Possible roles of AMPK and macropinocytosis in the defense responses against Δ9-THC toxicity on HL-1 cardiomyocytes
Department of Forensic Medicine, Graduate School of Medical and Dental Sciences, Tokyo Medical and Dental University, Tokyo, Japan
Graphical abstract
Untitled section
Keywords: Δ9-THC, ER stress, Macropinocytosis, AMPK, HL-1 cells
Highlights
- •Δ9-THC induced ER stress in HL-1 murine cardiomyocyte.
- •Δ9-THC also induced macropinocytosis, which was mediated by AMPK.
- •AMPK-macropinocytosis axis was one of the survival pathways against Δ9-THC.
Abstract
Cannabinoids are some of the most popular recreationally used illicit drugs, and are frequently consumed along with alcoholic beverages. Although the whole body effects of cannabinoids depend largely on their effects on the central nerve system, cannabinoids could harm the heart directly, due to the presence of the endocannabinoid system including cannabinoid receptor1 and 2 (CB-R1 and CB-R2) in the heart. The aim of this study is to examine the mechanism of direct cardiotoxicity of Δ9-tetrahydrocannabinol (Δ9-THC), the main psychoactive ingredient of cannabis. For this purpose, HL-1 murine atrial cardiac muscle cells were treated with 10 or 30 μM Δ9-THC, along with 100 mM ethanol to examine the possible synergistic effects of Δ9-THC and ethanol. Transcriptome analysis showed upregulation of the genes involved in the unfolded protein response (UPR), including Bip, CHOP, ATF4 and ATF6, in cells treated with Δ9-THC. Immunoblot analysis showed caspase3 activation, indicating apoptosis caused by ER stress in Δ9-THC-treated cells. Microscopic analysis showed that Δ9-THC enhances macropinocytosis, a process involved in the uptake of extracellular fluids including nutrients. Moreover Δ9-THC seemed to activate AMPK, a sensor of intracellular energy status and an activator of macropinocytosis. Finally, we found that compound C (AMPK inhibitor) aggravated cell death by Δ9-THC while AICAR (AMPK activator) ameliorated it. Collectively, these results indicate that the activation of AMPK is necessary for the survival of HL-1 cells against Δ9-THC toxicity. Macropinocytosis might serve as one of the survival pathways downstream of AMPK.
Article notes
Untitled section
Received 2021 Jan 13; Revised 2021 Apr 19; Accepted 2021 Apr 27; Collection date 2021.
1.Introduction
Cannabinoids are components of the cannabis plant which includes Cannabis Indica and Cannabis Sativa as the two major subspecies. Marijuana, which is widely used as a recreational drug, is made from dried parts of cannabis plant. Although the use of marijuana is associated with relatively few deaths, adverse effects on the cardiovascular system such as arrhythmias, ischemic attack, and cardiac infarction sometimes lead to sudden cardiac death [1]. The risk of sudden death due to the cardiovascular toxicity of cannabis has recently expanded due to the worldwide distribution of synthetic cannabinoids [[2], [3], [4], [5], [6]]. Alcohol can increase the harmful effects of cannabinoids; therefore, drinking alcoholic beverages while consuming marijuana may raise the possibility of sudden cardiac death [7,8]. Although responses of the heart to cannabinoids depend highly on the individual, in general, an acute increase in heart rate is followed by decreased heart function [1]. Among naturally occurring cannabinoids, Δ9-tetrahydrocannabinol (Δ9-THC) is the most potent psychoactive constituent of marijuana [9]. Δ9-THC elicits its effects by binding to cell surface G-protein coupled receptors, referred to as type-1 and -2 cannabinoid receptors (CB-R1 and CB-R2), both of which are expressed in cardiomyocytes [10,11]. Although CB-R1 and CB-R2 are the main transducers of Δ9-THC signals, other receptors, such as G-protein coupled receptor 55 (GPR55), are also expressed in the heart and are involved in Δ9-THC signal transduction [12].
ER stress and subsequent unfolded protein response (UPR) are processes involved not only in cell survival but also in cell death [13,14]. Upon accumulation of unfolded proteins within the ER, an ER-resident chaperone, Bip, initiates UPR. Downstream of Bip, UPR diverges 3 ways into the IRE1α, PERK, and ATF6 pathways [13]. IRE1α can induce pro-apoptotic JNK activation [15]. The activation of PERK leads to the activation of proapoptotic CHOP transcription factor through ATF4 [14,16]. Although ATF6 induces ER-resident chaperones such as Bip and PDI for the protection of cells against ER stress, prolonged ATF6 activation results in the induction of CHOP [14]. Therefore, excessive UPR can induce apoptotic cell death through any of these 3 pathways. Caspase-12 is considered to be responsible for ER-stress-induced apoptosis in murine cells [17], though other functions, such as an inflammatory caspase, are attributed to this caspase [18]. There are many reports describing the importance of ER stress in Δ9-THC -induced apoptosis in various cell types [[19], [20], [21]].
Macropinocytosis is a type of clathrin-independent endocytosis in which extracellular fluids, including nutrients, antigens, and small water-soluble molecules, are taken up nonspecifically [22]. Macropinocytosis begins with protrusion of the plasma membrane through the polymerization of actin, followed by the engulfment of extracellular fluids via closure of the membrane protrusions at their distal margins. Then, the luminal space of macropinosomes is delivered to the lysosome to digest their contents. Although excessive macropinocytosis sometimes results in massive cytoplasmic vacuolization and resultant catastrophic cell death, referred to as methuosis [23], macropinocytosis ordinarily participates in cellular homeostasis, especially for tumor cell survival as a nutrients-acquiring cellular strategy [22,24]. In accordance with its role in nutrient acquisition, macropinocytosis is facilitated by AMPK [25,26], which is activated during nutrient deficiency [27]. To the best of our knowledge, macropinocytosis has not been a topic in the context of Δ9-THC cytotoxicity, in contrast to ER stress, which has been repeatedly reported in Δ9-THC-treated cells.
In this study we examined the cytotoxicity mechanism of Δ9-THC and/or ethanol on HL-1 murine atrial cardiomyocytes, and found ER stress as a cell death mechanism. In addition, we found AMPK activation protects the cells against Δ9-THC cytotoxicity. We also observed cytoplasmic vacuolization through enhanced macropinocytosis, which was activated by AMPK and therefore might be involved in the protective role of AMPK against Δ9-THC cytotoxicity.
2.Materials and methods
2.1.Δ9-THC and other reagents
Δ9-Tetrahydrocannabinol (Δ9-THC, kindly provided by Dr. Satoshi Morimoto, Kyushu University) was dissolved in DMSO (FUJIFILM Wako Pure Chemical, Osaka, Japan) at a final concentration of 100 mM and stored at −80 °C until use. Ethanol, AM251, and AM630 were purchased from FUJIFILM Wako Pure Chemical. Tauroursodeoxycholic acid (TUDCA) was from Millipore Corp (USA). 5-Aminoimidazole-4-carboxamide-1-β-d-ribofuranoside (AICAR) was from Sigma-Aldrich (St. Louis, MO, USA). Compound C was from abcam (Cambridge, MA, USA).
2.2.Cell culture
HL-1 mouse atrial cardiomyocyte-derived cells were kindly provided by Dr. William C. Claycomb (Louisiana State University Medical Center) [28]. The cells were maintained as recommended by the Claycomb Laboratory. In brief, cells were cultured on gelatin/fibronectin-coated dishes at 37 °C in a humidified atmosphere containing 5% CO2 in Claycomb medium supplemented with 10 % fetal bovine serum, 100 U/mL penicillin, 100 μg/mL streptomycin, 0.1 mM norepinephrine, and 2 mM l-glutamine. Once the cells had grown to confluency and started to beat spontaneous, the indicated concentrations of Δ9-THC (10 or 30 μM) and/or 100 mM ethanol were added directly to the medium. The culture dishes were sealed with laboratory film throughout the incubation period to minimize ethanol evaporation.
2.3.Viability assays
Cells were incubated with 30 μM Δ9-THC and/or 100 mM ethanol for 48 h. In some experiments, the indicated concentrations of inhibitors or activators were added to the medium 1 h before the addition of Δ9-THC and/or ethanol, and included throughout the incubation period. Cell viability was determined by a modified MTT assay using a Cell Counting Kit-8 (CCK-8; Dojindo, Kumamoto, Japan).
2.4.Western blot analysis
Cells grown on 3 cm diameter dishes were scraped, collected together with floating cells by centrifugation, and subjected to ultrasonic wave disruption in STE buffer (0.32 M sucrose, 10 mM Tris−HCl, pH 7.4, 5 mM EDTA, 50 mM NaF, 2 mM Na₃VO₄) on ice. Equal amounts of protein were subjected to SDS-PAGE, transferred to a PVDF membrane, and blocked in TBS-Tween (150 mM NaCl, 10 mM Tris−HCl, pH 7.4, 0.05 % Tween 20) containing 3% skim milk. The membranes were incubated overnight at 4℃ with specific antibodies (Supporting information, S1 Table). After washing with TBS-Tween, the membranes were incubated with peroxidase-conjugated anti-rabbit antibody (1:10,000 dilution, Promega, USA) at room temperature for 45 min. Antigens were visualized using a Western Lightning Chemiluminescence Reagent Plus Kit (Perkin Elmer Life Science, USA), and the signal intensities were quantified using Image J (ver.1.52v, National Institutes of Health, USA).
2.5.Microarray and quantitative real-time PCR analysis
For DNA microarray and quantitative real-time RT-PCR (qPCR) analysis, total RNA was extracted from cells using TRlzol reagent (Invitrogen, USA). For DNA microarray analysis, the total RNA was further purified using a Monarch total RNA prep kit (New England Biolabs, USA). RNA integrity was assessed by a BioAnalyzer (Agilent Technologies, USA), and DNA microarray analysis was performed using Clariom™S array (Affymetrix, Thermo Fisher Scientific, USA). DAVID Bioinformatics Resources (https://david.ncifcrf.gov/summary.jsp) were used to analyze the results. For qPCR analysis, cDNA was synthesized using oligo (dT)15 primer and SuperScriptⅡreverse transcriptase (Invitrogen, USA). qPCR was performed with the StepOnePlus real-time PCR system (Applied Biosystems, USA). Primers used are listed in Supporting information (S2 Table).
2.6.Transfection of vectors and fluorescence microscopy
Cells grown on 3 cm dishes for 24 h were transfected with plasmid vectors expressing kinectin (1–106)-GFP [29] or GFP-HSP47 [30], which were kindly provided by Dr. Erika Abe (Akita University) or Dr. Kazuhiro Nagata (Kyoto University), respectively. Vectors were mixed with Lipofectamine2000 (Invitrogen), added to the cells, and the cells were incubated overnight. After treatment with 30 μM Δ9-THC for 24 h, cells were observed under a fluorescence microscope (DMi8, Leica, Wetzlar, Germany).
2.7.Uptake of FITC-dextran
To observe macropinocytosis, we used fluid-phase tracer FITC-dextran, which is widely known as a marker for macropinocytosis [31]. Cells grown on 3 cm diameter dishes for 2 days were treated with 30 μM Δ9-THC and 0.5 mg/ml FITC-dextran (average M.W. 70 kDa, Sigma-Aldrich) for 24 h. The cells were then washed twice with the medium and observed under a fluorescence microscope (DMi8, Leica).
2.8.Statistical analysis
All data comprising more than three experimental groups were analyzed using the Tukey-Kramer statistical method for multiple comparisons. Student’s t-test was also used for the comparison of two experimental groups. The data are expressed as mean ± S.D. of at least three samples. P values <0.05 were considered to be statistically significant.
3.Results
3.1.Δ9-THC decreases cellular viabilities in HL-1 cells
We first examined whether Δ9-THC decreases the viability of HL-1 cells, as well as whether or not ethanol affects Δ9-THC cytotoxicity. Given the indication that the cytotoxicity of Δ9-THC becomes detectable in cells at around 10 μM [32], and our previous observation that 0.5–1 % (86−172 mM) ethanol decreases the viability of HL-1 cells slightly but not significantly [33], cells were treated with 30 μM Δ9-THC and/or 100 mM ethanol for 48 h. The relative viabilities (mean ± S.D., expressed as % of control) of each experimental group were 82.9 ± 3.93 % (Δ9-THC), 92.0 ± 6.58 % (ethanol), and 63.6 ± 6.80 % (Δ9-THC + ethanol) (Fig. 1A). There are significant differences between Δ9-THC and Δ9-THC + ethanol groups, as well as ethanol and Δ9-THC + ethanol groups (Fig. 1A). Although the loss of viability in the Δ9-THC + ethanol group (36.4 %) was slightly higher than that of the sum (25.1 %) of Δ9-THC (17.1 %) and ethanol (8.0 %), there was no obvious synergistic effect between Δ9-THC and ethanol. Thus, the cytotoxicity of Δ9-THC and ethanol seems to be additive, rather than synergistic, under our experimental settings. Interestingly, we observed cytoplasmic vacuolization in Δ9-THC-treated cells, which was not observed in ethanol-treated cells (Fig. 1B), supporting the assumption that the toxicities of Δ9-THC and ethanol on HL-1 cells are independent, rather than interactive. Next, we examined whether the cytotoxic effects of Δ9-THC are transmitted through cannabinoid receptors. Neither AM251 (1 μM, CB-R1 antagonist) nor AM630 (1 μM, CB-R2 antagonist) could rescue the loss of viability caused by Δ9-THC (Fig. 1C). Thus, the Δ9-THC-induced loss of cell viability seems to be a CB-R1/2 -independent process.
3.3.Δ9-THC induces ER stress and subsequent apoptosis in HL-1 cells
We checked further whether ER stress responses are indeed induced by Δ9-THC. Cells were treated with 10 or 30 μM Δ9-THC with or without 100 mM ethanol for 24 and 48 h, and then evaluated by quantitative RT-PCR and western blot analysis. Both the mRNA and proteins levels of BIP, ATF4, ATF6 and CHOP, markers of the ER stress response, increased in response to 30 μM Δ9-THC (Fig. 2A-F), confirming the ER stress response. Although the co-administration of ethanol seemed to affect the expressions of several of the ER stress genes induced by Δ9-THC, there was no certain tendency for an effect of ethanol on Δ9-THC-induced ER stress gene expression (Fig. 2A-D). Significant increase of all the BIP, ATF4, ATF6 and CHOP gene expressions were observed in Δ9-THC + ethanol group compared to ethanol group (Fig. 2A-D), suggesting that these gene expressions were governed mainly by Δ9-THC. In contrast, only BIP and CHOP showed increased protein levels in Δ9-THC + ethanol group compared to ethanol group (Fig. 2, E and F). Therefore, there should be some differences between the regulations of protein and mRNA of these genes. Further, we examined the involvement of ER stress in the cytotoxicity of Δ9-THC using tauroursodeoxycholic acid (TUDCA), which has been shown to function as a chemical chaperone and suppresses ER stress [32,34] TUDCA pretreatment significantly alleviated Δ9-THC cytotoxicity (Fig. 2H). Thus, ER stress appears to be involved, at least in part, in the cytotoxicity of Δ9-THC on HL-1 cells. To examine whether apoptosis is involved in the observed loss of viability of Δ9-THC-treated cells (Fig. 1A), we evaluated the levels of the cleaved forms of caspase-12 and caspase-3. Interestingly, a significant increase in cleaved caspase-12 was observed only in the Δ9-THC + ethanol group, implying that Δ9-THC and ethanol may activate the caspase-12 pathway in a synergistic manner (Fig. 2G). In contrast, a significant increase in cleaved caspase-3 was observed in all experimental groups in which 30 μM Δ9-THC was included (Fig. 2G), suggesting that the loss of cell viability by Δ9-THC involves apoptotic cell death through caspase-3.
3.4.Δ9-THC decreases both MYH-6 and MYH-7 expression
Given the indication of the downregulation of myocardial function-related genes (Table 1), we examined the mRNA levels of MYH-6 and MYH-7 (also known as α- and β-myosin heavy chain) and found that both are decreased by Δ9-THC (Fig. 3 A and B). Expression of the MYH-7 gene was also decreased by ethanol (Fig. 3 B), suggesting that ethanol by itself can affect myocardial functional gene expression. Significant decreases were observed in both MYH-6 and MYH-7 gene expression in Δ9-THC + ethanol group compared to ethanol group (Fig. 3 A and B), indicating that Δ9-THC showed decreasing effect on MYH-7 gene even under the presence of ethanol. We also found a tendency towards an increase in the expression of atrogin-1, an E3 ubiquitin ligase implicated in the degradation of myosin [35], in response to ethanol and/or Δ9-THC (Fig. 3C). Thus, not only the decrease in gene expression, but also protein degradation might be involved in the downregulation of myocardial functional genes.
3.5.Cytoplasmic vacuolization in Δ9-THC-treated cells involves ER dilation as well as macropinocytosis
We next investigated the origin of the vacuoles that are observed in Δ9-THC-treated cells (Fig. 1B). We first suspected ER dilation as the origin of the cytoplasmic vacuoles, and so we transfected cells with plasmid vectors expressing kinectin (1–106)-GFP and GFP-HSP47, which localize to the membrane and luminal space of the ER, respectively [29,30]. In cells treated with Δ9-THC, kinectin-GFP localized to the edge of several vacuoles (Fig. 4A). In contrast, GFP-HSP47 localized to the lumen of large vacuoles, which were sometimes observed in Δ9-THC-treated cells (Fig. 4B). However, neither kinectin-GFP nor GFP-HSP47 localized to phase lucent vacuoles that have a perfect round shape (Fig. 4 A and B). We then explored the origin of these vacuoles. FITC-dextran was observed to be taken up into these phase lucent vacuoles (Fig. 4C), suggesting that they are macropinosomes. Taken together, cytoplasmic vacuolization by Δ9-THC involves at least two mechanisms: dilation of the ER and an enhancement of macropinocytosis.
3.6.AMPK is activated by Δ9-THC and involved in cytoprotection against Δ9-THC toxicity
Given the indication of enhanced macropinocytosis (Fig. 4C) and the fact that AMPK is involved in the induction of macropinocytosis [25,26], we examined whether Δ9-THC activates AMPK. Levels of the phosphorylated active form of AMPK (p-AMPK) as well as total AMPK were evaluated by immunoblotting. An increase in p-AMPK levels relative to total AMPK was observed in cells treated with Δ9-THC for both 24 and 48 h (Fig. 5A). Furthermore, cells treated with an AMPK activator (AICAR) or inhibitor (compound C) showed significantly mitigated or aggravated Δ9-THC cytotoxicity, respectively, (Fig. 5 B and C). Thus, AMPK activates a survival pathway against Δ9-THC toxicity in HL-1 cells. In addition, pretreatment with compound C indeed mitigated cytoplasmic vacuolization in Δ9-THC-treated cells (Fig. 5D), confirming that AMPK is involved in the induction of macropinocytosis in these cells.
4.Discussion
Many studies have shown that THC induces ER stress and subsequent cell death. For example, Carracedo et al., reported that Δ9-THC induces ER stress and subsequent cell death though CB-R2 in several human pancreatic tumor cell lines [19]. They also reported decreased growth of pancreatic tumor cells in animals administered Δ9-THC, showing that Δ9-THC reduces tumor growth through ER stress-mediated cell death in vivo [19]. Lojpur et al. also reported that in human trophoblast BeWo cells, Δ9-THC-induced ER stress as well as apoptosis is suppressed by a mixture of CB-R1 and CB-R2 antagonists [32]. Therefore, it is a bit surprising that Δ9-THC-induced death of HL-1 cells could be suppressed by antagonists of neither CB-R1 nor CB-R2 (Fig. 1C). Since there are other proteins that can function as cannabinoid receptors including GPR55 [12], TRP channels [36] and PPARs [37], Δ9-THC might induce UPR through receptors other than CB-R1/2. Alternatively, there is a possibility that Δ9-THC induces ER stress and subsequent apoptosis in a manner independent of these receptors. Indeed, the possible involvement of receptor-independent processes in the action of cannabinoids has been proposed to occur in addition to receptor-mediated processes [38]. Due to its hydrophobicity, Δ9-THC can interact directly with membrane phospholipids, thereby altering membrane properties such as fluidity, integrity, and the barrier function of micro- as well as macro-molecules. Indeed, membrane perturbation by Δ9-THC has been demonstrated [39]. Thus, future investigations should be undertaken to determine whether Δ9-THC induces ER stress and cell death through receptors other than CB-R1, CB-R2, or whether there is a direct interaction of Δ9-THC with the cardiomyocyte membrane.
A massive accumulation of cytoplasmic vacuoles, most of which are derived from macropinocytosis, was observed in Δ9-THC-treated cells. However, the Δ9-THC-induced death of HL-1 cells seems not to be caused by methuosis since cell death could be suppressed by an activator of AMPK, an inducer of macropinocytosis (Fig. 5); AMPK-macropinocytosis seems to be involved in the protection against Δ9-THC toxicity in HL-1 cells. Macropinocytosis plays crucial roles in nutrient uptake into cells from extracellular environments [22]. The incorporation of nutrients through macropinocytosis is especially important for the survival of tumor cells as well as for normal cells encountering nutrient deficiency [22]. Indeed, a recent study demonstrated that macropinocytosis-mediated nutrient uptake plays an important role in tumor cell resistance to chemotherapy drugs [40]. Furthermore, it has been demonstrated that Δ9-THC inhibits glycolysis in the testis of mice as well as rats in a dose dependent manner [41]. A recent in vitro study has also shown that both CB-R1- and -R2-specific synthetic cannabinoids (arachidonoyl cyclopropamide and GW405833, respectively) suppress glycolysis as well as glutamine uptake in Panc1 pancreatic tumor cells [42]. Thus, it might be reasonable to suppose macropinocytosis as one of the survival mechanisms downstream of AMPK. It is worth noting that the induction of autophagy, another cellular defense mechanism against nutrient deficiency [43], by Δ9-THC has been repeatedly reported [21,[44], [45], [46]].
In conclusion, this is the first report showing enhanced macropinocytosis in Δ9-THC-treated cells. AMPK is involved not only in the induction of macropinocytosis but also in cytoprotection against Δ9-THC in the cells. Along with autophagy, AMPK might protect against Δ9-THC cytotoxicity by inducing macropinocytosis.
Funding
This study was supported by a grant-in-aid from MEXT KAKENHI (grant number 19K19483 to K.N. and 18K19670 to T.A.).
Declaration of Competing Interest
The authors declare no conflict of interest.
Acknowledgment
We would like to thank Dr. Satoshi Morimoto (Kyushu University) for providing Δ9-THC.
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Edited by Dr. A.M Tsatsaka
Footnotes
Footnote Group
Appendix A.Supplementary data
The following is Supplementary data to this article:
References
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