Introduction
Sigma receptors have been intensely studied for their applications in both neuropharmacology and oncology. Two subtypes of sigma receptors are known, sigma-1 and −2, which were classically characterized by differences in their relative binding affinity of
3 H]-(+)-pentazocine (sigma-1 > sigma-2) [
1] and
3 H]-1,3 di-ortho-tolylguanidine (
3 H]-DTG) (sigma-1 = sigma-2) [
2] because of lack of genetic identification of the sigma-2 receptorfor many years. However, we have recently identified progesterone receptor membrane component 1 (PGRMC1) protein complex as containing the sigma-2 receptor binding site [
3]and others recently found PGRMC1/sigma-2 to be elevated in tumors and serum of lung cancer patients [
4].
Table 1
Pancreatic cancer cell line viability, IC
50
(μM), following sigma-2 receptor ligand treatment (24 hr)
| Mean | SEM | n | Mean | SEM | n | Mean | SEM | n |
SV119 | 92 | 10 | 4 | 97 | 16 | 3 | 192 | 41 | 4 |
SW43 | 26 | 5 | 4 | 56 | 14 | 3 | 65 | 12 | 4 |
PB28 | 73 | 10 | 4 | 96 | 16 | 3 | 244 | 48 | 4 |
PB282 | 79 | 16 | 4 | 82 | 20 | 3 | 135 | 10 | 4 |
Sigma-2 receptors are overexpressed in multiple tumor types including breast, pancreas, neuroblastoma, bladder, and lung as reviewed [
5], which has allowed further development of these ligands as radiotracers for the imaging of cancer [
6]. In addition, various sigma-2 receptor ligands have been extensively studied for their effectiveness in the treatment of solid tumors due to their preferential uptake in proliferating cells [
7]. We have previously shown that sigma-2 receptors are upregulated in pancreatic cancer, that sigma-2 ligands can induce caspase-3-mediated apoptisis, and are effective in preclinical models of pancreatic cancer [
8‐
10].
Sigma-2 receptor ligands that have been investigated for efficacy in the treatment of cancer induce apoptosis in caspase-3 dependent and independent manners, but the exact mechanism of cell death is still not well characterized. For example, in SK-N-SH neuroblastoma cells caspase-3 was not activated by CB-64D [
11], nor did caspase inhibitors afford protection against cell death in MCF-7 breast cancer cells [
12]. Caspase-3 is however activated in MCF-7 [
13] and in murine pancreatic adenocarcinoma Panc02cells [
10] bysiramesine, though caspase-3 inhibitor did not rescue viability in either case. With another compound, PB28, no caspase-3 activity was observed in MCF-7 [
14] or SK-N-SH cells [
15].
Thus, while various sigma-2 receptor ligands are capable of inducing apoptosis in tumor cells, the activation of caspase-3 and upstream signaling events leading to this appear to be specific to particular ligand and cell type. In this study, we sought to more closely study the apoptotic pathway induced by a number of structurally distinct sigma-2 receptor ligands in pancreatic cancer, which have proven efficacious in preclincal models. With knowledge of chemotherapy resistance to apoptotic stimuli depending on different mechanisms, we may more appopriately choose effective therapies.
Discussion
Recent synthesis of fluorescently labeled analogs of SV119 (SW120) and PB28 (PB385), allowing live cell imaging, has shown sigma-2 receptor ligand subcellular localization to the membrane components of the cell ultrastructure [
16,
17]. In various pancreatic cancer cell lines we have observed similar results, and hypothesized that strong uptake into the endo-lysosomal compartment induces lysosomal membrane permeabilization (LMP). In addition, weakly basic amines as a class of drugs have been shown to induce LMP [
24] and cell death [
25], and the amine groups present on sigma-2 receptor ligands suggest they can induce LMP. We examined here whether this could influence the caspase-3 activation in pancreatic cancer we observed earlier [
8‐
10] and found that LMP occurs shortly following treatment with a variety of structurally diverse sigma-2 receptor ligands, verified by both AO and LysoTracker release from the lysosome.
Uptake of fluorescently labeled compounds was inhibited by blocking the lysosomal pH gradient with concanamycin A (CMA), a specific inhibitor of the V-Type ATPase [
26,
27], and translated into significant viability protection following treatment. SW43 was a stronger inducer of LMP, with greater protection from CMA pretreatment than for PB282. This that some sigma-2 receptor ligands have a greater propensity to influence the lysosomal death pathway Chemical structure differences may be responsible for this difference
. For instance, the structure of the
N-(9-(6-Aminohexyl)-9-azabicyclo[3.3.1]-nonan-3α-yl)-
N-(2-methoxy-5-methylphenyl) carbamate hydrochloride (SV119) derivatives contain an alkyl extension with terminal amine group that is not present in the 1-cyclohexyl-4-[3-(5-methoxy-1,2,3,4-tetrahydro-naphthalen-1-yl)-propyl]-piperazine dihydrochloride (PB28) derivatives, a mo
ie ty that increases lysosomal membrane insertion and permeabilization [
28].
The lysosomal associated membrane proteins 1 and 2 (LAMP1/2) are homologous proteins of the lysosomal membrane [
21,
29,
30], where they are highly glycosylated and to contribute to protection of the lysosomal membrane and its proteins from the hostile constituents such as hydrogen ion and proteases [
31]. In addition, down-regulation of LAMP1/2 have been previously shown to sensitize cells to lysosomal mediated death pathways [
32], and we wished to confirm that sigma-2 receptor ligands act through a component of this pathway by decreasing LAMP1 expression with a lentivirus driven shRNA in Bxpc3 cells. Transformed cells had weaker lysosomes that retained less LysoTracker and the effect was additive with sigma-2 receptor ligand. Overall LysoTracker Green uptake was decreased as assessed by flow cytometry, which could have occurred by either a decreased number of lysosomes, or increased leakage across the membrane. We believe that the enhanced killing of transformed cells was due to compromise of the membrane integrity rather than decreased number of lysosomes based on the above finding that sigma-2 ligand accumulation in lysosomes is a necessary component of cell death.
LMP mediated cell death has been extensively studied recently in the context of apoptosis induction in cancer cells [
22,
33,
34]. The exact mechanism of LMP is still undetermined, and whether it involves pore formation or selective movement of contents, dyes of increasing molecular weight and size can be differentially released indicating some selectivity to LMP. A large number of known inducers of LMP exist, reviewed in [
22], and culminate in the release of proteases such as cathepsin B, D, and L, amonst others. Following treatment with sigma-2 receptor ligands, or hydroxychloroquine, we observed a near doubling of Z-RR-AMC cleavage within one hour, which was inhibited completely by CMA and CA-074-Me, supporting the above finding that uptake of the compound into the lysosome is a critical step in LMP mediated cell death.
Cancer cells can undergo both caspase-dependent and independent pathways of cell death following LMP, depending on the degree of insult [
22]. Cathepsins mediate crosstalk between the lysosome to the mitochondria [
35], where a caspase-dependent pathway is stimulated with cytochrome c release and superoxide production [
36]. With larger insults, a caspase-independent death pathway may be followed with release of cathepsins, cytosolic acidification, and caspase-2 activation [
22]. ROS production due to either pathway can act as both an effector and initiator of cell death. Amongst known inducers of LMP, oxidative stress itself ultimately leads to lipid peroxidation of the membrane with permeabilization [
37]. Thus, production of ROS following treatment can amplify LMP.
Protection against ROS can be by antioxidants or intracellular enzymes such as superoxide dimutase, catalase, and glutathione peroxidase. NAC is an small diffusible, hydrophobic antioxidant that is a precursor to glutathione, a cellular thiol-reducing agent oxidized by glutathione peroxidase in the reduction of hydrogen peroxide to water. In this study, NAC protected against cell death by SW43 to a greater extent than α-toco, while α-toco protected against PB282 more than NAC. While the mechanism of α-toco protection against oxidative stress is thought to be by prevention of membrane lipid peroxidation, and NAC as a general reducing agent, we believe this indicates key differences in the intracellular sites exposed to oxidative stress by sigma-2 receptor ligands. Intracellular ROS was detected with CM-H2DCFDA following SW43, but not PB282. This was decreased by both α-toco and NAC following SW43 treatment, but only with NAC following H2O2, suggesting that H2O2treatment did not induce oxidative stress in the membranes where the α-toco is present, while SW43 may have. PB282 viability protection by antioxidants is through a mechanism other than inhibiting oxidative stress.
Alpha-tocopherol has been previously established to protect cells from sigma-2 mediated mitochondrial ROS production and caspase-3 release [
10,
38,
39], and in this study we observed that caspase-3 stimulated by PB282 was inhibited in the presence of this antioxidant, while it did not protect that from SW43 or HCQ. In addition, caspase-3 inhibitor DEVD-FMK provided ample protection against cell death following PB282 treatment, but little following SW43 or HCQ despite detectable caspase-3 activity. The observation that the Aspc1 cell line did not induce caspase-3 activity following sigma-2 receptor ligand treatement, but retained cytotoxicity following lysosomal membrane permeabilization following SW43 treatment, further suggests the susceptibility differences are through slighty convergent pathways. Thus, it is most likely that PB282 undergoes caspase-dependent cell death following LMP that is mediated through a mitochondrial pathway, protected by α-toco. Conversely, SW43 undergoes caspase-independent cell death following LMP, with oxidative stress playing a stronger role in cell death.
Materials and Methods
Cell Culture
Cell lines were maintained in RPMI media (GIBCO) supplemented with L-glutamine (2 mM), (HEPES) (1 mM), pyruvate (1 mM), sodium bicarbonate (0.075 % w/v), penicillin and streptomycin (100 IU/mL), amphotericin (0.25 μg/mL), and 10 % fetal bovine serum (Atlanta Biologicals, Lawrenceville, GA). Cells were seeded at a density of 2 x 105/mL unless otherwise stated and maintained in a humidified atmosphere of 5 % CO2 at 37°C.
Compounds
Sigma-2 receptor ligands were synthesized as previously described [
10,
16,
17,
40‐
42]. The imaging dyes acridine orange and LysoTracker Red were obtained from Invitrogen (Carlsbad, CA), FITC mouse anti-human CD107a (LAMP1) and CD107b (LAMP2) antibodies from BD Biosciences (Franklin Lakes, NJ), peptidase inhibitors CA-074-Me and pepstatin A, and fluorogenic peptidase substrate Z-RR-AMC from Enzo Life Sciences (Plymouth Meeting, PA), caspase-3 inhibitor Z-DEVD-FMK from R&D Systems (Minneapolis, MN); caspase-3 substrate Ac-DEVD-AMC from Bachem Biosciences, Inc (King of Prussia, PA); All other reagents were obtained from Sigma-Alrich (St. Louis, MO) unless otherwise stated. Compounds were dissolved in DMSO with final concentrations less than 0.3 %.
In vivo tumor treatment
Athymic nude mice from Harlan Bioproducts, Inc. were inoculated subcutaneously with 1x106 Bxpc3 cells in the right flank. Tumor sizes were monitored with calipers and when tumors reached an average of 5 mm in diameter, mice were randomized and treated daily with equimolar doses of sigma-2 receptor ligands SV119 (1.0 mg), SW43 (1.1 mg), PB28 (0.9 mg), or PB282 (0.9 mg) resuspended in vehicle consisting of 5 % DMSO, 5 % EtOH, and 10 % Cremophor in 1X PBS and injected intraperitoneally. Data represents mean ± SEM, n = 7–10 per group.
Confocal microscopy
Cells grown on glass cover slips were incubated with SW120 or PB385 (100 nM) in the presence of LysoTracker Red (25 nM) for 30 minutes at 37°C. Cells were washed with PBS and fixed in 2 % paraformaldehyde for 30 minutes at 37°C prior to additional washing and mounting with ProLong Gold antifade reagent. Confocal imaging was performed on a Carl Zeiss Axiovert 100 inverted microscope, fitted with LSM 510 laser scanning microscope camera and software. Images were collected with filter bandwidths corresponding to 505–530 nm for green, 560–615 nm for red, and > 650 nm for far red, with 4 scans over 11.8 seconds.
Fluorescence microscopy
Cells grown on glass cover slips were loaded with acridine orange (2 μg/mL) for 15 minutes at 37°C prior to treatment for one hour with compounds. Cover slips were inverted onto slides and images taken immediately at 40X magnification on anOlympus BX51 microscope fitted with a U-LH100HE reflective fluorescence system and equipped with a Diagnositic Instruments, Inc. SPOT camera and software. Chroma Technology Corp filter sets were used for green (exciter: D480/30x, emitter: 535/40 m, beamsplitter: 505dclp), red (exciter: D540/25x, emitter: 606/55 m, beamsplitter: 556dclp), and blue (exciter: D360/40x, emitter: 460/50 m, beamsplitter: 400dclp). Scale bar equals 20 μm.
Dye retention analysis by flow cytometry
Cells were incubated with acridine orange (2 μg/mL) or LysoTracker Green (25 nM) for 30 minutes at 37°C prior to treatment with compounds for one hour. Cells were washed and mean fluorescence quantified with a FACSCalibur flow cytometer (BD Biosciences, San Jose, CA). Mean fluorescence was normalized to DMSO to determine the degree of lysosomal permeabilization. In addition, cells were pretreated with concanamycin A (10 μM) for one hour at 37°C prior to staining with either SW120 or PB385 (100 nM) for 30 minutes at 37°C and the difference in uptake represented by histogram.
Constructs
shRNAlentiviral constructs in pLKO.1 against human LAMP1 was purchased from Sigma Aldrich, and following verification of knockdown, clone ID NM_005561.2-1183s1c1 used to compromise lysosomal integrity. Packaging vectors were obtained through Addgene, Inc. (Cambridge, MA). Lentivirus particles were prepared by transfection of 293 T cells in T75 flasks with 3 μg construct, 2.8 μgpRSV-Rev, 2.4 μgpMDLg/pRRE, and 0.6 μg pMD2.G utilizing FuGENE® 6 Transfection Reagent from F. Hoffmann-La Roche Ltd. (Basel, Switzerland). Forty-eight and 72 hours following transfection, supernatant was transferred to Bxpc3 cells in the presence of polybrene (8 μg/mL). Transformed cells were selected with puromycin (1 μg/mL) and assayed accordingly.
Antibody staining
Cells were washed once with PBS prior to fixation with IC Fixation Buffer (eBiosciences) for 15 minutes at 37°C. Fixed cells were washed with PBS, resuspended in Permeabilization Buffer (eBiosciences), and incubated for 30 minutes at room temperature. Intracellular antigen staining was performed with FITC-antibody dilution of 1:100 in Permeabilization Buffer for 60 minutes at room temperature. Mean fluorescence in FL1 was quantified with a FACSCalibur flow cytometer.
Cell viability
Cell lines maintained at optimal culture conditions were seeded into 96-well white, clear-bottom plates and following treatment, viability determined with CellTiter-Glo Luminescent Viability Assay from Promega (Madison, WI). Luminescence was quantified with a SpectraMax Gemini microplate spectrofluorometer from Molecular Devices (Silicon Valley, CA). Viability relative to vehicle was fit by non-linear regression and plotted against concentration.
Cellular protease assay
Cells were treated in the presence of inhibitors and cytosolic extracts prepared using the digitonin extraction method as previously described [
43]. Washed cells were resuspended at 1x10
6 cells/mL in extraction buffer consisting of sucrose (250 mM), HEPES (20 mM), KCl (10 mM), MgCl
2 (1.5 mM), EDTA (1 mM), and digitonin (30 μM). Cells were placed on ice on an orbital shaker for 10 minutes prior to centrifugation for 1 min at 14,000 rpm at 4°C. Supernatants were collected and 20 μL used to detect cleavage of Z-RR-AMC in and equal volume of reaction buffer consisting of sodium acetate (100 mM), NaCl (200 mM), EDTA (4 mM), DTT (10 mM), and Z-RR-AMC (10 μM). Plates were read following incubation at 37 ° for 60 minutes with SpectraMax Gemini microplate spectrofluorometer, Molecular Devices (Silicon Valley, CA) (ex 355 nm, em 450 nm).
Detection of reactive oxygen species (ROS) by flow cytometry
Cells were seeded into 12-well plates one day prior to treatment, stained with 25 μM 5-(and-6)-carboxy-2’,7’-dichlorodihydro-fluorescein diacetate (carboxy-H2DCFDA) (Image-iT Live Green Reactive Oxygen Species Detection Kit, Molecular Probes, Eugene, OR) for 30 minutes at 37°C and treated overnight. Fluorescence intensity (max 529 nM) was quantified in the FL1 channel with a FACSCalibur flow cytometer.
Caspase-3 activity
Cells were maintained at optimal conditions and seeded in 96-well black-bottom plates in a volume of 100 μL. Following treatment, 5X assay buffer containing EDTA (10 mM), CHAPS (5 %), HEPES (100 mM), DTT (25 mM), and Ac-DEVD-AMC (250 μM) was added directly to the cell media and incubated for two hours at 37°C on a microplate shaker, and liberated AMC quantified with a SpectraMax Gemini microplate spectrofluorometer, Molecular Devices (ex 355 nm, em 450 nm). Caspase-3 activity is normalized to the absence of inhibitor.
Statistical analysis
Statistical analysis and data plotting was conducted using GraphPad Prism (GraphPad Software, San Diego, CA). Data represents the mean ± SEM. Viability IC50 values at 18 hours were calculated by line fitting normalized viability versus concentration with non-linear regression and statistical significance determined using one-way ANOVA. Differences in viability, caspase-3 activity, apoptosis, and oxidation status were analyzed using two-way ANOVA to identify differences and confirmed with paired two-tailed t-tests. Blood cytology and biochemistry results were analyzed using one-way ANOVA with Tukey’s multiple comparison test. Statistical analysis for the difference in tumor volume between treatments groups was determined with the repeated measures ANOVA. Kaplan-Meier survival curves were plotted and differences compared with a log-rank test. A p-value of less than 0.05 was considered significant for all tests.
Competing interests
No authors of this manuscript have any competing interests to disclose.
Authors’ contributions
JRH participated in the design and conduction of experiments, data analysis, and final drafting and writing of the manuscript. SV, RHM, CA, and FB all contributed new reagents for these experiments. PG and DS were involved in research design and contributed to the drafting of the manuscript. WGH was closely involved in research design and drafting of the final manuscript. All authors read and approved the final manuscript