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A proposed modulatory role of the endocannabinoid system on adipose tissue metabolism and appetite in periparturient dairy cows

Journal of Animal Science and Biotechnology volume 12, Article number: 21 (2021) Cite this article

Abstract

To sustain the nutrient demands of rapid fetal growth, parturition, and milk synthesis, periparturient dairy cows mobilize adipose tissue fatty acid stores through lipolysis. This process induces an inflammatory response within AT that is resolved as lactation progresses; however, excessive and protracted lipolysis compounds the risk for metabolic and inflammatory diseases. The suppression of lipolytic action and inflammation, along with amplification of adipogenesis and lipogenesis, serve as prospective therapeutic targets for improving the health of periparturient dairy cows. Generally, the activation of cannabinoid receptors by endocannabinoids enhances adipogenesis and lipogenesis, suppresses lipolysis, and increases appetite in mammals. These biological effects of activating the endocannabinoid system open the possibility of harnessing the endocannabinoid system through nutritional intervention in dairy herds as a potential tool to improve dairy cows’ health, although much is still to be revealed in this context. This review summarizes the current knowledge surrounding the components of the endocannabinoid system, elaborates on the metabolic effects of its activation, and explores the potential to modulate its activity in periparturient dairy cows.

Introduction

To meet the energy needs of her growing fetus, parturition, and onset of lactation during a dairy cow’s periparturient period, profound metabolic and endocrine adaptations must occur. It is well established that this period of high-energy requirement is coupled with a reduction in appetite (i.e., dry matter intake [1]), setting the stage for negative energy balance. To compensate for energy deficits, fatty acids (FA) stored as triacylglycerols (TAG) within adipose tissue’s (AT) cellular unit, the adipocyte, are mobilized (Fig. 1) [2]. Although this metabolic challenge is normal and necessary during the periparturient period, some cows fail to adapt, which increases their risk for metabolic and inflammatory diseases.

Fig. 1
figure 1

The ECS promotes energy conservation and reduces lipolysis in mature white adipocytes. Lipolysis: CB1 activation on the adipocyte surface inhibits the activity of the lipolytic enzymes HSL and PLIN, while CB1 activation in autonomous nerves limits the release of catecholamines, the primary ligand for β-adrenergic receptors. Lipogenesis and adipogenesis: eCBs bind and activate PPARγ directly, enhancing transcription of pro-lipogenic and pro-adipogenic genes: Improved expression of GLUT4 and LPL leads to greater levels of lipogenesis. Mitochondrial biogenesis: CB1 activation suppresses the activity of the transcriptional coactivator PGC-1α; the principal inducer of mitochondrial biogenesis. Abbreviations: 5′ AMP-activated protein kinase (AMPK), Adenosine triphosphate (ATP), Adenylyl cyclase (AC), Adipose triglyceride lipase (ATGL), Anandamide (AEA), Beta adrenergic receptor (β-ADR), Calcium (Ca2+), Calcium/calmodulin-dependent protein kinase kinase 2 (CaMKKβ), Cannabinoid receptor 1 (CB1), Chylomicron (CM), Cyclic adenosine monophosphate (camp), Diacylglycerol lipase (DAG), Endocannabinoid membrane transporter (EMT), Extracellular signal-regulated kinase (ERK1/2), Factor associated with neutral sphingomyelinase activation (FAN), Fatty acid (FA), Fatty acid transport protein (FATP), G alpha subunit (Gαs), G protein-coupled receptor 55 (GPR55), Gi protein subunit o (Gi/o), Glucose (GLU), Glucose transporter type 4 (GLUT-4), Guanine nucleotide binding protein subunit 12/13 (Gα12/13), Guanine nucleotide binding protein subunit q (GαQ), Hormone-sensitive lipase (HSL), Insulin (I), Insulin receptor (IR), Lipoprotein lipase (LPL), Mammalian target or rapamycin complex 1 (MTORC1), Mitogen-activated extracellular signal-regulated kinase (MEK), Mitogen-activated protein kinase (MAPK), Monoacylglycerol (MAG), Monoglyceride lipase (MGL), N-Acyltransferase (NAT), NAPE-phospholipase D (PLD), N-Arachidonyl phosphatidylethanolamine (NAPE), Neutral sphingomyelinase (EMN), Norepinephrine (NE), Perilipin (PLIN), Peroxisome proliferator-activated receptor gamma (PPARγ), Phosphatidylinositol 4,5 bisphosphate (PIP2), Phospholipase C (PLC), Phosphorylation (P), Potassium (K+), PPAR-gamma coactivator 1α (PGC-1α), Protein kinase A (PKA), Protein kinase B (Akt/PKB), Protein kinase C (PKC), Ras homolog family member A (RHOA), Retinoid X receptor (RXR), Rho-associated protein kinase (ROCK), Sphingomyelin (EM), Triacylglycerol (TAG), Tuberous sclerosis complex 2 (TSC2), Vallinoid receptor 1 (TRPV1)

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The AT is composed of adipocytes, fibroblasts, progenitor cells, endothelial cells, and immune cells. White adipocytes are largely comprised of a single substantial fat droplet (up to 90% of the cell’s volume), a limited number of mitochondria, and a compressed nucleus. In response to increased energy needs, TAG stored in the lipid droplet are hydrolyzed during lipolysis to release FA and glycerol. In times of excess energy, the AT expands by enlarging the size of adipocytes’ lipid droplets (lipogenesis), or by increasing the number of adipocytes (adipogenesis) (as displayed in Figs. 1 and 2). In addition to the provision of energy, AT serves as an endocrine organ and secretes several factors associated with the modulation of energy metabolism, including adipokines (e.g., adiponectin, leptin, resistin) and, as recently described, endocannabinoids (eCBs) [3]. Research over the past two decades highlights the endocannabinoid system (ECS) as a potent coordinator of AT function. The ECS consists of eCBs, cannabinoid receptors, and enzymes involved in the synthesis and degradation of eCBs. Functions of the ECS include regulation of physical exertion, immunomodulation, modification of cellular proliferation, and preservation of energy-storing reservoirs [4]. The ECS, when active, favors the accumulation of fat mass through both central and peripheral pathways [5]. Within AT, ECS activation promotes adipogenesis and lipogenesis and impedes lipolytic activity (Figs. 1 and 2). In addition to these functions, the ECS enhances appetite in mammals through paracrine and endocrine signals as well as neural pathways. The role of ECS on modulating these important metabolic processes emphasizes the potential of the ECS to reduce the intensity and duration of negative energy balance in periparturient cows.

Fig. 2
figure 2

The ECS enhances transcriptional machinery of PPARγ and lipid accumulation, promoting adipogenesis and lipogenesis in maturing progenitor cells. Red arrows: inhibitory effect downstream of eCB stimulation. Green arrows: stimulatory effect downstream of eCB stimulation. Abbreviations: Adenylyl cyclase (AC), adiponectin (ApN), Cannabinoid receptor 1 (CB1), Cyclic adenosine monophosphate response element-binding protein (CREB), Endocannabinoid (eCB), Extracellular signal-regulated kinase (ERK), Fatty acid binding protein 4 (FABP4), Fatty acid translocase (CD36), Fatty acid transport protein (FATP), Fibroblast growth factor 1, 2, 10 (FGF1, 2, 10), Free fatty acid (FFA), Gi protein subunit o (Gi/o), Glucose transporter type 4 (GLUT-4), insulin (I), Insulin receptor (IR), Insulin receptor substrate (IRS), Lipoprotein lipase (LPL), Peroxisome proliferator-activated receptor gamma (PPARγ), Retinoid X receptor (RXR), Tumor necrosis factor alpha (TNFα), Vascular endothelial growth factor D (VEGF-D)

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The adipose tissue endocannabinoid system

Endocannabinoids

eCBs consist of lipid intermediaries, including amides, esters, and ethers of polyunsaturated FAs [6]. eCBs possess structural similarities to exogenous cannabinoids, such as a phenolic hydroxyl at the carbon C-1 and an alkyl side chain at the carbon C-3 [7]. Both eCBs and exogenous CBs (such as (−)-trans-Δ9-tetrahydrocannabinol, THC) bind to CB receptors in mammalian tissues [8].

Synthesized rapidly in response to an increase in intracellular calcium levels, metabolic stress, or cellular damage, eCBs are derived from dietary FAs [9]. These ligands bind and activate the canonical CB receptors type 1 and 2 (CB1 and CB2, respectively), the vallinoid receptor TRPV1, G protein-coupled receptor 55 (GPR55), and members of the peroxisome proliferator-activated receptor (PPAR) family [10]. The two most abundant (and potent) eCBs are the arachidonic acid-containing AEA (anandamide, N-arachidonoylethanolamide) and 2-AG (2-arachidonyglycerol) [11]. Lesser-known eCB molecules include palmitoylethanolamine (PEA) and oleoylethanolamine (OEA). These compounds have not been studied in ruminants and, therefore, are beyond the scope of this review (readers are referred to a detailed literature revision elsewhere [12]).

In dairy cows, plasma 2-AG concentrations increase from 1.5 ± 0.94 nmol/mL during the dry period to 3.0 ± 0.94 nmol/mL one month after parturition [13]. In AT from cows exhibiting high postpartum weight loss (> 8% during the first month postpartum), AEA and 2-AG levels double from 0.94 ± 0.23 fmol/mg and 0.56 ± 0.10 nmol/mg at − 14 days relative to parturition, to 2.18 ± 0.23 fmol/mg and 0.97 ± 0.10 nmol/mg 4 days after calving [14]. In contrast, cows exhibiting low weight loss do not show dramatic increases in plasma and AT AEA or 2-AG levels when compared to high weight loss groups [13, 14]. These changes in plasma and AT eCB content suggest that the ECS may be activated to a greater extent in cows experiencing greater levels of lipolysis. It is presently unknown if high eCB content is an anti-lipolytic response of the AT to reduce TAG breakdown or if it is a consequence of the high availability of eCB precursors driven by lipolysis.

Biosynthesis of eCBs

AEA

There are three proposed biosynthetic pathways for AEA (illustrated in Fig. 3a): The first pathway begins with the N-acylation of the phospholipid membrane precursor phosphatidylethanolamine (PE) by the Ca2+-dependent N-acyltransferase (NA) to produce N-arachidonylphosphatidylethanolamine (NAPE) [15, 16]. Next Ca2+-activated enzyme N-arachidonylphosphatidylethanolamine-specific phospholipase D (NAPE-PLD) acts on NADE yielding AEA. The second pathway includes the hydrolysis of NAPE (after N-acylation by NA) by type-C phospholipase (PLC) to phosphoanandamide. This is followed by dephosphorylation by Src homology 2 domain-containing inositol-5-phosphatase 1 to produce AEA [17]. In pathway three, repeated hydrolytic cleavage of NAPE’s acyl groups by the serine hydrolase abhydrolase domain containing 4 to form lyso-NAPE and then glycerophospho-N-AEA. This product is then hydrolyzed by the metal-dependent glycerophosphodiester phosphodiesterase 1 to AEA [18].

Fig. 3
figure 3

Proposed biosynthetic pathways for AEA (a) and 2-AG (b) formation. Abbreviations: Arachidonic acid (AA), Arachidonoyl ethanolamine (AEA), Ethanolamine (EA), Fatty acid amide hydrolase (FAAH), Glycerophosphoanandamide (GP-N-AEA), Lyso-NAPE, abhydrolase domain-containing 4 (ABHD4), N-acyltransferase (NAT), NAPE-phospholipase D (NAPE-PLD), N-arachidonylphosphatidylethanolamine (NAPE), Phosphatidyl ethanolamine (PE), Phosphoanandamide (P-AEA), Phosphodiesterase (PDE), Phospholipase C (PLC), Protein tyrosine phosphatase (PTPN22), Src Homology 2 domain-containing inositol-5-phosphatase 1 (SH2DI5P1). 2-AG lysophosphatidyl inositol (2-AG-LPI), 2-arachidonoyl glycerol (2-AG), 2-arachidonoyl phospholipids (2-A PPL), 2-lysophosphatidic acid phosphatase (2-LPAP), Adipose triglyceride lipase (ATGL), Diacylglycerol (DAG), DAG lipase (DAGL), Hormone-sensitive lipase (HSL), Lyso-PLC, 2-AG-lysophosphatidic acid (2-AG-LPA), N-acyltransferase (NAT), Phosphatidyl inositol (PI), Phosphatidyl inositol bisphosphate 2 (PIP2), Phospholipase 1 (PLA1), PIP2 phosphatase (PIP2P), Triacylglycerol (TAG)

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2-AG

2-AG is the hydrolyzed product of 2-arachidonoyl-containing phospholipids (mainly arachidonoyl-containing phosphatidyl inositol bis-phosphate, PIP2). There are three main routes proposed for the intracellular biosynthesis of 2-AG (Fig. 3b): 1) diacylglycerol (DAG) is synthesized from PIP2 and then hydrolyzed by the enzyme diacylglycerol lipase (DAGL). 2) 2-arachidonoyl-lysophosphatidic acid is hydrolyzed by 2-lysophosphatidic acid phosphatase into the bioactive eCB. 3) 2-arachidonoyl-lysophosphatidylinositosol, a derivative of PIP2, is synthesized into 2-AG by lyso-PLC [19].

Degradation of eCBs

Non-oxidative enzymatic degradation of eCBs

The two primary enzymes that catabolize eCBs are the serine hydrolase FAAH and monoacylglycerol lipase (MAGL) [20]. FAAH, a membrane-bound enzyme, favors AEA as a substrate but hydrolyzes other long-chain amides and amines (detailed description in [21, 22]. The hydrolysis of AEA, OEA, and PEA by FAAH yields ethanolamine and AA, oleic acid, and palmitic acid, respectively [23]. The expression and activity of these non-oxidative pathways in AT are affected by anatomical location and degree of adiposity. Visceral AT exhibits a higher expression of these eCB catabolic pathways compared to subcutaneous depots [24]. In humans, levels of visceral FAAH are lower in obese humans compared to lean subjects [25], suggesting that eCB degradation by FAAH may be inhibited in larger adipocytes.

MAGL hydrolyzes 2-AG and is likely to be the primary route of degradation for 2-AG into AA and glycerol [26]. Unlike FAAH, which is expressed ubiquitously, MAGL is expressed predominantly in AT [27]. Notably, genetic or pharmacological blockade of MAGL in mice leads to elevated levels of 2-AG in the brain and enhances the sensitivity of CB1 to eCBs [20], unlike FAAH blockade, which causes CB1 desensitization [28].

MAGL appears to be a major degradative enzyme of eCBs in periparturient dairy cows. We demonstrated that MAGL protein abundance in AT is lower in cows experiencing high weight loss compared to those with minimal body weight changes [14]. In the same study, FAAH concentrations remained stable across groups throughout the sampling period [14]. However, MAGL protein abundance was higher in insulin-resistant vs. insulin-sensitive AT from postpartum cows [29]. More information on the role of MAGL in AT lipolysis and ECS activation in dairy cows is required to explore the possibility of using this enzyme as a pharmacological target for intervention.

Additional enzymes known to degrade eCBs include the serine hydrolases α/β hydrolase 6 (ABHD6), and α/β hydrolase 12 (ABHD12), which degrade 2-AG in the brain [30], and N-acylethanolamine-hydrolyzing acid amidase (NAAA), which hydrolyzes N-acylethanolamines under acidic conditions [31]. In dairy cows, the expression of genes encoding for ABHD12 and NAAA was reported in the reproductive tract but not in AT. Periparturient dairy cows with subclinical endometritis had a reduced endometrial mRNA expression of NAAA compared to healthy controls [32]. ABHD6 and ABHD12 levels are expressed differently during the follicular development of oocytes [33]; however, the role that these enzymes play in the ECS in AT remains to be explored in dairy cows.

Oxidative degradation of eCBs

Enzymes such as cyclooxygenases (COX), lipoxygenases (LOX), and cytochromes P450 (CYP450) are capable of oxidizing eCBs (reviewed in [34]). These enzymes are part of the inflammatory process as a source of inflammatory lipid mediators, also known as oxylipids. These products are oxidized FAs derived from phospholipid membranes or triglycerides contained in lipid droplets that regulate the different stages of inflammation from onset to resolution [35]. In AT from dairy cows, we demonstrated the expression and functionality of COX, LOX, and P450s [36]. The full extent to which these oxidative enzymes act on eCBs in ruminant AT remains unknown. However, pharmacological blockade of these eCB-oxidizing pathways in dairy cows’ AT may be beneficial during the periparturient period as eCBs may promote lipogenesis and thus counteract lipolysis. Also, there are reports of eCBs acting as suppressors of AT inflammation [37] and inhibitors of pain sensation [38]; therefore, inhibiting eCB-degrading enzymes could offer some advantages by reducing AT inflammation. Nevertheless, recent studies indicate that when eCB precursors are fed at high levels in mice and salmon, inflammatory responses within AT are observed along with enhanced levels of eCBs [39]. These conflicting findings highlight the complexity of the ECS in AT and emphasize the need for further research to elucidate the role of eCB in AT inflammatory responses of dairy cattle.

Cellular receptors of eCBs

CB1

The two primary receptors of the ECS are the G protein-coupled receptors (GCPRs) CB1 and CB2, encoded by the CNR1 and CNR2 genes, respectively. CB1 belongs to the Class A GCPRs, known to activate inward-propelling potassium channels and inhibit calcium channels [40]. In humans and rodents, CB1 receptors are expressed at the highest levels in neural tissue, and lower levels of expression are observed in AT, liver, skeletal muscle, and peripheral organs [41]. In adipocytes, CB1 receptor stimulation increases the uptake of glucose and lipogenesis while inhibiting lipolysis [42]. CB1 conducts its response via G protein Gi/o-mediated reduction in adenylate cyclase action, suppressing the activation of hormone-sensitive lipase (HSL) through the halt in cyclic adenosine monophosphate (cAMP) production [43].

CB2

CB2 is found primarily in microvascular endothelial cells and on the surface of immune cells, most commonly those derived from the hematopoietic lineage [44]. CB2 is known to exert anti-inflammatory effects in peripheral tissues [45], and only low levels of CB2 expression are detected in monogastric AT [46]. In humans, CB2 expression has been shown to decrease as pre-adipocytes mature into adipocytes in vitro [24]. This mRNA expression pattern suggests that within AT, CB2 content is higher in preadipocytes, macrophages, and vascular cells rather than in mature adipocytes [24].

GPR55

Belonging to the rhodopsin-like (Class A) family of GPCRs, GPR55 expression is detected in brain and neural tissues, immune cells, spleen, blood vessels, small intestine, endometrium, and AT [47]. This receptor activates PLC, which stimulates inward-propelling Ca2+ channels. PLC activation catalyzes the cleavage of PIP2 to inositol triphosphate and DAG (diacylglycerol) [48]; GPR55 activation also promotes insulin secretion in pancreatic β-cells [49], and its suppression is associated with adiposity [50] and impaired insulin signaling in AT [47].

TRPV1

TRPV1 is a non-selective ion channel expressed most prominently in neural tissues. This receptor is also found in a wide range of tissues, including blood vessels, the gastrointestinal tract, immune cells, endothelial cells lining the urinary tract, and adipocytes [51]. TRPV1’s direct role in AT metabolism lies in its ability to increase intracellular calcium levels, which activates mitochondrial biogenesis through enhanced 5′ adenosine monophosphate-activated protein kinase (AMPK) activity [52] and by peroxisome proliferator-activated receptor gamma coactivator 1 (PGC-1α) activation of uncoupling protein 1 (UCP-1) by route of sirtuin-1 (SIRT-1) [53]. The eCB AEA is known to activate the TRPV1 receptor and B-lymphocyte-derived (B1 cell-derived) leukotriene B4, which regulates the local inflammatory response in AT as a TRPV1 agonist [54].

CB receptors in AT of dairy cows

AT expression of CNR1 (encoding CB1) and CNR2 (encoding CB2) increase after calving in dairy cows exhibiting high rates of lipolysis [14]. Dirandeh et al. [55] demonstrated that higher gene expression of CNR2, NAPEPLD, and FAAH in AT coincides with enhanced expression of pro-inflammatory genes (TNF-α, IL-6, IL-1β) at 21 and 42 days postpartum in cows exhibiting intense AT lipolysis. Also, CB receptor expression is affected during inflammatory diseases, as shown in cows with endometritis, where endometrial CNR2 transcription is amplified [32]. These expression patterns indicate a possible link between ECS and AT inflammatory responses; however, further research is required to understand the role of ECS in adipose inflammation in dairy cows, specifically during the periparturient period when AT undergoes dramatic lipolysis and remodeling [56].

The ECS modulates adipogenesis and lipid mobilization in AT

Alteration of adipogenesis via the ECS

Adipogenesis defines the determination and terminal differentiation of adipose progenitor cells into adipocytes. De novo adipogenesis enhances the capacity of AT for storing energy when present adipocytes reach their maximum volume during positive energy balance (i.e., hyperplasia) [57]. Since adipogenesis reduces lipotoxicity, promoting the differentiation of new adipocytes may be effective in reducing the deleterious effects of excessive lipolysis in periparturient cows.

PPARγ is the master regulator of adipogenesis, although other PPARs – α, β/δ – contribute as well [58]. Three variants of PPARγ have been identified; the most prominent isoform is PPARγ2 as it is expressed primarily in AT and is heavily involved in energy homeostasis [42]. Upon activation by eCBs (or other ligands), the PPAR family binds to the retinoid X receptor (RXR) to form heterodimers. This complex then binds to DNA response elements, triggering the expression of adipogenic and lipogenic gene networks (Figs. 1 and 2) [59].

During the differentiation of adipocyte progenitor cells, expression of CB1, NAPE-PLD, and DAGL increase, while expression of the eCB-degradative enzymes FAAH, MAGL, and NAAA decrease [60]. CB1 and CB2 are present in adipocyte progenitor cells [61] and, as illustrated in Fig. 2, CB1 stimulation enhances the capacity of adipose stem cells to commit to preadipocytes through downstream activation of the cAMP response element-binding protein (CREB) and PPARγ2 [62]. Although CB1 stimulation decreases intracellular levels of cAMP [63], phosphorylation of CREB may occur through Gi/o activation of ERK [64]. CREB binds to adipogenic promoters such as FABP, FAS, and C/EBPβ. This enhances the adipogenic commitment cascade in progenitor cells. PPARγ2’s adipogenic activity, on the other hand, is directly improved by the binding of eCBs and CREB [65].

When murine 3 T3-F442A preadipocytes are treated with the CB1 stimulant HU210, these cells show enhanced expression of PPARγ2 and adiponectin and increase the number of lipid droplets formed [66]. In human preadipocytes, CB1 stimulation promotes glucose uptake through increased intracellular Ca2+ mobilization from the endoplasmic reticulum and insulin-dependent phosphatidylinositol 3 kinase (PI3K)/AKT (Protein Kinase B) pathway activation (see Fig. 1) [24]. CB1 inhibition with the selective agent Rimonabant (SR141716A) in co-incubation with CB1 activators was shown to mitigate adipogenesis via inhibition of p42/44 mitogen-activated protein kinase (MAPK) activity. In the same type of cells, adiponectin levels and glyceraldehyde-3-phosphate dehydrogenase activity increases during exposure to CB1 agonists, expounding the significance of CB1 stimulation in both adipogenesis and lipogenesis [67].

To our knowledge, there are no studies evaluating AT adipogenic responses during ECS activation in dairy cows. However, in periparturient cows exhibiting moderate to high body weight loss, the gene expression of NAPEPLD and PPARγ is upregulated and positively associated [55], suggesting a possible physiological response as AEA synthesized by NAPE-PLD is capable of activating PPARγ, enhancing adipogenesis directly.

Lipogenesis is amplified by ECS activation

In ruminants, de novo lipogenesis is the biological process by which neutral lipids and phospholipids (i.e., TAG, phospholipids, cholesterol, or sphingolipids) are biosynthesized from dietary volatile FAs within the cytoplasm of adipocytes or hepatocytes. A key stimulator of lipogenesis is insulin. This pancreatic peptide promotes glucose transporter type 4 (GLUT-4) and lipoprotein lipase (LPL) activity. In monogastric animals, upon ligand binding to CB1, lipogenesis is enhanced by three mechanisms: 1) the promotion of LPL activity; 2) the inhibition of AMPK; and 3) the augmentation of insulin-dependent glucose uptake. LPL hydrolyzes TAG found in circulating plasma lipoproteins and thus increases FA available for lipogenesis. In preadipocytes and adipocytes, LPL transcription and activity are heavily regulated by insulin. Glucose, on the other hand, glycosylates LPL intended for secretion from adipocytes to capture TAG and enhances LPL synthesis within adipocytes [68]. eCB binding to CB1 increases expression and activity of LPL [69]; however, the mechanism by which this occurs is unknown.

CB1 activation triggers Gi/o-dependent signaling pathways [63], enhancing the excretion of intracellular calcium into the extracellular matrix. This intracellular Ca2+ reduction hinders AMPK action via Ca2+/calmodulin-dependent protein kinase kinase β (CaMKKβ) [70]. AMPK, a serine/threonine protein kinase, regulates energy homeostasis by enriching pathways that generate ATP and diminishing energy-consuming pathways [71]. AMPK decreases FA synthesis by reducing ACC activity and, subsequently, malonyl-CoA availability. AMPK regulation occurs through mechanisms directly related to hindered cAMP production (Gi/o-dependent signaling pathways triggered by CB1 activation, for example), reductions of intracellular calcium, and elevations of the concentrations of ATP. Gi/o pathway activation also hinders the action of adenylate cyclase, most likely as a means to conserve ATP [63].

Intracellular glucose levels increase with CB1 activation [24]. Downstream of CB1, PI3K/AKT pathway stimulation promotes the translocation of glucose transporters to the cell surface from the cytoplasmic vesicles. This explains the increase in insulin-dependent glucose transport into the cell that has been stimulated with eCBs [72]. Like CB1, GPR55 is a positive regulator of insulin action and enhances levels of intracellular glucose in an insulin-dependent manner [47].

In dairy cows with intense body weight loss, AT CNR1 expression is greater than in those maintaining their body condition, suggesting that the eCB receptor CB1 activation is a response to increased free FA content in AT [14]. However, more information is required on the specific mechanisms that govern the ECS in periparturient cows in order to fully understand its involvement in the regulation of lipogenesis.

The ECS suppresses lipolysis

Lipolysis occurs during negative energy balance when stored TAG are broken down into free FAs and glycerol. Stimulation of TAG catabolism occurs upon binding of hormones (glucagon, growth hormone) and bioactive amines (adrenaline, norepinephrine) to either β-adrenergic or glucagon receptors, triggering the c-AMP-dependent lipolytic cascade via protein kinase A (PKA) phosphorylation of HSL and perilipin [73]. Within the adipocyte, TAG are hydrolyzed by adipose triglyceride lipase (ATGL) into diacylglycerol (DAG). From this point, DAG is hydrolyzed to monoacylglycerol (MAG) by HSL. Once broken down into free FAs and glycerol by MAGL, FA transport proteins (FAT/CD36, FATP1, FABP) can direct FAs to the mitochondria for oxidation or the RER where FA can be re-esterified into TAG or released into the vasculature surrounding the adipocyte for transport (extensively reviewed in [74]). Free FAs are then used as energy substrates primarily by cardiac, renal, or muscular tissues, but may also be utilized by most organs (exceptions being erythrocytes and the renal medulla).

The anti-lipolytic effect of CB1 stimulation in adipocytes occurs through Gi/o inhibition of cAMP production, which limits the downstream phosphorylation of HSL and perilipin [75]. Transcriptional effects downstream of CB1 activation in AT include the suppression of lipolysis-associated enzymes (carnitine-acyl-CoA transferase, carnitine palmitoyltransferase 2, and crotonase), along with downregulation of β-adrenergic and growth hormone receptor expression [76]. CB1 stimulation in AT sympathetic nerves suppresses catecholamine release, subsequently downregulating HSL activity through the decrease in cAMP produced by AC, which is no longer activated by β-adrenergic receptors [77] (Figs. 1 and 2).

Homeorhetic conditions in periparturient dairy cows drastically increase lipolysis around the time of parturition [78], yet excessive lipolysis leads to high disease incidence, reduced milk yield, and impaired reproductive performance. Considering the anti-lipolytic effects that follow CB1 stimulation and their potential benefits, the role of this receptor and the ECS should be further explored in periparturient cows.

The ECS modulates mitochondrial function in AT

Despite the limited number and relative mass of mitochondria in white adipocytes, their role in AT homeostasis and remodeling is significant. Based on microenvironmental signals, mitochondria oxidize FAs and carbohydrates in the tricarboxylic acid cycle, and the subsequent electron transport chain provides ATP to the cell [79]. In addition to the provision of energy, mitochondria also play a key role in the differentiation of preadipocytes into adipocytes. In fact, mitochondrial FA metabolism and production of reactive oxygen species (ROS) are necessary to initiate adipogenesis [80]. This may be attributed to ROS’ role in insulin signaling or its ability to enhance PPARγ’s transcriptional machinery [81].

In line with its lipogenic effects, CB1 stimulation has been shown to limit mitochondrial biogenesis and increase mitophagy in AT (as illustrated in Figs. 1 and 2). These effects may reduce mitochondrial oxidaton of FA and possibly redirect these energy molecules to reesterification into triglycerides in the endoplasmic reticulum. Both genetic (CNR1 knockout mice) and pharmacological (SR141716-treated mice) blockade of the CB1 receptor increased eNOS-dependent (endothelial nitric oxide synthase) mitochondrial biogenesis and AMPK activity in white adipocytes [82]. In another study, CB1 stimulation was associated with a decrease in PGC-1α expression, which corresponded to a direct decrease in mitochondrial mass and function [83].

Other molecules associated with suppressed mitochondrial function are ceramides [84]. These bioactive lipids are produced from a FA and sphingosine (de novo synthesis) or by the hydrolysis of sphingomyelin [85]. In monogastric AT, ceramides are known regulators of insulin signaling, inflammation, and intracellular metabolism [86]. Both CB1 and CB2 activation cause increases in intracellular ceramide production, likely a result of improved de novo ceramide synthesis through upregulation of the MAPKs extracellular signal-regulated kinase (ERK1/2), P38MAPK, and/or c-Jun N-terminal kinases (JNK) [87]. Heightened intracellular ceramide levels are associated with changes in mitochondrial membrane potential, the formation of new ion channels [88], and alterations in trifunctional proteins which are known to catalyze chain shortening reactions in mitochondrial FA β-oxidation [89].

Increased plasma ceramide in periparturient cows is positively associated with plasma acylcarnitine accretion, suggesting that FAs are partitioned away from β-oxidation in the mitochondria and toward the synthesis of sphingolipids [90]. The role of ceramide and sphingolipid biology in the metabolism of dairy cows is extensive (reviewed in [91]); however, it is currently unknown whether ceramides activate CB1 or CB2 in AT of dairy cows, and this warrants further investigation.

The ECS modulates inflammatory responses

The effects of ECS activation on inflammatory responses are complex and vary depending on the tissue, eCBs, and the type of receptor. For example, AEA has anti-inflammatory effects, including the inhibition of chemoattractant cytokines secretion, especially those released at the early stages of the inflammatory process such as IL-6, IL-8, and MCP-1, along with completely blocking lipopolysaccharide (LPS)-triggered activation of NF-kappa β pathway in periodontal tissues [92]. As for the receptors, activation of the CB1 suppresses the proliferation of cells of the adaptive immune system, especially T-cells [93]. Blocking CB1 activity has been shown to increase LPS-mediated inflammation in the gut [94]. CB2 activation in immune cells inhibits the release of pro-inflammatory cytokines [95] and therefore prevents leukocyte migration and adhesion in the brain [96]. Nevertheless, there are reports indicating that inhibition of ECS receptor activity causes inflammatory responses. Blocking of CB1 with Rimonabant in the presence of LPS decreases expression and secretion of the pro-inflammatory cytokines TNFα and IL-6 in adipocytes [97]. Therefore, more research is required to fully elucidate the effects of eCBs and the activation of CB1 and CB2 receptors on inflammation in different tissue types.

In dairy cows, there are reports indicating that ECS activation may be indicative of subclinical inflammatory diseases [32, 98]. For example, periparturient cows with subclinical endometritis had reduced expression (2- to 4- fold) of markers of eCB degradation (NAAA, FAAH) compared to healthy controls. At the same time, these animals had higher expression (2.5- to 4-fold) of components of the eCB synthesis pathways, and ECS markers (NAPEPLD, CNR2) compared to controls [32]. These findings indicate that the ECS is activated to a greater extent in cows experiencing uterine inflammation post-calving [14]. Remarkably, ECS activity in the reproductive tract appears to be modified, at least at the gene expression level, by nutritional interventions, as reported by Abolghasemi et al. [99]. In their study, conjugated linoleic acid supplementation (75 g/d) from days 21 to 42 after parturition reduced the expression of uterine CNR2 and NAPEPLD .

The interactions between ECS activation and inflammatory responses in AT of periparturient dairy cows is poorly characterized. However, we demonstrated that AT inflammation is triggered by high lipolysis rates postpartum, and this alters the activity of some components of the ECS system [14, 36]. Cows with high lipolysis have enhanced expression of components of the eCB biosynthetic pathways and ECS receptors, including NAPEPLD, CNR1, and CNR2 compared to periparturient cows with low lipolysis [14]. AT inflammation and lipolysis postpartum also affects the expression of eCBs degrading enzymes. Expression of ALOX5 and ALOX15 (encoding for 5- and 15-lipoxygenase, respectively), which are capable of metabolizing eCBs and subsequently produce oxylipid mediators of inflammation, varies throughout the periparturient period and also between cows displaying high or low levels of body weight loss [36]. AT ALOX15 expression declines in the postpartum period, whereas ALOX5 increases post-calving, and its transcription is enhanced in cows exhibiting higher levels of lipolysis [36]. Currently, the effect of ECS activation on bovine AT immune cells is unknown. In rodents, eCBs such as palmitoylethanolamide can polarize AT macrophages to the M2 anti-inflammatory phenotype when administered parenterally (SC, 30 mg/kg) for five weeks [100]. Considering the two-fold elevation observed in eCB levels during the postpartum period in cows with high weight loss [14], the altered gene expression of eCB oxidative enzymes between groups of cows exhibiting high and low levels of lipolysis [36], and the possible effect of eCBs on AT macrophage phenotype, the relationship between the ECS and AT inflammation should be further explored.

The ECS regulates appetite and nutrient uptake

CB1 activation stimulates appetite

In mammals, CB1 increases food intake by activating the binding of orexigenic peptides and inhibiting the attachment of anorexigenic proteins to hypothalamic neurons [101]. Leptin, a key hormone in this metabolic equation, is released from AT after feeding and binds to the hypothalamus where it induces the release of anorexigenic peptides (extensively reviewed in [102]). Hypothalamic eCB levels are negatively controlled by leptin [103, 104], and disruption of leptin signaling leads to an increase in eCB expression in neural tissues. Hypothalamic levels of NAPE (an AEA precursor) increases after treatment with leptin in rats [104]. This pattern of NAPE expression identifies leptin as a potential suppressor of NAPE-PLD; this is reasonable considering it inhibits the mobilization of intracellular calcium necessary for the activation of NAPE-PLD [105]. In addition, eCB levels increase in the limbic forebrain of fasted rats and return to basal levels after feeding [106], further pointing toward leptin as a potential regulator of circulating eCB levels.

Peripheral CB1 activation may also exhibit an inhibitory role over leptin in neural tissue [107]. Studies by Tam et al. using a peripherally-restricted CB1 inverse agonist in a diet-induced obese mouse model reversed hyperleptinemia and leptin resistance [108, 109] and improved anorexic melanocortin signaling in the hypothalamic arcuate nucleus [110]. These findings highlight the capabilities of CB1 to reduce leptin sensitivity and satiation signaling pathways in the hypothalamus.

The role of the ECS on the hedonic response to eating has recently been described in detail [111]. Taste is of special interest as this sensation can be altered by endocrine and paracrine signaling [112]. In lean mice, the sweet taste is suppressed by leptin [113]; however, eCBs block this effect and enhance sweet taste sensation [114]. The capacity of eCBs to enhance sensitivity to sweet taste at physiological levels was described in humans, and, remarkably, taste response to sweet stimulation increased by more than 120% [115]. This was also observed in mice with a dose-dependent response [116]. In the same study, CB1 knockout or pharmacological inhibition obliterated the response to sweet tastes, suggesting that CB1 modulates the effects of this sensation. Furthermore, Rimonabant decreases food intake in mice, yet CB2-selective inhibitor SR144528 has no direct impact on appetite. Based on these findings, the involvement of CB2 on the modulation of appetite may not be as extensive as that of CB1 [117].

In dairy cows, reduced intake of feed promotes mobilization of body fat, which leads to increased hepatic deposition of TAG and synthesis of ketones. Although conjecture, by reducing ruminant AT lipolysis in a CB1-dependent manner, satiety signaling may be suppressed through the limitation of FA oxidation in the liver, subsequently increasing dry matter intake and improving periparturient metabolic health. For these reasons, the relationship between CB1 activation in AT and feed intake in dairy cows should be explored in the future.

NAPE-PLD, the intestinal barrier, and nutrient absorption

Recent studies determined that AT NAPE-PLD levels improve the gut epithelial barrier and microbial function, which in turn, enhanced AT energy storage function in a cyclical manner [118]. The intestinal epithelium regulates metabolic function through its role in the uptake of nutrients, secretion of hormones, and production of eCBs [119]. In monogastrics, short-term dietary FA contact in the stomach induces jejunal AEA mobilization and movement of FAs into the duodenum, which leads to enhanced synthesis of OEA [120]. In addition to the enrichment of eCB synthesis, activation of the gut ECS also improves adipogenesis in AT [121]. In monogastric species, the intestinal ECS reduces LPS mobilization, barrier disruption, gut inflammation, and dysbiosis of gut microbes [121].

In dairy cows, LPS released from the rumen epithelium is translocated across the intestinal barrier and into the bloodstream. Increases in plasma concentrations of endotoxin lead to profound metabolic changes and systemic inflammation [122]. In the same study, Ametaj et al. discovered that blood glucose and non-esterified FA levels correspond to circulating LPS [122], and such increases are accompanied by depressed dry matter intake in dairy cows [123]. Interestingly, local CB1 activation limits LPS absorption in the gut, which may improve appetite and limit inflammation in dairy cows.

Conclusion

The past two decades of research have created a solid foundation in eCB biology with regards to the effects of ECS on the modulation of metabolic, behavioral, neurological, and immune functions in mammals. Targeting the systemic and adipose ECS shows promise to enhance periparturient period health through possibly promoting appetite, adipocyte proliferation, lipid accumulation, and suppressing lipolysis and AT inflammation. It is also important to determine the potential impact of ECS activity on fetal growth and neonatal health. Much work is still required to determine the biological significance of eCBs and ECS mechanisms of function in ruminant species but this research will help reducing periparturient disease incidence and enhace metabolic function in dairy cows.

Availability of data and materials

Not applicable.

Abbreviations

2-AG:

2-Arachidonyglycerol

AA:

Arachidonic acid

ABHD12:

α/β Hydrolase 12

ABHD6:

α/β Hydrolase 6

ACC:

Acetyl-CoA carboxylase

AEA:

N-Arachidonoylethanolamide

AKT:

Protein kinase B

AMPK:

5′ Adenosine monophosphate-activated protein kinase

AT:

Adipose tissue

CaMKKβ:

Ca2+/calmodulin-dependent protein kinase kinase β

cAMP:

Cyclic adenosine monophosphate

CB1:

Cannabinoid receptor type 1

CB2:

Cannabinoid receptor type 2

COX:

Cyclooxygenases

CYP450:

Cytochromes P450

DAG:

Diacylglycerol

DAGL:

Diacylglycerol lipase

eCBs:

Endocannabinoids

ECS:

Endocannabinoid system

ERK1/2:

Extracellular signal-regulated kinase

FA:

Fatty acid

FAAH:

Fatty acid amide hydrolase

FAS:

Fatty acid synthase

GLUT-4:

Glucose transporter type 4

GPCR:

G protein-coupled receptor

GPR55:

G protein-coupled receptor 55

HSL:

Hormone-sensitive lipase

LOX:

Lipoxygenases

LPL:

Lipoprotein lipase

MAG:

Monoacylglycerol

MAGL:

Monoacylglycerol lipase

MAGL:

Monoacylglycerol lipase

MAPK:

P42/44 mitogen-activated protein kinase

NAAA:

N-Acylethanolamine-hydrolyzing acid amidase

NAPE:

N-Arachidonylphosphatidylethanolamine

NAPE-PLD:

N-Arachidonylphosphatidylethanolamine-specific phospholipase D

NO:

Nitric oxide

OEA:

Oleoylethanolamide

PEA:

N-Palmitoylethanolamine

PGC-1α:

Peroxisome proliferator-activated receptor gamma coactivator 1

PLC:

Phospholipase C

PPAR:

Peroxisome proliferator-activated receptor

PUFA:

Polyunsaturated fatty acid

ROS:

Reactive oxygen species

RXR:

Retinoid X receptor

TAG:

Triacylglycerol

TRPV1:

Transient receptor potential cation channel subfamily V member 1

References

  1. Grummer RR, Hoffman PC, Luck ML, Bertics SJ. Effect of prepartum and postpartum dietary energy on growth and lactation of primiparous cows. J Dairy Sci. 1995;78(1):172–80.

    Article  CAS  PubMed  Google Scholar 

  2. Sina M, Dirandeh E, Deldar H, Shohreh B. Inflammatory status and its relationships with different patterns of postpartum luteal activity and reproductive performance in early lactating Holstein cows. Theriogenology. 2018;108:262–8.

    Article  CAS  PubMed  Google Scholar 

  3. Lowe CE, O'Rahilly S, Rochford JJ. Adipogenesis at a glance. J Cell Sci. 2011;124(Pt 16):2681–6.

    Article  CAS  PubMed  Google Scholar 

  4. Gamelin FX, Aucouturier J, Iannotti FA, Piscitelli F, Mazzarella E, Aveta T, et al. Effects of chronic exercise on the endocannabinoid system in Wistar rats with high-fat diet-induced obesity. J Physiol Biochem. 2016;72(2):183–99.

    Article  CAS  PubMed  Google Scholar 

  5. DiPatrizio NV, Piomelli D. The thrifty lipids: endocannabinoids and the neural control of energy conservation. Trends Neurosci. 2012;35(7):403–11.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

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

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  7. Lynch DL, Reggio PH. Molecular dynamics simulations of the endocannabinoid N-arachidonoylethanolamine (anandamide) in a phospholipid bilayer: probing structure and dynamics. J Med Chem. 2005;48(15):4824–33.

    Article  CAS  PubMed  Google Scholar 

  8. Niaz K, Khan F, Maqbool F, Momtaz S, Ismail Hassan F, Nobakht-Haghighi N, et al. Endo-cannabinoids system and the toxicity of cannabinoids with a biotechnological approach. EXCLI J. 2017;16:688–711.

    PubMed  PubMed Central  Google Scholar 

  9. Verderio C, Gabrielli M, Giussani P. Role of sphingolipids in the biogenesis and biological activity of extracellular vesicles. J Lipid Res. 2018;59(8):1325–40.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  10. Hillard CJ. Circulating endocannabinoids: From whence do they come and where are they going? Neuropsychopharmacology. 2018;43(1):155–72.

  11. Di Marzo V, Bisogno T, De Petrocellis L. Endocannabinoids and related compounds: walking back and forth between plant natural products and animal physiology. Chem Biol. 2007;14(7):741–56.

    Article  PubMed  CAS  Google Scholar 

  12. Cristino L, Bisogno T, Di Marzo V. Cannabinoids and the expanded endocannabinoid system in neurological disorders. Nat Rev Neurol. 2020;16(1):9–29.

    Article  PubMed  Google Scholar 

  13. Kuhla B, Kaever V, Tuchscherer A. Kuhla A. Neuroendocrinology: Involvement of plasma endocannabinoids and the hypothalamic endocannabinoid system in increasing feed intake after parturition of dairy cows; 2019.

    Google Scholar 

  14. Zachut M, Kra G, Moallem U, Livshitz L, Levin Y, Udi S, et al. Characterization of the endocannabinoid system in subcutaneous adipose tissue in periparturient dairy cows and its association to metabolic profiles. PLoS One. 2018;13(11):e0205996.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  15. Hansen HH, Hansen SH, Schousboe A, Hansen HS. Determination of the phospholipid precursor of anandamide and other N-acylethanolamine phospholipids before and after sodium azide-induced toxicity in cultured neocortical neurons. J Neurochem. 2000;75(2):861–71.

    Article  CAS  PubMed  Google Scholar 

  16. Okamoto Y, Morishita J, Tsuboi K, Tonai T, Ueda N. Molecular characterization of a phospholipase D generating anandamide and its congeners. J Biol Chem. 2004;279(7):5298–305.

    Article  CAS  PubMed  Google Scholar 

  17. Basavarajappa BS. Critical enzymes involved in endocannabinoid metabolism. Protein Pept Lett. 2007;14(3):237–46.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  18. Ueda N, Tsuboi K, Uyama T. Enzymological studies on the biosynthesis of N-acylethanolamines. Biochim Biophys Acta. 2010;1801(12):1274–85.

    Article  CAS  PubMed  Google Scholar 

  19. Murataeva N, Straiker A, Mackie K. Parsing the players: 2-arachidonoylglycerol synthesis and degradation in the CNS. Br J Pharmacol. 2014;171(6):1379–91.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  20. Cravatt BF, Lichtman AH. Fatty acid amide hydrolase: an emerging therapeutic target in the endocannabinoid system. Curr Opin Chem Biol. 2003;7(4):469–75.

    Article  CAS  PubMed  Google Scholar 

  21. Saghatelian A, Trauger SA, Want EJ, Hawkins EG, Siuzdak G, Cravatt BF. Assignment of endogenous substrates to enzymes by global metabolite profiling. Biochemistry. 2004;43(45):14332–9.

    Article  CAS  PubMed  Google Scholar 

  22. Huang SM, Bisogno T, Petros TJ, Chang SY, Zavitsanos PA, Zipkin RE, et al. Identification of a new class of molecules, the arachidonyl amino acids, and characterization of one member that inhibits pain. J Biol Chem. 2001;276(46):42639–44.

    Article  CAS  PubMed  Google Scholar 

  23. McKinney MK, Cravatt BF. Structure and function of fatty acid amide hydrolase. Annu Rev Biochem. 2005;74:411–32.

    Article  CAS  PubMed  Google Scholar 

  24. Pagano C, Pilon C, Calcagno A, Urbanet R, Rossato M, Milan G, et al. The endogenous cannabinoid system stimulates glucose uptake in human fat cells via phosphatidylinositol 3-kinase and calcium-dependent mechanisms. J Clin Endocrinol Metab. 2007;92(12):4810–9.

    Article  CAS  PubMed  Google Scholar 

  25. Bluher M, Engeli S, Kloting N, Berndt J, Fasshauer M, Batkai S, et al. Dysregulation of the peripheral and adipose tissue endocannabinoid system in human abdominal obesity. Diabetes. 2006;55(11):3053–60.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  26. Dinh TP, Carpenter D, Leslie FM, Freund TF, Katona I, Sensi SL, et al. Brain monoglyceride lipase participating in endocannabinoid inactivation. Proc Natl Acad Sci U S A. 2002;99(16):10819–24.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  27. Tornqvist H, Belfrage P. Purification and some properties of a monoacylglycerol-hydrolyzing enzyme of rat adipose tissue. J Biol Chem. 1976;251(3):813–9.

    Article  CAS  PubMed  Google Scholar 

  28. Schlosburg JE, Blankman JL, Long JZ, Nomura DK, Pan B, Kinsey SG, et al. Chronic monoacylglycerol lipase blockade causes functional antagonism of the endocannabinoid system. Nat Neurosci. 2010;13(9):1113–9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  29. Zachut M. Defining the adipose tissue proteome of dairy cows to reveal biomarkers related to peripartum insulin resistance and metabolic status. J Proteome Res. 2015;14(7):2863–71.

  30. Marrs WR, Blankman JL, Horne EA, Thomazeau A, Lin YH, Coy J, et al. The serine hydrolase ABHD6 controls the accumulation and efficacy of 2-AG at cannabinoid receptors. Nat Neurosci. 2010;13(8):951–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  31. Tsuboi K, Takezaki N, Ueda N. The N-acylethanolamine-hydrolyzing acid amidase (NAAA). Chem Biodivers. 2007;4(8):1914–25.

    Article  CAS  PubMed  Google Scholar 

  32. Bonsale R, Seyed Sharifi R, Dirandeh E, Hedayat N, Mojtahedin A, Ghorbanalinia M, et al. Endocannabinoids as endometrial inflammatory markers in lactating Holstein cows. Reprod Domest Anim. 2018;53(3):769–75.

    Article  CAS  PubMed  Google Scholar 

  33. Bertevello PS, Teixeira-Gomes AP, Seyer A, Vitorino Carvalho A, Labas V, Blache MC, et al. Lipid identification and transcriptional analysis of controlling enzymes in bovine ovarian follicle. Int J Mol Sci. 2018;19(10):3261.

  34. Rouzer CA, Marnett LJ. Endocannabinoid oxygenation by cyclooxygenases, lipoxygenases, and cytochromes P450: cross-talk between the eicosanoid and endocannabinoid signaling pathways. Chem Rev. 2011;111(10):5899–921.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  35. Sordillo LM. Symposium review: Oxylipids and the regulation of bovine mammary inflammatory responses. J Dairy Sci. 2018;101(6):5629–41.

    Article  CAS  PubMed  Google Scholar 

  36. Contreras GA, Strieder-Barboza C, de Souza J, Gandy J, Mavangira V, Lock AL, et al. Periparturient lipolysis and oxylipid biosynthesis in bovine adipose tissues. PLoS One. 2017;12(12):e0188621.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  37. Bartelt A, Orlando P, Mele C, Ligresti A, Toedter K, Scheja L, et al. Altered endocannabinoid signalling after a high-fat diet in Apoe(−/−) mice: relevance to adipose tissue inflammation, hepatic steatosis and insulin resistance. Diabetologia. 2011;54(11):2900–10.

    Article  CAS  PubMed  Google Scholar 

  38. Agarwal N, Pacher P, Tegeder I, Amaya F, Constantin CE, Brenner GJ, et al. Cannabinoids mediate analgesia largely via peripheral type 1 cannabinoid receptors in nociceptors. Nat Neurosci. 2007;10(7):870–9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  39. Alvheim AR, Torstensen BE, Lin YH, Lillefosse HH, Lock EJ, Madsen L, et al. Dietary linoleic acid elevates endogenous 2-arachidonoylglycerol and anandamide in Atlantic salmon (Salmo salar L.) and mice, and induces weight gain and inflammation in mice. Br J Nutr. 2013;109(8):1508–17.

    Article  CAS  PubMed  Google Scholar 

  40. Felder CC, Joyce KE, Briley EM, Mansouri J, Mackie K, Blond O, et al. Comparison of the pharmacology and signal transduction of the human cannabinoid CB1 and CB2 receptors. Mol Pharmacol. 1995;48(3):443–50.

    CAS  PubMed  Google Scholar 

  41. Cota D. CB1 receptors: emerging evidence for central and peripheral mechanisms that regulate energy balance, metabolism, and cardiovascular health. Diabetes Metab Res Rev. 2007;23(7):507–17.

    Article  CAS  PubMed  Google Scholar 

  42. Isabelle Matias IB, and Daniela Cota. The fat side of the endocannabinoid system: Role of endocannabinoids in the adipocyte. Cannabis and Cannabinoid Research. 2016;1:1. https://doi.org/10.1089/can.2016.0014.

  43. Piomelli D. The molecular logic of endocannabinoid signalling. Nat Rev Neurosci. 2003;4(11):873–84.

    Article  CAS  PubMed  Google Scholar 

  44. Staiano RI, Loffredo S, Borriello F, Iannotti FA, Piscitelli F, Orlando P, et al. Human lung-resident macrophages express CB1 and CB2 receptors whose activation inhibits the release of angiogenic and lymphangiogenic factors. J Leukoc Biol. 2016;99(4):531–40.

    Article  CAS  PubMed  Google Scholar 

  45. Turcotte C, Blanchet MR, Laviolette M, Flamand N. The CB2 receptor and its role as a regulator of inflammation. Cell Mol Life Sci. 2016;73(23):4449–70.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  46. 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 (Silver Spring). 2008;16(3):553–65.

    Article  CAS  Google Scholar 

  47. Lipina C, Walsh SK, Mitchell SE, Speakman JR, Wainwright CL, Hundal HS. GPR55 deficiency is associated with increased adiposity and impaired insulin signaling in peripheral metabolic tissues. FASEB J. 2019;33(1):1299–312.

    Article  CAS  PubMed  Google Scholar 

  48. Liu P, Peng HJ, Zhu J. Juvenile hormone-activated phospholipase C pathway enhances transcriptional activation by the methoprene-tolerant protein. Proc Natl Acad Sci U S A. 2015;112(15):E1871–9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  49. Romero-Zerbo SY, Rafacho A, Diaz-Arteaga A, Suarez J, Quesada I, Imbernon M, et al. A role for the putative cannabinoid receptor GPR55 in the islets of Langerhans. J Endocrinol. 2011;211(2):177–85.

    Article  CAS  PubMed  Google Scholar 

  50. Bjursell M, Ryberg E, Wu T, Greasley PJ, Bohlooly YM, Hjorth S. Deletion of Gpr55 results in subtle effects on energy metabolism, motor activity and thermal pain sensation. PLoS One. 2016;11(12):e0167965.

  51. Gram DX, Holst JJ, Szallasi A. TRPV1: A potential therapeutic target in type 2 diabetes and comorbidities? Trends Mol Med. 2017;23(11):1002–13.

  52. Maiese K. Warming up to new possibilities with the capsaicin receptor TRPV1: mTOR, AMPK, and erythropoietin. Curr Neurovasc Res. 2017;14(2):184–9.

  53. Luo Z, Ma L, Zhao Z, He H, Yang D, Feng X, et al. TRPV1 activation improves exercise endurance and energy metabolism through PGC-1alpha upregulation in mice. Cell Res. 2012;22(3):551–64.

    Article  CAS  PubMed  Google Scholar 

  54. Szallasi A, Cortright DN, Blum CA, Eid SR. The vanilloid receptor TRPV1: 10 years from channel cloning to antagonist proof-of-concept. Nat Rev Drug Discov. 2007;6(5):357–72.

    Article  CAS  PubMed  Google Scholar 

  55. Dirandeh E, Ghorbanalinia M, Rezaei-Roodbari A, Colazo MG. Relationship between body condition score loss and mRNA of genes related to fatty acid metabolism and the endocannabinoid system in adipose tissue of periparturient cows. Animal. 2020:1–9.

  56. Contreras GA, Strieder-Barboza C, De Koster J. Symposium review: Modulating adipose tissue lipolysis and remodeling to improve immune function during the transition period and early lactation of dairy cows. J Dairy Sci. 2018;101(3):2737–52.

    Article  CAS  PubMed  Google Scholar 

  57. Poulos SP, Dodson MV, Culver MF, Hausman GJ. The increasingly complex regulation of adipocyte differentiation. Exp Biol Med (Maywood). 2016;241(5):449–56.

    Article  CAS  Google Scholar 

  58. Muller T, Demizieux L, Troy-Fioramonti S, Gresti J. Pais de Barros JP, Berger H et al. Overactivation of the endocannabinoid system alters the antilipolytic action of insulin in mouse adipose tissue. Am J Physiol Endocrinol Metab. 2017;313(1):E26–36.

    Article  PubMed  Google Scholar 

  59. O'Sullivan SE. An update on PPAR activation by cannabinoids. Br J Pharmacol. 2016;173(12):1899–910.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  60. Nahon KJ, Kantae V, den Haan R, Hanssen MJW, Harms AC, van der Stelt M, et al. Gene expression of endocannabinoid system components in skeletal muscle and adipose tissue of South Asians and White Caucasians with overweight. Obesity (Silver Spring). 2018;26(8):1332–7.

  61. Rossi F, Bernardo ME, Bellini G, Luongo L, Conforti A, Manzo I, et al. The cannabinoid receptor type 2 as mediator of mesenchymal stromal cell immunosuppressive properties. PLoS One. 2013;8(11):e80022.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  62. Gimble JM, Katz AJ, Bunnell BA. Adipose-derived stem cells for regenerative medicine. Circ Res. 2007;100(9):1249–60.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  63. Eldeeb K, Leone-Kabler S, Howlett AC. CB1 cannabinoid receptor-mediated increases in cyclic AMP accumulation are correlated with reduced Gi/o function. J Basic Clin Physiol Pharmacol. 2016;27(3):311–22.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  64. Kelleher RJ 3rd, Govindarajan A, Jung HY, Kang H, Tonegawa S. Translational control by MAPK signaling in long-term synaptic plasticity and memory. Cell. 2004;116(3):467–79.

    Article  CAS  PubMed  Google Scholar 

  65. Siersbaek RN, R. Mandrup, S. Transcriptional networks and chromatin remodeling controlling adipogenesis. Trends in Endocrinology & Metabolism 2011, 23(2):56–64.

  66. Matias I, Bisogno T, Di Marzo V. Endogenous cannabinoids in the brain and peripheral tissues: regulation of their levels and control of food intake. Int J Obes (Lond). 2006;30(Suppl 1):S7–S12.

    Article  CAS  Google Scholar 

  67. Gary-Bobo M, Elachouri G, Scatton B, Le Fur G, Oury-Donat F, Bensaid M. The cannabinoid CB1 receptor antagonist rimonabant (SR141716) inhibits cell proliferation and increases markers of adipocyte maturation in cultured mouse 3T3 F442A preadipocytes. Mol Pharmacol. 2006;69(2):471–8.

    Article  CAS  PubMed  Google Scholar 

  68. Goldberg IJ, Eckel RH, Abumrad NA. Regulation of fatty acid uptake into tissues: lipoprotein lipase- and CD36-mediated pathways. J Lipid Res. 2009;50(Suppl):S86–90.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  69. Cota D, Marsicano G, Tschop M, Grubler Y, Flachskamm C, Schubert M, et al. The endogenous cannabinoid system affects energy balance via central orexigenic drive and peripheral lipogenesis. J Clin Invest. 2003;112(3):423–31.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  70. Sundararaman A, Amirtham U, Rangarajan A. Calcium-Oxidant Signaling Network Regulates AMP-activated Protein Kinase (AMPK) Activation upon Matrix Deprivation. J Biol Chem. 2016;291(28):14410–29.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  71. Zhang BB, Zhou G, Li C. AMPK: an emerging drug target for diabetes and the metabolic syndrome. Cell Metab. 2009;9(5):407–16.

    Article  PubMed  CAS  Google Scholar 

  72. Sanchez MG, Ruiz-Llorente L, Sanchez AM, Diaz-Laviada I. Activation of phosphoinositide 3-kinase/PKB pathway by CB (1) and CB (2) cannabinoid receptors expressed in prostate PC-3 cells. Involvement in Raf-1 stimulation and NGF induction. Cell Signal. 2003;15(9):851–9.

    Article  CAS  PubMed  Google Scholar 

  73. Hafidi ME, Buelna-Chontal M, Sanchez-Munoz F, Carbo R. Adipogenesis: A Necessary but Harmful Strategy. Int J Mol Sci 2019, 20(15).

  74. Lafontan M, Langin D. Lipolysis and lipid mobilization in human adipose tissue. Prog Lipid Res. 2009;48(5):275–97.

    Article  CAS  PubMed  Google Scholar 

  75. Sidibeh CO, Pereira MJ, Lau Borjesson J, Kamble PG, Skrtic S, Katsogiannos P, et al. Role of cannabinoid receptor 1 in human adipose tissue for lipolysis regulation and insulin resistance. Endocrine. 2017;55(3):839–52.

    Article  CAS  PubMed  Google Scholar 

  76. Jbilo O, Ravinet-Trillou C, Arnone M, Buisson I, Bribes E, Peleraux A, et al. The CB1 receptor antagonist rimonabant reverses the diet-induced obesity phenotype through the regulation of lipolysis and energy balance. FASEB J. 2005;19(11):1567–9.

    Article  CAS  PubMed  Google Scholar 

  77. Lowin T, Straub RH. Cannabinoid-based drugs targeting CB1 and TRPV1, the sympathetic nervous system, and arthritis. Arthritis Res Ther. 2015;17:226.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  78. Bauman DE, Currie WB. Partitioning of nutrients during pregnancy and lactation: a review of mechanisms involving homeostasis and homeorhesis. J Dairy Sci. 1980;63(9):1514–29.

    Article  CAS  PubMed  Google Scholar 

  79. Sun K, Kusminski CM, Scherer PE. Adipose tissue remodeling and obesity. J Clin Invest. 2011;121(6):2094–101.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  80. Tormos KV, Anso E, Hamanaka RB, Eisenbart J, Joseph J, Kalyanaraman B, et al. Mitochondrial complex III ROS regulate adipocyte differentiation. Cell Metab. 2011;14(4):537–44.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  81. Wang W, Zhang Y, Lu W, Liu K. Mitochondrial reactive oxygen species regulate adipocyte differentiation of mesenchymal stem cells in hematopoietic stress induced by arabinosylcytosine. PLoS One. 2015;10(3):e0120629.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  82. Tedesco L, Valerio A, Cervino C, Cardile A, Pagano C, Vettor R, et al. Cannabinoid type 1 receptor blockade promotes mitochondrial biogenesis through endothelial nitric oxide synthase expression in white adipocytes. Diabetes. 2008;57(8):2028–36.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  83. Tedesco L, Valerio A, Dossena M, Cardile A, Ragni M, Pagano C, et al. Cannabinoid receptor stimulation impairs mitochondrial biogenesis in mouse white adipose tissue, muscle, and liver: the role of eNOS, p38 MAPK, and AMPK pathways. Diabetes. 2010;59(11):2826–36.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  84. Law BA, Liao X, Moore KS, Southard A, Roddy P, Ji R, et al. Lipotoxic very-long-chain ceramides cause mitochondrial dysfunction, oxidative stress, and cell death in cardiomyocytes. FASEB J. 2018;32(3):1403–16.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  85. Chaurasia B, Summers SA. Ceramides - lipotoxic inducers of metabolic disorders. Trends Endocrinol Metab. 2015;26(10):538–50.

  86. Pyne S, Adams DR, Pyne NJ. Sphingosine 1-phosphate and sphingosine kinases in health and disease: Recent advances. Prog Lipid Res. 2016;62:93–106.

    Article  CAS  PubMed  Google Scholar 

  87. Rueda D, Navarro B, Martinez-Serrano A, Guzman M, Galve-Roperh I. The endocannabinoid anandamide inhibits neuronal progenitor cell differentiation through attenuation of the Rap1/B-Raf/ERK pathway. J Biol Chem. 2002;277(48):46645–50.

    Article  CAS  PubMed  Google Scholar 

  88. Ueda N. Ceramide-induced apoptosis in renal tubular cells: a role of mitochondria and sphingosine-1-phoshate. Int J Mol Sci. 2015;16(3):5076–124.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  89. Fonseca BM, Correia-da-Silva G, Teixeira NA. The endocannabinoid anandamide induces apoptosis of rat decidual cells through a mechanism involving ceramide synthesis and p38 MAPK activation. Apoptosis. 2013;18(12):1526–35.

    Article  CAS  PubMed  Google Scholar 

  90. Rico JE, Zang Y, Haughey NJ, Rius AG, McFadden JW. Short communication: Circulating fatty acylcarnitines are elevated in overweight periparturient dairy cows in association with sphingolipid biomarkers of insulin resistance. J Dairy Sci. 2018;101(1):812–9.

    Article  CAS  PubMed  Google Scholar 

  91. McFadden JW, Rico JE. Invited review: Sphingolipid biology in the dairy cow: The emerging role of ceramide. J Dairy Sci. 2019;102(9):7619–39.

    Article  CAS  PubMed  Google Scholar 

  92. Nakajima Y, Furuichi Y, Biswas KK, Hashiguchi T, Kawahara K, Yamaji K, et al. Endocannabinoid, anandamide in gingival tissue regulates the periodontal inflammation through NF-kappaB pathway inhibition. FEBS Lett. 2006;580(2):613–9.

    Article  CAS  PubMed  Google Scholar 

  93. Katona S, Kaminski E, Sanders H, Zajicek J. Cannabinoid influence on cytokine profile in multiple sclerosis. Clin Exp Immunol. 2005;140(3):580–5.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  94. Mehrpouya-Bahrami P, Chitrala KN, Ganewatta MS, Tang C, Murphy EA, Enos RT, et al. Blockade of CB1 cannabinoid receptor alters gut microbiota and attenuates inflammation and diet-induced obesity. Sci Rep. 2017;7(1):15645.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  95. Silver RJ. The Endocannabinoid System of Animals. Animals (Basel) 2019, 9(9).

  96. Rom S, Zuluaga-Ramirez V, Dykstra H, Reichenbach NL, Pacher P, Persidsky Y. Selective activation of cannabinoid receptor 2 in leukocytes suppresses their engagement of the brain endothelium and protects the blood-brain barrier. Am J Pathol. 2013;183(5):1548–58.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  97. Murumalla R, Bencharif K, Gence L, Bhattacharya A, Tallet F, Gonthier MP, et al. Effect of the Cannabinoid Receptor-1 antagonist SR141716A on human adipocyte inflammatory profile and differentiation. J Inflamm (Lond). 2011;8:33.

    Article  CAS  Google Scholar 

  98. Dirandeh E, Ghaffari J. Effects of feeding a source of omega-3 fatty acid during the early postpartum period on the endocannabinoid system in the bovine endometrium. Theriogenology. 2018;121:141–6.

    Article  CAS  PubMed  Google Scholar 

  99. Abolghasemi A, Dirandeh E, Ansari Pirsaraei Z, Shohreh B. Dietary conjugated linoleic acid supplementation alters the expression of genes involved in the endocannabinoid system in the bovine endometrium and increases plasma progesterone concentrations. Theriogenology. 2016;86(6):1453–9.

    Article  CAS  PubMed  Google Scholar 

  100. Mattace Raso G, Santoro A, Russo R, Simeoli R, Paciello O, Di Carlo C, et al. Palmitoylethanolamide prevents metabolic alterations and restores leptin sensitivity in ovariectomized rats. Endocrinology. 2014;155(4):1291–301.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  101. Miller CC, Murray TF, Freeman KG, Edwards GL. Cannabinoid agonist, CP 55,940, facilitates intake of palatable foods when injected into the hindbrain. Physiol Behav. 2004;80(5):611–6.

    Article  CAS  PubMed  Google Scholar 

  102. Sobrino Crespo C, Perianes Cachero A, Puebla Jimenez L, Barrios V, Arilla FE. Peptides and food intake. Front Endocrinol (Lausanne). 2014;5:58.

    Article  Google Scholar 

  103. Thanos PK, Ramalhete RC, Michaelides M, Piyis YK, Wang GJ, Volkow ND. Leptin receptor deficiency is associated with upregulation of cannabinoid 1 receptors in limbic brain regions. Synapse. 2008;62(9):637–42.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  104. Di Marzo V, Goparaju SK, Wang L, Liu J, Batkai S, Jarai Z, et al. Leptin-regulated endocannabinoids are involved in maintaining food intake. Nature. 2001;410(6830):822–5.

    Article  PubMed  Google Scholar 

  105. Ueda N. Endocannabinoid hydrolases. Prostaglandins Other Lipid Mediat. 2002;68–69:521–34.

    Article  PubMed  Google Scholar 

  106. Kirkham TC, Williams CM, Fezza F, Di Marzo V. Endocannabinoid levels in rat limbic forebrain and hypothalamus in relation to fasting, feeding and satiation: stimulation of eating by 2-arachidonoyl glycerol. Br J Pharmacol. 2002;136(4):550–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  107. Palomba L, Silvestri C, Imperatore R, Morello G, Piscitelli F, Martella A, et al. Negative Regulation of Leptin-induced Reactive Oxygen Species (ROS) Formation by Cannabinoid CB1 Receptor Activation in Hypothalamic Neurons. J Biol Chem. 2015;290(22):13669–77.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  108. Tam J, Cinar R, Liu J, Godlewski G, Wesley D, Jourdan T, et al. Peripheral cannabinoid-1 receptor inverse agonism reduces obesity by reversing leptin resistance. Cell Metab. 2012;16(2):167–79.

    Article  CAS  PubMed  Google Scholar 

  109. Tam J, Vemuri VK, Liu J, Batkai S, Mukhopadhyay B, Godlewski G, et al. Peripheral CB1 cannabinoid receptor blockade improves cardiometabolic risk in mouse models of obesity. J Clin Invest. 2010;120(8):2953–66.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  110. Tam J, Szanda G, Drori A, Liu Z, Cinar R, Kashiwaya Y, et al. Peripheral cannabinoid-1 receptor blockade restores hypothalamic leptin signaling. Mol Metab. 2017;6(10):1113–25.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  111. Monteleone AM, Di Marzo V, Monteleone P, Dalle Grave R, Aveta T, Ghoch ME, et al. Responses of peripheral endocannabinoids and endocannabinoid-related compounds to hedonic eating in obesity. Eur J Nutr. 2016;55(4):1799–805.

    Article  CAS  PubMed  Google Scholar 

  112. Loper HB, La Sala M, Dotson C, Steinle N. Taste perception, associated hormonal modulation, and nutrient intake. Nutr Rev. 2015;73(2):83–91.

    Article  PubMed  PubMed Central  Google Scholar 

  113. Yoshida R, Noguchi K, Shigemura N, Jyotaki M, Takahashi I, Margolskee RF, et al. Leptin Suppresses Mouse Taste Cell Responses to Sweet Compounds. Diabetes. 2015;64(11):3751–62.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  114. Niki M, Jyotaki M, Yoshida R, Yasumatsu K, Shigemura N, DiPatrizio NV, et al. Modulation of sweet taste sensitivities by endogenous leptin and endocannabinoids in mice. J Physiol. 2015;593(11):2527–45.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  115. Yoshida R, Ohkuri T, Jyotaki M, Yasuo T, Horio N, Yasumatsu K, et al. Endocannabinoids selectively enhance sweet taste. Proc Natl Acad Sci U S A. 2010;107(2):935–9.

    Article  CAS  PubMed  Google Scholar 

  116. Higgs S, Williams CM, Kirkham TC. Cannabinoid influences on palatability: microstructural analysis of sucrose drinking after delta (9)-tetrahydrocannabinol, anandamide, 2-arachidonoyl glycerol and SR141716. Psychopharmacology (Berl). 2003;165(4):370–7.

    Article  CAS  Google Scholar 

  117. Wiley JL, Burston JJ, Leggett DC, Alekseeva OO, Razdan RK, Mahadevan A, et al. CB1 cannabinoid receptor-mediated modulation of food intake in mice. Br J Pharmacol. 2005;145(3):293–300.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  118. Geurts L, Everard A, Van Hul M, Essaghir A, Duparc T, Matamoros S, et al. Adipose tissue NAPE-PLD controls fat mass development by altering the browning process and gut microbiota. Nat Commun. 2015;6:6495.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  119. Tellez LA, Medina S, Han W, Ferreira JG, Licona-Limon P, Ren X, et al. A gut lipid messenger links excess dietary fat to dopamine deficiency. Science. 2013;341(6147):800–2.

    Article  CAS  PubMed  Google Scholar 

  120. DiPatrizio NV, Astarita G, Schwartz G, Li X, Piomelli D. Endocannabinoid signal in the gut controls dietary fat intake. Proc Natl Acad Sci U S A. 2011;108(31):12904–8.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  121. Muccioli GG, Naslain D, Backhed F, Reigstad CS, Lambert DM, Delzenne NM, et al. The endocannabinoid system links gut microbiota to adipogenesis. Mol Syst Biol. 2010;6:392.

    Article  PubMed  PubMed Central  CAS  Google Scholar 

  122. Ametaj BN, Emmanuel DG, Zebeli Q, Dunn SM. Feeding high proportions of barley grain in a total mixed ration perturbs diurnal patterns of plasma metabolites in lactating dairy cows. J Dairy Sci. 2009;92(3):1084–91.

    Article  CAS  PubMed  Google Scholar 

  123. Plaizier JC, Krause DO, Gozho GN, McBride BW. Subacute ruminal acidosis in dairy cows: the physiological causes, incidence and consequences. Vet J. 2008;176(1):21–31.

    Article  CAS  PubMed  Google Scholar 

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Funding

This project was funded by the US-Israel Binational Agricultural Research and Development Fund (Grant IS-5167-19). MNS was supported in part by the USDA National Institute for Food and Agriculture (Washington, DC, USA) competitive project 2019-67015-29443.

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Authors and Affiliations

  1. Department of Large Animal Clinical Sciences, College of Veterinary Medicine, Michigan State University, East Lansing, MI, 48824, USA

    Madison N. Myers & G. Andres Contreras

  2. Department of Ruminant Science, Institute of Animal Sciences, Agricultural Research Organization / Volcani Center, 7505101, Rishon LeZion, Israel

    Maya Zachut

  3. Obesity and Metabolism Laboratory, The Institute for Drug Research, School of Pharmacy, Faculty of Medicine, The Hebrew University of Jerusalem, 9112001, Jerusalem, Israel

    Joseph Tam

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  1. Madison N. Myers
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  2. Maya Zachut
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  4. G. Andres Contreras
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MNS drafted the manuscript. MZ, JT, and GAC edited and added content to the manuscript. All authors approved the final version of the article.

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Correspondence to Maya Zachut or G. Andres Contreras.

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Myers, M.N., Zachut, M., Tam, J. et al. A proposed modulatory role of the endocannabinoid system on adipose tissue metabolism and appetite in periparturient dairy cows. J Animal Sci Biotechnol 12, 21 (2021). https://doi.org/10.1186/s40104-021-00549-3

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Keywords

Journal of Animal Science and Biotechnology

ISSN: 2049-1891