Martin M, Roca C, Molas M, Bura AS, Zimmer A, et al. Deficiency of CB2 cannabinoid receptor in mice improves insulin sensitivity but increases food intake and obesity with age. Diabetologia. 2010;53:2629-40.

37. Deveaux V, Cadoudal T, Ichigotani Y, Teixeira-Clerc F, Louvet A, Manin S, et al. Cannabinoid CB2 Receptor Potentiates Obesity-Associated Inflammation, Insulin Resistance and Hepatic Steatosis. PLOS ONE. Public Libr Sci. 2009;4:e5844.

38. Bowen KJ, Kris-Etherton PM, Shearer GC, West SG, Reddivari L, Jones PJH. Oleic acid-derived oleoylethanolamide: a nutritional science perspective. Prog Lipid Res. 2017;67:1-15.

39. Guzmán M, Verme JL, Fu J, Oveisi F, Blázquez C, Piomelli D. Oleoylethanolamide stimulates lipolysis by activating the nuclear receptor peroxisome proliferator-activated receptor α (PPAR-α). J Biol Chem. 2004; 279:27849-54.

40. Kirkwood JS, Broeckling CD, Donahue S, Prenni JE. A novel microflow LC-MS method for the quantitation of endocannabinoids in serum. J Chromatogr B Analyt Technol Biomed Life Sci. 2016;1033-1034:271-7.

41. Mulawa EA, Kirkwood JS, Wolfe LM, Wojda SJ, Prenni JE, Florant GL, et al. Seasonal changes in Endocannabinoid concentrations between active and hibernating marmots (Marmota flaviventris). J Biol Rhythm. 2018;33:388-401.

42. Stewart JM, Boudreau NM, Blakely JA, Storey KB. A comparison of oleamide in the brains of hibernating and non-hibernating Richardson's ground squirrel (Spermophilus richardsonii) and its inability to bind to brain fatty acid binding protein. J Therm Biol. 2002;27:309-15.

43. Graesli AR, Evans AL, Fahlman Å, Bertelsen MF, Blanc S, Arnemo JM. Seasonal variation in haematological and biochemical variables in free-ranging subadult brown bears (Ursus arctos) in Sweden. BMC Vet Res. 2015;11:301.

44. Deval C, Capel F, Laillet B, Polge C, Béchet D, Taillandier D, et al. Docosahexaenoic acid-supplementation prior to fasting prevents muscle atrophy in mice. J Cachexia Sarcopenia Muscle. 2016;7:587-603.

45. McGlory C, Calder PC, Nunes EA. The influence of Omega-3 fatty acids on skeletal muscle protein turnover in health, disuse, and disease. Front Nutr. 2019;6:144.

46. Wei H-K, Zhou Y, Jiang S, Tao Y-X, Sun H, Peng J, et al. Feeding a DHA-enriched diet increases skeletal muscle protein synthesis in growing pigs: association with increased skeletal muscle insulin action and local mRNA expression of insulin-like growth factor 1. Br J Nutr. 2013;110:671-80.

47. Simopoulos AP. The importance of the ratio of omega-6/omega-3 essential fatty acids. Biomed Pharmacother. 2002;56:365-79.

48. Bosch-Bouju C, Layé S. Dietary Omega-6/Omega-3 and Endocannabinoids: implications for brain health and diseases. 2016; in "cannabinoids in health and disease", (Meccariello R. and Chianese R. eds). IntechOpen (Rijeka).

49. Naughton SS, Mathai ML, Hryciw DH, McAinch AJ. Fatty acid modulation of the Endocannabinoid system and the effect on food intake and metabolism. Int J Endocrinol. 2013;2013:361895.

50. Alvheim AR, Torstensen BE, Lin YH, Lillefosse HH, Lock E-J, Madsen L, et al. Dietary linoleic acid elevates the Endocannabinoids 2-AG and Anandamide and promotes weight gain in mice fed a low fat diet. Lipids. 2014;49:59-69.

51. Alvheim AR, Malde MK, Osei-Hyiaman D, Lin YH, Pawlosky RJ, Madsen L, et al. Dietary linoleic acid elevates endogenous 2-AG and anandamide and induces obesity. Obes Silver Spring Md. 2012;20:1984-94.

52. Ghosh S, O'Connell JF, Carlson OD, González-Mariscal I, Kim Y, Moaddel R, et al. Linoleic acid in diets of mice increases total endocannabinoid levels in bowel and liver: modification by dietary glucose. Obes Sci Pract. 2019;5:383-94.

53. Schwartz GJ, Fu J, Astarita G, Li X, Gaetani S, Campolongo P, et al. The lipid messenger OEA links dietary fat intake to satiety. Cell Metab. 2008;8:281-8.

54. Walker C, West A, Browning L, Madden J, Gambell J, Jebb S, et al. The pattern of fatty acids displaced by EPA and DHA following 12 months supplementation varies between blood cell and plasma fractions. Nutrients. 2015;7:6281-93.

55. Matias I, Carta G, Murru E, Petrosino S, Banni S, Di Marzo V. Effect of polyunsaturated fatty acids on endocannabinoid and N-acyl-ethanolamine levels in mouse adipocytes. Biochim Biophys Acta BBA - Mol Cell Biol Lipids. 1781;2008;52-60.

56. DiPatrizio NV, Igarashi M, Narayanaswami V, Murray C, Gancayco J, Russell A, et al. Fasting stimulates 2-AG biosynthesis in the small intestine: role of cholinergic pathways. Am J Physiol - Regul Integr Comp Physiol. 2015;309: R805-13.

57. Cavuoto P, McAinch AJ, Hatzinikolas G, Cameron-Smith D, Wittert GA. Effects of cannabinoid receptors on skeletal muscle oxidative pathways. Mol Cell Endocrinol. 2007;267:63-9.

58. Mugahid DA, Sengul TG, You X, Wang Y, Steil L, Bergmann N, et al. Proteomic and Transcriptomic changes in hibernating grizzly bears reveal metabolic and signaling pathways that protect against muscle atrophy. Sci Rep. 2019;9:19976.

59. Esposito I, Proto MC, Gazzerro P, Laezza C, Miele C, Alberobello AT, et al. The cannabinoid CB1 receptor antagonist Rimonabant stimulates 2-Deoxyglucose uptake in skeletal muscle cells by regulating the expression of Phosphatidylinositol-3-kinase. Mol Pharmacol. 2008;74:1678-86.

60. Vella CA, Nelson OL, Jansen HT, Robbins CT, Jensen AE, Constantinescu S, et al. Regulation of metabolism during hibernation in brown bears (Ursus arctos): involvement of cortisol, PGC-1α and AMPK in adipose tissue and skeletal muscle. Comp Biochem Physiol A Mol Integr Physiol. 2019;240:110591.

61. Engeli S. Dysregulation of the endocannabinoid system in obesity. J Neuroendocrinol. 2008;20(Suppl 1):110-5.

62. Nesto RW, Mackie K. Endocannabinoid system and its implications for obesity and cardiometabolic risk. Eur Heart J Suppl Oxford Academic. 2008; 10:B34-41.

63. Di Marzo V. The endocannabinoid system in obesity and type 2 diabetes. Diabetologia. 2008;51:1356-67.

64. Rigano KS, Gehring JL, Evans Hutzenbiler BD, Chen AV, Nelson OL, Vella CA, et al. Life in the fat lane: seasonal regulation of insulin sensitivity, food intake, and adipose biology in brown bears. J Comp Physiol B. 2017;187:649-76.

65. Fröbert O, Fröbert AM, Kindberg J, Arnemo JM, Overgaard MT. The brown bear as a translational model for sedentary lifestyle-related diseases. J Intern Med. 2019;joim.12983.

66. Proulx K, Cota D, Castañeda TR, Tschöp MH, D'Alessio DA, Tso P, et al. Mechanisms of oleoylethanolamide-induced changes in feeding behavior and motor activity. Am J Physiol-Regul Integr Comp Physiol. 2005;289:R729-37.

67. Sarro-Ramirez A, Sanchez-Lopez D, Tejeda-Padron A, Frias C, Zaldivar- Rae J, Murillo-Rodriguez E. Brain Molecules and Appetite: The Case of Oleoylethanolamide. Cent Nerv Syst Agents Med Chem. 2013;13:88-91

68. Fu J, Astarita G, Gaetani S, Kim J, Cravatt BF, Mackie K, et al. Food Intake Regulates Oleoylethanolamide Formation and Degradation in the Proximal Small Intestine. J Biol Chem. 2007;282:1518-28.

69. Izzo AA, Piscitelli F, Capasso R, Marini P, Cristino L, Petrosino S, et al. Basal and fasting/refeeding-regulated tissue levels of endogenous PPAR-alpha ligands in Zucker rats. Obes Silver Spring Md. 2010;18:55-62.

70. Fedele S, Arnold M, Krieger J-P, Wolfstädter B, Meyer U, Langhans W, et al. Oleoylethanolamide-induced anorexia in rats is associated with locomotor impairment. Physiol Rep. 2018;6:e13517.

71. Murillo-Rodriguez E, Palomero-Rivero M, Millán-Aldaco D, Arias-Carrión O, Drucker-Colín R. Administration of URB597, Oleoylethanolamide or
Palmitoylethanolamide Increases Waking and Dopamine in Rats. PLOS ONE.
2011;6:e20766.

72. Swenson JE, Sandegren F, Brunberg S, Wabakken P. Winter den abandonment by brown bears Ursus arctos: causes and consequences. Wildl Biol. Nordic Board for Wildlife Research; 1997;3:35-8.

73. Linnell JDC, Swenson JE, Andersen R, Barnes B. How Vulnerable Are Denning Bears to Disturbance? Wildl Soc Bull. 2000;28:400-13.

74. Evans AL, Singh NJ, Fuchs B, Blanc S, Friebe A, Laske TG, et al. Physiological reactions to capture in hibernating brown bears. Conserv Physiol. 2016;4: cow61.

75. Chanon S, Chazarin B, Toubhans B, Durand C, Chery I, Robert M, et al. Proteolysis inhibition by hibernating bear serum leads to increased protein content in human muscle cells. Sci Rep. 2018;8:5525.

76. Lefils J, Géloën A, Vidal H, Lagarde M, Bernoud-Hubac N. Dietary DHA: time course of tissue uptake and effects on cytokine secretion in mice. Br J Nutr. 2010;104:1304-12.

77. R Development Core Team. R: a language and environment for statistical computing. R Foundation for Statistical Computing, Vienna. 2008; ISBN 3-900051-07-0. Available from: https://www.r-project.org/.

**Publisher's Note**

Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Ready to submit your research? Choose BMC and benefit from:

* fast, convenient online submission

* thorough peer review by experienced researchers in your field

* rapid publication on acceptance

* support for research data, including large and complex data types

* gold Open Access which fosters wider collaboration and increased citations

* maximum visibility for your research: over 100M website views per year

At BMC, research is always in progress.

Learn more biomedcentral.com/submissions

<figure><img src="image_10.png" /></figure>