Transcriptional Mapping of the Human Cannabinoid Receptor 1 (CNR1) Gene Promoter

Article type: Research Article

Keywords: CNR1, cannabinoid receptor 1, cAMP, transcriptional regulation, promoter

Authors: Alonso Cortez-Resendiz, Shivani S. Godbole, Nurgul Carkaci-Salli, Kent E. Vrana ⚬, Wesley M. Raup-Konsavage ⚬

Affiliations: Department of Neuroscience and Experimental Therapeutics, Penn State College of Medicine, Penn State University, Hershey, PA 17033, USA; Center for Cannabis and Natural Product Pharmaceutics (CCNPP), Penn State College of Medicine, Penn State University, Hershey, PA 17033, USA; Department of Molecular and Precision Medicine, Penn State College of Medicine, Penn State University, Hershey, PA 17033, USA

License: © 2026 by the authors. CC BY 4.0 Licensee MDPI, Basel, Switzerland. This article is an open access article distributed under the terms and conditions of the Creative Commons Attribution (CC BY) license.

Article links: DOI: 10.3390/molecules31132387  |  PMC: PMC13363282

Relevance: Moderate: mentioned 3+ times in text

Full text: PDF (2.6 MB)

1. Introduction

The cannabinoid type 1 receptor (CB1R) is a G_i/G_o-coupled receptor activated by endocannabinoids (N-arachidonoylethanolamine [AEA] and 2-arachidonoylglycerol [2-AG]), phytocannabinoids (Δ⁹-tetrahydrocannabinol [(Δ⁹-THC]) as well as synthetic cannabinoids (WIN55212 and CP55940) and is primarily expressed in the central nervous system (CNS) [ref. 1,ref. 2,ref. 3,ref. 4,ref. 5,ref. 6]. Specifically, CB1R is highly expressed in the limbic system, cerebral cortex, and cerebellum [ref. 1,ref. 2,ref. 3,ref. 4,ref. 5,ref. 6]. The human cannabinoid type 1 receptor gene (CNR1) is located on chromosome 6q14-15, (the 91.8~96.1 cM locus) and lies within 15 cM of the D6S474 and D6S424 markers linked to schizophrenia [ref. 1,ref. 5,ref. 7]. The structure and transcriptional regulation of the CNR1 gene, including its promoter, are currently not well understood and have received limited attention [ref. 1,ref. 2,ref. 3,ref. 4,ref. 5,ref. 7].

To date, research has focused on the activation/inhibition of the CB1R along with the upregulation/downregulation of this receptor in different human cell types, and disorders such as Alzheimer’s disease and schizophrenia. The overuse of cannabis can lead to the development of tolerance, which has been associated with decreased CB1R on the plasma membrane, that may ultimately lead to cannabis use disorder (CUD). Nevertheless, only a few publications have examined the transcriptional regulation of the CNR1 gene promoter (located in the 5′ flanking region of the CNR1 gene) responsible for the transcription of the CB1R protein [ref. 1,ref. 8]. While searching for the cause of these disorders and the regulation of the CNR1 gene, investigators have examined changes in the CNR1 promoter region, including an (AAT)_n triplet repeat in the promoter region of the CNR1 gene thought to be associated with the pathogenesis of schizophrenic disorders [ref. 7]. Studies involving luciferase reporter gene assays have shown transcriptional regulation in the CNR1 gene [ref. 1,ref. 8]. First, the 1.0 kb 5′ flanking sequence of CNR1 gene exon 1 showed significant promoter/enhancer-like activities [ref. 1]. Second, a single nucleotide polymorphism (SNP) found within the 3.0 kb immediately 5′ from the CNR1 coding exon 3 showed reduced reporter gene expression when compared to the wild type [ref. 8]. More recently, the rs2180619 polymorphism (located about 3.0 kb from CNR1 gene exon 1) and its related genotypes have been associated with attention deficits and reduction in working memory, behaviors like addiction and anxiety, as well as lowered levels of CB1R expression [ref. 1,ref. 9,ref. 10,ref. 11]. Finally, other studies have examined the role of transcriptional factors in the regulation of CB1R [ref. 4,ref. 12]. These findings clearly emphasize the need to explore the transcriptional regulation and structural composition of the CNR1 gene and consequently the expression of the CB1R. An understanding of how the CNR1 gene is regulated will contribute insights into human diseases and conditions.

To map the promoter regions of the human CNR1 gene, a 997-bp fragment from the sequence upstream of the CNR1 gene (similar to the 1.0 kb sequence theorized to contain the core promoter region in Zhang et al. [ref. 1]) was cloned into a secreted luciferase reporter construct (pNL2.3). A series of deletion fragments were constructed, and their activity was assessed in three different human cell lines. Through this mapping, we identified two key regions of transcriptional regulation. Additional data indicate that increases in cAMP levels can suppress CNR1 gene expression in a cell-type specific manner. We report that the core promoter is located within the first 100 bp upstream of the CNR1 gene sequence and predict several transcription factors that play a role in its regulation and implication in disease.

2. Results

2.1. Luciferase Activity of Full-Length CNR1 Promoter and Promoter Deletions

A 997-bp fragment immediately upstream of the reported CNR1 transcription start site (TSS) (Full-Length, FL) and its deletion fragments (illustrated in Figure 1 and Figure S1) were cloned into a pNL2.3 luciferase reporter construct and transiently transfected into HEK293T (Figure 2A), HCT116 (Figure 2B) and SHSY5Y (Figure 2C) cells [ref. 1]. As noted in the Discussion section, these are commonly used human cell lines from tissues known to express the CB1R and where the receptor is thought to contribute to organ physiology and/or pathology. Deletion mapping of the promoter region revealed two major regulatory regions within the promoter, as assessed by a decrease in luciferase activity (Figure 2). The first major decrease occurred following the deletion of the first 600 bp, resulting in about a 50% reduction in luciferase activity across all three cell lines. Deletion of the region between Δ900 and Δ950 promoter fragments completely abolished luciferase activity (reducing it to empty vector levels). These data suggest that a key regulatory region is between the Δ400 and Δ600 fragments, and the core promoter sequences are between Δ900 and Δ950 fragments (within 100 bp of the reported transcription start site) [ref. 1].

2.2. Luciferase Activity of Full-Length CNR1 Promoter After Forskolin (FSK) Treatment

We next examined the possible regulation of transcription by GPCRs, (such as the G_i/G_o-coupled CB1R). To test this, we used forskolin (FSK) which activates adenylyl cyclase and increases cyclic AMP (cAMP) levels, a major downstream pathway component of GPCR activation. Increased cAMP levels within a cell ultimately activate CREB/CREM transcription factors. Cells transfected with the full-length CNR1 promoter construct were treated with 5 μM FSK for 24 h (Figure 3). After FSK treatment, the luciferase reporter activity in HEK293T (Figure 3A) and HCT116 cells (Figure 3B) was significantly decreased. However, this decrease in reporter activity was less pronounced and not significant in SHSY5Y (Figure 3C). These results demonstrate a slight cell-type specific response to FSK and cAMP levels on transcriptional activation/inhibition of the CNR1 promoter.

2.3. Luciferase Activity of Promoter Deletions After Forskolin (FSK) Treatment

Because of the observed cAMP-induced decreases in luciferase activity with the full-length construct, suggesting the presence of cAMP-responsive elements (CRE) within the promoter, we next mapped the location of potential elements using the promoter fragment constructs (Figure 4). Treatment of transfected HEK293T (Figure 4A) and HCT116 (Figure 4B) showed a decrease in promoter activity with the three largest constructs, but the effect of forskolin on luciferase activity was greatly reduced following deletion of the first 600 bp (Δ600 fragments and larger deletions). Interestingly, we also observed a smaller, but still significant decrease in cAMP responsiveness in SHSY5Y cells for these three larger promoter fragments (Figure 4C). These results should be considered with reservations as the transient transfection in SHSY5Y cells was less effective, and luciferase assay results showed a greater degree of variability. Furthermore, while the cAMP-induced reduction was less, we observed a continued impact of FSK treatment across the smaller promoter fragments in HCT116 cells. In sum, these data suggest the presence of a potential CRE within the major regulatory region—the 200 bp between the Δ400–Δ600 fragments—of the CNR1 promoter. This suggests that this element(s) may be responsible for the decrease in expression observed in the deletion series described in Figure 2.

2.4. CREB/CREM Expression in HEK293T, HCT116, and SHSY5Y Cells

Because of observed cAMP-induced responses to, and potential differences in cell lines to forskolin (FSK) treatment(Figure 3 and Figure 4), we examined the expression levels of CREB and CREM mRNA in each of these cell lines. We tested CREM (Figure 5A), CREB1 (Figure 5B), ATF4 (formerly CREB2; Figure 5C), CREB3 (Figure 5D), and CREB5 (Figure 5E) in all three cell lines. Expression of ATF4 (Figure 5C) was the highest for each of the three cell lines, while expression of CREM (Figure 5A) was the lowest in each cell line. Regardless, we did not observe any significant differences in CREB or CREM gene expression that could account for these differences; however, CREM and CREB5 expression are notably low in HCT116 cells.

2.5. CNR1 Gene Endogenous-Expression Regulation After Forskolin (FSK) Treatment

We next tested the effect of forskolin (FSK) treatment on the endogenous expression of the CNR1 gene. In contrast to what we observed with FSK treatment of the luciferase constructs, we found FSK treatment had no significant impact on the endogenous expression of the CNR1 gene in HEK293T (Figure 6A), HCT116 (Figure 6B) and SHSY5Y (Figure 6C) cell lines. Not surprisingly, this observation suggests that additional regulatory elements, outside of the 997-bp promoter region, regulate CNR1 expression.

2.6. In Silico Identification of Promoter Elements

Two software packages for predicting transcription-factor binding profiles of CREB/CREM elements were utilized to identify potential regulatory elements within the key regulatory region between Δ400–Δ600 (−600 bp and −400 bp) of our luciferase promoter constructs (Figure 4). JASPAR predicted multiple binding sequences, while PROMO only predicted one area of binding; additionally, another potential CRE site was visually identified upon analysis of the sequence (Figure 7A). Of particular interest is a CRE site predicted by both PROMO and JASPAR located close to the start of the Δ400 fragment (located about −600 bp from the transcription start site), which is the last fragment to maintain a large luciferase promoter activity.

The online software package YAPP was used to identify potential core promoter elements found between the Δ900 and Δ950 fragments, which represented deletion of the core promoter region (Figure 2). This analysis predicted two overlapping BRE elements and an INR element within this region that may represent the core promoter elements of CNR1 (Figure 7B).

2.7. Transcriptional Activity of BRE and Inr Mutations Within Full-Length CNR1 Promoter

After identifying two different types of predicted promoter elements within the last ~100bp of the reported transcription start site (TSS), the proximal BRE and Inr were mutated within the full-length (FL) CNR1 promoter sequence, as previously reported [ref. 13,ref. 14,ref. 15,ref. 16,ref. 17,ref. 18,ref. 19,ref. 20]. Specifically, the proposed BRE sequence of CGGCGCC was modified to CAGGACC and the proposed Inr sequence of CTACTCC was converted to CTTCGCC. Luciferase reporter assays were performed with all three cell lines to quantify the transcriptional activity of the FL containing each mutation (Figure 8). In HEK293T and SHSY5Y cells, the mutation of either BRE or Inr did not produce any significant changes in transcriptional activity when compared to unmutated FL CNR1 promoter. However, in HCT116 cells, a two-fold increase in activity of the BRE mutated construct was observed when compared to unmutated CNR1 promoter. Meanwhile, the Inr-mutated FL only showed a minimal reduction in activity without statistical significance.

3. Discussion

In this study, we mapped potential regulatory regions within the CNR1 promoter. Our findings indicate that two major regulatory regions exist: one distal between Δ400 and Δ600 (−600 bp and −400 bp relative to the reported transcription start site), and a second more proximal region between Δ900 and Δ950 (−100 bp and −50 bp relative to the reported transcription start site) [ref. 1]. The deletion of the region between Δ400 and Δ600 reduced luciferase expression in all three cell lines by about 50%, while the deletion of the region between Δ900 and Δ950 abolished all remaining luciferase expression. These findings suggest that an active basal promoter region for CNR1 lies within these 50 base pairs, and the 200 base pairs between Δ400 and Δ600 contain a major transcriptional regulatory region.

To evaluate the functional relevance of these regulatory regions across biologically distinct cellular contexts, promoter activity was examined in three commonly used human cell lines representing tissues in which CB1 receptor signaling is known to play important physiological or pathological roles [ref. 13,ref. 14,ref. 15,ref. 16,ref. 17,ref. 18,ref. 19]. HEK293T cells were selected as a broadly utilized human cell line that serves as a standard platform for molecular and transcriptional studies and is frequently used in cannabinoid receptor binding assays, generally over-expressing the receptor of interest [ref. 20,ref. 21,ref. 22]. Furthermore, CNR1 has been found to play a role in kidney disease, renal fibrosis and diabetic nephropathy. HCT116 colorectal cancer cells were included because alterations in CB1 receptor expression and endocannabinoid signaling have been reported in both inflammatory bowel disease (IBD) and colorectal cancer, suggesting a role for CNR1 regulation in gastrointestinal health and disease. Previously, we confirmed the expression of CNR1 mRNA in both HEK293T and HCT116 cells [ref. 23]. SH-SY5Y neuroblastoma cells were selected as a neuronal model because CB1 is the most abundant GPCR in the brain and is widely expressed on neurons. CB1R has also been found to have protective roles in neurodegenerative disorders, and decreased CNR1 mRNA is a known feature of Huntington’s disease [ref. 24,ref. 25].

To begin to identify pathways that may contribute to regulation of the CNR1 promoter, the impact of cAMP levels on transcription was tested. We found that HEK293T and HCT116 cell treatment with FSK produced a significant reduction in luciferase expression of the full-length construct; however, this effect was more modest in SHSY5Y cells, suggesting differential regulation by cAMP response element (CRE) transcription factors between the cell lines. Treatment of the deletion fragments with FSK decreased luciferase expression by varying degrees; of note, the FSK-mediated decrease was absent in constructs that deleted the first 600 bp, with some exceptions in HCT116 cells. This suggests that a regulatory CRE element resides within the 200 bp separating the Δ400 and Δ600 constructs (the region between −600 bp and −400 bp relative to the transcription start site). Consistent with this hypothesis, in silico analysis identified potential cAMP responsive elements (CRE) within the 200-bp region between Δ400–Δ600. To account for the cell-type differences in cAMP responsiveness, we examined the expression levels of CREB/CREM transcription factors across the three cell lines; however, no notable differences in CREB/CREM transcription factor expression were observed. This further suggests that other elements were mediating part of the reduced promoter activity with FSK treatment. Furthermore, endogenous expression of CNR1 was not impacted by FSK treatment. This discrepancy between the promoter-reporter assays and the endogenous gene expression raises the possibility that additional regulatory elements outside the cloned promoter region or chromatin-dependent mechanisms not captured by the reporter constructs may contribute to the regulation of endogenous CNR1 transcription.

Beyond the putative CRE, in silico mapping identified potential BRE and Inr promoter elements between Δ900 and Δ950 and within Δ950, respectively, that may account for the changes in expression we observed. The BRE (B recognition element) and Inr (initiator element) interact with transcription factor II B (TFIIB) and RNA polymerase II (PolII), respectively, and collaborate in direct transcription initiation [ref. 26,ref. 27,ref. 28]; while still consistent with a minimal promoter being present in this small region, this demonstrates that the suggested BRE and Inr may not play a key role in regulating transcription. Additionally, other elements may be present in the larger constructs that can drive transcription, and the identified BRE and INR may only be active in the smaller promoter fragment constructs. Further studies to refine the map of the CNR1 promoter, including the impact of mutations of the BRE and INR in a smaller construct, will provide additional, important insight into the regulation of CNR1.

Most of the information regarding CNR1 gene regulation comes from genomic variation, transcription-factor binding, and associated single-nucleotide polymorphisms (SNPs) [ref. 1,ref. 4,ref. 8,ref. 9,ref. 10,ref. 12]. Zhang et al. investigated promoter/enhancer activity in sequences that extended 1.0, 2.0 and 3.0 kb 5′ from the human CNR1 gene exon 1 transcription start site (TSS) [ref. 1]. This group reported higher luciferase expression from the 1.0 kb sequence, compared to the 2.0 and 3.0 kb fragments, suggesting distal inhibitory elements. Beyond the promoter region, the expression of genes can be influenced by enhancer/repressor sequences, the expression of transcriptional factors or co-factors, and/or by mutations in the DNA sequence (i.e., SNPs) [ref. 4,ref. 8,ref. 9,ref. 10,ref. 12]. Studies have identified potential crosstalk, co-expression, and co-localization of the CB1R with other receptors [ref. 2,ref. 3,ref. 29]. One study found that the testosterone-androgen receptor (AR) complex, known to function as a transcription factor, enhances the transcription of CNR1 in SHSY-5Y cells transfected with AR and rCNR1 [ref. 2,ref. 29]. The increase in expression of the rCNR1 was due to two potential AR binding sites in the 1.5 kb rat CNR1 promoter region. The location of these AR binding sites, within the first 500 and 900 bp upstream of the rCNR1 TSS, coincides with the promoter region investigated in our study and may exert similar influences in the transcriptional regulation of the human CNR1 gene. This is worth further study because AR has been reported to be a target for some phytocannabinoids and could suggest that phytocannabinoids’ inhibition of AR may impact CNR1 expression [ref. 30,ref. 31].

A less considered factor that can lead to the transcriptional regulation of genes, including the CNR1 gene, and can contribute to the development of other disorders is the occurrence of SNPs [ref. 1,ref. 8,ref. 9,ref. 10]. The SNP-related downregulation of rs806371, located 5′ from the coding CNR1 exon 3, was studied as a variant associated with lower levels of high-density lipoprotein (HDL) cholesterol in humans [ref. 8]. Feng et al. concluded that this SNP acted as a novel regulatory binding element reducing the level of CNR1 expression [ref. 8]. At the same time, rs2180619, along with related genotypes (GG), located 2.0 kb upstream of our promoter sequence, was shown to lower the efficiency of the endocannabinoid system due to lowered CNR1 expression, producing a reduction in attention control and working memory as well as the increased risk of addiction and anxiety [ref. 1,ref. 9,ref. 11]. Lowered expression of CNR1 is not the only way in which SNPs can lead to disorders. The rs1049353, identified in individuals with anorexia nervosa (AN), bulimia nervosa (BN), obesity, type 2 diabetes mellitus and major depression, is silent and does not alter the amino acid sequence, but it is thought to alter the mRNA stability [ref. 5,ref. 32,ref. 33,ref. 34].

Altered CB1R expression has been associated with numerous diseases and conditions. Increased CB1R expression has been reported in neuropathic pain, certain cancers (notably prostate cancer), cirrhosis, fatty liver disease, and depression [ref. 4,ref. 15,ref. 25,ref. 34,ref. 35,ref. 36,ref. 37,ref. 38,ref. 39,ref. 40,ref. 41,ref. 42,ref. 43,ref. 44]. Expression has been found to be decreased in Huntington’s disease, breast cancer, inflammatory bowel disease (IBD) and cannabis use disorder (CUD) [ref. 16,ref. 24,ref. 45,ref. 46,ref. 47,ref. 48,ref. 49]. In animal models of neuropathic pain, CB1R upregulation may reduce neurotransmitter release while enhancing responsiveness to exogenous cannabinoids such as THC [ref. 35,ref. 36,ref. 37]. Similarly, elevated CB1R expression in high-fat-diet-fed mice can be reversed by CB1R antagonists such as rimonabant [ref. 35,ref. 44]. In colorectal cancer there are conflicting data; loss of CB1R expression has been attributed to methylation of the CNR1 promoter, whereas other studies have found higher levels of CB1R expression in patients with a poorer prognosis [ref. 15,ref. 50,ref. 51]. These observations highlight the importance of understanding the mechanisms regulating CNR1 transcription. Changes in CB1 expression may also result from receptor internalization and degradation, processes implicated in cannabis tolerance [ref. 52,ref. 53]. Cannabis dependence and tolerance are associated with CB1R downregulation that correlates with the duration of chronic cannabis use and is largely reversible following prolonged abstinence [ref. 45,ref. 46]. Notably, reduced CNR1 mRNA expression is an early marker of Huntington’s disease [ref. 41].

Cannabis is widely used to manage symptoms associated with pain, depression, anxiety, and IBD, with many patients reporting therapeutic benefit [ref. 52,ref. 53,ref. 54]. At the same time, increasing use of high-THC cannabis products has raised concerns regarding adverse outcomes, including tolerance, CUD, cannabis-induced persistent psychosis, and cannabis-induced hyperemesis [ref. 55,ref. 56] A better understanding of the regulatory regions that modulate CNR1 transcription may provide novel insights into the mechanisms contributing to these conditions and side effects.

The focus of the current study was to map regulatory regions within the promoter region of CNR1; however, a key limitation of this study is that it does not address other enhancer and insulator DNA elements. Two regulatory regions were identified; the first region showed a cAMP response element (CRE) and, after in silico analysis, the second region showed two overlapping BRE promoter elements and an Inr promoter element. Our data on the impact of FSK on endogenous CNR1 expression, and other studies linking CNR1 expression to cAMP levels, clearly indicate that these factors will be involved in regulating CNR1 expression [ref. 3,ref. 57,ref. 58,ref. 59]. Mutation of the proximal BRE or Inr did not display core promoter functionality and, in the case of HCT116, it showed the opposite effect by resulting in a two-fold increase in expression only in the BRE-mutated FL promoter. Mapping of these additional elements will be key to better understanding how CNR1 is potentially regulated and will provide additional insights into the observed cell-type-dependent differences observed here. Nonetheless, our results bring light to a new area in the transcriptional regulation of the CNR1 expression, focusing on transcription factors and the activation of other GPCRs.

In conclusion, our results provide evidence for the presence of multiple regulatory elements within the 1000-bp sequence upstream of the CNR1 transcriptional start site. Deletion analysis identified a proximal region located within the first 100 bp upstream of the transcriptional start site (between the comprised Δ900 and Δ950 fragments) that appears to be important for basal promoter activity and contains putative INR and BRE elements identified through in silico analyses. In addition, upstream we identified a potential regulatory region located between Δ400 and Δ600 that contains a putative cAMP response element (CRE). While the promoter-reporter studies are consistent with a role for this region in cAMP-responsive transcription, the absence of changes in the endogenous CNR1 mRNA following forskolin treatment suggests that regulation of the endogenous gene is more complex and may involve additional regulatory elements, chromatin-dependent mechanisms, or distal enhancer regions not present in the construct tested in this study.

Taken together, these results expand the current understanding of the CNR1 promoter architecture and identify candidate regulatory regions that warrant further investigation. However, because the conclusions are based primarily on transient reporter assays and in silico predictions, additional studies will be required to confirm the functionality of the proposed regulatory elements and to define their contribution to endogenous CNR1 expression in physiologically relevant cellular contexts. Notably, the function of the INR and BRE may be more relevant to the smaller fragments than the full-length construct, and this warrants further evaluation. Additional promoter elements may lie upstream in the larger constructs, and these should be analyzed in greater detail as well. As such, this work provides a framework for future studies aimed at more comprehensively characterizing the transcriptional regulation of CNR1 and ultimately CB1 receptor expression.

4. Materials and Methods

4.1. DNA Cloning and Preparation of CNR1 Gene-Promoter Deletion Fragments

Genomic DNA was extracted from the human colorectal adenocarcinoma cell line, DLD-1, using the QIAmp DNA Mini Kit (Qiagen, Germantown, MD, USA) following the manufacturer’s protocol. A 997-bp region of CNR1 5′ flanking region was amplified utilizing HotStarTaq^® DNA Polymerase (Qiagen, Germantown, MD, USA) between 88165981 and 88166977 on chromosome 6 (Figure 1). The identity of the amplified fragment was confirmed by DNA sequencing (Figure 1A). The amplified genomic DNA of 997 base pairs were cloned into the pNL2.3 [secNluc Hygro] vector (Promega, Madison, WI, USA) using KpnI and BglII restriction enzymes (Thermo Fisher Scientific, Waltham, MA, USA) to create a secreted luciferase reporter gene construct. The reporter plasmid was purified from transformed E. coli using the QIAprep Spin Miniprep Kit (Qiagen, Germantown, MD, USA). A series of 5′ deletions of 200 bp (Δ200), 400 bp (Δ400), 600 bp (Δ600), 800 bp (Δ800), 850 bp (Δ850), 900 bp (Δ900) and 950 bp (Δ950) were generated using QuickChange Lightning Site-Directed Mutagenesis Kits (Agilent, Santa Clara, CA, USA). The primers utilized for the amplification, cloning, deletion, and sequencing of DNA are provided in Supplemental Table S1.

4.2. Cell Culture and Transient Transfection

The human embryonic kidney cell line, HEK293T, the human colon cancer cell line, HCT116, and the human neuroblastoma cell line, SHSY5Y, were cultured in DMEM (Corning, Manassas, VA, USA) supplemented with 10% fetal bovine serum (FBS) (Cytiva, Logan, UT, USA, and GeminiBio, Sacramento, CA, USA), and 1% Antibiotic-Antimycotic (Anti-Anti) (Gibco, Grand Island, NY, USA). Cells were seeded at a concentration of 100,000 cells per well in 24-well culture plates. Cells were incubated overnight for 12 to 16 h and then transfected with recombinant plasmids and Lipofectamine 2000 Reagent (Invitrogen, Carlsbad, CA, USA) following the manufacturer’s recommendations. Following 4–6 h of incubation, medium was replaced with DMEM (with 10% FBS and 1% Anti-Anti) and cultured for 24 h. Cells were treated with forskolin (Sigma-Aldrich, Saint Louis, MO, USA) where indicated (at 5 μM) and cultured for 24 h before performing the luciferase assay on culture medium.

4.3. Luciferase Reporter Assay

After transfection, cells were incubated for 24 h with or without forskolin treatment. The culture medium was collected and centrifuged at 9500× g for 5 min at 4 °C. For HEK293T cells, 10μL of cleared supernatant was added per well into a 96-well Lumitrac microplate (Greiner Bio-One, Frickenhausen, Germany). For HCT116 and SHSY5Y cells, 20μL of cleared supernatant were added per well. Full-length promoter and deletion fragment reporter activity were measured using a SpectraMax i3 imaging cytometer (Molecular Devises, San Jose, CA, USA) and the Nano-Glo^® Luciferase Assay System (Promega, Madison, WI, USA) according to the manufacturer’s instructions. Each reaction was carried out in duplicate, and the results of these technical replicates were averaged. Experiments were conducted independently, with multiple replicates. Luciferase reporter activity assay results were calculated as z-scores by dividing the average of duplicate reactions by the average luminescence for each well in the plate (luciferase assay run).

4.4. qRT-PCR for Gene Expression

Cells utilized for the expression of cAMP response element (CRE)-related transcription factors were cultured without treatment. Cells utilized for cannabinoid receptor type 1 (CNR1) gene expression were treated with FSK as described above. In both cases, RNA was isolated using a RNeasy^® Mini Kit (Qiagen, Hilden, Germany). cDNA was synthesized utilizing a High-Capacity cDNA Reverse Transcription Kit with RNase inhibitor (AppliedBiosystems, Vilnius, Lithuania) with 1 µg of isolated RNA. cDNA was diluted to 1:50 (transcription factors) and 1:5 (CNR1) for RT-PCR using a TaqMan^® Fast Advanced Master Mix (AppliedBiosystems, Vilnius, Lithuania) utilizing Human TaqMan probes for CREM (Assay ID: Hs01582003_g1), CREB1 (Assay ID: Hs00231713_m1), ATF4 (Assay ID: Hs00909569_g1), CREB3 (Assay ID: Hs00197255_m1), CREB5 (Assay ID: Hs00191719_m1), CNR1 (Assay ID: Hs01038522_s1), Actin (Assay ID: Hs99999903_m1), and GAPDH (Assay ID: Hs02786624_g1) (AppliedBiosystems, ThermoFisher, Waltham, MA, USA). The resulting C_T values were analyzed to calculate the expression of CRE-related transcription factors and CNR1 relative to GAPDH or β-actin (2^−ΔCt) in each of the cell lines.

4.5. In Silico Promoter Analysis

The online software packages JASPR (https://jaspar.elixir.no/, version 11, accessed on 2 February 2025) and PROMO (https://bioinformaticaupf.crg.eu/2003/projectes03/2.2/promotor/ALGGEN%20-%20Algorismica%20i%20Genetica.Promotors.html, accessed on 2 February 2025) were used to search the DNA sequence of the region between the Δ400 and Δ600 bp fragments for human cAMP response elements. Core promoter elements were searched within the full 997-bp promoter fragment studied using YAPP (https://bioinformaticshome.com/db/tool/YAPP) accessed on 2 February 2025).

4.6. BRE and Inr Mutations and Luciferase Reporter Assay

Mutations of the predicted proximal BRE and Inr were generated using Q5 Site-Directed Mutagenesis Kit (New England BioLabs, Ipbswich, MA, USA) and the plasmids were isolated from transformed E. coli as previously described. The primers utilized for the amplification, cloning and sequencing of DNA are provided in Supplemental Table S2. Luciferase reporter assays were performed independently, with multiple replicates, as previously described.

4.7. Statistical Analysis

Statistical analysis was conducted using Prism Software (GraphPad, Boston, MA, USA, version 10.4.1). Ordinary one-way and two-way ANOVA with Dunnett’s/Tukey’s and Šidák’s multiple comparison test was used to evaluate luciferase data. Levels of endogenous CNR1 were compared using one-way ANOVA with Tukey’s multiple comparison test. All data are presented as mean ± standard deviation.

5. Conclusions

In conclusion, our results show the existence of two regulatory regions in the 1000-bp sequence upstream of the CNR1 gene transcription start site. The core promoter is located within the first 100 bp comprising Δ900 and Δ950 (between −100 bp and −5 bp upstream of the TSS), and an upstream regulatory region is located between Δ400 and Δ600 (−600 bp and −400 bp upstream of the TSS) that contains a cAMP response element (CRE). These results add to the current knowledge of the regulation of CNR1/CB1R expression and provide insights into key regulatory regions of the promoter.

References

1. P.W. Zhang, H. Ishiguro, T. Ohtsuki, J. Hess, F. Carillo, D. Walther, E.S. Onaivi, T. Arinami, G.R. Uhl. Human cannabinoid receptor 1: 5′ exons, candidate regulatory regions, polymorphisms, haplotypes and association with polysubstance abuse. Mol. Psychiatry, 2004. [DOI | PubMed]
2. K.S. Lee, J. Asgar, Y. Zhang, M.K. Chung, J.Y. Ro. The role of androgen receptor in transcriptional modulation of cannabinoid receptor type 1 gene in rat trigeminal ganglia. Neuroscience, 2013. [DOI | PubMed]
3. Y.C. Chiang, Y.N. Lo, J.C. Chen. Crosstalk between dopamine D2 receptors and cannabinoid CB1 receptors regulates CNR1 promoter activity via ERK1/2 signaling. J. Neurochem., 2013. [DOI | PubMed]
4. B. Mukhopadhyay, J. Liu, D. Osei-Hyiaman, G. Godlewski, P. Mukhopadhyay, L. Wang, W.I. Jeong, B. Gao, G. Duester, K. Mackie. Transcriptional regulation of cannabinoid receptor-1 expression in the liver by retinoic acid acting via retinoic acid receptor-gamma. J. Biol. Chem., 2010. [DOI | PubMed]
5. M. Pucci, E. Zaplatic, M.V. Micioni Di Bonaventura, E. Micioni Di Bonaventura, P. De Cristofaro, M. Maccarrone, C. Cifani, C. D’Addario. On the Role of Central Type-1 Cannabinoid Receptor Gene Regulation in Food Intake and Eating Behaviors. Int. J. Mol. Sci., 2021. [DOI | PubMed]
6. S. Hryhorowicz, M. Kaczmarek-Ryś, A. Andrzejewska, K. Staszak, M. Hryhorowicz, A. Korcz, R. Słomski. Allosteric Modulation of Cannabinoid Receptor 1-Current Challenges and Future Opportunities. Int. J. Mol. Sci., 2019. [DOI | PubMed]
7. S.J. Tsai, Y.C. Wang, C.J. Hong. Association study of a cannabinoid receptor gene (CNR1) polymorphism and schizophrenia. Psychiatr. Genet., 2000. [DOI | PubMed]
8. Q. Feng, K.C. Vickers, M.P. Anderson, M.G. Levin, W. Chen, D.G. Harrison, R.A. Wilke. A common functional promoter variant links CNR1 gene expression to HDL cholesterol level. Nat. Commun., 2013. [DOI | PubMed]
9. A.E. Ruiz-Contreras, K. Carrillo-Sánchez, I. Ortega-Mora, M.A. Barrera-Tlapa, T.V. Román-López, C.B. Rosas-Escobar, L. Flores-Barrera, U. Caballero-Sánchez, Z. Muñoz-Torres, S. Romero-Hidalgo. Performance in working memory and attentional control is associated with the rs2180619 SNP in the CNR1 gene. Genes Brain Behav., 2014. [DOI | PubMed]
10. B. Fairfield, N. Mammarella, M. Franzago, A. Di Domenico, L. Stuppia, V. Gatta. A variant on promoter of the cannabinoid receptor 1 gene (CNR1) moderates the effect of valence on working memory. Memory, 2018. [DOI | PubMed]
11. J. Lazary, A. Lazary, X. Gonda, A. Benko, E. Molnar, L. Hunyady, G. Juhasz, G. Bagdy. Promoter variants of the cannabinoid receptor 1 gene (CNR1) in interaction with 5-HTTLPR affect the anxious phenotype. Am. J. Med. Genet. B Neuropsychiatr. Genet., 2009. [DOI | PubMed]
12. A. Subedi, A. Etemad, A. Tiwari, Y. Huang, B. Chatterjee, S.M. McLeod, Y. Lu, D. Gonzalez, K. Ghosh, M. Sirito. Nerve injury inhibits Oprd1 and Cnr1 transcription through REST in primary sensory neurons. Sci. Rep., 2024. [DOI | PubMed]
13. B. Malla, X. Guo, G. Senger, Z. Chasapopoulou, F. Yildirim. A Systematic Review of Transcriptional Dysregulation in Huntington’s Disease Studied by RNA Sequencing. Front. Genet., 2021. [DOI | PubMed]
14. E. Kloster, C. Saft, J.T. Epplen, L. Arning. CNR1 variation is associated with the age at onset in Huntington disease. Eur. J. Med. Genet., 2013. [DOI | PubMed]
15. D. Wang, H. Wang, W. Ning, M.G. Backlund, S.K. Dey, R.N. DuBois. Loss of cannabinoid receptor 1 accelerates intestinal tumor growth. Cancer Res., 2008. [DOI | PubMed]
16. M. Grill, C. Högenauer, A. Blesl, J. Haybaeck, N. Golob-Schwarzl, N. Ferreirós, D. Thomas, R. Gurke, M. Trötzmüller, H.C. Köfeler. Members of the endocannabinoid system are distinctly regulated in inflammatory bowel disease and colorectal cancer. Sci. Rep., 2019. [DOI | PubMed]
17. L. Cohen, M.G. Neuman. Cannabis and the Gastrointestinal Tract. J. Pharm. Pharm. Sci., 2020. [DOI | PubMed]
18. T. Jourdan, J.K. Park, Z.V. Varga, J. Pálóczi, N.J. Coffey, A.Z. Rosenberg, G. Godlewski, R. Cinar, K. Mackie, P. Pacher. Cannabinoid-1 receptor deletion in podocytes mitigates both glomerular and tubular dysfunction in a mouse model of diabetic nephropathy. Diabetes Obes. Metab., 2018. [DOI | PubMed]
19. L. Lecru, C. Desterke, S. Grassin-Delyle, C. Chatziantoniou, S. Vandermeersch, A. Devocelle, A. Vernochet, N. Ivanovski, C. Ledent, S. Ferlicot. Cannabinoid receptor 1 is a major mediator of renal fibrosis. Kidney Int., 2015. [DOI | PubMed]
20. N. AlAli, B.J. Wheaton, S.O.P. Jacobsson. Functional selectivity of cannabinoids at CB1 receptors: Comprehensive analysis of G proteins, β-arrestin and cAMP signalling dynamics in HEK293T cells. Eur. J. Pharmacol., 2026. [DOI | PubMed]
21. W.J. Costain, J.S. Tauskela, I. Rasquinha, T. Comas, M. Hewitt, V. Marleau, E.C. Soo. Pharmacological characterization of emerging synthetic cannabinoids in HEK293T cells and hippocampal neurons. Eur. J. Pharmacol., 2016. [DOI | PubMed]
22. G. Navarro, I. Reyes-Resina, R. Rivas-Santisteban, V. Sánchez de Medina, P. Morales, S. Casano, C. Ferreiro-Vera, A. Lillo, D. Aguinaga, N. Jagerovic. Cannabidiol skews biased agonism at cannabinoid CB1 and CB2 receptors with smaller effect in CB1-CB2 heteroreceptor complexes. Biochem. Pharmacol., 2018. [DOI | PubMed]
23. W.M. Raup-Konsavage, M. Johnson, C.A. Legare, G.S. Yochum, D.J. Morgan, K.E. Vrana. Synthetic Cannabinoid Activity Against Colorectal Cancer Cells. Cannabis Cannabinoid Res., 2018. [DOI | PubMed]
24. E.A. McCaw, H. Hu, G.T. Gomez, A.L. Hebb, M.E. Kelly, E.M. Denovan-Wright. Structure, expression and regulation of the cannabinoid receptor gene (CB1) in Huntington’s disease transgenic mice. Eur. J. Biochem., 2004. [DOI | PubMed]
25. D. Navarro, A. Gasparyan, F. Navarrete, A.B. Torregrosa, G. Rubio, M. Marín-Mayor, G.B. Acosta, M.S. Garcia-Gutiérrez, J. Manzanares. Molecular Alterations of the Endocannabinoid System in Psychiatric Disorders. Int. J. Mol. Sci., 2022. [DOI | PubMed]
26. R. Evans, J.A. Fairley, S.G. Roberts. Activator-mediated disruption of sequence-specific DNA contacts by the general transcription factor TFIIB. Genes Dev., 2001. [DOI | PubMed]
27. T. Lagrange, A.N. Kapanidis, H. Tang, D. Reinberg, R.H. Ebright. New core promoter element in RNA polymerase II-dependent transcription: Sequence-specific DNA binding by transcription factor IIB. Genes Dev., 1998. [DOI | PubMed]
28. J.E. Butler, J.T. Kadonaga. The RNA polymerase II core promoter: A key component in the regulation of gene expression. Genes Dev., 2002. [DOI | PubMed]
29. C.A. Heinlein, C. Chang. Androgen receptor (AR) coregulators: An overview. Endocr. Rev., 2002. [DOI | PubMed]
30. S.K. Mobisson, D.E. Ikpi, I. Wopara, A.O. Obembe, O. Omotuyi. Inhibition of human androgen receptor by delta 9-tetrahydro-cannabinol and cannabidiol related to reproductive dysfunction: A computational study. Andrologia, 2022. [DOI | PubMed]
31. V. Purohit, B.S. Ahluwahlia, R.A. Vigersky. Marihuana inhibits dihydrotestosterone binding to the androgen receptor. Endocrinology, 1980. [DOI | PubMed]
32. P. Monteleone, M. Bifulco, C. Di Filippo, P. Gazzerro, B. Canestrelli, F. Monteleone, M.C. Proto, M. Di Genio, C. Grimaldi, M. Maj. Association of CNR1 and FAAH endocannabinoid gene polymorphisms with anorexia nervosa and bulimia nervosa: Evidence for synergistic effects. Genes Brain Behav., 2009. [DOI | PubMed]
33. M. Sadeghian, S. Rahmani, A. Mansoori. G1359A Variant of the Cannabinoid Receptor Gene (rs1049353) and Obesity-Related Traits and Related Endophenotypes: A Meta-Analysis. Ann. Nutr. Metab., 2018. [DOI | PubMed]
34. K. Domschke, U. Dannlowski, P. Ohrmann, B. Lawford, J. Bauer, H. Kugel, W. Heindel, R. Young, P. Morris, V. Arolt. Cannabinoid receptor 1 (CNR1) gene: Impact on antidepressant treatment response and emotion processing in major depression. Eur. Neuropsychopharmacol., 2008. [DOI | PubMed]
35. L.K. Miller, L.A. Devi. The highs and lows of cannabinoid receptor expression in disease: Mechanisms and their therapeutic implications. Pharmacol. Rev., 2011. [DOI | PubMed]
36. G. Lim, B. Sung, R.R. Ji, J. Mao. Upregulation of spinal cannabinoid-1-receptors following nerve injury enhances the effects of Win 55,212-2 on neuropathic pain behaviors in rats. Pain, 2003. [DOI | PubMed]
37. A. Siegling, H.A. Hofmann, D. Denzer, F. Mauler, J. De Vry. Cannabinoid CB(1) receptor upregulation in a rat model of chronic neuropathic pain. Eur. J. Pharmacol., 2001. [DOI | PubMed]
38. J.S. Walczak, V. Pichette, F. Leblond, K. Desbiens, P. Beaulieu. Behavioral, pharmacological and molecular characterization of the saphenous nerve partial ligation: A new model of neuropathic pain. Neuroscience, 2005. [DOI | PubMed]
39. S. Mitrirattanakul, N. Ramakul, A.V. Guerrero, Y. Matsuka, T. Ono, H. Iwase, K. Mackie, K.F. Faull, I. Spigelman. Site-specific increases in peripheral cannabinoid receptors and their endogenous ligands in a model of neuropathic pain. Pain, 2006. [DOI | PubMed]
40. F. Teixeira-Clerc, B. Julien, P. Grenard, J. Tran Van Nhieu, V. Deveaux, L. Li, V. Serriere-Lanneau, C. Ledent, A. Mallat, S. Lotersztajn. CB1 cannabinoid receptor antagonism: A new strategy for the treatment of liver fibrosis. Nat. Med., 2006. [DOI | PubMed]
41. W.I. Jeong, D. Osei-Hyiaman, O. Park, J. Liu, S. Bátkai, P. Mukhopadhyay, N. Horiguchi, J. Harvey-White, G. Marsicano, B. Lutz. Paracrine activation of hepatic CB1 receptors by stellate cell-derived endocannabinoids mediates alcoholic fatty liver. Cell Metab., 2008. [DOI | PubMed]
42. B.L. Hungund, K.Y. Vinod, S.A. Kassir, B.S. Basavarajappa, R. Yalamanchili, T.B. Cooper, J.J. Mann, V. Arango. Upregulation of CB1 receptors and agonist-stimulated [35S]GTPgammaS binding in the prefrontal cortex of depressed suicide victims. Mol. Psychiatry, 2004. [DOI | PubMed]
43. S. Sarfaraz, V.M. Adhami, D.N. Syed, F. Afaq, H. Mukhtar. Cannabinoids for cancer treatment: Progress and promise. Cancer Res., 2008. [DOI | PubMed]
44. T. Jourdan, L. Djaouti, L. Demizieux, J. Gresti, B. Vergès, P. Degrace. CB1 antagonism exerts specific molecular effects on visceral and subcutaneous fat and reverses liver steatosis in diet-induced obese mice. Diabetes, 2010. [DOI | PubMed]
45. A. Ligresti, A.S. Moriello, K. Starowicz, I. Matias, S. Pisanti, L. De Petrocellis, C. Laezza, G. Portella, M. Bifulco, V. Di Marzo. Antitumor activity of plant cannabinoids with emphasis on the effect of cannabidiol on human breast carcinoma. J. Pharmacol. Exp. Ther., 2006. [DOI | PubMed]
46. C. Grimaldi, S. Pisanti, C. Laezza, A.M. Malfitano, A. Santoro, M. Vitale, M.G. Caruso, M. Notarnicola, I. Iacuzzo, G. Portella. Anandamide inhibits adhesion and migration of breast cancer cells. Exp. Cell Res., 2006. [DOI | PubMed]
47. R.J. McKallip, M. Nagarkatti, P.S. Nagarkatti. Delta-9-tetrahydrocannabinol enhances breast cancer growth and metastasis by suppression of the antitumor immune response. J. Immunol., 2005. [DOI | PubMed]
48. T.R. Spindle, H. Kuwabara, A. Eversole, A. Nandi, R. Vandrey, D.G. Antoine, A. Umbricht, A.S. Guarda, D.F. Wong, E.M. Weerts. Brain imaging of cannabinoid type I (CB1) receptors in women with cannabis use disorder and male and female healthy controls. Addict. Biol., 2021. [DOI | PubMed]
49. D.C. D’Souza, J.A. Cortes-Briones, M. Ranganathan, H. Thurnauer, G. Creatura, T. Surti, B. Planeta, A. Neumeister, B. Pittman, M. Normandin. Rapid Changes in CB1 Receptor Availability in Cannabis Dependent Males after Abstinence from Cannabis. Biol. Psychiatry Cogn. Neurosci. Neuroimaging, 2016. [DOI | PubMed]
50. S.B. Gustafsson, R. Palmqvist, M.L. Henriksson, A.M. Dahlin, S. Edin, S.O. Jacobsson, Å. Öberg, C.J. Fowler. High tumour cannabinoid CB1 receptor immunoreactivity negatively impacts disease-specific survival in stage II microsatellite stable colorectal cancer. PLoS ONE, 2011. [DOI | PubMed]
51. C.K. Jung, W.K. Kang, J.M. Park, H.J. Ahn, S.W. Kim, S. Taek Oh, K.Y. Choi. Expression of the cannabinoid type I receptor and prognosis following surgery in colorectal cancer. Oncol. Lett., 2013. [DOI | PubMed]
52. P.F. Whiting, R.F. Wolff, S. Deshpande, M. Di Nisio, S. Duffy, A.V. Hernandez, J.C. Keurentjes, S. Lang, K. Misso, S. Ryder. Cannabinoids for Medical Use: A Systematic Review and Meta-analysis. JAMA, 2015. [DOI | PubMed]
53. A.M. Kerlin, M. Long, M. Kappelman, C. Martin, R.S. Sandler. Profiles of Patients Who Use Marijuana for Inflammatory Bowel Disease. Dig. Dis. Sci., 2018. [DOI | PubMed]
54. K. Bogale, W. Raup-Konsavage, S. Dalessio, K. Vrana, M.D. Coates. Cannabis and Cannabis Derivatives for Abdominal Pain Management in Inflammatory Bowel Disease. Med. Cannabis Cannabinoids, 2021. [DOI | PubMed]
55. L. Karila, P. Roux, B. Rolland, A. Benyamina, M. Reynaud, H.J. Aubin, C. Lançon. Acute and long-term effects of cannabis use: A review. Curr. Pharm. Des., 2014. [DOI | PubMed]
56. D. Shah, P. Chand, M. Bandawar, V. Benegal, P. Murthy. Cannabis induced psychosis and subsequent psychiatric disorders. Asian J. Psychiatr., 2017. [DOI | PubMed]
57. M.R. Wade, E.T. Tzavara, G.G. Nomikos. Cannabinoids reduce cAMP levels in the striatum of freely moving rats: An in vivo microdialysis study. Brain Res., 2004. [DOI | PubMed]
58. K. Eldeeb, S. Leone-Kabler, A.C. Howlett. CB1 cannabinoid receptor-mediated increases in cyclic AMP accumulation are correlated with reduced Gi/o function. J. Basic Clin. Physiol. Pharmacol., 2016. [DOI | PubMed]
59. E.E. Cawston, W.J. Redmond, C.M. Breen, N.L. Grimsey, M. Connor, M. Glass. Real-time characterization of cannabinoid receptor 1 (CB1) allosteric modulators reveals novel mechanism of action. Br. J. Pharmacol., 2013. [DOI | PubMed]