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Article

Identification of the Ghrelin and Cannabinoid CB2 Receptor Heteromer Functionality and Marked Upregulation in Striatal Neurons from Offspring of Mice under a High-Fat Diet

by
Jaume Lillo
1,2,†,
Alejandro Lillo
3,†,
David A. Zafra
3,
Cristina Miralpeix
4,
Rafael Rivas-Santisteban
1,2,
Núria Casals
4,5,
Gemma Navarro
1,3,6,*,‡ and
Rafael Franco
1,2,7,*,‡
1
Centro de Investigación Biomédica en Red Enfermedades Neurodegenerativas (CiberNed), National Institute of Health Carlos III, Valderrebollo, 5, 28031 Madrid, Spain
2
Department of Biochemistry and Molecular Biomedicine, Universitat de Barcelona, 08028 Barcelona, Spain
3
Department of Biochemistry and Physiology, Faculty of Pharmacy and Food Science, University of Barcelona, 08028 Barcelona, Spain
4
Basic Sciences Department, Faculty of Medicine and Health Sciences, Universitat Internacional de Catalunya, 08190 Sant Cugat del Vallès, Spain
5
Centro de Investigación Biomédica en Red de Fisiopatología de la Obesidad y la Nutrición (CIBEROBN), Instituto de Salud Carlos III, Monforte de Lemos, 3, 28029 Madrid, Spain
6
Institut de Neurociències, Universitat de Barcelona (UBNeuro), 08035 Barcelona, Spain
7
School of Chemistry, University of Barcelona, 08028 Barcelona, Spain
*
Authors to whom correspondence should be addressed.
†
These authors contributed equally to this work.
‡
Equally contributed.
Int. J. Mol. Sci. 2021, 22(16), 8928; https://0-doi-org.brum.beds.ac.uk/10.3390/ijms22168928
Submission received: 1 July 2021 / Revised: 11 August 2021 / Accepted: 13 August 2021 / Published: 19 August 2021
(This article belongs to the Section Bioactives and Nutraceuticals)
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Versions Notes

Abstract

:
Cannabinoids have been reported as orexigenic, i.e., as promoting food intake that, among others, is controlled by the so-called “hunger” hormone, ghrelin. The aim of this paper was to look for functional and/or molecular interactions between ghrelin GHSR1a and cannabinoid CB2 receptors at the central nervous system (CNS) level. In a heterologous system we identified CB2-GHSR1a receptor complexes with a particular heteromer print consisting of impairment of CB2 receptor/Gi-mediated signaling. The blockade was due to allosteric interactions within the heteromeric complex as it was reverted by antagonists of the GHSR1a receptor. Cannabinoids acting on the CB2 receptor did not affect cytosolic increases of calcium ions induced by ghrelin acting on the GHSR1a receptor. In situ proximity ligation imaging assays confirmed the expression of CB2-GHSR1a receptor complexes in both heterologous cells and primary striatal neurons. We tested heteromer expression in neurons from offspring of high-fat-diet mouse mothers as they have more risk to be obese. Interestingly, there was a marked upregulation of those complexes in striatal neurons from siblings of pregnant female mice under a high-fat diet.

1. Introduction

The psychotropic effects of marihuana smoking led to the discovery of cannabinoid receptors and of endocannabinoids. Since the discovery of tetrahydrocannabinol (THC) and cannabidiol (CBD) in Cannabis sativa L., decades of research have led to the identification of multiple phytocannabinoids that show biological activity. The characterization of cannabinoid receptors, the use of animal models of disease, and the experience of marihuana users have led to the discovery of the health-promoting benefits of natural cannabinoids. In addition to the already approved cannabinoid-containing drugs (Dronabinol/Marinol® -LGM Pharma Boca Raton, USA)- and Sativex® and Epidiolex® -Jazz Pharmaceuticals, Dublin, Ireland-), non-psychotropic compounds such as cannabidiol and cannabigerol extracted from Cannabis sativa L. have been proposed to aid in a variety of diseases (see [1,2] for review). Although cannabinoids can act via a variety of targets (GPR55, GPCR18, peroxisome proliferator-activated receptor gamma, serotonin receptors, etc.), their canonical targets are the cannabinoid CB1 and CB2 receptors. Both belong to the superfamily of G-protein-coupled-receptors (GPCRs) and both couple to the Gi heterotrimeric protein, i.e., receptor activation leads to Gi-mediated deactivation of adenylyl cyclase and reduction of intracellular cAMP levels. The CB1 receptor (CB1R), expressed mainly in neurons, is the most abundant GPCR in the nervous system; while the CB2R is expressed at lower levels both in glia and neurons located in specific regions of the brain [3,4,5,6,7]. The CB2R is considered a target for neuroprotection, especially in diseases coursing with neuroinflammation. For instance, cannabinoids acting on the CB2R in striatal neural cells reduce the neuronal loss in synucleinopathies such as Parkinson’s disease [8,9,10,11,12,13]. The underlying mechanism is mainly related to the reduction of inflammation, but the CB2R expressed in some striatal neurons may also have a relevant role [3,7,14,15,16]. A selective antagonist of the CB1R, rimonabant, approved to combat obesity was, unfortunately, withdrawn due to side effects [17,18,19,20]. The anti-obesity potential of targeting the CB2R has not yet been addressed.
Although the molecular mechanism has not been fully elucidated, the orexigenic properties of marihuana consumption are well known [21]. Ghrelin is often considered the “hunger” hormone because its appearance in blood leads to an increase under food intake [22,23]. Ghrelin, a 28-amino acid peptide, mainly produced by specialized cells of the gastrointestinal act, may reach the central nervous system where it activates central mechanisms that control food intake [24,25,26,27]. Its main target there is the ghrelin GHSR1a receptor, also a member of the GPCR superfamily [28]. The aim of this paper was to investigate the molecular and/or functional interactions between CB2 and GHS1a receptors that could explain the orexigenic effects of marihuana consumption and whether ghrelin affects the neuroprotective effects induced by cannabinoids acting on the CB2R. As offspring from obese mothers have more risk to be obese, the potential expression of complexes formed by these two receptors was also studied in neurons isolated from fetuses of pregnant female mice in a high-fat diet.

2. Results

2.1. The CB2R May Interact with the GHSR1a

Consumption of Cannabis sativa L. increases appetite via a mechanism in which ghrelin, a hormone of the endocrine system, participates. To investigate whether there may be a functional interaction between the cannabinoidergic and the orexinergic systems, we first investigated a potential interaction between the cannabinoid receptor CB2 and the functional form of the ghrelin receptor, GHSR1a. Immunocytochemical assays in HEK-293T cells transfected with the cDNA for the CB2R fused to the Green Fluorescent Protein (GFP2) and the cDNA of the GHSR1a fused to Renilla luciferase (RLuc) led to detect the receptors at the plasma membrane level with a marked colocalization (Figure 1A). As colocalization may be found for proteins that are close (approximately 200 nm apart) but not directly interacting, a Bioluminescence Resonance Energy Transfer (BRET) assay was performed in HEK-293T cells cotransfected with a constant amount of the cDNA for GHSR1a-RLuc and increasing amounts of cDNA for CB2R-GFP2. A saturation curve (BRETmax: 550 ± 50 mBU, BRET50: 18 ± 4) was obtained, demonstrating a direct interaction between the two receptors in the heterologous expression system (Figure 1B). As negative control, HEK-293T cells were transfected with a constant amount of GABABR-RLuc cDNA and increasing amounts of GHSR1a-GFP2 cDNA; the nonspecific linear signal indicated a lack of interaction between these two proteins.
It is well known that GPCRs may form homodimers of heterodimers and higher order structures. One of the first examples has been provided for the adenosine A1 and A2A receptors that can form tetrameric structures complexed with two heterotrimeric G proteins, one Gi and one Gs [29,30]. To investigate the possible formation of tetramers formed by CB2 and GHS1a receptors, BRET with bimolecular complementation experiments was performed in HEK-293T cells transfected with a constant amount of Rluc8 N/C hemiproteins fused to GHSR1a (GHSR1a-cRLuc and GHSR1a-nRLuc) and increasing amounts of YFP N/C hemiproteins fused to CB2R (CB2R-cYFP and CB2R-nYFP). As observed in Figure 1C, both CB2R and GHSR1a were able to reconstitute RLuc and YFP proteins, emitting, respectively, bioluminescence and fluorescence. This result proves homodimerization. However, a saturation BRET curve was possible in cells expressing a constant amount of donor complemented hemiproteins and increasing levels of acceptor complemented hemiproteins (BRETmax: 56 ± 5 mBU, BRET50: 280 ± 70 mBU). Taken together, these results constitute evidence of heterotetramer formation with two protomers of each receptor, i.e., a heterotetramer constituted by two homodimers. As a negative control, we obtained a negligible signal when substituting one of the fused proteins by the non-fused version (one example is provided in Figure 1D that shows data in assays where CB2R-cYFP cDNA was substituted by that of cYFP).

2.2. CB2R-Mediated Signaling Is Blocked in the CB2-GHSR1a Receptor Heteromer (CB2-GHSR1aHet)

Once a direct interaction between CB2R and GHSR1a was identified, we investigated the functional consequences of interprotomer cross-talk within the heteromer. Signaling assays were performed taking into account that both CB2 and GHS1a receptors may couple to Gi. The activation of the receptors leads to reduced adenylate cyclase activity and a decrease in cytosolic cAMP levels. Accordingly, intracellular cAMP levels following receptor activation were measured in HEK-293T cells expressing CB2R, GHSR1a or both. In cells expressing the GHSR1a, ghrelin induced a 25% decrease of forskolin-induced cAMP levels that was completely counteracted by YIL 781 (1 µM), the selective GHSR1a antagonist. Moreover, the selective CB2R agonist, JWH-133 induced no effect, demonstrating the ligand selectivity and lack of nonspecific effects (Figure 2A). On the other hand, in cells expressing the CB2R, 200 nM JWH-133 induced a 30% decrease with respect to forskolin-induced cAMP levels, an effect that was completely blocked by pretreatment with the selective antagonist (AM 630, 1 µM). The control that was performed with 200 nM ghrelin induced no effect (Figure 2B). In HEK-293T cells expressing both receptors, the effect of ghrelin was similar to that found in cells only expressing the ghrelin receptor (Figure 3A); remarkably, the selective CB2R agonist, JWH-133, did not induced any effect suggesting that CB2R, in the heteromeric context, is not functionally coupled to Gi. Simultaneous treatment with both agonists resulted in a 37% decrease of the intracellular cAMP levels, i.e., similar to levels obtained upon ghrelin treatment. However, when the same cells were pretreated with ghrelin selective antagonist (YIL 781, 1µM) JWH-133 was able to allow the CB2R-Gi coupling (Figure 3A). Additionally, the finding that 1 µM AM 630 in co-transfected HEK-293T cells potentiated GHSR1a-mediated signaling was also noticeable. These results indicate that (i) the basal structure restrains activation and/or decreases the functional signal, and (ii) the CB2R blockade disappears in the presence of the selective antagonists of the partner receptor in the macromolecular complex.
We next analyzed the possibility of calcium mobilization upon activation of receptors. It is well known that GHSR1a receptor may couple to Gq, thus being linked to phospholipase C activation and calcium release from endoplasmic reticulum stores towards the cytosol. In GHSR1a-expressing HEK-293T cells, 200 nM ghrelin led to calcium mobilization (Figure 2B), that was counteracted by the pretreatment of the GHSR1a antagonist but not by the CB2R antagonist (and did not occur in cells only expressing the CB2R). In GHSR1a- or in CB2-receptor-expressing cells, JWH-133 treatment did not lead to any effect (Figure 2D).
When calcium mobilization was assayed in cotransfected cells, ghrelin treatment resulted in a characteristic curve of calcium mobilization that was not significantly modified upon simultaneous treatment with JWH-133 (Figure 3B). Pretreatment with the CB2R antagonist, AM 630, partially blocked the ghrelin effect. This phenomenon, known as cross-antagonism is, often, a print of the heteromer that is instrumental to detect it in natural sources. In these cells the CB2R was not coupled to Gq, i.e., JWH-133 did not lead to any signal related to changes in cytosolic levels of the calcium ion.
Finally, as CB2R and GHSR1a activation leads to activation of the mitogen-activated protein kinase (MAPK) pathway [31,32], we tested the properties of the heteromer in the link to the MAPK signaling cascade. Hence, we measured ERK1/2 phosphorylation in HEK-293T cells expressing the two receptors. Treatment with 200 nM ghrelin resulted in a significant signal whereas 200 nM JWH-133 did not induce any effect (Figure 3C). Interestingly, pretreatment with the ghrelin receptor antagonist, YIL 781, allowed the activation of the MAPK pathway via the CB2R. This action that results from antagonizing the GHSR1a was similar to that found in cAMP assays, i.e., blockade of the ghrelin receptor releases the brake posed on CB2R-mediated signaling.

2.3. CB2R Activation Is Blocked in Striatal Neurons via Formation of Heteromers of CB2R and GHSR1a (CB2R-GHSR1aHets)

Upon the demonstration that CB2R-GHSR1aHets may be formed in a heterologous system and upon the detection of particular heteromer prints, we undertook the search for detecting the prints in a more physiological context; for such purpose we used primary striatal neurons isolated from fetuses of mothers under a standard (STD) diet (see Section 4, Materials and Methods). Primary striatal neurons from fetuses of pregnant female mothers were isolated and cultured for 15 days prior to undertake signaling assays.
First, in regard to the forskolin-induced levels, the cAMP assays showed that stimulation of CB2R with JWH-133 did not induce any significant effect (Figure 4A). These findings may be due to lack of CB2R or to the presence of CB2R-GHSR1aHets. However, the results using antagonists did show that the CB2R is expressed and that is likely forming complexes with the ghrelin receptor. In fact, YIL 781 allowed the Gi coupling of the CB2R as JWH-133 was then able to decrease the forskolin-induced cytosolic cAMP levels (Figure 4A). These results are fully consistent with those obtained in the heterologous expression system (HEK-293T cells). In addition, analysis of the link to the MAPK pathway showed the effect of ghrelin whereas the effect of JWH-133 was only possible in cells pretreated with the selective ghrelin receptor antagonist (Figure 4B).
Finally, we used an imaging technique, the Proximity Ligation Assay (PLA), to demonstrate the occurrence of CB2R-GHSR1aHets in striatal neurons. PLA has been instrumental for detecting, in natural scenarios (cells or tissues), complexes formed by two proteins. Clusters of macromolecules formed by two different proteins appear as red dots using a confocal microscope (see Section 4, Materials and Methods for details); such red dots, which surrounded Hoechst stained nuclei, demonstrated the existence in striatal neurons of complexes of CB2R and GHSR1a (Figure 4C).

2.4. Expression of CB2R and GHSR1a Complexes Is Increased in Neurons of Progeny from Mothers on a High-Fat Diet

The ghrelin GHS1a receptor has an important role in controlling food intake, with some authors referring to ghrelin as the peripheral “hunger hormone” [22]. Moreover, it is known both an association between child obesity and maternal body mass index [33] and that diet-induced obesity leads to neuroinflammation and synapsis structure modification [34]. Herein, we investigated the expression of the CB2R-GHSR1aHet in striatal neurons of the progeny from female mice under a high-fat (HFD) diet. Primary striatal neurons from fetuses of pregnant HFD mothers were isolated and cultured for 15 days prior to undertaking signaling assays, and the results were compared with those obtained from neurons isolated from fetuses of mothers under a standard diet (see results presented in the previous section).
By analyzing the cAMP levels in primary striatal neurons from mothers in a HFD (Figure 5A) the results were qualitatively similar to those observed in the control group (Figure 4A) although more marked, i.e., the decreases obtained with respect to forskolin-induced cAMP levels were higher. One print of the CB2R-GHSR1aHet was noticed as JWH-133 was only efficacious in the presence of the selective GHS1a receptor antagonist (YIL 781). The results related to the phosphorylation of pERK1/2 (Figure 5B) were virtually identical to those found in the samples of the control group (Figure 4B), being necessary YIL 781 to observe an effect of JWH-133.
Finally, when analyzing by PLA the CB2R-GHSR1aHet expression, a marked increase in samples from the HFD group was noticed. An average of 12 red dots per Hoechst stained nuclei were observed in neurons derived from the HFD group, whereas neurons derived from the standard diet group only presented three red dots per stained nuclei (Figure 4C and Figure 5C,D the negative control is provided in Supplementary Figure S1). Remarkably, the striatal neurons of the siblings of HFD mothers show a much higher number of CB2R-GHSR1aHets than neurons of the siblings of mothers in standard diet, suggesting an enhanced suppression of CB2R function in HFD mother’s siblings.

3. Discussion

There is interest in the potential of targeting cannabinoid receptors for combating a variety of diseases. Despite targeting the CB1R was the main objective in cannabinoid-related drug discovery, the psychotropic action of some cannabinoids acting on its receptors and the side effects of a CB1R antagonist approved to combat obesity, rimonabant, has shifted the focus toward the CB2R. The limited expression of the CB2R in some CNS regions and its upregulation in activated glial cells have led to propose this receptor as target to limit neuroinflammation, to limit neurotoxicity induced by oxidative stress, to afford neuroprotection and/or the increase neurogenesis/gliogenesis [11,35,36,37,38,39,40,41]. Medications targeting cannabinoid receptors have been approved for a very limited therapeutic interventions (Sativex®, Marinol®, Epidiolex®; mainly to combat spasticity and emesis). The potential is higher and there are clinical trials already running or in preparation to test the efficacy of cannabidiol, an allosteric modulator of the CB2R [42], and of other cannabinoids for treating from the hypoxia of the neonate to improving the course of amyotrophic lateral or multiple sclerosis [15,43,44,45,46,47,48,49,50,51]. The number of registered clinical trials indicated in https://clinicaltrials.gov/ for testing cannabidiol in a variety of pathological conditions is 321 (date: 1 July 2021). As commented in the introduction, the CB2R is, also, an attractive target to afford neuroprotection in Parkinson’s disease [3,7,8,9,10,11,12,13,14].
The ghrelin receptor expressed in the hypothalamus and in reward circuits of the brain is key to mediating the control of food intake [24,25,52,53,54]. Several of the known phytocannabinoids are able to enter the brain where they exert multiple actions [1,12,55,56,57,58,59,60,61,62]. This study was undertaken to identify possible interactions between the orexinergic and the cannabinoidergic systems. The discovery of complexes formed by GHS1a and CB2 receptors and their identification in striatal neurons show that the ghrelin receptor modulates the effect of cannabinoids in the brain. From the molecular point of view our results suggest a tetrameric structure in complex with, at least, one Gi and one Gq protein. These results are qualitatively similar to those reported in the first reliable structural model of two interacting GPCRs, namely A1 and A2A adenosine receptors that arrange into a tetramer formed by two homodimers and are coupled to two different G proteins (one Gs and one Gi) [29,30]. In this example, the activation of one receptor blocks the activation of the partner receptor in the heteromer. However, the allosteric interactions within the CB2R-GHSR1aHet are such that CB2R-mediated signaling is blocked even in the absence of ghrelin, i.e., irrespective of the presence of the hormone, the CB2R cannot be activated within the CB2R-GHSR1aHet. Cannabinoid receptor activation is only possible in the presence of a selective GHS1a receptor antagonist, YIL 781. Although this atypical behavior is not found in many of the already identified GPCR heteromers (http://www.gpcr-hetnet.com/, accessed on 24 June 2021; [63]), it has been reported that the mere presence of the A2B receptor and the formation of A2A–A2B receptor heteromers decreases both agonist affinity and function of the A2A receptor. At present, the only reasonable hypothesis to explain the physiological role of the of CB2R-GHSR1aHet and of A2AR-A2BRHet is that they are formed to suppress the functionality of one of the two receptors in the heteromer.
Heteromer formation in GPCRs appear as a means for achieving functional diversification [64,65,66], i.e., heteromers are functional units that behave differently than individually-expressed receptors. There have been few ghrelin receptor-containing heteromers reported in the literature. To our knowledge, GHSR1a may interact with the class A dopamine D1 and D2 receptors or with class B secretin receptors [67,68]. It should be noted that cocaine interacting with sigma1-receptors modulate the GHSR1a-D1 receptor interaction in hypothalamic cells to suppress appetite [69]. Results in the present paper show that CB2R functionality is blunted by formation of the CB2R-GHSR1aHet. This discovery is complemented by another result of the present study, namely that the expression of the CB2R-GHSR1aHet in primary striatal neurons is altered in the progeny of obese mothers. The increased CB2R-GHSR1aHets expression in samples from fetuses of mothers subjected to a HFD (when compared with samples from fetuses of mothers subjected to a STD) may explain some of the findings related to obesity and unbalanced diets. On the one hand, genetic inactivation of the gene coding for the receptor leads to improved insulin function but leads to age-related obesity [70]. On the other hand, neuroinflammation often occurs in obesity [71] and, interestingly, balancing the diet improves both maternal deficits and neuroinflammation in offspring [72]. These findings are relevant as cumulative research has found a higher proportion of obesity cases among children with obese parents [73]. Upregulation of the CB2R-GHSR1aHet in offspring of mothers with HFD would indicate that already at birth these animals have CB2R function compromised, i.e., the benefits of cannabinoids acting on striatal CB2Rs would be lost by the blockade exerted by the ghrelin receptor. In addition, our results suggest that GHSR1a antagonists could have a double benefit: (i) reducing food intake and (ii) revert the detrimental effects of HFD on the functionality of striatal CB2Rs.

4. Materials and Methods

4.1. Reagents

JWH-133, AM 630, Ghrelin and YIL 781 were purchased from Tocris Bioscience (Bristol, UK).

4.2. High Fat Diet Model Generation

C57BL/6J female mice were used for the experiments. All animals were housed on a 12 h/12 h light/ dark cycle in a temperature- and humidity-controlled room and were allowed free access to water and standard laboratory chow. C57BL/6J mice were randomly assigned to a high fat diet (HFD) (60% kcal from fat; catalog no. D12492, Research Diets, New Brunswick, NJ, USA) or standard diet (STD) (10% kcal from fat; catalog no. D12450B, Research Diets) for 60 days. Primary striatal neurons were obtained from fetuses of mother on STD or HFD. Pregnant animals were killed by cervical dislocation during the light phase. All animal procedures were performed in agreement with European guidelines (2010/63/EU) and approved by the University of Barcelona Ethical Committee, which reports to the regional Government (Protocol #9659; Generalitat de Catalunya, 24 May 2019).

4.3. Cell Culture and Transient Transfection

Human embryonic Kidney HEK-293T (lot 612968) cells were acquired from the American Type Culture Collection (ATCC, Manassas, VA, USA). They were amplified and frozen in liquid nitrogen in several aliquots. Cells from each aliquot were used until passage 19. HEK-293T cells were grown in Dulbecco’s modified Eagle’s medium (DMEM) (Gibco, Waltham, MA, USA) supplemented with 2 mM L-glutamine, 100 U/mL penicillin/streptomycin, MEM Non-Essential Amino Acid Solution (1/100) and 5% (v/v) heat-inactivated fetal bovine serum (FBS) (all supplements were from Invitrogen, Paisley, Scotland, UK) and maintained in a humid atmosphere of 5% CO2 at 37 °C.
Cells were transiently transfected with the corresponding cDNAs using the PEI (PolyEthylenImine, Sigma-Aldrich, St. Louis, MO, USA) method as previously described [74,75]. 4 h after transfection, growth medium was replaced by complete medium. Experiments were carried out 48 h later.
To prepare primary striatal neurons, brains from fetuses of pregnant C57/BL6 mice were removed (gestational age: 17 days). Neurons were isolated as described in Hradsky et al. [1] and plated at a confluence of 40,000 cells/0.32 cm2. Briefly, the samples were dissected and, after careful removal of the meninges, digested for 20 min at 37 °C with 0.25% trypsin. Trypsinization was stopped by adding an equal volume of culture medium (Dulbecco’s modified Eagle medium-F-12 nutrient mixture, Invitrogen). Cells were brought to a single cell suspension by repeated pipetting followed by passage through a 100 μm-pore mesh. Pelleted (7 min, 200× g) cells were resuspended in supplemented DMEM and seeded at a density of 3.5 × 105 cells/mL in 6-well plates. The day after, medium was replaced by neurobasal medium supplemented with 2 mM L-glutamine, 100 U/mL penicillin/streptomycin and 2% (v/v) B27 medium (GIBCO). Neuronal cultures were used for assays after 15 days of culture. Using NeuN as a marker, the percentage of neurons in the cultures was >90%.

4.4. Expression Vectors

The human cDNAs for the CB2, GHS1a and GABAB receptors cloned in pcDNA3.1 were amplified without their stop codons using sense and antisense primers. The primers harbored either unique BamHI and HindIII sites for GHS1a and GABAB receptors and BamHI and KpnI sites for the CB2R. The fragments were subcloned to be in frame with an enhanced green fluorescent protein (GFP2-N2, Clontech, Heidelberg, Germany), the Renilla luciferase protein (RLuc) (pRluc-N1; PerkinElmer, Wellesley, MA, USA) or the hemiproteins nRLuc8, cRLuc8, nVenus or cVenus (pcDNA3.1-nRLuc8, pcDNA3.1-cRLuc8, pcDNA3.1-nVenus and pcDNA3.1-cVenus) on the C-terminal end of the receptor to produce CB2R-GFP2, GHSR1a-GFP2, GHSR1a-RLuc, GABABR-RLuc, GHSR1a-nRLuc, GHSR1a-cRLuc, CB2R-nYFP and CB2R-cYFP fusion proteins.

4.5. Immunofluorescence

HEK-293T cells transfected with cDNAs for CB2R-GFP2 and GHSR1a-RLuc were fixed in 4% paraformaldehyde for 15 min and then washed twice with PBS containing 20 mM glycine before permeabilization with the same buffer containing 0.2% Triton X-100 (5 min incubation). The samples were treated for 1 h with blocking solution (PBS containing 1% bovine serum albumin) and labeled with a mouse anti-RLuc (1/100; MAB4400, Millipore, Burlington, MA, USA) as primary antibody and a Cy3-conjugated anti-mouse IgG (1/200; 715-166-150; Jackson ImmunoResearch) as secondary antibody. The samples were washed several times and mounted with 30% Mowiol (Calbiochem, San Diego, CA, USA). Nuclei were stained with Hoechst (1/100). Samples were observed under a Zeiss 880 confocal microscope (Leica Microsystems, Wetzlar, Germany).

4.6. Bioluminescence Resonance Energy Transfer (BRET) Assay

HEK-293T cells growing in 6-well plates were transiently co-transfected with a constant amount of cDNA encoding for GHSR1a-Rluc and with increasing amounts of cDNA for CB2R-GFP2. For negative control, cells were co-transfected with a constant amount of cDNA encoding for GABABR-Rluc and with increasing amounts of cDNA for GHSR1a-GFP2. 48 h post-transfection, cells were washed twice in quick succession with HBSS (137 mM NaCl; 5 mM KCl; 0.34 mM Na2HPO4; 0.44 mM KH2PO4; 1.26 mM CaCl2; 0.4 mM MgSO4; 0.5 mM MgCl2 and 10 mM HEPES, pH 7.4) supplemented with 0.1% glucose (w/v), detached by gently pipetting and resuspended in the same buffer. To have an estimation of the number of cells per plate, protein concentration was determined using a Bradford assay kit (Bio-Rad, Munich, Germany) using bovine serum albumin dilutions for standardization. To quantify GFP2-fluorescence expression, cells were distributed (20 μg protein) in 96-well microplates (black plates with a transparent bottom; Porvair, Leatherhead, UK). Fluorescence was read using a fluorimeter FluoStar Optima (BMG Labtechnologies, Offenburg, Germany) equipped with a high-energy xenon flash lamp, reading at 510 nm. GFP2-fluorescence expression was determined as the fluorescence of the sample minus the fluorescence of cells only expressing protein-RLuc. For the BRET2 measurements, the equivalent of 20 μg protein of cell suspension was distributed in 96-well microplates (white plates; Porvair), and 5 μM Deep-Blue C was added (PJK GMBH, Kleinblittersdorf, Germany). 30 s after, readings were collected using a Mithras LB 940 (Berthold, Bad Wildbad, Germany), which allowed the integration of the signals detected in the short-wavelength filter at 410 nm (400–420 nm) and the long-wavelength filter at 510 nm (500–520 nm). To quantify receptor-RLuc expression, luminescence readings were collected 10 min after 5 μM coelenterazine H addition. The net BRET is defined as [(long-wavelength emission)/(short-wavelength emission)]-Cf where Cf corresponds to [(long-wavelength emission)/(short-wavelength emission)] for the RLuc construct expressed alone in the same experiment. The BRET curves were fitted assuming a single phase by a non-linear regression equation using the GraphPad Prism software (San Diego, CA, USA). BRET values are given as milli BRET units (mBU: 1000 × net BRET).

4.7. BRET with Bimolecular Luminescence and Fluorescence Complementation (BiLFC)

For BRET with bimolecular luminescence and fluorescence complementation (BiLFC) assays, HEK-293T cells were transiently transfected with a constant amount of cDNAs for GHSR1a-cRLuc and for GHSR1a-nRLuc cDNAs and increasing amounts of cDNAs for CB2R-cYFP and for CB2R-nYFP cDNAs. For negative controls, the cDNA for one of the fusion proteins was substituted by the corresponding empty vector (pcDNA3.1-cYFP) maintaining the other three plasmids. Protein determination was performed as described in the previous section. 48 h post-transfection, the equivalent of 20 μg protein of cell suspension was distributed in 96-well microplates. To quantify protein-YFP expression, fluorescence was read in a Mithras LB 940 equipped with a high-energy xenon flash lamp, using a 30 nm bandwidth excitation filter at 485 nm and an emission filter at 530 nm (510–550 nm). For BRET measurements, readings were collected 1 min after the addition of 5 μM coelenterazine H (Molecular Probes, Eugene, OR, USA) using a Mithras LB 940, which allows the integration of the signals detected in the short-wavelength filter at 485 nm and the long-wavelength filter at 530 nm. To quantify protein-RLuc expression, luminescence readings were obtained 10 min after 5 μM coelenterazine H addition using a Mithras LB 940.

4.8. cAMP Determination

HEK-293T cells transfected with the cDNAs for CB2R (0.5 µg) and/or GHSR1a (1 µg) and neuronal primary cultures were plated in 6 well plates. Two hours before initiating the experiment, neuronal culture or HEK-293T cell-culture media were exchanged to non-supplemented DMEM medium. Then, cells were detached, re-suspended in non-supplemented medium containing 50 µM zardaverine, and plated in 384-well microplates (2500 cells/well). Cells were pretreated (15 min) with the corresponding antagonists (1 µM AM 630 for CB2R or 1 µM YIL 781 for GHSR1a) or vehicle and stimulated with agonists (200 nM JWH-133 for CB2R or 200 nM ghrelin for GHSR1a) (15 min) before the addition of 0.5 μM forskolin or vehicle. Finally, reaction was stopped by addition of the Eu-cAMP tracer and the ULight-cAMP monoclonal antibody prepared in the “cAMP detection buffer” (PerkinElmer). All steps were performed at 25º. Homogeneous time-resolved fluorescence energy transfer (HTRF) measures were performed after 60 min incubation using the Lance Ultra cAMP kit (PerkinElmer, Waltham, MA, USA). Fluorescence at 665 nm was analyzed on a PHERAstar Flagship microplate reader equipped with an HTRF optical module (BMG Lab technologies, Offenburg, Germany).

4.9. MAPK Phosphorylation Assays

To determine MAP kinase 1/2 (ERK1/2) phosphorylation, striatal neurons were plated in transparent Deltalab 96-well plates and kept in the incubator for 15 days. 2 to 4 h before the experiment, the medium was replaced by serum starved medium. Next, the cells were pre-treated at 25 °C for 10 min with antagonists (1 µM AM 630 for CB2R or 1 µM YIL 781 for GHSR1a) or vehicle and stimulated for an additional 7 min with selective agonists (200 nM JWH-133 for CB2R or 200 nM ghrelin for GHSR1a). Then, neurons were washed twice with cold PBS before the addition of 30 µL/well “Ultra lysis buffer” -PerkinElmer- (20 min treatment). Afterwards, 10 µL of each supernatant were placed in white ProxiPlate 384-well plates and ERK1/2 phosphorylation was determined using an AlphaScreen® SureFire® kit (PerkinElmer), following the instructions of the supplier, and using an EnSpire® Multimode Plate Reader (PerkinElmer, Waltham, MA, USA). The reference value (100%) was the value achieved in the absence of any treatment (basal). The ligands effect was given in percentage with respect to the basal value.
On the other hand, HEK-293T cells were cultured into 25 cm2 flasks and transfected with the cDNAs for CB2R (0.5 µg) and/or GHSR1a (1 µg). Two hours before initiating the experiment, cell-culture medium was exchanged to serum-starved DMEM medium. The cells were, subsequently, pre-treated at 25 °C for 10 min with antagonists (1 µM AM 630 for CB2R or 1 µM YIL 781 for GHSR1a) or vehicle and stimulated for an additional 7 min with selective agonists (200 nM JWH-133 for CB2R or 200 nM ghrelin for GHSR1a). Stimulation was ended by a rapid rinse with ice-cold PBS, and the cell lysis was performed by the addition of 250 µL of ice-cold lysis buffer. Cellular debris were removed by centrifugation at 13,000× g for 5 min at 4 °C, and protein was quantified by the bicinchoninic acid method using bovine serum albumin dilutions as standard. To determine the level of ERK1/2 phosphorylation, equivalent amounts of protein (10 μg) were separated by electrophoresis on a denaturing 10% SDS-polyacrylamide gel and transferred onto PVDF-FL membranes. Membranes were blocked with Odyssey blocking buffer (LI-COR Biosciences, Lincoln, NE, USA) for 60 min and probed with a mixture of a mouse anti-phospho-ERK1/2 antibody (1:2500, Sigma-Aldrich) and rabbit anti-ERK1/2 antibody (1:40,000, Sigma-Aldrich) for 2 h. The 42 and 44 kDa bands corresponding to ERK 1 and ERK 2 were visualized by the addition of a mixture of IRDye 800 (anti-mouse) antibody (1:10,000, Sigma-Aldrich) and IRDye 680 (anti-rabbit) antibody (1:10,000, Sigma-Aldrich) for 1 h and scanned by the Odyssey infrared scanner (LI-COR Biosciences). Band densities were quantified using the scanner software and exported to Microsoft Excel. The level of phosphorylated ERK 1/2 was normalized for differences in loading using the total ERK1/2 protein band intensities.

4.10. Intracellular Calcium Mobilization

HEK-293T cells were co-transfected with cDNAs for CB2R (0.5 µg) and/or GHSR1a (1 µg) in the presence of 1 μg cDNA for the calmodulin-based calcium GCaMP6 sensor. Forty-eight hours after transfection, cells were detached using Mg2+-free Locke’s buffer pH 7.4 (154 mM NaCl, 5.6 mM KCl, 3.6 mM NaHCO3, 2.3 mM CaCl2, 5.6 mM glucose and 5 mM HEPES) supplemented with 10 μM glycine. 1500 cells per well were plated in 96-well black, clear bottom, microtiter plates. Then, cells were incubated for 10 min with the CB2R and GHSR1a antagonists (1 µM AM 630 or 1 µM YIL 781), and subsequently stimulated with selective agonists (200 nM JWH-133 or 200 nM ghrelin). Upon excitation at 488 nm, real-time 515 nm fluorescence emission due to calcium-ion complexed GCaMP6 was recorded on the EnSpire® Multimode Plate Reader (every 5 s, 100 flashes per well).

4.11. Proximity Ligation Assays (PLAs)

Physical interaction between CB2R and GHSR1a were detected using the Duolink in situ PLA detection Kit (OLink; Bioscience, Uppsala, Sweden) following the instructions of the supplier. Primary neurons were grown on glass coverslips, fixed in 4% paraformaldehyde for 15 min, washed with PBS containing 20 mM glycine to quench the aldehyde groups and permeabilized with the same buffer containing 0.05% Triton X-100 (20 min). Then, samples were extensively washed with PBS. After 1 h incubation at 37 °C with the blocking solution in a pre-heated humidity chamber, primary cultures were incubated overnight in the antibody diluent medium with a mixture of equal amounts of mouse anti-CB2R (1/100; sc-293188, Santa Cruz Technologies, Dallas, TX, USA) and rabbit anti-GHSR1a (1/100; ab95250, Abcam, Cambridge, United Kingdom) to detect CB2R–GHSR1a complexes. Neurons were processed using the PLA probes detecting primary antibodies (Duolink II PLA probe plus and Duolink II PLA probe minus) diluted in the antibody diluent solution (1:5). Ligation and amplification were done as indicated by the supplier. Samples were mounted using the mounting medium with Hoechst (1/100; Sigma-Aldrich) to stain nuclei. Samples were observed in a Leica SP2 confocal microscope (Leica Microsystems, Mannheim, Germany) equipped with an apochromatic 63× oil immersion objective (N.A. 1.4) and 405 and a 561 nm laser lines. For each field of view, a stack of two channels (one per staining) and four Z stacks with a step size of 1 μm were acquired. The number of neurons containing one or more red spots versus total cells (blue nucleus) was determined, and the unpaired Student’s t-test was used to compare the values (red dots/cell) obtained in the two groups.

Supplementary Materials

Supplementary materials can be found at https://0-www-mdpi-com.brum.beds.ac.uk/article/10.3390/ijms22168928/s1.

Author Contributions

Conceptualization, G.N. and R.F.; Data Curation, R.F.; Formal Analysis, J.L., A.L. and G.N.; Investigation, J.L., A.L., D.A.Z., C.M. and G.N.; Methodology, J.L., A.L. and R.R.-S.; Project Administration, R.R.-S.; Resources, C.M., N.C., G.N. and R.F.; Software, R.R.-S.; Supervision, G.N. and R.F.; Validation, G.N.; Writing—Original Draft, G.N. and R.F.; Writing—Review and Editing, J.L., A.L., C.M., R.R.-S., N.C. and G.N. All authors have read and agreed to the published version of the manuscript.

Funding

This work was partially supported by the AARFD-17-503612 grant the US Alzheimer’s Association, and by grants SAF2017-84117-R and PID2020-113430RB-I00 from the Spanish Ministerio de Ciencia, Innovación y Universidades (MCIU; or equivalent) and Spanish Agencia Estatal de Investigación (AEI); they include UE FEDER funds.

Institutional Review Board Statement

The study was conducted according to the guidelines of the Declaration of Helsinki, and approved by the Institutional Ethics Committee (Protocol #9659; Generalitat de Catalunya).

Informed Consent Statement

Not applicable.

Data Availability Statement

Data are available upon reasonable request to corresponding authors. A Western blot compilation file accompanies the submission and may be found via IJMS.

Acknowledgments

In memoriam, María Teresa Miras-Portugal a great scientist and a beloved friend of R.F.

Conflicts of Interest

The authors declare no conflict of interest. The funders had no role in the design of the study; in the collection, analyses, or interpretation of data; in the writing of the manuscript, or in the decision to publish the results.

References

  1. Franco, R.; Rivas-Santisteban, R.; Reyes-Resina, I.; Casanovas, M.; Pérez-Olives, C.; Ferreiro-Vera, C.; Navarro, G.; Sánchez de Medina, V.; Nadal, X. Pharmacological potential of varinic-, minor-, and acidic phytocannabinoids. Pharmacol. Res. 2020, 158, 104801. [Google Scholar] [CrossRef] [PubMed]
  2. Gonçalves, E.; Baldasso, G.; Bicca, M.; Paes, R.; Capasso, R.; Dutra, R. Terpenoids, Cannabimimetic Ligands, beyond the Cannabis Plant. Molecules 2020, 25, 1567. [Google Scholar] [CrossRef] [Green Version]
  3. Lanciego, J.L.; Barroso-Chinea, P.; Rico, A.J.; Conte-Perales, L.; Callén, L.; Roda, E.; Gómez-Bautista, V.; López, I.P.; Lluis, C.; Labandeira-García, J.L.; et al. Expression of the mRNA coding the cannabinoid receptor 2 in the pallidal complex of Macaca fascicularis. J. Psychopharmacol. 2011, 25, 97–104. [Google Scholar] [CrossRef] [PubMed]
  4. Sierra, S.; Luquin, N.; Rico, A.J.; Gómez-Bautista, V.; Roda, E.; Dopeso-Reyes, I.G.; Vázquez, A.; Martínez-Pinilla, E.; Labandeira-García, J.L.; Franco, R.; et al. Detection of cannabinoid receptors CB1 and CB2 within basal ganglia output neurons in macaques: Changes following experimental parkinsonism. Brain Struct. Funct. 2015, 220, 2721–2738. [Google Scholar] [CrossRef] [Green Version]
  5. Reyes-Resina, I.; Navarro, G.; Aguinaga, D.; Canela, E.I.; Schoeder, C.T.; Załuski, M.; Kieć-Kononowicz, K.; Saura, C.A.; Müller, C.E.; Franco, R. Molecular and functional interaction between GPR18 and cannabinoid CB2 G-protein-coupled receptors. Relevance in neurodegenerative diseases. Biochem. Pharmacol. 2018, 157, 169–179. [Google Scholar] [CrossRef] [Green Version]
  6. García-Gutiérrez, M.S.; Navarrete, F.; Navarro, G.; Reyes-Resina, I.; Franco, R.; Lanciego, J.L.; Giner, S.; Manzanares, J. Alterations in gene and protein expression of cannabinoid cb2 and gpr55 receptors in the dorsolateral prefrontal cortex of suicide victims. Neurotherapeutics 2018, 15, 796–806. [Google Scholar] [CrossRef] [Green Version]
  7. Navarro, G.; Borroto-Escuela, D.; Angelats, E.; Etayo, I.; Reyes-Resina, I.; Pulido-Salgado, M.; Rodríguez-Pérez, A.; Canela, E.; Saura, J.; Lanciego, J.L.; et al. Receptor-heteromer mediated regulation of endocannabinoid signaling in activated microglia. Role of CB1 and CB2 receptors and relevance for Alzheimer’s disease and levodopa-induced dyskinesia. Brain. Behav. Immun. 2018, 67, 139–151. [Google Scholar] [CrossRef] [PubMed]
  8. Rentsch, P.; Stayte, S.; Egan, T.; Clark, I.; Vissel, B. Targeting the cannabinoid receptor CB2 in a mouse model of l-dopa induced dyskinesia. Neurobiol. Dis. 2020, 134, 104646. [Google Scholar] [CrossRef] [PubMed]
  9. Antonazzo, M.; Botta, M.; Bengoetxea, H.; Ruiz-Ortega, J.Á.; Morera-Herreras, T. Therapeutic potential of cannabinoids as neuroprotective agents for damaged cells conducing to movement disorders. In International Review of Neurobiology; Academic Press Inc.: Cambridge, MA, USA, 2019; Volume 146, pp. 229–257. [Google Scholar]
  10. He, X.; Yang, L.; Huang, R.; Lin, L.; Shen, Y.; Cheng, L.; Jin, L.; Wang, S.; Zhu, R. Activation of CB2R with AM1241 ameliorates neurodegeneration via the Xist/miR-133b-3p/Pitx3 axis. J. Cell. Physiol. 2020, 235, 6032–6042. [Google Scholar] [CrossRef]
  11. Navarro, G.; Morales, P.; Rodríguez-Cueto, C.; Fernández-Ruiz, J.; Jagerovic, N.; Franco, R. Targeting cannabinoid CB2 receptors in the central nervous system. Medicinal chemistry approaches with focus on neurodegenerative disorders. Front. Neurosci. 2016, 10, 406. [Google Scholar] [CrossRef] [Green Version]
  12. Palomo-Garo, C.; Gómez-Gálvez, Y.; García, C.; Fernández-Ruiz, J. Targeting the cannabinoid CB 2 receptor to attenuate the progression of motor deficits in LRRK2-transgenic mice. Pharmacol. Res. 2016, 110, 181–192. [Google Scholar] [CrossRef]
  13. Fernández-Ruiz, J.; Romero, J.; Ramos, J. Endocannabinoids and neurodegenerative disorders: Parkinson’s disease, Huntington’s chorea, Alzheimer’s disease, and others. Handb. Exp. Pharmacol. 2015, 231, 233–259. [Google Scholar]
  14. Gómez-Gálvez, Y.; Palomo-Garo, C.; Fernández-Ruiz, J.; García, C. Potential of the cannabinoid CB2 receptor as a pharmacological target against inflammation in Parkinson’s disease. Prog. Neuro-Psychopharmacol. Biol. Psychiatry 2016, 64, 200–208. [Google Scholar] [CrossRef] [PubMed]
  15. Franco, R.; Villa, M.; Morales, P.; Reyes-Resina, I.; Gutiérrez-Rodríguez, A.; Jiménez, J.; Jagerovic, N.; Martínez-Orgado, J.; Navarro, G. Increased expression of cannabinoid CB2 and serotonin 5-HT1A heteroreceptor complexes in a model of newborn hypoxic-ischemic brain damage. Neuropharmacology 2019, 152, 58–66. [Google Scholar] [CrossRef]
  16. Song, W.M.; Colonna, M. The identity and function of microglia in neurodegeneration. Nat. Immunol. 2018, 19, 1048–1058. [Google Scholar] [CrossRef]
  17. Christensen, R.; Kristensen, P.K.; Bartels, E.M.; Bliddal, H.; Astrup, A. Efficacy and safety of the weight-loss drug rimonabant: A meta-analysis of randomised trials. Lancet 2007, 370, 1706–1713. [Google Scholar] [CrossRef]
  18. Carai, M.A.M.; Colombo, G.; Maccioni, P.; Gessa, G.L. Efficacy of rimonabant and other cannabinoid CB1 receptor antagonists in reducing food intake and body weight: Preclinical and clinical data. CNS Drug Rev. 2006, 12, 91–99. [Google Scholar] [CrossRef]
  19. Christensen, R.; Kristensen, P.K.; Bartels, E.M.; Bliddal, H.; Astrup, A.V. A meta-analysis of the efficacy and safety of the anti-obesity agent Rimonabant. Ugeskr. Laeger 2007, 169, 4360–4363. [Google Scholar]
  20. Sam, A.H.; Salem, V.; Ghatei, M.A. Rimonabant: From RIO to Ban. J. Obes. 2011, 2011, 432607. [Google Scholar] [CrossRef]
  21. Pagotto, U.; Cervino, C.; Vicennati, V.; Marsicano, G.; Lutz, B.; Pasquali, R. How many sites of action for endocannabinoids to control energy metabolism? Int. J. Obes. 2006, 30, S39–S43. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  22. Higgins, S.C.; Gueorguiev, M.; Korbonits, M. Ghrelin, the peripheral hunger hormone. Ann. Med. 2007, 39, 116–136. [Google Scholar] [CrossRef]
  23. Pradhan, G.; Samson, S.L.; Sun, Y. Ghrelin: Much more than a hunger hormone. Curr. Opin. Clin. Nutr. Metab. Care 2013, 16, 619–624. [Google Scholar] [CrossRef] [Green Version]
  24. Cassidy, R.M.; Tong, Q. Hunger and satiety gauge reward sensitivity. Front. Endocrinol. 2017, 8, 104. [Google Scholar] [CrossRef] [PubMed]
  25. Funahashi, H.; Takenoya, F.; Guan, J.-L.; Kageyama, H.; Yada, T.; Shioda, S. Hypothalamic neuronal networks and feeding-related peptides involved in the regulation of feeding. Anat. Sci. Int. Jpn. Assoc. Anat. 2003, 78, 123–138. [Google Scholar] [CrossRef] [PubMed]
  26. Abizaid, A.; Horvath, T.L. Brain circuits regulating energy homeostasis. Regul. Pept. 2008, 149, 3–10. [Google Scholar] [CrossRef]
  27. Schellekens, H.; Dinan, T.G.; Cryan, J.F. Lean mean fat reducing “ghrelin” machine: Hypothalamic ghrelin and ghrelin receptors as therapeutic targets in obesity. Neuropharmacology 2010, 58, 2–16. [Google Scholar] [CrossRef] [PubMed]
  28. Alexander, S.P.; Christopoulos, A.; Davenport, A.P.; Kelly, E.; Mathie, A.; Peters, J.A.; Veale, E.L.; Armstrong, J.F.; Faccenda, E.; Harding, S.D.; et al. The concise guide to pharmacology 2019/20: G protein-coupled receptors. Br. J. Pharmacol. 2019, 176, S21–S141. [Google Scholar] [CrossRef] [Green Version]
  29. Navarro, G.; Cordomí, A.; Brugarolas, M.; Moreno, E.; Aguinaga, D.; Pérez-Benito, L.; Ferre, S.; Cortés, A.; Casadó, V.; Mallol, J.; et al. Cross-communication between Gi and Gs in a G-protein-coupled receptor heterotetramer guided by a receptor C-terminal domain. BMC Biol. 2018, 16, 24. [Google Scholar] [CrossRef]
  30. Navarro, G.; Cordomí, A.; Zelman-Femiak, M.; Brugarolas, M.; Moreno, E.; Aguinaga, D.; Perez-Benito, L.; Cortés, A.; Casadó, V.; Mallol, J.; et al. Quaternary structure of a G-protein-coupled receptor heterotetramer in complex with Gi and Gs. BMC Biol. 2016, 14, 26. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  31. Navarro, G.; Reyes-Resina, I.; Rivas-Santisteban, R.; Sánchez de Medina, V.; Morales, P.; Casano, S.; Ferreiro-Vera, C.; Lillo, A.; Aguinaga, D.; Jagerovic, N.; et al. Cannabidiol skews biased agonism at cannabinoid CB1 and CB2 receptors with smaller effect in CB1-CB2 heteroreceptor complexes. Biochem. Pharmacol. 2018, 157, 148–158. [Google Scholar] [CrossRef]
  32. Mousseaux, D.; Le Gallic, L.; Ryan, J.; Oiry, C.; Gagne, D.; Fehrentz, J.-A.; Galleyrand, J.-C.; Martinez, J. Regulation of ERK1/2 activity by ghrelin-activated growth hormone secretagogue receptor 1A involves a PLC/PKCɛ pathway. Br. J. Pharmacol. 2006, 148, 350–365. [Google Scholar] [CrossRef] [Green Version]
  33. Heslehurst, H.; Vieira, R.; Akhter, Z.; Bailey, H.; Slack, E.; Ngongalah, L.; Pemu, A.; Rankin, J. The association between maternal body mass index and child obesity: A systematic review and meta-analysis. PLoS Med. 2019, 16, e1002817. [Google Scholar] [CrossRef] [PubMed]
  34. Guillemot-Legris, O.; Muccioli, G.G. Obesity-induced neuroinflammation: Beyond the hypothalamus. Trends Neurosci. 2017, 40, 237–253. [Google Scholar] [CrossRef] [PubMed]
  35. Mecha, M.; Feliú, A.; Carrillo-Salinas, F.J.; Rueda-Zubiaurre, A.; Ortega-Gutiérrez, S.; de Sola, R.G.; Guaza, C. Endocannabinoids drive the acquisition of an alternative phenotype in microglia. Brain. Behav. Immun. 2015, 49, 233–245. [Google Scholar] [CrossRef] [PubMed]
  36. Cottone, E.; Pomatto, V.; Rapelli, S.; Scandiffio, R.; Mackie, K.; Bovolin, P. Cannabinoid receptor modulation of neurogenesis: ST14A striatal neural progenitor cells as a simplified in vitro model. Molecules 2021, 26, 1448. [Google Scholar] [CrossRef] [PubMed]
  37. Cassano, T.; Calcagnini, S.; Pace, L.; De Marco, F.; Romano, A.; Gaetani, S. Cannabinoid receptor 2 signaling in neurodegenerative disorders: From pathogenesis to a promising therapeutic target. Front. Neurosci. 2017, 11, 30. [Google Scholar] [CrossRef] [Green Version]
  38. García-Ovejero, D.; Arévalo-Martín, Á.; Navarro-Galve, B.; Pinteaux, E.; Molina-Holgado, E.; Molina-Holgado, F. Neuroimmmune interactions of cannabinoids in neurogenesis: Focus on interleukin-1β (IL-1β) signalling. Biochem. Soc. Trans. 2013, 41, 1577–1582. [Google Scholar] [CrossRef] [Green Version]
  39. Komorowska-Müller, J.A.; Schmöle, A.C. CB2 receptor in microglia: The guardian of self-control. Int. J. Mol. Sci. 2021, 22, 19. [Google Scholar] [CrossRef]
  40. Docagne, F.; Mestre, L.; Loría, F.; Hernangómez, M.; Correa, F.; Guaza, C. Therapeutic potential of CB2 targeting in multiple sclerosis. Expert Opin. Ther. Targets 2008, 12, 185–195. [Google Scholar] [CrossRef] [Green Version]
  41. Ilyasov, A.A.; Milligan, C.E.; Pharr, E.P.; Howlett, A.C. The endocannabinoid system and oligodendrocytes in health and disease. Front. Neurosci. 2018, 12, 733. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  42. Martínez-Pinilla, E.; Varani, K.; Reyes-Resina, I.; Angelats, E.; Vincenzi, F.; Ferreiro-Vera, C.; Oyarzabal, J.; Canela, E.I.; Lanciego, J.L.; Nadal, X.; et al. Binding and signaling studies disclose a potential allosteric site for cannabidiol in cannabinoid CB2 receptors. Front. Pharmacol. 2017, 8, 744. [Google Scholar] [CrossRef] [PubMed]
  43. Ceprián, M.; Jiménez-Sánchez, L.; Vargas, C.; Barata, L.; Hind, W.; Martínez-Orgado, J. Cannabidiol reduces brain damage and improves functional recovery in a neonatal rat model of arterial ischemic stroke. Neuropharmacology 2017, 116, 151–159. [Google Scholar] [CrossRef]
  44. Mohammed, N.; Ceprian, M.; Jimenez, L.; Pazos, M.R.; Martinez-Orgado, J. Neuroprotective effects of cannabidiol in hypoxic ischemic insult: The therapeutic window in newborn mice. CNS Neurol. Disord. Drug Targets 2016, 27, 27. [Google Scholar] [CrossRef]
  45. Garberg, H.T.; Huun, M.U.; Escobar, J.; Martinez-Orgado, J.; Løberg, E.M.; Solberg, R.; Saugstad, O.D. Short-term effects of cannabidiol after global hypoxia-ischemia in newborn piglets. Pediatr. Res. 2016, 80, 710–718. [Google Scholar] [CrossRef] [PubMed]
  46. De Lago, E.; Fernández-Ruiz, J. Cannabinoids and neuroprotection in motor-related disorders. CNS Neurol. Disord. Drug Targets 2007, 6, 377–387. [Google Scholar] [CrossRef]
  47. Molina-Holgado, E.; Vela, J.M.; Arévalo-Martín, A.; Almazán, G.; Molina-Holgado, F.; Borrell, J.; Guaza, C. Cannabinoids promote oligodendrocyte progenitor survival: Involvement of cannabinoid receptors and phosphatidylinositol-3 kinase/Akt signaling. J. Neurosci. 2002, 22, 9742–9753. [Google Scholar] [CrossRef] [PubMed]
  48. Carrillo-Salinas, F.J.; Mestre, L.; Mecha, M.; Feliú, A.; Del Campo, R.; Villarrubia, N.; Espejo, C.; Montalbán, X.; Álvarez-Cermeño, J.C.; Villar, L.M.; et al. Gut dysbiosis and neuroimmune responses to brain infection with Theiler’s murine encephalomyelitis virus. Sci. Rep. 2017, 7, 44377. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  49. Mecha, M.; Yanguas-Casás, N.; Feliú, A.; Mestre, L.; Carrillo-Salinas, F.; Azcoitia, I.; Yong, V.W.; Guaza, C. The endocannabinoid 2-AG enhances spontaneous remyelination by targeting microglia. Brain. Behav. Immun. 2019, 77, 110–126. [Google Scholar] [CrossRef]
  50. Mecha, M.; Carrillo-Salinas, F.J.; Feliú, A.; Mestre, L.; Guaza, C. Microglia activation states and cannabinoid system: Therapeutic implications. Pharmacol. Ther. 2016, 166, 40–55. [Google Scholar] [CrossRef]
  51. Correa, F.; Docagne, F.; Mestre, L.; Loría, F.; Hernangómez, M.; Borrell, J.; Guaza, C. Cannabinoid system and neuroinflammation: Implications for multiple sclerosis. Neuroimmunomodulation 2007, 14, 182–187. [Google Scholar] [CrossRef]
  52. Argente-Arizon, P.; Freire-Regatillo, A.; Argente, J.; Chowen, J.A. Role of non-neuronal cells in body weight and appetite control. Front. Endocrinol. 2015, 6, 42. [Google Scholar]
  53. Geelissen, S.M.E.; Beck, I.M.E.; Darras, V.M.; Kühn, E.R.; Van der Geyten, S.; Kuhn, E.R.; Van der, G.S. Distribution and regulation of chicken growth hormone secretagogue receptor isoforms. Gen. Comp. Endocrinol. 2003, 134, 167–174. [Google Scholar] [CrossRef]
  54. Guan, X.; Yu, H.; Palyha, O.; McKee, K.; Feighner, S.; Sirinathsinghji, D.; Smith, R.; Van der Ploeg, L.; Howard, A. Distribution of mRNA encoding the growth hormone secretagogue receptor in brain and peripheral tissues. Mol. Brain Res. 1997, 48, 23–29. [Google Scholar] [CrossRef]
  55. Sagredo, O.; García-Arencibia, M.; de Lago, E.; Finetti, S.; Decio, A.; Fernández-Ruiz, J. Cannabinoids and neuroprotection in basal ganglia disorders. Mol. Neurobiol. 2007, 36, 82–91. [Google Scholar] [CrossRef]
  56. Espejo-Porras, F.; Fernández-Ruiz, J.; Pertwee, R.G.; Mechoulam, R.; García, C. Motor effects of the non-psychotropic phytocannabinoid cannabidiol that are mediated by 5-HT1Areceptors. Neuropharmacology 2013, 75, 155–163. [Google Scholar] [CrossRef]
  57. García, C.; Palomo-Garo, C.; Gómez-Gálvez, Y.; Fernández-Ruiz, J. Cannabinoid–dopamine interactions in the physiology and physiopathology of the basal ganglia. Br. J. Pharmacol. 2016, 173, 2069–2079. [Google Scholar] [CrossRef] [PubMed]
  58. Valdeolivas, S.; Sagredo, O.; Delgado, M.; Pozo, M.; Fernández-Ruiz, J. Effects of a sativex-like combination of phytocannabinoids on disease progression in R6/2 mice, an experimental model of Huntington’s disease. Int. J. Mol. Sci. 2017, 18, 684. [Google Scholar] [CrossRef]
  59. Libro, R.; Diomede, F.; Scionti, D.; Piattelli, A.; Grassi, G.; Pollastro, F.; Bramanti, P.; Mazzon, E.; Trubiani, O. Cannabidiol modulates the expression of Alzheimer’s disease-related genes in mesenchymal stem cells. Int. J. Mol. Sci. 2016, 18, 26. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  60. Haider, A.; Spinelli, F.; Herde, A.M.; Mu, B.; Keller, C.; Margelisch, M.; Weber, M.; Schibli, R.; Mu, L.; Ametamey, S.M. Evaluation of 4-oxo-quinoline-based CB2 PET radioligands in R6/2 chorea huntington mouse model and human ALS spinal cord tissue. Eur. J. Med. Chem. 2018, 145, 746–759. [Google Scholar] [CrossRef]
  61. Zeissler, M.-L.; Eastwood, J.; McCorry, K.; Hanemann, O.C.; Zajicek, J.P.; Carroll, C.B. Delta-9-tetrahydrocannabinol protects against MPP+ toxicity in SH-SY5Y cells by restoring proteins involved in mitochondrial biogenesis. Oncotarget 2016, 7, 46603–46614. [Google Scholar] [CrossRef] [Green Version]
  62. Lafuente, H.; Alvarez, F.J.; Pazos, M.R.; Alvarez, A.; Rey-Santano, M.C.; Mielgo, V.; Murgia-Esteve, X.; Hilario, E.; Martinez-Orgado, J. Cannabidiol reduces brain damage and improves functional recovery after acute hypoxia-ischemia in newborn pigs. Pediatr. Res. 2011, 70, 272–277. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  63. Borroto-Escuela, D.O.; Brito, I.; Romero-Fernandez, W.; Di Palma, M.; Oflijan, J.; Skieterska, K.; Duchou, J.; Van Craenenbroeck, K.; Suárez-Boomgaard, D.; Rivera, A.; et al. The G protein-coupled receptor heterodimer network (GPCR-HetNet) and its hub components. Int. J. Mol. Sci. 2014, 15, 8570–8590. [Google Scholar] [CrossRef]
  64. Ferré, S.; Baler, R.; Bouvier, M.; Caron, M.G.; Devi, L.A.; Durroux, T.; Fuxe, K.; George, S.R.; Javitch, J.A.; Lohse, M.J.; et al. Building a new conceptual framework for receptor heteromers. Nat. Chem. Biol. 2009, 5, 131–134. [Google Scholar] [CrossRef] [Green Version]
  65. Franco, R.; Martínez-Pinilla, E.; Lanciego, J.L.; Navarro, G. Basic pharmacological and structural evidence for class A G-protein-coupled receptor heteromerization. Front. Pharmacol. 2016, 7, 76. [Google Scholar] [CrossRef]
  66. Franco, R.; Aguinaga, D.; Jiménez, J.; Lillo, J.; Martínez-Pinilla, E.; Navarro, G. Biased receptor functionality versus biased agonism in G-protein-coupled receptors. Biomol. Concepts 2018, 9, 143–154. [Google Scholar] [CrossRef]
  67. Harikumar, K.G.; Morfis, M.M.; Sexton, P.M.; Miller, L.J. Pattern of intra-family hetero-oligomerization involving the G-protein-coupled secretin receptor. J. Mol. Neurosci. 2008, 36, 279–285. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  68. Casanovas, M.; Jiménez-Rosés, M.; Cordomí, A.; Lillo, A.; Vega-Quiroga, I.; Izquierdo, J.; Medrano, M.; Gysling, K.; Pardo, L.; Navarro, G.; et al. Discovery of a macromolecular complex mediating the hunger suppressive actions of cocaine: Structural and functional properties. Addict. Biol. 2021, e13017. [Google Scholar] [CrossRef]
  69. Medrano, M.; Aguinaga, D.; Reyes-Resina, I.; Canela, E.I.; Mallol, J.; Navarro, G.; Franco, R. Orexin A/hypocretin modulates leptin receptor-mediated signaling by allosteric modulations mediated by the ghrelin GHS-R1A receptor in hypothalamic neurons. Mol. Neurobiol. 2018, 55, 4718–4730. [Google Scholar] [CrossRef] [PubMed]
  70. Agudo, J.; Martin, M.; Roca, C.; Molas, M.; Bura, A.S.; Zimmer, A.; Bosch, F.; Maldonado, R. Deficiency of CB2 cannabinoid receptor in mice improves insulin sensitivity but increases food intake and obesity with age. Diabetologia 2010, 53, 2629–2640. [Google Scholar] [CrossRef] [Green Version]
  71. Miller, A.A.; Spencer, S.J. Obesity and neuroinflammation: A pathway to cognitive impairment. Brain. Behav. Immun. 2014, 42, 10–21. [Google Scholar] [CrossRef]
  72. Kang, S.S.; Kurti, A.; Fair, D.A.; Fryer, J.D. Dietary intervention rescues maternal obesity induced behavior deficits and neuroinflammation in offspring. J. Neuroinflammation 2014, 11, 156. [Google Scholar] [CrossRef] [PubMed]
  73. Abu-Rmeileh, N.M.E.; Hart, C.L.; McConnachie, A.; Upton, M.N.; Lean, M.E.J.; Watt, G.C.M. Contribution of midparental BMI and other determinants of obesity in adult offspring. Obesity 2008, 16, 1388–1393. [Google Scholar] [CrossRef] [PubMed]
  74. Carriba, P.; Navarro, G.; Ciruela, F.; Ferré, S.; Casadó, V.; Agnati, L.; Cortés, A.; Mallol, J.; Fuxe, K.; Canela, E.I.E.I.; et al. Detection of heteromerization of more than two proteins by sequential BRET-FRET. Nat. Methods 2008, 5, 727–733. [Google Scholar] [CrossRef] [PubMed]
  75. Navarro, G.; Hradsky, J.; Lluís, C.; Casadó, V.; McCormick, P.J.; Kreutz, M.R.; Mikhaylova, M. NCS-1 associates with adenosine A(2A) receptors and modulates receptor function. Front. Mol. Neurosci. 2012, 5, 53. [Google Scholar] [CrossRef] [Green Version]
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Figure 1. Molecular interaction between GHS1a and CB2 receptors expressed in transfected HEK-293T cells. (A) Confocal microscopy images of HEK-293T cells co-transfected with cDNAs for GHSR1a-RLuc (0.75 µg) and for CB2R-GFP2 (0.5 µg). GHSR1a-RLuc (red) was identified by immunocytochemistry using an anti-RLuc antibody (Merck-Millipore, 1/100). The CB2R-GFP2 (green) was identified by the fluorescence due to GFP2. colocalization is shown in yellow (image in the right). Cell nuclei were stained with Hoechst (blue). Scale bar: 5 μm. (B) BRET saturation experiments were performed using HEK-293T cells co-transfected with (i) a constant amount of GHSR1a-RLuc cDNA (1.5 μg) and increasing amounts of CB2R-GFP2 cDNA (0–2 μg) or (ii) a constant amount of GABAB-RLuc cDNA (0.75 μg) and increasing amounts of GHSR1a-GFP2 cDNA (0–2 μg) as negative control. BRET data are expressed as the mean ± SEM of 8 different experiments performed in duplicates. (C) Bimolecular luminescence and fluorescence complementation (BiLFC) assays were performed in HEK-293T cells co-transfected with a constant amount of GHSR1a-cRLuc and GHSR1a-nRLuc cDNAs (1.5 μg each) and increasing amounts of CB2R-cYFP and CB2R-nYFP cDNAs (0–3 μg each). (D) HEK-293T cells were co-transfected with 1.5 μg of the GHSR1a-cRLuc and GHSR1a-nRLuc cDNAs and 3 μg of the CB2R-nYFP and CB2R-cYFP cDNAs or with the non-fused cYFP as negative control. BRET data are expressed as the mean ± SEM of 7 different experiments performed in duplicates. * p < 0.05. mBU: milliBret units.
Figure 1. Molecular interaction between GHS1a and CB2 receptors expressed in transfected HEK-293T cells. (A) Confocal microscopy images of HEK-293T cells co-transfected with cDNAs for GHSR1a-RLuc (0.75 µg) and for CB2R-GFP2 (0.5 µg). GHSR1a-RLuc (red) was identified by immunocytochemistry using an anti-RLuc antibody (Merck-Millipore, 1/100). The CB2R-GFP2 (green) was identified by the fluorescence due to GFP2. colocalization is shown in yellow (image in the right). Cell nuclei were stained with Hoechst (blue). Scale bar: 5 μm. (B) BRET saturation experiments were performed using HEK-293T cells co-transfected with (i) a constant amount of GHSR1a-RLuc cDNA (1.5 μg) and increasing amounts of CB2R-GFP2 cDNA (0–2 μg) or (ii) a constant amount of GABAB-RLuc cDNA (0.75 μg) and increasing amounts of GHSR1a-GFP2 cDNA (0–2 μg) as negative control. BRET data are expressed as the mean ± SEM of 8 different experiments performed in duplicates. (C) Bimolecular luminescence and fluorescence complementation (BiLFC) assays were performed in HEK-293T cells co-transfected with a constant amount of GHSR1a-cRLuc and GHSR1a-nRLuc cDNAs (1.5 μg each) and increasing amounts of CB2R-cYFP and CB2R-nYFP cDNAs (0–3 μg each). (D) HEK-293T cells were co-transfected with 1.5 μg of the GHSR1a-cRLuc and GHSR1a-nRLuc cDNAs and 3 μg of the CB2R-nYFP and CB2R-cYFP cDNAs or with the non-fused cYFP as negative control. BRET data are expressed as the mean ± SEM of 7 different experiments performed in duplicates. * p < 0.05. mBU: milliBret units.
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Figure 2. Functional characterization of GHS1a and CB2 receptors expressed in HEK-293T cells. (A,B) HEK-293T cells transfected with plasmids encoding for either GHSR1a (1.5 μg) (A) or CB2R (1 μg) (B) were pre-treated with selective antagonists, 1 μM YIL 781-GHSR1a- or 1 μM AM 630-CB2R, and subsequently treated with the selective agonists, 200 nM ghrelin -GHSR1a- or 200 nM JWH-133 -CB2R-. cAMP levels after 0.5 μM forskolin stimulation were detected by the Lance Ultra cAMP kit and the results were expressed in % respect to levels obtained upon forskolin stimulation. The values are the mean ± SEM of 10 different experiments performed in triplicates. One-way ANOVA followed by Dunnett’s multiple comparison post-hoc test were used for statistical analysis. ** p < 0.01, versus forskolin treatment. (C,D) HEK-293T cells expressing an engineered calcium sensor, GCaMP6 and GHSR1a (C) or CB2R (D) were pre-treated with selective antagonists for 10 min followed by agonist stimulation. Representative traces of intracellular Ca2+ responses over time are shown (6 independent experiments).
Figure 2. Functional characterization of GHS1a and CB2 receptors expressed in HEK-293T cells. (A,B) HEK-293T cells transfected with plasmids encoding for either GHSR1a (1.5 μg) (A) or CB2R (1 μg) (B) were pre-treated with selective antagonists, 1 μM YIL 781-GHSR1a- or 1 μM AM 630-CB2R, and subsequently treated with the selective agonists, 200 nM ghrelin -GHSR1a- or 200 nM JWH-133 -CB2R-. cAMP levels after 0.5 μM forskolin stimulation were detected by the Lance Ultra cAMP kit and the results were expressed in % respect to levels obtained upon forskolin stimulation. The values are the mean ± SEM of 10 different experiments performed in triplicates. One-way ANOVA followed by Dunnett’s multiple comparison post-hoc test were used for statistical analysis. ** p < 0.01, versus forskolin treatment. (C,D) HEK-293T cells expressing an engineered calcium sensor, GCaMP6 and GHSR1a (C) or CB2R (D) were pre-treated with selective antagonists for 10 min followed by agonist stimulation. Representative traces of intracellular Ca2+ responses over time are shown (6 independent experiments).
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Figure 3. CB2-GHSR1aHet-mediated signaling in transfected HEK-293T cells. Panels (A–C) HEK-293T cells were transfected with cDNAs encoding for GHSR1a (1.5 μg) and CB2R (1 μg) (A,C) or with GHSR1a (1.5 μg), CB2R (1 μg) and the GCaMP6 calcium sensor (B) and pre-treated with antagonists, 1 μM YIL 781 -for GHSR1a- and 1 μM AM 630 -for CB2R, and subsequently stimulated with selective agonists, 200 nM ghrelin -for GHSR1a- and 200 nM JWH-133 -for CB2R, individually or in combination. cAMP levels were analyzed by the Lance Ultra cAMP kit and results were expressed in % respect to levels obtained upon 0.5 μM forskolin stimulation (A). Representative traces of intracellular Ca2+ responses over time are shown (9 independent experiments) (B). ERK 1/2 phosphorylation was determined by immunoblot using the Odyssey infrared scanner (LI-COR Biosciences) (C,D). In cAMP accumulation and MAPK pathway signaling-related assays, the values are the mean ± SEM of 8 different experiments performed in triplicates. One-way ANOVA followed by Dunnett’s multiple comparison post-hoc test were used for statistical analysis..* p < 0.05, ** p < 0.01, versus basal in pERK1/2 assays; *** p < 0.001; versus forskolin treatment in cAMP or versus basal in pERK1/2 assays, # p < 0.05 versus JWH-133 treatment in pERK assays, ## p < 0.01 versus JWH-133+FK treatment in cAMP assays; $$$ p < 0.001; versus ghrelin+FK treatment.
Figure 3. CB2-GHSR1aHet-mediated signaling in transfected HEK-293T cells. Panels (A–C) HEK-293T cells were transfected with cDNAs encoding for GHSR1a (1.5 μg) and CB2R (1 μg) (A,C) or with GHSR1a (1.5 μg), CB2R (1 μg) and the GCaMP6 calcium sensor (B) and pre-treated with antagonists, 1 μM YIL 781 -for GHSR1a- and 1 μM AM 630 -for CB2R, and subsequently stimulated with selective agonists, 200 nM ghrelin -for GHSR1a- and 200 nM JWH-133 -for CB2R, individually or in combination. cAMP levels were analyzed by the Lance Ultra cAMP kit and results were expressed in % respect to levels obtained upon 0.5 μM forskolin stimulation (A). Representative traces of intracellular Ca2+ responses over time are shown (9 independent experiments) (B). ERK 1/2 phosphorylation was determined by immunoblot using the Odyssey infrared scanner (LI-COR Biosciences) (C,D). In cAMP accumulation and MAPK pathway signaling-related assays, the values are the mean ± SEM of 8 different experiments performed in triplicates. One-way ANOVA followed by Dunnett’s multiple comparison post-hoc test were used for statistical analysis..* p < 0.05, ** p < 0.01, versus basal in pERK1/2 assays; *** p < 0.001; versus forskolin treatment in cAMP or versus basal in pERK1/2 assays, # p < 0.05 versus JWH-133 treatment in pERK assays, ## p < 0.01 versus JWH-133+FK treatment in cAMP assays; $$$ p < 0.001; versus ghrelin+FK treatment.
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Figure 4. Expression and function of CB2R-GHSR1aHets in primary neurons from C57BL/6J mice. (A,B) Primary striatal neurons isolated from C57BL/6J mice were pre-treated with antagonists, 1 μM YIL 781 -for GHSR1a- or 1 μM AM 630 -for CB2R-, and subsequently stimulated with selective agonists, 200 nM ghrelin -for GHSR1a- or 200 nM JWH-133 -for CB2R-, individually or in combination. cAMP levels were determined using the Lance Ultra cAMP kit and results were expressed in % respect to levels obtained upon 0.5 μM forskolin stimulation (A), while ERK1/2 phosphorylation was analyzed using the AlphaScreen®SureFire® kit (PerkinElmer; Wellesley, MA, USA) (B). Values are the mean ± SEM of 6 different experiments performed in triplicates. One-way ANOVA followed by Dunnett’s multiple comparison post-hoc tests were used for statistical analysis. ** p<0.01, *** p < 0.001 versus basal, ### p < 0.001; versus JWH-133+FK treatment in cAMP or versus JWH-133 treatment in p-ERK1/2 assays. (C) CB2R-GHSR1aHets were detected in primary striatal neurons by the in situ proximity ligation assay (PLA) using specific antibodies. Cell nuclei was stained with Hoechst (blue). Samples from 5 different animals were processed and analyzed and quantitation is shown in Figure 5. Scale bar: 20 μm.
Figure 4. Expression and function of CB2R-GHSR1aHets in primary neurons from C57BL/6J mice. (A,B) Primary striatal neurons isolated from C57BL/6J mice were pre-treated with antagonists, 1 μM YIL 781 -for GHSR1a- or 1 μM AM 630 -for CB2R-, and subsequently stimulated with selective agonists, 200 nM ghrelin -for GHSR1a- or 200 nM JWH-133 -for CB2R-, individually or in combination. cAMP levels were determined using the Lance Ultra cAMP kit and results were expressed in % respect to levels obtained upon 0.5 μM forskolin stimulation (A), while ERK1/2 phosphorylation was analyzed using the AlphaScreen®SureFire® kit (PerkinElmer; Wellesley, MA, USA) (B). Values are the mean ± SEM of 6 different experiments performed in triplicates. One-way ANOVA followed by Dunnett’s multiple comparison post-hoc tests were used for statistical analysis. ** p<0.01, *** p < 0.001 versus basal, ### p < 0.001; versus JWH-133+FK treatment in cAMP or versus JWH-133 treatment in p-ERK1/2 assays. (C) CB2R-GHSR1aHets were detected in primary striatal neurons by the in situ proximity ligation assay (PLA) using specific antibodies. Cell nuclei was stained with Hoechst (blue). Samples from 5 different animals were processed and analyzed and quantitation is shown in Figure 5. Scale bar: 20 μm.
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Figure 5. Expression and function of CB2R-GHSR1aHets in primary neurons isolated from fetuses of pregnant C57BL/6J female mice subjected to a high-fat diet. (A,B) Primary striatal neurons isolated from fetuses of pregnant females mice subjected to a high-fat diet for 60 days were pre-treated with antagonists, 1 μM YIL 781 -for GHSR1a- or 1 μM AM 630 -for CB2R-, followed by stimulation with selective agonists, 200 nM ghrelin -for GHSR1a- or 200 nM JWH-133 -for CB2R-, individually or in combination. cAMP levels were determined using the Lance Ultra cAMP kit and results were expressed in % versus 0.5 µM forskolin treatment (A) while ERK1/2 phosphorylation was analyzed using the AlphaScreen® SureFire® kit (PerkinElmer) (B). Values are the mean ± SEM of 5 different experiments performed in triplicates. One-way ANOVA followed by Dunnett’s multiple comparison post-hoc test were used for statistical analysis. # p < 0.05, ## p < 0.005 versus JWH-133+FK treatment in cAMP or versus JWH-133 treatment in p-ERK1/2 assays. * p < 0.05, basal. (C). CB2R-GHSR1aHets were detected by the in situ proximity ligation assay (PLA) in primary striatal neurons; the negative control undertaken by omitting one of the primary antibodies is shown in Supplementary Figure S1. Experiments were performed in samples from 5 animals. The number of red dots/cell was quantified using the Andy’s algorithm Fiji’s plug-in and represented over cell stained nuclei with Hoechst (blue) (D). The number of dots-clusters/cell were compared to those in neurons from control mice (mice fed with standard diet). Unpaired t-test was used for statistics analysis. *** p < 0.001, versus control. Scale bar: 20 μm.
Figure 5. Expression and function of CB2R-GHSR1aHets in primary neurons isolated from fetuses of pregnant C57BL/6J female mice subjected to a high-fat diet. (A,B) Primary striatal neurons isolated from fetuses of pregnant females mice subjected to a high-fat diet for 60 days were pre-treated with antagonists, 1 μM YIL 781 -for GHSR1a- or 1 μM AM 630 -for CB2R-, followed by stimulation with selective agonists, 200 nM ghrelin -for GHSR1a- or 200 nM JWH-133 -for CB2R-, individually or in combination. cAMP levels were determined using the Lance Ultra cAMP kit and results were expressed in % versus 0.5 µM forskolin treatment (A) while ERK1/2 phosphorylation was analyzed using the AlphaScreen® SureFire® kit (PerkinElmer) (B). Values are the mean ± SEM of 5 different experiments performed in triplicates. One-way ANOVA followed by Dunnett’s multiple comparison post-hoc test were used for statistical analysis. # p < 0.05, ## p < 0.005 versus JWH-133+FK treatment in cAMP or versus JWH-133 treatment in p-ERK1/2 assays. * p < 0.05, basal. (C). CB2R-GHSR1aHets were detected by the in situ proximity ligation assay (PLA) in primary striatal neurons; the negative control undertaken by omitting one of the primary antibodies is shown in Supplementary Figure S1. Experiments were performed in samples from 5 animals. The number of red dots/cell was quantified using the Andy’s algorithm Fiji’s plug-in and represented over cell stained nuclei with Hoechst (blue) (D). The number of dots-clusters/cell were compared to those in neurons from control mice (mice fed with standard diet). Unpaired t-test was used for statistics analysis. *** p < 0.001, versus control. Scale bar: 20 μm.
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Lillo, J.; Lillo, A.; Zafra, D.A.; Miralpeix, C.; Rivas-Santisteban, R.; Casals, N.; Navarro, G.; Franco, R. Identification of the Ghrelin and Cannabinoid CB2 Receptor Heteromer Functionality and Marked Upregulation in Striatal Neurons from Offspring of Mice under a High-Fat Diet. Int. J. Mol. Sci. 2021, 22, 8928. https://0-doi-org.brum.beds.ac.uk/10.3390/ijms22168928

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Lillo J, Lillo A, Zafra DA, Miralpeix C, Rivas-Santisteban R, Casals N, Navarro G, Franco R. Identification of the Ghrelin and Cannabinoid CB2 Receptor Heteromer Functionality and Marked Upregulation in Striatal Neurons from Offspring of Mice under a High-Fat Diet. International Journal of Molecular Sciences. 2021; 22(16):8928. https://0-doi-org.brum.beds.ac.uk/10.3390/ijms22168928

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Lillo, Jaume, Alejandro Lillo, David A. Zafra, Cristina Miralpeix, Rafael Rivas-Santisteban, Núria Casals, Gemma Navarro, and Rafael Franco. 2021. "Identification of the Ghrelin and Cannabinoid CB2 Receptor Heteromer Functionality and Marked Upregulation in Striatal Neurons from Offspring of Mice under a High-Fat Diet" International Journal of Molecular Sciences 22, no. 16: 8928. https://0-doi-org.brum.beds.ac.uk/10.3390/ijms22168928

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