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Calcium-dependent enhancement by extracellular acidity of the cytotoxicity of
mitochondrial inhibitors against melanoma
Fumihito Noguchi1,2,7, Shigeki Inui1, Clare Fedele2, Mark Shackleton2,3,4,5,6, Satoshi Itami1,6
1Department of Regenerative Dermatology, Graduate School of Medicine, Osaka University, 2-2,
Yamada-oka, Suita-shi, Osaka 565-0871, Japan, Tel: 81 6 6879 3032; Fax: 81 6 6879 3039,
E-mail: [email protected]
2Cancer Development and Treatment Laboratory and 3Division of Cancer Medicine, Peter
MacCallum Cancer Centre, 305 Grattan Street, Melbourne VIC 3000, Australia, Tel: 61 3 8559
5000; Fax: 61 3 8559 7379
4Sir Peter MacCallum Department of Oncology and 5Department of Pathology, University of
Melbourne, Parkville VIC 3052, Australia
6Equal contribution
7Correspondance: [email protected] ; Tel: 61 3 8559 5000; Fax: 61 3 8559
7379
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Keywords
acidic pH; OXPHOS; calcium; alkalizer therapy; ROS
Running title
OXPHOS-inhibition, calcium and pHe in melanoma
Abbreviations
pHe, extracellular pH; OXPHOS, oxidative phosphorylation; TIS, therapy-induced senescence;
ROS, reactive oxygen species; PGC1alpha, peroxisome proliferator-activated receptor gamma
coactivator 1-alpha; JARID1B, Jumonji/ARID Domain-Containing Protein 1B; OCR, oxygen
consumption rate; FCCP, trifluoromethoxy carbonyl cyanide phenylhydrazine; AIF,
apoptosis-inducing factor; ATA, aurintricarboxylic Acid; MFI, median fluorescence intensity
Disclosure of potential conflict of interest
There are no conflicts of interest.
Financial Support
F. Noguchi was supported by Uehara Memorial Foundation. M. Shackleton was supported by
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Pfizer Australia, the Victorian Cancer Agency, the Australian National Health and Medical
Research Council (NHMRC) and veski.
Abstract
Extracellular acidity is a hallmark of cancers and is independent of hypoxia. Since acidity
potentiates malignant phenotypes, therapeutic strategies that enhance the targeting of oncogenic
mechanisms in an acidic microenvironment should be effective. We report here that drugs which
abrogate mitochondrial respiration show enhanced cytotoxicity against melanoma cells in a
normoxic but acidic extracellular pH, independent from P53 mutations, BRAF (V600E)
mutations and/or resistance against BRAF inhibitors. Conversely, the cytotoxicity against
melanoma cells of mitochondrial inhibitors is impaired by a neutral or alkaline extracellular pH
and in vivo systemic alkalinization with NaHCO3 enhanced subcutaneous tumor growth and
lung metastasis of B16F10 cells in mice treated with the mitochondrial inhibitor phenformin.
Intracellular calcium (Ca2+) was significantly increased in melanoma cells treated with
mitochondrial inhibitors at an acidic extracellular pH and an intracellular Ca2+ chelator,
BAPTA/AM, inhibited cytoplasmic Ca2+ as well as melanoma cell death. Surprisingly, ROS
scavengers synergized with increased apoptosis in cells treated with mitochondrial inhibitors,
suggesting that ROS contributes to cell survival in this context. Notably, the cytotoxic
enhancement of mitochondrial inhibitors by acidity was distinct from PGC1alpha-driven
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mitochondrial addiction, from therapy-induced senescence and from slow,
JARID1B-high-associated cell cycling, all of which have been shown to promote vulnerability
to mitochondrial inhibition. These data indicate that extracellular pH profoundly modulates the
cytotoxicity of mitochondrial inhibitors against cancer cells.
Introduction
Melanoma, the most aggressive form of skin cancer, typically responds poorly to conventional
cancer therapies, including chemotherapy and radiation therapy, after it progresses and
subsequently metastasizes (1). Although new therapies such as BRAF inhibitors (e.g.
vemurafenib) and immunotherapies prolong the survival of many patients, relapses occur in
most cases (2,3). Accordingly, identifying new therapies and ascertaining ways in which to
combine and potentiate existing therapies are high research priorities in this disease.
Recently, a subpopulation was identified of proliferative but slow-cycling melanoma cells that
express the histone3 K4 demethylase JARID1B (4,5). These cells showed enhanced
mitochondrial oxidative phosphorylation (OXPHOS) and were relatively resistant to various
drugs including vemurafenib, thus playing a critical role in melanoma cell survival. Furthermore,
it was reported that the mitochondrial master regulator gene PGC1alpha is regulated in
melanoma cells through microphthalmia-associated transcription factor (MITF), the central
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melanocytic lineage regulator, resulting in mitochondrial addiction, tolerance to vemurafenib (6)
and oxidative stress (7). As PGC1alpha-driven mitochondria-addicted melanoma cells (6) as
well as JARID1B-high slow-cycling cells (5,8) are sensitive to drugs that inhibit OXPHOS
(OXPHOSi), OXPHOSi have therapeutic potential against melanoma (9-11).
Interest in OXPHOSi is also driven by links between mitochondrial activity and
therapy-induced senescence (TIS) (12). Therapies such as radiation and chemotherapy can drive
either apoptosis or senescence in cancer cells, with senescent cells appearing in tumor remnants
that remain after therapy. These cells are important as they may possess a slow-cycling,
drug-resistant phenotype that serves as a reservoir for recurrent disease (12). Importantly,
senescent cancer cells also exhibit activation of OXPHOS and sensitivity to OXPHOSi (12,13).
The extracellular pH (pHe) is acidic in most cancers due to hypoxia, insufficient perfusion and
aerobic glycolysis (the so-called “Warburg effect”), although hypoxia and extracellular acidity
often lack spatial correlation (14). The pHe is reportedly 6.2–6.9 in tumor tissues, while the pHe
is 7.3-7.4 in normal tissues (15,16). Extracellular acidity, independently from hypoxia,
facilitates malignant behaviors of cancer cells including migration, invasion,
epithelial-mesenchymal transition, metastasis, lymphangiogenesis, autophagy, mutagenesis,
chemoresistance, immune evasion and dedifferentiation (17-29). Indeed, high intratumoral
acidity is linked to poor patient prognosis (30) and alkalizer therapy that manipulates the acidic
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pHe in a tumor towards neutral was reported to inhibit tumor growth and metastasis in several
types of cancers (20,28,31,32). These observations highlight the importance of considering pHe
in cancer treatment. In this study, we assessed the effects of an acidic pHe on melanoma cells
and on modulating the anti-melanoma effects of OXPHOSi.
Materials and Methods
Cell lines and cell culture
B16F10 (ATCC Number CRL-6475) mouse melanoma cells were purchased from the American
Type Culture Collection (ATCC) (Manassas, VA, USA) in April 2009. Human melanoma cell
lines MEWO (ATCC Number HTB-65, in January 2012), SK-MEL-28 (ATCC Number
HTB-72, in October 2014) and A375 (ATCC Number CRL-1619, in November 2014) were
purchased from ATCC. Normal human dermal fibroblasts were derived from the scalp skin of a
14-year-old female patient in Jun 2003. All cell lines were stored in liquid nitrogen and
authenticated for viability a month before use. Cells were grown in Dulbecco's Modified Eagle
Medium (DMEM) (MediaTech, Herndon, VA, USA) supplemented with 4.5 g/L glucose, 2 mM
L-glutamine, 5% penicillin-streptomycin, 2.5 μg/ml amphotericin B and 10% fetal bovine serum
(FBS) at pH 7.4. All cell lines were cultured in a humidified 5% CO2 atmosphere at 37°C. The
pH of media was adjusted with hydrochloric acid, sodium hydroxide or bicarbonate to 6.2, 6.7
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and 8.0 for extracellular pH-manipulation in vitro. The medium was changed every day to
normal/acidic medium with/without oligomycin (1404-19-9, Wako Pure Chemical Industries,
Ltd, Osaka, Japan), phenformin (P7045, Sigma-Aldrich, St. Louis, MO, USA), rotenone (R8875,
Sigma-Aldrich), 2-thenoyltrifluoroacetone (TTFA) (T27006, Sigma-Aldrich), cisplatin
(15663-27-1, Wako Pure Chemical Industries, Ltd.), vemurafenib (PLX4032, RG7204) (S1267,
Selleckchem.com, Houston, TX, USA), Z-VAD-FMK (sc-3067, Santa Cruz Biotechnology,
Santa Cruz, CA, USA), Z-DEVD-FMK (FMK004, R&D Systems, Minneapolis, MN, USA),
Trolox (sc-200810, Santa Cruz Biotechnology), sodium pyruvate (sc-208397, Santa Cruz
Biotechnology), (aurintricarboxylic Acid (ATA) (sc-3525, Santa Cruz Biotechnology), E64
(sc-201276, Santa Cruz Biotechnology), antipain (sc-291907, Santa Cruz Biotechnology) and/or
BAPTA/AM (1,2-Bis(2-aminophenoxy)ethane-N,N,N′,N′-tetraacetic acid
tetrakis(acetoxymethyl ester) (sc-202488, Santa Cruz Biotechnology). To derive
vemurafenib-resistant sublines, SK-MEL-28 and A375 cells were seeded at low density, treated
with vemurafenib at 10 µM for 6 weeks and clonal colonies isolated and maintained. All in vitro
experiments were performed with cells at 70-80% confluency in normoxic conditions.
Cell viability assay
The viability of drug-treated cells at each pH was calculated using a Cell Counting Kit-8
(CCK8) (Dojindo Laboratories, Kumamoto, Japan) by the following formula: relative viability
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= value of drug-treated cells / value of cells with no treatment.
Western Blotting
Immunoblotting was performed as previously described (33). Antibodies used were: mouse
monoclonal anti-ATP synthase beta IgG (1:10000) (612518, BD Biosciences), rabbit polyclonal
anti-PGC-1 IgG (1:200) (sc-13067, Santa Cruz Biotechnology), rabbit polyclonal anti-cleaved
caspase-3 p11 IgG (1:200) (sc-22171-R, Santa Cruz Biotechnology), rabbit polyclonal
anti-cleaved caspase-6 (Asp162) IgG (1:1000) (#9761, Cell Signaling) and anti-β-actin
(1:20000) (A5441, Sigma-Aldrich).
Detection of mitochondrial membrane potential
For detection of mitochondrial membrane potential, MitoRed (PromoKine, PK-CA707-70055,
Heidelberg, Germany) was used following the manufacturer’s protocol.
Oxygen Consumption
The oxygen consumption rate was measured using a Seahorse Bioscience XF96 Extracellular
Flux Analyzer. Briefly, cells (2 × 104 /well) were cultured in XF96 tissue culture plates at pH 7.4
or pH 6.7 for 72 h and then media was changed into unbuffered XF Base Medium 1 h before the
measurement. Maximal oxygen consumption rate was measured under a mitochondrial
uncoupler trifluoromethoxy carbonyl cyanide phenylhydrazine (FCCP) (0.25 µM for
SK-MEL-28 and 0.1 µM for MEWO, respectively). The number of cells was normalized using
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CCK8.
Immunocytochemistry
Cells were fixed in 4% paraformaldehyde for 10 min at room temperature, and then
permeabilized with 0.5% Triton X-100 for 5 min. The expression of P53 and P21 was detected
by incubating cells with rabbit polyclonal anti-p53 IgG (1:100) (sc-6243, Santa Cruz) or rabbit
polyclonal anti-p21 IgG (1:100) (sc-756, Santa Cruz) for 1 h at room temperature followed by
incubation with Alexa fluor 488 conjugated goat anti-rabbit IgG. DAPI was added to label cell
nuclei. The expression of senescence associated β-galactosidase was detected using Cellular
Senescence Kit (GX0003, OZ Biosciences) following the manufacturer’s protocol. Cells were
observed using an All-in-one Fluorescence Microscope BZ-9000 (Keyence, Osaka, Japan).
Immunohistochemistry
For TUNEL staining, a TACS2 TdT in situ Apoptosis Detection Kit (Trevigen, Gaithersburg,
MD, 20877) and a ChemMate ENVISION/ HRP kit (Dako, Glostrup, Denmark) were used. In
brief, 3 μm thick tumor sections on the slides were covered with Proteinase K Solution for 15
min and were then immersed in Quenching Solution for 5 min. After washing with PBS, the
slides were immersed in 1×TdT Labeling Buffer for 5 min and were then covered with Labeling
Reaction Mix for 60 min at 37°C, followed by covering with Stop Buffer for 5 min. The slides
were then washed 2 times in deionized H2O for 5 min each, followed by treatment with alkaline
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phosphatase-conjugated streptavidin (K1018, Dako) for 15 min. Reaction products were
visualized using the Fuchsin+ Substrate-Chromogen System (K0625, Dako). 1% Methyl Green
was used as a counterstain.
Ki67 staining was performed as previously described (34). Briefly, sections were autoclaved
and stained with rabbit polyclonal anti-Ki67 IgG (1:500; Leica Microsystems, Buffalo Grove,
IL), followed by incubation and visualization with a ChemMate ENVISION/ HRP kit (Dako).
FACS analysis
Cellular ROS was labeled with CellROX Deep Red Reagent (Ex/Em = 644/665 nm) (C10422,
Life Technologies, Frederick, MD, USA) and measured using a BD FACS Canto II (BD
Biosciences). Briefly, cells were treated with the reagent (5 μM) with/without the drug(s) at pH
7.4 or 6.7 and were then incubated at 37°C for 30 min and collected. Menadione (100 μM,
M5625, Sigma-Aldrich) was used for a positive control. After distinguishing dead cells, median
fluorescence intensities (MFIs) of cells were determined (Ex/Em = 650/660 nm). MFIs of cells
in each condition were normalized to cells at pH 7.4 with no treatment.
For apoptosis assays, cells were cultured with/without the drug(s) at pH 7.4 or 6.7 for the
indicated periods and then apoptotic cells were detected using FITC Annexin V (640905,
BioLegend, San Diego, CA, USA) according to the manufacturer’s protocol using a BD FACS
Canto II.
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For intracellular calcium measurement, cells were cultured with/without the drug(s) at pH 7.4 or
6.7 for the indicated periods and then loaded with Fluo3/AM (sc-202612, Santa Cruz
Biotechnology) (5 μM) in PBS at 37°C for 1 h. After 2 washes, cells were cultured in PBS at
37°C for 30 min (de-esterification) and then analyzed on a BD FACS Canto II with excitation
wavelength of 488 mm. For cell sorting, cells stained by Fluo3/AM were analyzed on a BD
FACS Aria and sorted by Fluo3/AM fluorescence.
For cell cycle analysis, 1×105 cells were fixed with ice cold 70% EtOH for 4 h and then
suspended in DNA staining solution including 2.5 μg/ml propidium iodide and 0.5 mg/ml
RNase A in PBS. They were then analyzed using a BD FACS Canto II.
For analysis of JARID1B expression after incubation with/without the drug(s) at pH 7.4 or 6.7
for the indicated periods, 1×106 cells were fixed in 70% ethanol for 10 min on ice and then
washed with 2% bovine serum albumin (BSA) in PBS. Cells were then incubated with rabbit
polyclonal anti-JARID1B antibody (1:1000) (22260002, Novus Biologicals, Littleton, CO,
USA) for 30 min on ice. After washing, cells were incubated with a secondary fluorescein
isothiocyanate conjugated anti-rabbit antibody for 20 min on ice and analyzed using a BD FACS
Canto II.
Measurement of lactate
Measurement of lactate was performed using a Lactate Colorimetric Assay Kit II (#K627,
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BioVision, Milpitas, CA, USA). Briefly, cells were seeded (5×103/well) in 96-well plates and
were incubated at pH 7.4 or 6.7 for the indicated periods. The culture medium of each well was
then recovered and mixed with Reaction Mix. After incubation for 30 min at room temperature,
OD 450 nm was measured using a microplate reader. Values were normalized by the number of
viable cells evaluated using the CCK8 kit. The values of cells in acidic conditions were
normalized to cells at pH 7.4.
Measurement of ATP
Cellular ATP was measured using “Cellno” ATP ASSAY reagent (CA50, Toyo Inc, Tokyo,
Japan). Briefly, cells were seeded (5 × 103/well) in 96-well plates and incubated at pH 7.4 or 6.7
with/without the drug(s) for the indicated periods. The reagent was added to each well and the
plates were stirred for 1 min. Luminescence was measured using a CentroXS3 LB960 plate
reader (Berthold Technologies, Bad Wildbad, Germany). Values were normalized as described
in the section of Lactate measurement.
Animals
All animal studies were performed according to protocols approved by the Institutional Animal
Care and Use Committee at Osaka University. C57BL/6J mice (7-week-old, female) were
purchased from Nippon Charles River (Tokyo, Japan). Mice were maintained under light/dark
(12 h/12 h) cycles with free access to standard chow and water. For mice treated with oral
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administration of NaHCO3, water was replaced with 200 mM NaHCO3.
Subcutaneous tumor growth
For studies of subcutaneous tumor growth, mice (n = 6 per group) were inoculated with 2.5×105
B16F10 cells in their flanks. Mice were randomly divided into four groups: a) no treatment, b)
oral administration of 200 mM NaHCO3 ad libitum, c) daily intraperitoneal injection (i.p.) of
100 mg/kg phenformin, and d) both NaHCO3 and phenformin. Treatments started from the day
of inoculation and were continued for the duration of the experiment. Tumor diameters were
measured at the indicated time points. Tumor volumes were estimated by V = (a2×b)/2, where ‘a’
is the short axis and ‘b’ is the long axis of the tumor.
Metastasis assay
Mice were injected intravenously with 5 × 104 B16F10 cells in 0.1 ml PBS via the tail vein and
were treated daily with phenformin (100 mg/kg, i.p.) and/or NaHCO3 (200 mM, oral
administration ad libitum) from the day of injection, which continued for the duration of the
experiment (n = 5 per group). After 21 days, mice were sacrificed and their lungs resected and
photographed. The numbers of metastases on the surfaces of the lungs were counted
macroscopically.
Statistics
Data are expressed as means ± SE. To compare two mean values, an unpaired Welch’s t test was
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used. For comparisons of multiple mean values, a Tukey-Kramer test following a single-factor
ANOVA was used. For subcutaneous tumor growth analysis, an unpaired Welch’s t test was
used. For metastasis analysis, a nonparametric Mann-Whitney U test was used. Differences of
*P <0.05 were considered statistically significant.
Results
Extracellular pH modulates the cytotoxicity of OXPHOSi on melanoma cells in vitro
To elucidate whether cytotoxicity of mitochondrial inhibitors on melanoma cells is affected by
pHe in vitro, we examined human melanoma cells at pH 7.4 or 6.7 treated with oligomycin
(0.01 μg/ml), an inhibitor of mitochondrial ATP synthase, or phenformin (1 mM), an
anti-diabetic drug from the biguanide class known to inhibit mitochondrial complex I. Increased
numbers of apoptotic cells were detected when A375, SK-MEL-28 or MEWO cells were
cultured with oligomycin or phenformin at an acidic pHe, while there were only modest
numbers of apoptotic cells when cells were cultured without the drugs at an acidic pHe or with
the drugs at pHe 7.4 (Fig. 1A to 1D, S1A to S1C). A similar enhancement of apoptosis was
observed in cells treated with the mitochondrial complex II inhibitor TTFA (0.1 mM) at an
acidic pHe (Fig. S1D, S1E). An increase in apoptosis was also seen in A375 cells cultured with
oligomycin at pH 6.2 rather than at pH 6.7, and even in A375 cells cultured at pH 6.2 without
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the drug (Fig. S1F, S1G). The number of apoptotic A375 cells cultured at pH 8.0 was
comparable to that at pH 7.4 (Fig. S1F, S1G). These data indicate that extracellular acidity
enhances the cytotoxic effect of OXPHOSi on melanoma cells in vitro. Interestingly,
patient-derived normal human dermal fibroblasts were also sensitive to phenformin (1 mM) at
an acidic pHe (Fig. S1J to S1L), indicating that this phenomenon occurs in normal as well as
malignant cells.
Since cancer cells in an acidic microenvironment generally acquire multidrug-resistance (15,28),
we tested the cytotoxicity of cisplatin (20 μM) on melanoma cells at varying pHe. In contrast to
the effects of OXPHOSi, A375 and SK-MEL-28 cells displayed less apoptosis following
cisplatin exposure at pH 6.7 compared to pH 7.4, although comparable levels of apoptosis were
detected across pHs after treatment of MEWO cells with cisplatin (Fig. 1E to 1G, S1H, S1I).
Since a low pHe augments the cytotoxicity of weak acids and as cisplatin is a weak acid (35),
the cytotoxicity enhancement of OXPHOSi by acidity must not merely be because cells are
damaged by acidity. Rather, OXPHOS-inhibition by these drugs may specifically cooperate with
an acidic pHe to augment cytotoxicity.
Systemic buffering attenuates the anti-cancer effect of phenformin on B16F10 cells in vivo
Given that an acidic pHe enhanced cytotoxicity of OXPHOSi (including phenformin) against
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melanoma cells in vitro (Fig. 1), we hypothesized that systemic alkali buffering with NaHCO3
would reduce anti-tumor effects of phenformin in vivo, which have been shown for cancers such
as melanoma (8,36). Since it was reported that extracellular acidity promotes immune evasion
of cancer cells (26) and that host immune responses critically affect tumor development (37),
we utilized B16F10 cells and a syngeneic allograft model using C57BL/6 mice to test this.
In preparatory in vitro work, phenformin decreased the viability of B16F10 cells at pHe 7.4 as
well as pHe 6.7 (Fig. S2A, S2B). However, far more apoptosis was induced in B16F10 cells at
the acidic pHe compared to the normal pHe (Fig. 2A, 2B). Consistent with previous studies
(8,36), in vivo tumor growth was significantly inhibited in mice treated with phenformin (148
mm3 ± 28 SE) compared to untreated mice (1504 mm3 ± 106 SE) (Fig. 2C, 2D). As
hypothesized, a significant increase in tumor growth was observed in phenformin +
NaHCO3-treated mice compared to phenformin only treated mice (303 mm3 ± 39 SE on day 16
post-injection) (Fig. 2C, 2D). Correspondingly, immunohistochemical analysis suggested that
apoptotic cells were decreased while proliferating cells were increased in tumors from
phenformin + NaHCO3-treated mice (Fig. 2E, 2F). Interestingly, tumor growth was also
inhibited in mice treated with oral bicarbonate (452 mm3 ± 81 SE on day 16 post-injection)
compared to mice without treatment (Fig. 2C, 2D), regardless of phenformin administration.
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We also evaluated experimental metastasis. Twenty-one days after injection, the number of lung
atmetastases was reduced in mice treated with daily phenformin, compared to mice with no
treatment (Fig. 2G, 2H). Noticeably, metastasis was increased in mice with daily phenformin +
NaHCO3 treatment compared to phenformin only treated mice (Fig. 2G, 2H). Collectively, these
data are consistent with the possibility that OXPHOS inhibition preferentially targets melanoma
cells in the acidic in vivo tumor microenvironment that otherwise facilitates malignant
progression.
OXPHOS-inhibition causes the activation of caspase-dependent apoptosis at an acidic pHe
We next interrogated mechanisms of action of OXPHOSi targeting in an acidic
microenvironment. Cleavage of caspase-3 as well as caspase-6 was increased in A375 cells after
treatment with oligomycin at an acidic pHe (Fig. 3A, 3B). Although the substrate-specific
caspase inhibitor Z-DEVD-FMK failed to suppress apoptosis in A375 cells after treatment with
oligomycin at pH 6.7 (Fig. S3A), the pan-caspase inhibitor Z-VAD-FMK suppressed apoptosis
in these cells (Fig. 3C, 3D). In contrast, treatment with the apoptosis-inducing factor (AIF)
specific inhibitor ATA (38) and E64 and antipain both of which inhibit cathepsin-B (39) failed to
suppress apoptosis in A375 cells treated with oligomycin at pH 6.7 (Figs. S3B and S3C). These
data indicate caspase-dependent apoptosis in the cytotoxicity of OXPHOSi elicited by acidity.
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Inhibition of both caspase-3 and caspase-6 by Z-VAD-FMK, but not caspase-3-specific
inhibition by Z-DEVD-FMK, may be necessary to suppress apoptosis in A375 cells treated with
oligomycin at an acidic pHe.
Intracellular Ca2+ level is increased in melanoma cells after treatment with OXPHOSi at
an acidic pHe
Since oxidative stress increases the concentration of intracellular Ca2+ (40), leading to
intracellular Ca2+ overload and apoptosis (41), we next tested if intracellular Ca2+ is altered in
melanoma cells after treatment with OXPHOSi at an acidic pHe. When A375 cells were treated
with the OXPHOSi at pH 6.7, large fractions of surviving cells showed high cytoplasmic Ca2+.
This was not seen following OXPHOSi at pH 7.4 or at pH 6.7 without OXPHOSi (Fig. 4A, 4B).
Similar results were obtained with SK-MEL-28 cells and MEWO cells (Fig. S4A to S4D). The
viable Ca2+-high cell population induced by OXPHOSi at pH 6.7 was impaired, as A375 cells
sorted from the propidium iodide-excluding Ca2+-high gate showed markedly impaired in vitro
proliferation (Fig. 4C to 4E). The importance of intracellular Ca2+ in this context was further
revealed by treatment with BAPTA/AM, an intracellular calcium chelator, which decreased
Ca2+-high cells as well as death in A375 cells treated with oligomycin at pH 6.7 (Fig. 4F to 4I).
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These results indicate that intracellular Ca2+ overload contributes substantially to the enhanced
cytotoxicity of OXPHOSi in an acidic pH.
ROS scavenging synergizes with OXPHOSi against melanoma cells in an acidic pHe
Cytotoxicity of OXPHOSi against cancer cells may be due to deleterious effects of ROS
production (12). Since extracellular acidosis enhances ROS in cancer cells (42,43), we next
studied whether increased ROS production in melanoma cells at acidic pHe modulates the
cytotoxic effects of OXPHOSi. As expected, ROS production in A375 and MEWO cells was
significantly increased after OXPHOS-inhibition at pH 6.7 compared to pH 7.4 and Trolox and
Sodium pyruvate, both ROS scavengers, suppressed ROS production at pH 6.7 (Fig. 5A, S5A).
However, when ROS production was suppressed after treatment with OXPHOSi at pH 6.7,
more rather than less apoptosis was unexpectedly seen in both A375 (Fig. 5B to 5E) and
MEWO cells (Fig. S5B to S5E). As a moderate increase of ROS correlates with aggressive
cancer cell phenotypes (44), these data raise the possibility that OXPHOSi in an acidic pH
increases ROS to a threshold that provides a level of adaptive cytoprotection that may be
exploited therapeutically by concurrent ROS scavengers (44).
Enhanced cytotoxicity in melanoma cells of OXPHOSi in acid pHe is independent of
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PGC1alpha
PGC1alpha is up-regulated in some melanoma cells, resulting in mitochondrial addiction,
tolerance to oxidative stress (7) and vulnerability against OXPHOSi (6). As expected (7), we
found that MEWO cells robustly expressed PGC1alpha (Fig. 6A). Interestingly, expression of
PGC1alpha and ATP synthase were increased by acidification in MEWO cells, indicating the
activation of OXPHOS (Fig. 6A). Consistent with this, mitochondrial membrane potential was
activated (Fig. 6B) and oxygen consumption rate was increased (Fig. 6D) in acid pHe,
suggesting that acidification potentiates mitochondrial activity in MEWO cells. However,
although SK-MEL-28 and A375 cells were also sensitive to OXPHOSi at acidic pHe, they
expressed very low levels of PGC1alpha (Fig. 6A) and had much lower mitochondrial
membrane potentials and oxygen consumption rates after acidification (Fig. 6B, 6C). This
argues against a consistent PGC1alpha-dependency of the cytotoxicity elicited by OXPHOSi in
acidic pHe (6,7).
Melanoma cells at an acidic pHe acquire senescent phenotypes that do not mediate the
cytotoxicity of OXPHOSi
To examine further potential mechanisms of OXPHOSi cytotoxicity in acidic pHe and as cells
undergoing senescence have increased sensitivity to OXPHOSi (12,13), we tested whether
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melanoma cells that survive an acidic milieu are senescent (12). Some cell lines showed some
but not all features of senescence in acidic pHe. Consistent with previous data (17), A375 cells
were slow-cycling and had increased G1 phase cells (Fig. S6A to S6C). SK-MEL-28 cells, but
not A375 or MEWO cells, showed increased expression of senescence-associated
β-galactosidase (Fig. S6G) (45). In metabolism studies, both lactate and ATP production were
increased by acidification in A375, SK-MEL-28 and MEWO cells (Fig. S6H, S6I), consistent
with a hyperactive hybrid metabolism, characterized by increased glycolysis as well as
mitochondrial respiration, that is linked to the senescent state (12,13). However, A375 and
SK-MEL-28 cells did not display increased mitochondrial membrane potential after
acidification (Fig. 6B, 6C), which would be expected of senescent cells (12). As P53 and P21
upregulation characterize the senescent state, we also tested expression of these proteins in
acidic pHe in A375, SK-MEL-28 and MEWO cells, with contrasting results. Although P53 and
P21 were increased after acidification in A375 cells (which harbor wild-type p53 (46)) (Fig.
S6D), neither protein was increased in MEWO cells (which carry p53 mutations (47)) (Fig.
S6F). In SK-MEL-28 cells, which are also p53 mutant (48), P53 but not P21 was increased after
acidification (Fig. S6E). Thus, P53 and P21 expression was not consistently linked to sensitivity
to OXPHOSi. Altogether, these data indicate that although some melanoma cells at an acidic
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pHe show some features of senescence, this phenotype is not unequivocally and universally
linked to the cytotoxicity conferred by OXPHOSi in an acidic pHe.
The JARID1B-high population is not increased in melanoma cells by an acidic pHe
Treatment with vemurafenib has been shown to enrich JARID1B-high slow-cycling melanoma
cells, which are sensitive to OXPHOSi (5). Since melanoma cells exhibited enhanced sensitivity
to OXPHOSi after acidification, we also tested whether JARID1B-high cells are increased by
acidification. SK-MEL-28-R and A375-R cells, resistant to vemurafenib, were generated from
SK-MEL-28 and A375 cells, which harbor a homozygous BRAF (V600E) mutation (Fig. 6E,
S6J). Apoptotic SK-MEL-28-R and in A375-R cells were significantly increased by treatment
with oligomycin at pH 6.7, compared to oligomycin at pH 7.4 or untreated cells at pH 6.7 (Fig.
6F, 6G, S6K, S6L). However, this was not associated with an increase in JARID1B-high cells at
pH 6.7 (Fig. 6H), although JARID1B-high SK-MEL-28-R cells were decreased after treatment
with oligomycin or rotenone at pH 6.7 (Fig. 6I). JARID1B-high A375-R cells were also
decreased after treatment with oligomycin or rotenone at acidic pHe (Fig. S6M, 6I). Thus, the
augmented sensitivity of melanoma cells to OXPHOSi at an acidic pHe cannot be attributed to
increased JARID1B-high cells in an acidic milieu. Despite this, the vulnerability of
JARID1B-high cells to OXPHOSi is preserved after acidification.
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Discussion
We demonstrate that the cytotoxicity of OXPHOSi against melanoma is strongly mediated by
pHe. Since not only melanoma cells but also normal human dermal fibroblasts are relatively
protected against phenformin by a neutral pH (Fig. S1J to S1L), the neutral pHe in normal
tissues (15,16) should ameliorate potential side-effects in patients of OXPHOSi, while
preserving cytotoxic effects that will be more specific for acidic tumor microenvironments. On
the other hand, when tissue physiological oxygenation is disturbed in patients with pathological
conditions like severe diabetes, coronary heart disease or stroke (49), acidosis can occur in
involved organs and tissues. It is thus possible that OXPHOSi could exert untoward toxicities
on non-malignant tissues that are unusually acidotic as a result of non-malignant pathological
conditions.
As an acidic pHe promotes aggressive phenotypes in cancers (15), manipulation of intratumoral
pHe has been considered as a potential cancer therapy (32,50,51). Systemic buffering by oral
administration of NaHCO3 increased intratumoral pHe and inhibited local invasion and tumor
growth in breast and in colon cancer cells (20). Moreover, treatment with oral bicarbonate
increased the average tumor pHe from 7.0 to 7.4 and inhibited the spontaneous metastasis of
metastatic breast and prostate cancer cells in immunodeficient mice (31). Our data show that the
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acidic microenvironment that promotes tumor progression also renders cancer cells susceptible
to therapies that target mitochondrial metabolism, and that systemic alkalinization ameliorates
this susceptibility.
It is notable that the vulnerability of melanoma cells to OXPHOSi in acidic pHe was
independent of P53 mutation status, BRAF (V600E) mutation status and resistance against
vemurafenib. This indicates potential application of OXPHOSi across a range of clinical
contexts, such as a second-line treatment against drug-resistant melanomas or combined with
first-line therapies (12) to reduce primary resistance. Regardless, identifying biomarkers of
acidic pHe, perhaps by tumor sampling (52,53), will be important to identify subgroups of
patients likely to respond to OXPHOSi, as recent clinical trials in unselected patients failed to
show improved survival in cancer patients treated with OXPHOSi (54,55). Clearly, concurrent
use of alkalizer therapy and OXPHOSi should not be applied to melanoma patients.
In examining mechanisms of action of the increased susceptibility of melanoma cells to
OXPHOSi in acidic pHe, we unexpectedly found that this vulnerability is not consistently
dependent on PGC1alpha (6,7), induction of senescence (12) or JARID1B expression (5,8).
Rather, we found that caspase- and pHe dependent apoptotic effects of OXPHOSi were closely
linked to increased intracellular calcium levels. The role of calcium in regulating cell
metabolism in some pathophysiological states is well understood. For example, myocardial cells
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undergo intracellular Ca2+ overload upon myocardial ischemia-reperfusion injury (56). In this
context, a decrease in extracellular as well as intracellular pH during ischemia leads to Na+/H+
exchange and Na+ overload in myocardial cells. Subsequently, Ca2+ uptake occurs through
reverse-mode Na+/Ca2+ exchange, resulting in intracellular Ca2+ overload. Concurrently
impaired ATP production in mitochondria inhibits Ca2+ extrusion by plasmalemmal Ca2+-ATPase,
compounding the intracellular Ca2+ increase, which results in mitochondrial-driven myocardial
cell apoptosis (40,41,56,57).
We speculate that the acidification of melanoma cells mimics this by inducing compensatory ion
fluxes that increase intracellular calcium to synergize with reduced ATP production conferred by
OXPHOSi. On the other hand, in A375 and SK-MEL-28 cells mitochondrial activities are
already decreased at acidic pHe without OXPHOSi (Fig. 6B, 6C). Therefore, it is possible that
inhibition of OXPHOS at acidic pH might induce intracellular Ca2+ increase and activation of
cell death signaling pathway in a manner independent from a decrease in ATP production
(58,59), although further studies are needed to address this mechanism. Our demonstration of
intracellular Ca2+ overload and activation of apoptosis in acidic melanoma cells after treatment
with OXPHOSi (Fig. 3, Fig. 4, Fig. S3, Fig. S4) suggests that the combination of OXPHOSi and
drugs that increase cytoplasmic Ca2+ level via manipulating Ca2+ channels, pumps or storage
(57) might have synergistic cytotoxicity against melanoma cells. This highlights the importance
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of understanding complex interactions between cell metabolism, tumoral pHe and ionic
homeostasis in developing novel therapy combinations that target specific susceptibilities in
cancer cells.
Acknowledgements
We appreciate Professor Seiji Takashima and Dr. Yasunori Shintani, Department of Medical
Biochemistry, Osaka University Graduate School of Medicine, for provision of convenience in
measuring oxygen consumption rates. We also greatly appreciate Ms. Ayako Sato, Ms. Yuko
Yoshikawa and Ms. Miyuki Nakamura for their technical assistance.
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Figure Legends
Figure 1. pHe is a threshold that modulates the cytotoxicity of OXPHOSi on melanoma
cells in vitro
A, Representative microscopic images of A375 and of MEWO cells treated with/without
oligomycin (0.01 µg/ml) or phenformin (1 mM) at pHs of 7.4 and 6.7 for 48 h (A375) or 72 h
(MEWO) (magnification × 100). Bar, 100 µm.
B, C, D, Apoptosis (late apoptotic + early apoptotic) detected in A375 and in MEWO cells after
treatment with/without oligomycin (0.01 µg/ml) or phenformin (1 mM) for 48 h (A375) or 72 h
(MEWO). (n = 3).
E, Representative microscopic images of A375 cells treated with/without cisplatin (20 µM) for
48 h at pHs of 7.4 and 6.7 (magnification × 100). Bar, 100 µm.
F, G, Apoptosis (late apoptotic + early apoptotic) detected in A375 cells after treatment
with/without cisplatin (20 µM) at pHs of 7.4 and 6.7 for 72 h (n = 3).
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Images are representative of 3 independent experiments. Bars = means ± SE. **P<0.01, N.S.,
not significant.
Figure 2. Systemic buffering attenuates the anti-cancer effect of phenformin on B16F10
cells in vivo
A, B, Apoptosis (late apoptotic + early apoptotic) detected in B16F10 cells after treatment
with/without phenformin (1 mM) at pH 7.4 or 6.7 for 48 h (n = 3).
C, Representative images of tumors in each group of mice 15 days after the subcutaneous
injection of B16F10 cells; dashed lines indicate areas of tumors.
D, Tumor volumes after the subcutaneous injection of B16F10 cells in mice with the indicated
treatments (n = 6). Bars = means ± SE. *P <0.05, **P<0.01.
E, F, TUNEL and Ki67 staining of tumors 16 days after treatment with phenformin with/without
NaHCO3 (magnification × 200). Bars, 100 µm. Arrows indicate Ki67-positive nucleuses.
Images are representative of 3 independent experiments.
G, Representative photographs of lungs resected from mice treated with/without phenformin
and/or NaHCO3 for 21 days after the intravenous injection of B16F10 cells.
H, Numbers of metastases on the surfaces of lungs (n = 5). Bars = means ± SE. *P <0.05,
**P<0.01, N.S., not significant.
Figure 3. OXPHOS-inhibition causes the activation of caspase-dependent apoptosis at an
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acidic pHe
A, Western blot analysis of cleaved caspase-3 p11 in A375 cells after treatment with/without
oligomycin (0.01 µg/ml) and/or Z-DEVD-FMK (10 µM) at pH 7.4 (N) or 6.7 (A) for 48 h; 9 μg
total protein extract was loaded in each lane.
B, Western blot analysis of cleaved caspase-6 in A375 cells after treatment with/without
oligomycin (0.01 µg/ml) and/or Z-VAD -FMK (100 µM) at pH 7.4 (N) or 6.7 (A) for 48 h; 9 μg
total protein extract was loaded in each lane.
C, D, Apoptosis (late apoptotic + early apoptotic) detected in A375 cells after treatment with
oligomycin (0.01 µg/ml), phenformin (1 mM) and/or Z-VAD-FMK (100 µM) at pH 6.7 for 48 h
(n = 3).
Images are representative of 3 independent experiments. Bars = means ± SE. *P <0.05, N.S., not
significant.
Figure 4. Intracellular Ca2+ level is increased in melanoma cells after treatment with
OXPHOSi at an acidic pHe, leading to cell death
A, A375 cells were treated with indicated drugs at pH 7.4 or pH 6.7 for 16 h and stained by
Fluo3/AM. Oligomycin: 0.01 μg/ml, Phenformin: 1 mM, TTFA: 0.1 mM
Images are representative of 3 independent experiments.
B, The ratio of A375 cells which show high (Ca-h) and low-intermediate (Ca-m) cytoplasmic
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Ca2+ level after treatment with the OXPHOSi at pH 7.4 or pH 6.7. (n = 3).
C, D, A375 cells were cultured with oligomycin (0.01 μg/ml) at pH 6.7 for 16 h. Ca-m/Ca-h
cells were sorted and cultured at pH 7.4 (2000/well).
E, Sorted cells were seeded in 24 well plates (2000/well) and cultured at pH 7.4. The number of
viable cells was counted and normalized to that of day 1(n=3).
Images are representative of 3 independent experiments.
F, A375 cells were treated with BAPTA/AM (1 μM) 1 h before treatment with Oligomycin (0.01
μg/ml) for 24 h at pH 6.7 and stained by Fluo3/AM.
G, The ratio of dead cells in the cells treated with oligomycin and oligomycin + BAPTA/AM (n
= 12).
H, I, The ratio of Ca-h/Ca-m cells in the cells treated with oligomycin or oligomycin +
BAPTA/AM (n = 12).
Images are representative of 12 independent experiments.
Bars = means ± SE. *P <0.05, **P<0.01.
Figure 5. ROS scavenging synergizes with the cytotoxicity enhancement of OXPHOSi
elicited by acidity
A, Measurement of ROS production in A375 cells after treatment with/without oligomycin
(0.01 μg/ml) and phenformin (1 mM) with/without Trolox (100 µM) or Sodium pyruvate (10
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mM) for 30 min at pHs of 7.4 and 6.7 (n = 3). The MFI of cells in each condition was
normalized to cells with no treatment at pH 7.4.
B to E, Apoptosis (late apoptotic + early apoptotic) detected in A375 cells after treatment
with/without oligomycin (0.01 µg/ml), phenformin (1 mM), TTFA (0.1 mM) with/without
Trolox (100 µM) (B, C) or Sodium pyruvate (10 mM) (D, E) at pH 6.7 for 48 h (n = 3). Trolox
and Sodium pyruvate were pre-treated 1 h before OXPHOS-inhibitors.
Images are representative of 3 independent experiments. Bars = means ± SE. *P <0.05,
**P<0.01, N.S., not significant.
Figure 6. The cytotoxicity enhancement of OXPHOSi elicited by acidity is distinct from
PGC1alpha-driven mitochondrial addiction and JARID1B-high slow-cycling cells
A, Western blot analysis of PGC1alpha and ATP synthase after acidification of melanoma cell
lines; 9 μg total protein extract was loaded in each lane.
B, MitoRed staining of melanoma cell lines cultured at pH 7.4 or 6.7 for 72 h (magnification ×
200). Bar, 100 µm.
C, D, Basal and maximal oxygen consumption rates in SK-MEL-28 or MEWO cells after
acidification for 72 h (n = 12).
E, Viability of SK-MEL-28 and SK-MEL-28-R cells after treatment with vemurafenib
(PLX4032, 10 µM) at the indicated concentration for 72 h. The value of vemurafenib-treated
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cells was normalized to cells with no treatment (n = 6).
F, G, Apoptosis (late apoptotic + early apoptotic) in SK-MEL-28-R cells after treatment
with/without oligomycin (0.01 μg/ml) at pH 7.4 or 6.7 for 72 h (n = 3).
H, FACS analysis of JARID1B-positive cells after acidification of SK-MEL-28 and
SK-MEL-28-R cells for 72 h. The ratio of JARID1B-positive cells are shown.
I, FACS analysis for JARID1B-positive cells after treatment of SK-MEL-28-R and A375-R
cells with/without oligomycin (0.01 µg/ml) for 48 h at pH 6.7. The ratio of JARID1B-positive
cells are shown.
Images are representative of 3 independent experiments. Bars = means ± SE. *P <0.05,
**P<0.01.
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Published OnlineFirst February 21, 2017.Mol Cancer Ther Fumihito Noguchi, Shigeki Inui, Clare Fedele, et al. cytotoxicity of mitochondrial inhibitors against melanomaCalcium-dependent enhancement by extracellular acidity of the
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