Upload
others
View
2
Download
0
Embed Size (px)
Citation preview
Studies on the synergistic effects of combined treatment of
gamma-tocotrienol and statin on human malignant
mesothelioma cells
2014
Guligena Tuerdi
1
Contents
List of abbreviations…………………………………….…………………………….…..2
Preface………………………………………………………………………………….…...4
Chapter1 Synergistic effect of combined treatment with gamma-tocotrienol and
statin on human malignant mesothelioma cells……………………………...8
Introduction…………………………………………………………………………….8
1.1 Cytotoxic effects of a combined treatment with gamma-T3 and statin…..…..9
1.1.1 Materials and methods…………………………………………………………9
1.1.2 Results……………………………………………………………………..…….12
1.2 Combination effects of on HMGR levels…………………………………….….…16
1.2.1 Materials and methods…………………………………………………..….…16
1.2.2 Results………………………………………………………………..……....….18
1.3 Antiproliferative effect of the mevalonate pathway and downstream
factors…………………………………………………………………………….....….20
1.3.1 Materials and methods………………………………………………..….…...20
1.3.2 Results……………………………………………………………………...…....22
1.4 Effect on intrinsic apoptosis ………………………………………………..…...…27
1.4.1 Materials and methods…………………………………………….…........…27
1.4.2 Results…………………………………………………………………....…..…29
1.5 Discussion……………………………………………………………………....…..…33
1.6 Summary………………………………………………………………………...….…37
Chapter2 Involvement of endoplasmic reticulum stress with the combination
effect of gamma-tocotrienol and statin……………………………..…….38
Introduction…………………………………………………………………..….…....38
2.1 Materials and methods………………………………………………………...……40
2.2 Results……………………………………………………………………………....…42
2.3 Discussion……………………………………………………………………………..50
2.4 Summary………………………………………………………………………………53
Conclusion ……………………………………………………………………..…….……54
References……………………………………………………………………………….…57
List of publication……………………………………………………………..……….…69
Acknowledgements……………………………….………………………….....….….…70
Examiners……………………………………………………………………....………....71
2
List of abbreviations
・APS : ammonium peroxodisulfate
・ATV : atorvastatin
・ASK1: apoptosis signaling regulation kinase
・BPB : bromophenol blue
・BSA : bovine serum albumine
・CDDP : cisplatin
・CHOP : C/EBP-homologous protein
・DMSO : dimethylsulfoxide
・DTT : dithiothreitol
・D.W : diluted water
・EDTA : ethylenediamine-N,N,N’,N’-tetraacetic acid
・ER : endoplasmic reticulum
・FACS : fluorescence-activated cell sorter
・FBS : fetal bovine serum
・FPP : farnesyl pyrophosphate
・GGPP : geranylgeranyl pyrophosphate
・GRP78 : glucose-regulated protein 78
・HMGR : 3-hydroxy-3-methylglutaryl-CoA reductase
・IPP : isopentenyl pyrophosphate
・IE : immuno enhancer
・JNK : c-jun N-terminal kinase
・MAPK : mitogen-activated protein kinase
・MVL : mevalonate
・PBS : phosphate buffered saline
・PCR : polymerase chain reaction
・PI : propidium iodide
・PVDF : polyvinylidene difluoride
・PMSF : phenylmethanesulfonyl fluoride
・RPL : ribosomal protein L
・RT : reverse transcription
・SDS : sodium dodecyl sulfate
・SMV : simvastatin
・Sal : salubrinal
3
・SP600125 : JNK inhibitor
・SREBPs : sterol regulatory element binding proteins
・T3 : tocotrienol
・TBS : tris bufferd saline
・TE : Tris-HCl + EDTA
・TEMED : N,N,N’,N’-tetramethyl-ethylenediamine
・TM : tunicamycin
・UPR : unfolded protein response
4
Preface
Cancer continues to be a worldwide killer; there are more than 20 different types
of cancer. In 2008 approximately 12.7 million cancers were diagnosed [1] and in
2010 nearly 7.98 million people died [2]. Cancer can develop from almost any type of
cell in the body. Cancers as a group account for approximately 13% of all deaths
each year with the most common being: lung cancer (1.4 million deaths), stomach
cancer (740,000 deaths), liver cancer (700,000 deaths), colorectal cancer (610,000
deaths), and breast cancer (460,000 deaths) [3]. Cancer is caused by both internal
factors such as inherited mutations, hormones, and immune conditions and
environmental/acquired factors such as tobacco, diet, radiation, and infectious
organisms; This makes invasive cancer the leading cause of death in the developed
world and the second leading cause of death in the developing world [1,3].
Malignant mesothelioma (MM), is an aggressive, treatment-resistant tumor, which
is increasing in frequency throughout the world [4]. Moreover, although MM is still
a rare cancer, its incidence is increasing in many countries [5–8]. From 1994 to 2008
the 15-year magnitude of mesothelioma is estimated to be 174,300 in a group of 56
countries that report the disease, and 38,900 for the same 15-year period by
extrapolation to a group of 33 countries that do not systematically report the
disease [9]. Key changes that occur during the development of the disease include
the loss of the normal restraints on proliferation and the acquisition of resistance to
apoptosis, and asbestos, a complete carcinogen for mesothelial cells, plays a complex
role in altering both proliferation and apoptosis [10].
MM patients have a history of asbestos exposure. Asbestos refers to a family of six
mineral fibers and is classified into two subgroups: (i) the amphiboles, a group of
rod-like fibers including amosite (brown asbestos), crocidolite (blue asbestos),
anthophyllite, actinolite and tremolite; (ii) the serpentine group, consisting of
chrysotile (white asbestos) [11], which promotes difficult disease 30-40 years after
the exposure [12]. There is a direct causal relationship between asbestos exposure
and the development of mesothelioma, with an etiological fraction of 80% or more
[4]. And several mechanisms might account for this finding that the asbestos fibers
stick out from the lung surface and cause repeated cycles of scratching, damage,
inflammation, and repair in the adjacent parietal mesothelial cell layer [13].
Although the association between MM and asbestos is well established, other
5
carcinogenic factors must be involved in MM development because only 10% of all
MM cases occur in asbestos exposed subjects [14]. Simian virus 40 (SV40), a DNA
virus, has been implicated in the development of several cancers including MM [15].
That report showed that SV40 oncogenes could lead to malignant transformation of
mesothelial cells and used an in vitro mouse model mesothelial cells which were
more susceptible to asbestos induced apoptosis than normal mesothelial cells [15].
However, the putative involvement of SV40 in the pathogenesis of MM has become
a controversial issue, and its role remains unclear and unproved [13]. One study
showed that long-term exposure (100 days) to both SV40 and asbestos, primary
peritoneal mouse mesothelioma cells become resistant to stress induced senescence
[15]. On the other hand, occur by silencing promoter of the Cdk inhibitor p21 (p21)
through p53 inactivation by SV40 proteins and/or the weaker activation of p21 by
alternative pathways [16]. A greater reduction in p21 expression will cause greater
aggression and result in a poorer prognosis of human mesothelioma [16]. Therefore,
new therapeutic approaches are urgently needed for MM patients.
The anti-folate pemetrexed was the first licensed drug in combination with
cisplatin (CDDP) for malignant mesothelioma. Results were presented at the
Society of Clinical Oncology and the European Crohn’s and Colitis Organization in
2007 [12]. Pemetrexed is a potent inhibitor of thymidylate synthase, which is
required for DNA synthesis. A multicentre phase Ⅲ study in 448 patients
compared this drug combination with CDDP alone, and showed an improvement in
overall survival of nearly 3 months with the combination, with an objective
response rate of 41% [4]. The addition of folic acid and vitamin B12 supplementation
resulted in a significant reduction in pemetrexed related toxicity. Thus, pemetrexed
and CDDP is likely to be used widely as first-line chemotherapy for MM [17].
Vitamin E administration is an attractive alternative therapy for cancer patients.
Since the discovery of this fat-soluble vitamin in 1922, many studies have focused
on the potential health benefits and therapeutic use of α-, β-, δ- and γ-tocopherol
[18,19]. Similarly, γ-tocotrienol (γ-T3) (Fig.A), another isoform of vitamin E, induces
apoptosis in a variety of cancer cell types [20,21]. Additionally, γ-T3 has gained
much interest owing to its lipid-lowering effects in cell-based studies and especially
for its ability to lower cholesterol by inhibiting 3-hydroxymethyl-3-methylglutaryl
coenzyme A reductase (HMGR) [22]. Compared to other vitamin E isomers, γ-T3
has superiorperior abilities in anticancer, neuroprotective and cholesterol-lowering
activities [23,24]. Most recently, γ-T3 has exhibited anticancer activity in numerous
human cancers, including prostate [25], breast [26], colon [27], liver [28] cancers.
6
Statins are currently some of the most widely used pharmaceutical agents in the
world [29,30] which include atorvastatin (Fig.B), simvastatin (Fig.C), lovastatin,
and pravastatin. Their main function is to inhibit the endogenous synthesis of
cholesterol [29]; in addition to that, they appear to have pleiotropic effects such as
modulation of cell growth, apoptosis, and inflammation [31]. Statins are competitive
inhibitors of HMGR, which has been found to directly block tumor cell growth both
in vitro and in vivo [32], thus making it a unique molecular target for anticancer
therapy. Furthermore, statins have been found to induce apoptosis [33]. In most
clinical studies, the debate has centered on whether the use of statins causes
cognitive decline, diabetes mellitus [34], or cancers such as prostate [33], breast [35],
colorectal [31], liver [29], and pancreatic tumors [36]. Thus statins are attractive
therapeutic compounds for life style diseases, however, high concentration of statins
would induce severe side-effect. Clinical trials with prostate, breast, colorectal,
ovarian, and lung cancer patients determined that high-dose treatment was
associated with severe myopathy with the maximum dose of lovastatin that could be
tolerated to be 25 mg/kg, which produced a peak plasma concentration of 3.9 μM
[37]. Since the dose of lovastatin required to inhibit growth and apoptosis of cancer
cells in culture ranged between 0.1 and 100 μM, toxic doses of lovastatin must be
used to effectively treat cancer patients. Moreover, to be achieved apoptosis of
cancer cells, more than several tens μM of lovastatins was required. Therefore it
limits clinical use of statins though they possess strong anticancer effects.
The endoplasmic reticulum (ER) is an essential intracellular organelle with
multiple roles including the synthesis of nascent proteins, Ca2+ storage,
glycosylation, and the trafficking of newly-synthesized membrane and secretory
proteins. Perturbations of these processes have been demonstrated to interfere with
the proper functioning of ER, thus leading to a condition defined as ER stress [38].
Inadequate supplies of glucose affect the glycosylation of secretory pathway
proteins and ATP production, both of which lead to the accumulation of unfolded
proteins in the ER, resulting in ER stress [39]. The tumor microenvironment is
characterized by poor vascularization, low oxygen supply, and nutrient deprivation
all of which are activators of ER stress. In rapidly growing cancers, unfolded protein
response (UPR) has been shown to exert an important cytoprotective role that
assists folding of newly synthesized proteins necessary for tumor growth [40]. These
integrated mechanisms, although they may reflect tumor cell specificities related to
their metabolism or proliferation ability, could represent interesting avenue for
therapeutic strategy as their inhibition/activation would prevent tumor cell
7
adaptation to environmental challenges [41].
Thus, combination chemotherapy could optimize the effectiveness of each drug by
inciting a complimentary and synergetic therapeutic response while concurrently
reducing toxic adverse side effects associated with high-dose single-agent therapy.
In this context, the present study for the first time investigates the possible
synergistic effects of γ-T3 in combination with statin in human MM cell lines. As
estimated molecular targets, we concentrated on HMGR expression and the
following signaling (common targets of γ-T3 and statins), ER stress markers
(targets of γ-T3), and intrinsic apoptotic factors; Bcl-2 family in mitochondria and
caspase 3 (common targets of γ-T3 and statins).
Fig. A structural formula of tocotrienol
Fig. B structural formula of atorvastatin Fig. C structural formula of simvastatin
R1
HO
R2
R3
O CH3
CH3CH3 CH3 CH3
R1 R2 R3
α -tocotrienol CH3 CH3 CH3
β -tocotrienol CH3 H CH3
γ -tocotrienol H CH3 CH3
δ -tocotrienol H H CH3
2
NNH
OH3C CH3
O-
OOH OHHH
F
Ca2+
3H2O
CH3H
O
H3C
H
H
O
OOH
O
CH3H3C
H3C
8
Chapter1
Synergistic effect of combined treatment with gamma-tocotrienol
and statin on human malignant mesothelioma cells
Introduction
The product of HMGR, mevalonate (MVL), is the precursor for many important
intermediates in a pathway commonly known as “mevalonate pathway”. Inhibition
of HMGR leads to block the formation of many intermediate products such as
farnesyl pyrophosphate (FPP) and geranylgeranyl pyrophosphate (GGPP), which
isoprenylate various proteins, including small G-proteins such as the Ras/Rho super
family proteins [42]. Ras communicates with a number of downstream targets
involved in cell function. Two targets, the PI3K/Akt pathway and the
Raf/MEK/MAPK/ERK pathways are involved in apoptosis and cell cycle progression.
Therefore, the cancer prevention activity reported for statin is believed to be due to
their inhibition of isoprenylation of G-proteins and subsequent alteration of
downstream signaling pathways. On the other hand, the mechanisms of action by
which γ-T3 and statins suppress HMGR activity are different [43]. In most cases,
the combination of γ-T3 with statin exhibits better anticancer activity than either
agent alone [26,27,44,45]. For example, combining low dose γ-T3 and statin was
shown to inhibit the growth of highly malignant mammary epithelial cells [44]. In
addition, atorvastatin (ATV) and γ-T3 exhibited a strong synergistic effect against
human colon cancer cells and caused cell cycle arrest and apoptosis [27]. Moreover,
both γ-T3 and statin also have reported to have HMGR-independent targets. For
example, statins inhibit the protein degradation machinery, specifically the
proteasomes. Inhibition of proteasome activity is likely to be related to the effect of
statins in G1 cell cycle arrest [27]. In general, statins exert their cancer prevention
effects by regulating several disease-associated cellular events including
inflammation, immunomodulation, angiogenesis, apoptosis and proliferation [26,27].
With regard to γ-T3, it has been well-studied about its endoplasmic reticulum (ER)
stress inducing effect. Wali et al. suggested that levels of HMGR (it is an
ER-transmembrane enzyme) decreased following γ-T3 treatment but it might not be
required for γ-T3 induced apoptosis, whereas ER stress apoptotic signaling was
associated with γ-T3-induced apoptosis in mammary tumor cells [20].
9
1.1Cytotoxic effects of a combined treatment with gamma-T3
and statin
In chapter 1-1, present study is the first to demonstrate the synergetic effect of
statins (atorvastatin; ATV and simvastatin; SMV) and gamma-tocotrienol (γ-T3) on
human malignant mesothelioma (MM) at 24 and 48 h.
1.1.1 Materials and methods
[Cell lines and culture conditions]
The human MM cell lines H2052 (a sarcomatoid), H28 (an epithelioid), H2452
(an epithelioid), and MSTO-211H (a biphasic; MSTO) cells were obtained from
the American Type Culture Collection (Rockville, MD, USA) and were cultured
in RPMI-1640 medium.
MSTO and H2052 cells were grown in medium containing 10% fetal bovine
serum (FBS) (Equitech-Bio, Kerrville, TX, USA), 0.5 units/mL of penicillin,
and 1 μg/mL of streptomycin.
H2452 and H28 cells were grown in the same medium supplemented with 4.5
g/L of glucose, 1 mM sodium pyruvate, and 10 mM HEPES buffer solution
(GIBCO, Life Technologies Japan Ltd., Minato-ku, Tokyo, Japan). All cell
lines were maintained at 37 °C in a fully humidified atmosphere of 5% CO2.
[Reagents]
All cultures and reagents were purchased from Sigma Chemical Company (St.
Louis, MO, USA) unless otherwise indicated. γ-T3 was a gift from Dr. Yano T (Toyo
University). Simvastatin (SMV) was purchased from Cayman Chemical Company
(Ann Arbor, MI, USA) and atorvastatin (ATV) was purchased from LKT
Laboratories, Inc. (St. Paul, MN, USA).
1) RPMI1640 (SIGMA)
2) FBS (EQUITECH-BIO, SIGMA)
3) Penicillin-Streptomycin (Antibiotics) (GIBCO)
4) 100mM Sodium Pyrvate (GIBCO)
5) HEPES Buffer Solution (1M) (GIBCO)
6) D-Glucose (GIBCO)
10
7) Dulbecco’s PBS(-) (Nissui Pharmaceutical Co.,Ltd)
8) 0.25% Trypsin-EDTA solution (SIGMA)
9) 0.4% Trypan blue solution (SIGMA)
10) Dimethyl sulfoxide(DMSO) (Wako)
11) Ethanol(Wako)
12) T3 content 39.3% of γ-T3
→γ-T3 is 3mM Was dissolved in FBS and ethanol.
13) Simvastatin (SMV) (Cayman Chemical)
14) Atorvastatin (ATV) (LKT Laboratories, Inc)
→Was dissolved in DMSO so that the 100mM.
3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT) (DOJINDO)
→MTT was dissolved in PBS so as to have a 5 mg / ml, was prepared at the
time to 0.25 mg / ml by using (1% Antibiotics) serum-free medium.
[Cytotoxicity assay (MTT assay)]
Cytotoxicity studies were performed in 96-well plates. The cells were cultured at a
density of 3.0 × 103 cells per well in 100 μL of RPMI-1640 medium for 24 h, then
started incubation with γ-T3, statin (ATV, SMV), combination of “γ-T3 + ATV” and
“γ-T3 + SMV”. After the cells were incubated for 24 or 48 h, 100 μL of MTT
solution (500 μg/mL) was added to each well and incubated for 1 h. Formazan
crystals were dissolved in DMSO (100 μL/well). The absorbance was measured at
540 nm with a Multiskan JX microplate reader (Thermo Lab Systems, Cheshire,
UK).
[Cell cycle analysis]
Cells were plated at a density of 2.0 × 105 cells in a 60-mm dish and incubated
for 24 h prior to treatment with γ-T3, statin (ATV, SMV), or a combination of γ-T3
and statin for 24 h. Thereafter, the cells were collected and fixed in 70% ice-cold
ethanol at −30 °C. Before the analysis, the cells were treated with 200 μg/mL
RNase A and 50 μg/mL of propidium iodide for 30 min in the dark at 37 °C. The
stained cells were analyzed using flow cytometry by using a MoFlo cell sorter (Dako
Cytomation, Kyoto, Japan).
[Statistical analysis]
We performed at least three independent experiments, and all data are presented
as mean ± standard deviation (SD) or standard error of the mean (SEM).
11
Statistical analysis was performed using the Tukey–Kramer test for the comparison
of multiple groups. Values with p < 0.05 were considered statistically significant.
12
1.1.2 Results
The cytotoxic effects of γ-T3 and statin either alone or in combination on human
MM cells were examined. As shown in Fig. 1.1.1, ATV (Fig. 1.1.1a) and SMV (Fig.
1.1.1b) decreased the cell viability of human MM cells; however, each statin alone
did not exert significant effects compared to the control. Compared to γ-T3 or statin
alone, the combination treatment significantly inhibited the growth of human MM
cells. Additionally, the combination treatment effect occurred in a time-dependent
manner. To examine the mechanism of the combination effect, MSTO and H2452
cells, which were especially sensitive to the combination among four cell lines, were
selected for the experiments that follow.
DNA damage causes cell cycle arrest. Cells with irreversible damage might
undergo apoptosis, causing an accumulation of cells in sub-G1 phase [46]. As shown
in Fig. 1.1.2, almost no phase shift was observed in MSTO cells that were treated
with γ-T3 (20 μM), ATV, or SMV (6.25 μM) alone for 24 h. On the other hand, the
sub-G1 population appeared to slightly increase in the group treated with a
combination of γ-T3 and statin. This population was also higher in groups treated
with ATV or SMV for 48 h than that in untreated control cells. Moreover, there was
a 3- to 8-fold increase in sub-G1 cells in groups treated for 48 h with a combination
of γ-T3 and ATV (or SMV) than in untreated control cells.
13
(a) γ-T3+ATV
14
Fig. 1.1.1 Effects of γ-T3 given alone or in combination with statins on human
MM cells. Cells (MSTO, H2452, H2052, and H28) were seeded in 96-well plates and
treated for 24 or 48 h with γ-T3 (20 μM) alone or in combination with (a) ATV (6.25
μM) or (b) SMV (6.25 μM). Cell viability was evaluated using the MTT assay. Data
are expressed as mean ± S.D of at least three independent experiments.
Significant differences between each of the indicated groups were determined using
the Tukey–Kramer test. **p < 0.01; ***p < 0.001.
(b) γ-T3+SMV
15
(a)
Fig. 1.1.2 Effects of combination treatment with γ-T3 and statins on the cell cycle
distribution in MSTO cells. Cells were treated with γ-T3 (20 μM) alone or in
combination with ATV (6.25 μM) or SMV (6.25 μM) for (a) 24 h or (b) 48 h. Each
parameter was determined using fluorescence-activated cell sorting (FACS)
analysis. Columns represent the mean value of a relative percentage of cells in each
cell cycle phase over the time course. Data were obtained from three independent
experiments.
control γT3 ATV γT3
+ATV
γT3
+SMV
SMV
control γT3 ATV γT3
+ATV
γT3
+SMV
SMV
(b)
16
1.2 Combination effects of on HMGR levels
In chapter 1-2, demonstrate the synergetic effect of statins (ATV and SMV) and
γ-T3 on human MM cells. Involvement of Mevalonate upstream pathway HMGR
mRNA expression.
1.2.1 Materials and methods
[Cell lines and culture conditions]
Refer to 1.2.1 Materials and methods.
[Real-time RT-PCR analysis]
Total RNA was isolated using an RNeasy® Mini Kit (Qiagen, Valencia, CA, USA),
and cDNA was synthesized using a PrimeScript RT Reagent Kit (Takara, Shiga,
Japan). Real-time reverse transcription (RT) PCR was performed using the ABI
StepOne Real-time PCR System (Applied Biosystems Japan Ltd, Tokyo, Japan)
using SYBR® Premix ExTaq™ (TaKaRa Bio Inc., Shiga, Japan) according to the
manufacturer ’ s instructions. The sequences of primers used to amplify
3-hydroxy-3-methylglutaryl CoA reductase (HMGR), and ribosomal protein L32
(RPL32) are shown in Table 1. The PCR was performed at 95 ℃ for 10 s followed by
40 cycles of 95 °C for 5 s and 60 °C for 31 s. All data were normalized to the
internal standard RPL32.
17
<Reverse transcription (RT) reaction>
Reagents:PrimeScript RT reagent Kit (Perfect Real Time) (TaKaRa)
Equipment:PCR Thermal Cycler (TaKaRa)
Composition:
Volume(/tube)
①5×PrimeScript Buffer (for Real Time) 2 l
②PrimeScript RT Enzyme Mix I 0.5 l
③Oligo dT Primer 0.5 l
④Random 6 mers 0.5 l
RNA template 0.25 g
⑤RNase Free dH2O
Total 10 l
<Real-time PCR>
Reagents:SYBR Premix Ex Taq (Perfect Real Time) (TaKaRa)
Equipment:ABI StepOne Real Time PCR System (Applied Biosystems)
Composition: Volume(/well)
HMGR / RPL
SYBR Premix Ex Taq (2×) 10 l
Primer Mix(10 M) 0.4 l
ROX Reference Dye (50×) 0.4 l
D.W 7.2l
cDNA template 2 l
Total 20 l
Table1
Sequence of oligonucleotide primers used for real-time quantitative RT-PCR.
Primer Sequence
HMGR (F) 5’-TACCATGTCAGGGGTACGTC-3’ Tm=62.3℃
(R) 5’-CAAGCCTAGAGACATAATCATC-3’ Tm=57.0℃
<Product: 153bp>
RPL32 (F) 5’-CATCTCCTTCTCGGCATCA-3’ Tm=64.0℃
(R) 5’-AACCCTGTTGTCAATGCCTC-3’ Tm=63.9℃
RPL32 was used as an internal standard.
Transcription reaction
37℃ 15 min
85℃ 5 sec
4℃ ∞
Transcription reaction
95℃ 10 sec
95℃ 5 sec 40 cycle
60℃ 31 sec
18
1.2.2 Results
The effects of single treatment of γ-T3 (20 μM)/ATV (6.25 μM)/SMV (6.25 μM) or
combined treatment with γ-T3 and one of the statins on HMGR mRNA levels were
measured using real-time PCR. As shown in Fig. 1.2.1, ATV or SMV (6.25 μM) alone
significantly increased HMGR mRNA expression approximately 1.5-fold above the
control levels, although the effect of SMV in H2452 was not significant. On the other
hand, combined treatment with γ-T3 and ATV or SMV maintained the HMGR
expression as control level.
19
Fig. 1.2.1 Effects of γ-T3 and statins on HMG-CoA reductase (HMGR) mRNA
levels in MSTO and H2452 cells. Cells were treated with γ-T3 (20 μM) given alone
or in combination with ATV (6.25 μM) or SMV (6.25 μM). The mRNA levels were
determined using real-time RT-PCR after a 24 h incubation, and each mRNA level
was normalized to the mRNA level of RPL32. Data are expressed as mean ± SEM
from three independent experiments. Significant differences between each of the
indicated groups were determined using the Tukey–Kramer test. ***p < 0.001.
20
1.3 Antiproliferative effect of the mevalonate pathway and
downstream factors
In chapter 1-3, demonstrate the synergetic effect of statins (ATV and SMV) and
γ-T3 on human MM cells. Involvement of the mevalonate pathway downstream
intermediates, including FPP, GGPP and MVL. Then investigation of downstream
factors Akt and ERK protein expression.
1.3.1 Materials and methods
[Cell lines and culture conditions]
Refer to 1.2.1 Materials and methods.
[Reagents and antibodies]
P44/42 MAP Kinase (137F5), Phospho-p44/42 MAPK (Thr202/Tyr204), and
Rabbit monoclonal antibodies were obtained from Cell Signaling Technology Inc.
(Danvers, MA, USA). Anti-AKT (rabbit) polyclonal and Anti-AKT pS473 (mouse)
monoclonal antibodies were purchased from Rockland Immunochemicals
(Gilbertsville, PA, USA).
[Cytotoxicity assay (MTT assay) with intermediates of mevalonate
pathway]
Cytotoxicity studies were performed in 96-well plates. The cells were cultured at a
density of 3.0 × 103 cells per well in 100 μL of RPMI-1640 medium for 24 h, then
started incubation with γ-T3, statin (ATV, SMV), combination of “γ-T3 + ATV”, and
“γ-T3 + SMV”. After the cells were incubated for 24 or 48 h, 100 μL of MTT solution
(500 μg/mL) was added to each well and incubated for 1 h. Formazan crystals were
dissolved in DMSO (100 μL/well). The absorbance was measured at 540 nm with a
Multiskan JX microplate reader (Thermo Lab Systems, Cheshire, UK). Mevalonate
(MVL) pathway is one of the main and common targets for both γ-T3 and statins.
Therefore, to examine the involvement of this pathway with cytotoxic effect induced
by γ-T3 and statins, cells were then co-treated with intermediate metabolites of
MVL pathway (these compounds promote the pathway), such as farnesyl
pyrophosphate (FPP; 5 μM), geranylgeranyl pyrophosphate (GGPP; 5 μM), or MVL
(50 μM) in addition to γ-T3 and statins. High concentrations of MVL (100, 200 μM)
21
were also examined to elucidate if the effect is concentration dependent or not.
[Western blotting analysis]
Human MM cells were cultured at a density of 1.0 × 106 cells in a 60-mm dish for
24 h. The cells were then harvested and lysed in ice-cold lysis buffer (50 mM
Tris–HCl [pH 6.5], 10% glycerol, 10% β-mercaptoethanol, 0.5 mM phenylmethane
sulfonyl fluoride [PMSF] solution, 2% sodium dodecyl sulfate [SDS] [Wako], 1 mM
sodium orthovanadate, and 1% protease inhibitor cocktail). The cells were
incubated on ice for 20 min following centrifugation for 10 min at 12,000 rpm and
4 °C. Samples containing 20 μg of protein were electrophoresed through a 10%
SDS–polyacrylamide gel and transferred to a polyvinylidene difluoride (PVDF)
membrane (Atto Corp, Tokyo, Japan). The membranes were blocked with TBS-T
(13.7 mM NaCl, 2.5 mM Tris, 0.05% Tween20 [Wako]) containing 5% skim milk
(Yukijirushi, Tokyo, Japan) for 1 h, incubated with primary antibodies for 1 h, and
incubated with secondary antibody for 1 h. The antibody dilutions were as follows:
ERK (1:1000), P-ERK and AKT (1:2000), P-AKT (1:3000), and ß-actin (1:2000). All
antibodies were diluted with TBS-T containing 0.1% skim milk. ß-actin was used as
the internal standard. Detection was accomplished using Immobilon Western
Chemiluminescent HRP Substrate (Millipore, Tokyo, Japan) and an LAS-1000plus
Image Analyzing System (Fujifilm, Tokyo, Japan).
[Statistical analysis]
Refer to 1.1.1 statistical analysis.
22
1.3.2 Results
To examine whether cytotoxicity induced by γ-T3 and statin was involved in the
modulatory effects of the MVL pathway, the cells were cultured with γ-T3, ATV, and
SMV in the absence (control) or presence of 5 μM FPP, 5 μM GGPP, and 50 μM MVL
Cell viability was measured using the MTT assay. FPP did not have a significant
effect on the viability of MSTO or H2452 cells. On the other hand, the addition of
GGPP and MVL increased cell viability, which was more readily apparent at 48 h
than at 24 h in MSTO cells (Fig. 1.3.1a). Additionally, the viability of cells treated
with γ-T3, ATV, and SMV was examined in the absence or presence of 50 μM, 100
μM, and 200 μM MVL (Fig. 1.3.1b). The results suggest that MVL treatment
reversed the growth inhibitory effect of the combined treatment (γ-T3 with ATV or
SMV) in both MSTO and H2452 cells.
Oncogenes promote cell cycle progression (i.e., cell proliferation) via regulation of
intracellular signaling pathways. Two major pathways that are intimately involved
in the G1-to-S transition are the RAS-activated RAF-MEK-ERK and PI3-AKT
pathways. PI3K-AKT is known to impart a strong survival signal that potentially
raises the cellular threshold for apoptosis. Therefore, AKT is frequently activated in
MM cells [47]. However, γ-T3 and statin (either alone or in combination) did not
affect AKT phosphorylation (Fig. 1.3.2a). On the other hand, γ-T3 and statin (alone
or in combination) significantly inhibited ERK phosphorylation in MSTO cells (***:
p < 0.001). No effects were noted in H2452 cells. These results suggest that γ-T3 and
statin inhibit the downstream signaling of the MVL pathway, which partially
contributes to the inhibition of cell growth (Fig. 1.3.2b).
23
(a)
24
Fig. 1.3.1 Effect of combined treatment with γ-T3 and statins on the MVL
pathway in MSTO and H2452 cells. (a) Under stimulation with FPP (5 μM), GGPP
(5 μM), and MVL (50 μM), growth inhibitory effects induced by γ-T3, ATV, and SMV
were examined in MSTO and H2452 cells. (b) The effect of MVL (50–200 μM) on the
growth inhibition induced by γ-T3, ATV, and SMV in MSTO and H2452 cells was
examined. Cell viability was determined using the MTT assay. Data are expressed
as mean ± S.D from three independent experiments. In each treatment group,
significant differences from (a) no metabolites or (b) MVL 0 μM were determined
using the Tukey–Kramer’s test. *p < 0.05; **p < 0.01; ***p < 0.001.
(b)
25
p-Akt/Akt (MSTO)
(a) Akt activation
26
Fig. 1.3.2 Effects of a combined treatment with γ-T3 and statins on the expression
levels of growth factors located downstream of the MVL pathway in MSTO and
H2452 cells. Cells were treated with γ-T3 (20 μM), ATV (6.25 μM), or SMV (6.25 μM)
given alone or in combination for 24 h. Subsequently, (a) Akt activation and (b) ERK
activation levels were examined. Protein expression levels were determined using
western blotting analysis. The bar graph shows the ratio of phosphoprotein density
to total protein density. Data are expressed as mean ± SEM of four independent
experiments. ***p < 0.001 vs. control by the Tukey–Kramer test.
(b) ERK activation
27
1.4 Effect on intrinsic apoptosis
In chapter 1-4, demonstrate the synergetic effects of intrinsic apoptosis,
unchanged expression of Bcl-2 family proteins and activation of caspase 3 on statins
(ATV and/or SMV) and γ-T3 in human MM cells.
1.4.1 Materials and methods
[Cell lines and culture conditions]
Refer to 1.2.1 Materials and methods.
[Reagents and antibodies]
Bax (N-20), Purified mouse anti-Bcl-2 and monoclonal anti-ß-actin were obtained
from Sigma Chemical Company (St. Louis, MO, USA). Donkey anti-rabbit IgG,
HRP-conjugate and Goat anti-mouse IgG, HRP-conjugate were purchased from
Beckam Coulter (Tokyo, Japan).
[Cytotoxicity assay (MTT assay)]
Refer to 1.1.1 Materials and methods.
[Western blotting analysis]
It is the same as 1.3.1 Materials and methods except for antibodies’ condition.
The antibody dilutions were as follows: The antibody dilutions were as follows:
Bax (1:1000), Bcl-2 (1:500), and ß-actin (1:2000). Bax and ß-actin were diluted with
TBS-T containing 0.1% skim milk. Bcl-2 was diluted with Immuno Enhancer (IE).
ß-actin was used as the internal standard.
[Caspase 3 activity assay]
1.0 × 106 cells were cultured in 60-mm dishes for 24 h. Subsequently, the cells
were harvested and centrifuged, and the cell pellets were washed with 2 mL of PBS.
Then the caspase 3-activity assay was performed according to the manufacturer’s
protocol (Biovision, Mountain View, CA, USA). In brief, 100 μL of cold lysis buffer
was added to the cell pellets. Subsequently, the cell pellets were incubated for 10
min on ice, and the lysate was centrifuged at 10,000 rpm for 1 min at 4 °C. The
supernatant was transferred into a micro-centrifuge tube and mixed with the DC
28
Protein Assay Reagent (Bio-Rad, Tokyo, Japan). Supernatants (50 μL) were
dispensed into a 96-well plate (100 μg of protein/well). We then added 10 μL of DTT
to 1 mL of 2 × reaction buffer and dispensed 50 μL of this mixture into each well in
addition to 5 μL of 4 mM DEVD-pNA substrate. The plate was then incubated for
2 h at 37 °C. To detect caspase 3 activity, the absorbance was measured at 405 nm
with a microplate reader.
[Statistical analysis]
Refer to o 1.1.1 statistical analysis.
29
1.4.2 Results
The expression of Bax, a pro-apoptotic protein, did not change after γ-T3 or statin
treatment. Similarly, the expression of Bcl-2, another cell death-associated protein,
did not change (Fig. 1.4.1). On the other hand, a combination of γ-T3 and ATV or
SMV caused a strong induction of caspase 3 activity in both in MSTO and H2452
cells (Fig. 1.4.2). Treatment with ATV alone also strongly activated caspase 3 in
MSTO cells (Fig. 1.4.2a); therefore, the effect might be mainly due to statins. The
caspase 3 inhibitor Z-DEVD-FMK significantly inhibited the reduction in MSTO
cell viability in response to ATV treatment, although the cell viability was not
reversed in H2452 cells even after treatment with Z-DEVD-FMK (Fig. 1.4.2b).
30
Fig. 1.4.1 Effects of a combined treatment with γ-T3 and statins on the expression
levels of Bcl-2 and Bax proteins in MSTO and H2452 cells. Cells were treated with
γ-T3 (20 μM), ATV (6.25 μM), or SMV (6.25 μM) given alone or in combination for 24
h. Subsequently, Bax and Bcl-2 protein expression levels were examined. Each
protein expression level was determined and quantified using western blotting.
ß-actin was used as an internal standard. The lower columns indicate the Bax/Bcl-2
ratio, which illustrates the apoptotic balance. Data are expressed as mean ± SEM
of four independent experiments.
31
(a)
32
Fig. 1.4.2 Effects of a combined treatment with γ-T3 and statins on caspase 3
activity in MSTO and H2452 cells. Cells were treated with γ-T3 (20 μM), ATV
(6.25 μM), or SMV (6.25 μM) given alone or in combination for 24 h. Subsequently,
(a) the activity of casepase-3 in MSTO and H2452 cells was examined. Caspase 3
activity was detected as absorbance at 405 nm. (b) The effect of a caspase 3
inhibitor (Z-DEVD-FMK) on apoptosis induced by ATV in MSTO and H2452 cells
was analyzed. The cells were treated with ATV (6.25 μM) in the absence or
presence of Z-DEVD-FMK (2 μM). Cell viability was measured using the MTT
assay. ***p < 0.001 vs. control; ##p < 0.05 vs. ATV by the Tukey–Kramer test.
Data are expressed as mean ± S.D of three independent experiments. Cell
viability was measured using the MTT assay. ***p < 0.001 vs. control; ##p < 0.05
vs. ATV by the Tukey–Kramer test. Data are expressed as mean ± S.D of three
independent experiments.
(b)
33
1.5 Discussion
Malignant mesothelioma cells exhibit resistance to single-agent and combination
chemotherapy strategies, therefore successful chemotherapy is a key point for the
treatment of these patients [48]. Now pemetrexed and cisplatin combination
chemotherapy is the first-line treatment in inoperable disease with a median
survival of 9 – 12.4 months [49]. Despite notable improvement using this
combination therapy, disease recurrence and progression remain a problem. On the
other hand, one previous study addressing the efficacy of γ-T3 combination
treatment with cisplatin-induced cytotoxicity in human mesothelioma H28 cells in
culture has been reported [50]. Additionally, several in vitro [27] and in vivo [51]
studies support the anticancer effect of γ-T3 alone or in combination with statin.
Cytostatic effects were observed when 20 μM of γ-T3 was combined with 6.5 μM
of ATV or 6.5 μM of SMV (Fig. 1.1.1). Previous study has shown that combining
low-dose γ-T3 and statin induced cell cycle arrest at G1 in mammary tumor, leading
to a large reduction in cyclin D1 and a marked increase in p27 expression; however,
γ-T3 or statin alone had little or no effect on the distribution of cells in different cell
cycle phases compared with the combining group [52]. On the other hand, γ-T3
inhibited human gastric adenocarcinoma (SGC-7901) cell growth at the G0/G1
phase [53]. Our results indicate that the sub-G1 population is increased by
combination treatment with γ-T3 and statins, and such an increase is an indicator
of apoptosis. No phase shift was observed in MSTO cells treated with γ-T3 (20 μM),
ATV (6.25 μM), or SMV (6.25 μM) alone for 24 and 48 h (Fig. 1.1.2). These results
suggest that the effects of γ-T3 or statin on cell cycle distribution may be dependent
on cell types. Further studies are needed to confirm which phase is a major target.
It has been reported that the synergistic effects of γ-T3 and statin appear to result
from the cooperative action of γ-T3, which down-regulates HMGR mRNA expression,
and statins, which directly inhibit HMGR activity [43]. Several studies have been
performed to determine if the antiproliferative effects of combined statin and γ-T3
treatment result solely from the inhibition of HMGR or if additional
HMGR-independent mechanisms are involved [26,43]. In the present study, a
decreasing trend of HMGR mRNA expression was observed in both MSTO and
H2452 cells treated with γ-T3; however, this decrease was not significant compared
to control in both cell lines. On the other hand, statins alone increased the mRNA
expression, which was also shown in previous reports [54,55]. This statin-induced
increase was reversed by co-treatment with γ-T3 (Fig. 1.2.1). Previous reports
34
support our results: tocotrienols have been shown to reduce HMGR activity by
triggering (1) the retention of sterol regulatory element binding proteins (SREBPs),
which are membrane-bound transcription factors that activate all of the genes
required to produce cholesterol, in the ER and (2) the degradation of HMGR by
stimulating ubiquitination or reduction in mRNA level [45,56]. Moreover, the ability
of sub-effective doses of γ-T3 to synergistically enhance the growth inhibitory effects
of statins can be explained, at least in part, on the basis of the finding that statin
inhibition of HMGR activity is associated with a compensatory feedback mechanism
that results in the up-regulation of HMGR expression [44]. Therefore, synergistic
attenuation of HMGR activity via the application of the 2 compounds might
contribute to strong growth inhibition.
Next, to investigate whether the anticancer activity of combination (γ-T3 + statin)
therapy is mediated via inhibition of the MVL pathway, the effects of exogenous
intermediates of this pathway on cell growth were examined. The inhibition of
HMGR by statins leads to reduced production of cholesterol and isoprenoids as well
as downstream intermediates, including MVL (the first product of this pathway),
FPP, and GGPP [57]. Human farnesyl pyrophosphate synthase (hFPPS) is
responsible for the catalytic elongation of dimethylallyl pyrophosphate (DMAPP) to
FPP via the successive condensation of 2 isopentenyl pyrophosphate (IPP) units,
and it controls the intracellular levels of all downstream isoprenoids, including
GGPP [58]. Moreover, the angiostatic effects of statins at high therapeutic
concentrations are lipid-independent and are reversible by supplementation with
MVL and GGPP [59]. Both FPP and GGPP are important lipid attachments
required for the post-translational modification of a variety of small GTPase
proteins such as Ras and Rho GTPases. Thus, inhibitors of the MVL pathway might
have the opportunity to inhibit the invasion of cancer cells, as was reported for
HMGR inhibitors [60]. In the present study, the inhibition of cell growth by γ-T3
and statin was reversed after the addition of MVL or GGPP in a dose-dependent
manner (Fig. 1.3.1). Therefore, the synergistic antiproliferative effects of combined
γ-T3 and statin treatment may result directly from an inhibition of HMGR activity
and subsequent suppression of MVL synthesis.
The Raf/MEK/MAPK/ERK pathway and the PI3K/AKT pathway are important
downstream targets of activated Ras. ERK and AKT are vital growth factors
involved in cell cycle promotion and apoptosis regulation. We investigated whether
there was any change in protein expression among the treated cells; however,
neither the single nor the combination treatment altered AKT expression (Fig.
35
1.3.2). On the other hand, γ-T3 and statin (alone or in combination) significantly
inhibited ERK phosphorylation in MSTO cells (Fig. 1.3.2). Therefore, the growth
inhibition observed in the present study might mainly occur via ERK signaling. It
was previously shown that γ-T3 inhibits cell growth in sympathoadrenal (SA) +
mammary cells specifically by suppressing EGF-dependent Stat and AKT mitogenic
signaling [45]. This disparity in response to γ-T3 might be derived from the
different characteristics of each cancer type.
Indeed, AKT is often activated in both primary tumor and MM cell lines [47]. Our
results also showed positive AKT phosphorylation in all the cells, which was not
affected by any treatment. MMs with a positive AKT phosphorylation status have
also been shown to be phosphorylated (activated) mammalian targets of rapamycin
(mTOR), a molecule that functions downstream of the AKT pathway [47]. Moreover,
a PTEN homozygous deletion, which was also responsible for AKT activation, was
detected in a small subset of MM cell lines [61]. Based on these observations, one of
the small molecule inhibitors of receptor tyrosine kinases (RTKs), imatinib
mesylate was used in clinical trial for MM patients; however, a clear effectiveness
was not observed [62]. This lower-than-expected level of responsiveness was
thought to be due to the intrinsic resistance of MM cells against RTK inhibitor [47].
As a result of this acquired secondary resistance, the effectiveness of inhibitors
targeted against constitutive activation of a specific RTK is thought to be abrogated
via a new mutation in the RTK gene or the activation of another RTK. Taken
together, these results indicate that mono-target therapy will be ineffective in the
near future for aggressive cancer types such as MM.
Finally, the effects on the intrinsic apoptotic pathway were investigated. Statins
initiate apoptosis by suppressing Bcl-2, increasing Bax expression, and activating
caspase 3 [35]. The propensity of a cell to undergo apoptosis is finely balanced by
anti-apoptotic and pro-apoptotic factors. The Bcl-2 family has been shown to play an
important regulatory role in apoptosis either as an activator (i.e., Bax and Bak) or
as an inhibitor (i.e., Bcl-2 and Bcl-xL). The ratio of Bcl-2 to Bax proteins is
recognized as a key factor in the regulation of the apoptotic process or cell death [63].
Additionally, because the Bcl-2 family proteins are involved in most of the apoptosis
pathways, they are attractive targets for cancer therapy [64]. Our studies have
shown that Bax and Bcl-2 were expressed in both MSTO and H2452 cells, but they
were not affected by γ-T3 and statin. These results are consistent with a previous
report indicating that γ-T3 induced a mitochondrial disruption pathway without
affecting Bax/Bcl-2 expression in human breast cancer MDA-MB-231 cells [65].
36
MM cell lines and tumors were shown to express the Bcl-2 family members Bcl-xL
and Mcl-1 [66]. The Bcl-2 family is a group of more than 20 protein-coding genes.
Among these, the Bcl-xL protein is at least as effective as Bcl-2 for preventing
apoptosis in a variety of human tumors, including MM, when challenged with
pro-apoptotic stimuli [67]. On the other hand, we found that caspase 3 was
activated in human MM cell lines by the γ-T3 and statin combination treatment
(Fig. 1.4.1). Cao et al. showed that Bcl-2/Bcl-xL inhibitors, such as 2-methoxy
antimycin A3, increased caspase 3 activation without altering the protein
expression of members of the Bcl-2 family [68]. Therefore, the expression of Bcl-2
family members should be further examined, and functional assays should be
performed.
On the other hand, extent of caspase 3 reactivity induced by statins, especially
ATV, was the most different point between MSTO and H2452 cells (Fig. 1.4.1). In
this study, H2452 cells seems to response mildly to stains compared with MSTO
cells, for example, regarding to ERK activation (Fig. 1.3.2b), casepase 3 activation
(Fig. 1.4.1). The cause of such difference between cells did not clear out in this study,
however, caspase 3 original levels might be involved with the different responses.
Soini et al. showed that there was a tendency for better prognosis of mesotheliomas
from patients with moderate or intense caspase 3 immunoreativity as compared to
cases with negative or low caspase 3 [66]. They also indicated that another famous
apoptotic inducing factor, Fas ligand was not detected in the most drug resistant
mesothelioma cell line although Fas/Fas ligand has been suggested to participate in
the apoptosis in mesothelioma cells [69]. Additionally it is suggested that cell origin
difference might be involved to each responses in MSTO and H2452; MSTO is
derived from metastatic site (lung) of mesothelioma patients while H2452 is from
primary tumor though both cell lines are biphasic type. To explore the factor which
determines drug sensitivity, levels of caspase 3 and other apoptotic markers should
be examined and be compared between cell lines.
37
1.6 Summary
Combination with γ-T3 and statin induced apoptosis.
γ-T3 was down-regulated HMGR mRNA expression.
Growth inhibiting effect by γ-T3 and statin was reversed with MVL or GGPP
in a dose-dependent.
γ-T3 and statin alone or combination inhibited ERK phosphorylation.
Extent of caspase 3 activation was induced by statin, and combination with
γ-T3 further made further stronger activation.
38
Chapter2
Involvement of endoplasmic reticulum stress with the
combination effect of gamma-tocotrienol and statin
Introduction
The endoplasmic reticulum (ER) stress is defined as accumulation of unfolded or
misfolded proteins in the ER, which induces monitored and maintained via a
coordinated adaptive program, the unfolded protein response (UPR) [70]. The
biochemistry of the ER stress and UPR pathways has been the subject of many
recent reviews [71]. The investigation of ER-nuclear signaling transduction has
three signaling pathways [72]: (1) the presence of misfolded or unfolded protein in
the organelle (unfolded protein response, UPR). (2) The overloading of the ER with
correctly folded proteins (ER-overload proteins, EOR). (3) The starvation of
cholesterol (sterol regulatory element binding protein, SREBP).
There are three branches of UPR that are detected by distinct ER stress
transducers located on the ER membrane [73]: (1) PER-like endoplasmic reticulum
kinase (PERK), (2) inositol-requiring enzyme (IRE1), and (3) activating
transcription factor 6 (ATF6). Moreover, ER stress activates a large number of genes
involved in the control of cell fate, including antiapoptotic and proapoptotic
molecules like C/EB homologous protein (CHOP), c-Jun N-terminal kinases (JNK)
or members of the BCL-2 proteins family [74].
PERK is a type 1 transmembrane protein. This activates and phosphorylates
phosphorylated α subunit of eukaryotic initiation factor 2 (eIF2α) causing a
translation arrest [75]. IRE1α is an ER transmembrane sensor that activates the
UPR to maintain the ER and cellular function. Further understanding of IRE1α
substrate preferences will reveal how IRE1α coordinates cellular homeostasis to
determine cell fate under ER stress [76]. During ER stress, Ask1 is recruited to
oligomerized IRE1α complexes containing TRAF2, activating Ask1 kinase and
causing downstream activation of JNK and P38 MAPK [38]. Release of GRP78 from
N-terminus of ATF6 triggers different mechanism of protein activation, compared
with PERK and IRE1α [38].
In chapter 2, present study is the first to demonstrate the synergetic effect of
statins and γ-T3 on ER stress in human MM cells. ER stress was evaluated by
39
expression of typical ER stress markers such as CHOP, GRP78, caspase 4
apoptosis-related cysteine protease (caspase 4) and JNK signaling. Finally
involvement of caspase family was examined as well.
40
2.1 Materials and methods
[Cell lines and culture conditions]
The human MM cell lines H2452 (an epithelial), and MSTO-211H (a biphasic;
MSTO) cells were obtained from the American Type Culture Collection
(Rockville, MD, USA) and were cultured in RPMI-1640 medium.
MSTO cells were grown in medium containing 10% fetal bovine serum (FBS)
(Equitech-Bio, Kerrville, TX, USA), 0.5 units/mL of penicillin, and 1 μg/mL of
streptomycin.
H2452 cells were grown in the same medium supplemented with 4.5 g/L of
glucose, 1 mM sodium pyruvate, and 10 mM HEPES buffer solution (GIBCO,
Life Technologies Japan Ltd., Minato-ku, Tokyo, Japan). All cell lines were
maintained at 37 °C in a fully humidified atmosphere of 5% CO2.
[Reagents]
All cultures and reagents were purchased from Sigma Chemical Company (St.
Louis, MO, USA) unless otherwise indicated. γ-T3 was a gift from Dr. Yano T (Toyo
University). Simvastatin (SMV) was purchased from Cayman Chemical Company
(Ann Arbor, MI, USA) and atorvastatin (ATV) was purchased from LKT
Laboratories, Inc. (St. Paul, MN, USA).
[Cytotoxicity assay (MTT assay)]
Refer to Chapter 1, 1.1.1 Materials and methods.
Use the following agents to examine ER stress induced apoptosis:
Tunicamycin (0.125 μg/ML); ER stress inducer
Salubrinal (12.5 μM); Protector from ER stress-induced apoptosis
JNK inhibitor (SP600125; 2 μM)
Caspase inhibitors (2 μM) [caspase 8 inhibitor (Z-IETD-FMK), caspase 9
inhibitor (Z-LEHD-FMK), and pan caspase inhibitor (Z-VAD-FMK)] and
caspase 4 inhibitor (Z-LEVD-FMK; 10 μM)
[Real-time RT-PCR analysis for ER stress markers]
Refer to Chapter 1, 1.2.1 Materials and methods.
The sequences of primers used to amplify CHOP, Caspase 4, GRP78, and RPL32
(internal standard) are shown in Table 2. All data were normalized to the internal
41
standard RPL32.
Table 2
Sequence of oligonucleotide primers used for real-time quantitative RT-PCR.
Primer Sequence
RPL32 (F) 5’-CATCTCCTTCTCGGCATCA-3’ Tm=64.0℃
(R) 5’-AACCCTGTTGTCAATGCCTC-3’ Tm=63.9℃
<Product: 247bp>
GRP78 (F)5’-GCTCGACTCGAATTCCAAAG-3’ Tm=63.7℃
(R) 5’-TTTGTCAGGGGTCTTTCACC-3’ Tm=63.8℃
<Product: 331bp>
CHOP (F) 5’-GAGTCATTGCCTTTCTCCTTCG-3’ Tm=66.0℃
(R) 5’-TTTGATTCTTCCTCTTCATTTCCA-3’ Tm=64.5℃
<Product: 140bp>
Caspase 4 (F) 5’-CTGAAGGACAAACCCAAGGTCA-3’ Tm=67.2℃
(R) 5’-CACTTCCAAGGATGCTGGAGAG-3’ Tm=67.1℃
<Product: 96bp>
RPL32 was used as an internal standard.
[Western blotting analysis]
Refer to Chapter 1, 1-3-1 Materials and methods.
The antibody dilutions were shown as follows: JNK (1:1000), pJNK, and ß-actin
(1:2000). All antibodies were diluted with TBS-T containing 0.1% skim milk. ß-actin
was used as the internal standard. Detection was accomplished using Immobilon
Western Chemiluminescent HRP Substrate (Millipore, Tokyo, Japan) and an
LAS-1000plus Image Analyzing System (Fujifilm, Tokyo, Japan).
[Statistical analysis]
Refer to Chapter 1, 1.1.1 statistical analysis.
42
2.2 Results
GRP78, CHOP, and caspase 4 are key molecules involved in the ER
stress-associated apoptosis pathway. Their mRNA expression levels were quantified
using real-time RT-PCR after 24 h of treatment with γ-T3 and statins given alone or
in combination. As shown in Fig. 2.2.1a and Fig. 2.2.1b, the expression levels of
GRP78 and CHOP in MSTO cells significantly increased from baseline in the
presence of γ-T3. ATV or SMV alone did not affect them at all. In H2452 cells, γ-T3
also increased GRP78 and CHOP expressions though it seemed milder compared
with those in MSTO cells (Fig. 2.2.1a and 2.2.1b). Although no differences were
observed in caspase 4 expression levels in MSTO cells, treatment with γ-T3 alone
caused a significant increase in the levels in H2452 cells (Fig. 2.2.1c). The response
to γ-T3 seems also relatively weak in H2452 regarding to ER stress markers, CHOP
(Fig. 2.2.1a) and GRP78 (Fig. 2.2.1b), although caspase 4 increase by γ-T3 was only
observed in H2452 cells. Additionally we examined if caspase 4 activation involves
the combination effect or not with caspase 4 inhibitor (Fig.2.2.2) but cell viability
after γ-T3 and statin treatment were unchanged both in presence or absence the
inhibitor.
Tunicamycin (TM) is an ER glycosylation inhibitor that impairs the synthesis of
proteins in the ER which induces apoptosis. And Salubrinal (Sal) is a selective
inhibitor of eIF2α dephosphorylation that was recently developed as a protective
agent against ER stress-mediated apoptosis [77]. Sal alone did not affect cell
viability so much whereas TM alone decreased the viability to almost 30% compared
with control (no treatment). In case of the combination with TM and Sal, cell
viability had been kept around 50%, which was significantly higher than in case of
TM alone (Fig.2.2.3a). On the other hand, γ-T3 seemed to exhibit similar effect like
TM; γT3 induced-growth inhibition was recovered with Sal although there was no
significant difference between γT3 alone and γT3 was combination Sal (Fig.2.2.3b).
It was considered that the growth inhibitory effect of γ-T3 might be partly occurred
via ER stress.
Next, as shown in Fig.2.2.4 γ-T3 and statin treated samples were probed by
western blot analysis for JNK and p-JNK. γ-T3 and ATV alone did not significantly
alter either JNK or p-JNK levels. On the other hand, p-JNK/JNK ratio was
significantly increased by γ-T3 and ATV combination comparing with control (p≺
43
0.05) in human MM cells.
Then we examined whether such as JNK activation could contribute to the
growth inhibitory effect or not, using JNK kinase inhibitor, SP600125 with γ-T3 and
statins. Contrary to our expectation, our results showed that SP600125 did not
significantly alter the cell viability in cells which were treated with γ-T3, ATV alone
or combination in neither MSTO nor H2452 cells (Fig.2.2.5).
To determine which caspase are required for the induction of apoptosis by γ-T3,
ATV alone or combination, cells were treated with caspase 8 inhibitor
(Z-IETD-FMK), caspase 9 inhibitor (Z-LEHD-FMK) or pan caspase inhibitor
(Z-VAD-FMK) at a concentration of 2 μM. Any of caspase inhibitors did not block
cell growth inhibition induced by γ-T3 and statins in MSTO and H2452 cells
(Fig.2.2.6).
44
Fig. 2.2.1 Effects of combined treatment with γ-T3 and statins on the relative
mRNA levels of ER stress-associated factors in MSTO and H2452 cells. Cells were
treated with γ-T3 (20 μM), ATV (6.25 μM), or SMV (6.25 μM) given alone or in
combination for 24 h. Subsequently, (a) CHOP, (b) GRP78, and (c) caspase 4 mRNA
expression levels were analyzed. Each mRNA expression level was determined
using real-time RT-PCR and quantified. The expression levels of each gene were
normalized to the expression level of RPL32. Data are expressed as mean ± SEM
of at least three independent experiments. ***p < 0.001; **p < 0.01 vs. control by
the Tukey–Kramer test.
MSTO
H2452
(a) CHOP
(b) GRP78
(c) Caspase 4
45
Fig.2.2.2 Effects of caspase 4 inhibitor (Z-LEVD-FMK; 10 μM) treatment with
γ-T3 (20 μM) and ATV (6.25 μM) alone or combination in MSTO and H2452 cells for
24 h. Cell viabilities were determined by MTT assay. Data are expressed as mean
±S.D of at least three independent experiments.
0
20
40
60
80
100
120
control γT3 ATV γT3+ATV
Ce
ll v
iab
ilit
y (
% o
f c
on
tro
l)
MSTO
0
20
40
60
80
100
120
control γT3 ATV γT3+ ATV
Ce
ll v
iab
ilit
y (
% o
f c
on
tro
l) H2452
Caspase4 inhibitor (-)
Caspase4 inhibitor (+)
46
Fig.2.2.3 The effects of Salubrinal (Sal) (12.5 μM), Tunicamycin (TM) (0.125 μg/ml)
and γ-T3 (50 μM) given alone and in combination of each other in MSTO cells for 24
h. (a) TM induced ER stress (b) γ-T3 induced ER stress. Cell viabilities were
determined by MTT assay. Data are expressed as mean ±S.E. of at least three
independent experiments. ***: p<0.001, **: p<0.01 vs. control by Tukey-kramer’s
test.
(a)
TM induced ER stress
(b)
γ-T3 induced ER stress
47
Fig.2.2.4 Effects of combined treatment with γ-T3 (20 μM), and statins (6.25 μM)
on the relative expressions of JNK and phosphorylated-JNK (p-JNK) protein in
MSTO and H2452 cells. p-JNK/JNK ratio was normalized to control in MSTO and
H2452 cells. Each protein level was determined by western blotting. Data are
expressed as mean ± S.D of at least three independent experiments. *:p<0.05 vs.
control by Tukey-Kramer’s test.
48
Fig.2.2.5 Effects of JNK inhibitor (SP600125; 2 μM) treatment with γ-T3 and ATV
alone or combination in MSTO and H2452 cells for 24 h. Cell viabilities were
determined by MTT assay. Data are expressed as mean ±S.D of at least three
independent experiments. ***: p<0.001 vs. control by Tukey-kramer’s test.
49
Fig.2.2.6 Contribution of caspase family to cell growth inhibition of γ-T3 and ATV
in MSTO and H2452 cells. Cells were seeded in 96-well plates and treated for 48 h
with γ-T3 (20 μM), ATV (6.25 μM) alone or in combination with caspase 8 inhibitor
(Z-IETD-FMK), caspase 9 inhibitor (Z-LEHD-FMK) and pan caspase (Z-VAD-FMK)
(2 μM). Cell viability was evaluated using the MTT assay. Data are expressed as
mean ± S.D of at least three independent experiments. ***: p<0.001 vs. control, ###:
p<0.001 vs. γ-T3 or ATV Tukey-Kramer’s test.
50
2.3 Discussion
In this chapter, we examined the involvement of ER stress with the synergistic
effect of γ-T3 and statins. ER stress is another expected target of γ-T3. Until now,
several apoptotic pathways have been identified in cells that are responsive to
cytotoxic insult, including apoptosis mediated by the activation of death receptors
(extrinsic), mitochondria-dependent signaling (intrinsic), and ER-induced apoptotic
cell death. In many instances, deregulation of ER homeostasis has been correlated
with pathologic states and particularly with cancer [78]. ER stress can lead to
adaptive responses or apoptosis, both of which follow activation of the UPR [79].
The UPR regulator GRP78, an ER chaperone, induces ER stress and is widely
up-regulated in cancer [51]. Similarly, the activation of CHOP and caspase 4 is a key
step in ER stress-induced apoptosis [80]. In fact, γ-T3 induced apoptosis may be
associated with induction of early response genes and the transcriptional response
to ER stress in breast cancer cells [81]. In the present study, the observed
up-regulation of GRP78 and CHOP led us to further investigate the involvement of
ER stress in γ-T3-induced apoptosis. We found that the expression levels of GRP78
and CHOP were unchanged by treatment with ATV or SMV alone (Fig. 2.2.1a and
Fig. 2.2.1b). It indicates that statins in the present study did not affect ER stress,
and also that statins did not inhibit γ-T3 -induced ER stress which might lead the
following apoptosis. Therefore, this supports the idea that γ-T3 enhances
statin-induced apoptosis. Although caspase 4 is also a known critical mediator of
programmed cell death [82], we found that the caspase 4 level was altered only by
treatment with γ-T3 alone in H2452 cells (Fig. 2.2.1c). Result of MTT assay using
caspase 4 inhibitor also suggested it was not significant factor for growth inhibitory
effect of γ-T3 and statins in the present study (Fig. 2.2.2).
The TM inhibits protein glycosylation in the ER, there by inducing ER stress.
Apoptosis is induced by severe and prolonged ER stress [77]. Salubrinal protected
MSTO cells from cytotoxicity induced by TM, as demonstrated by increased cell
viability. A recent study has shown that phosphorylation of eIF2α protected cells
from ER stress [83]. And TM is the most commonly used pharmacological agent to
experimentally induce ER stress [84]. As shown in Fig.2.2.3b, γ-T3 induced
cytotoxicity was slightly recovered by salubrinal which suggests the ER stress has a
role in γ-T3-induced growth inhibition; however, it was not significant change.
Another assay which detects apoptosis from the different aspect, such as
flowcytometry and TUNEL assay, will support to understand the role of ER stress
51
in the present case.
The, JNK belong to the mitogen-activated protein kinase (MAPK) family. JNK
studies provided a mechanistic link between stress and growth factor [85]. Moreover,
JNK is important role in cell stress reactions and being activated by many
extracellular stress signals, JNK is also called stress activated protein kinase
(SAPK), and is involved in stress reaction and cell death [86]. Our results indicated
that p-JNK/JNK ratio was significantly increased by γ-T3 combination with ATV,
but not affected by γ-T3 or ATV single treatment (Fig.2.2.4). A recent report
suggested JNK as a mediator of simvastatin- induced growth inhibition and cell
death in breast cancer cells [87]. Another report suggested that γ-T3 induces
apoptosis through activation of JNK signaling via ER stress in breast cancer cells
[88]. Moreover, the regulation of JNK transduction pathway also has been
mentioned in tumorigenesis and metastatic potential of gastric cancer [89]. JNK is
known to be activated by ER stress through the IRE1α pathway, but the interplay
with mitochondria and the mechanism for sustained JNK activation in ER stress is
not known [90]. In response to ER stress, the kinase domain of IRE1 binds to the
TRAF2 adaptor molecule and activates the apoptosis signaling regulation kinase
(ASK1), which in turn the causes the phosphorylation and activation of JNK.
However, JNK signaling elicits many cellular responses besides cell death and can
even promote cell survival in specific circumstances [91].
SP600125 is a specific, small molecule inhibition of JNK that prevents the
phosphorylation of c-Jun and blocks the expression of proinflammatory cytokines
and subsequent apoptosis cell death [92]. Hence, SP600125 treatment significantly
induced apoptosis consistent with the increasing levels of phosphorylated
anti-apoptotic proteins like Bcl-2 and Bcl-xL (un-activated form) in U937 leukemia
cells [93]. In recent report shown that downstream of JNK activates caspases via
the translation of Bax to mitochondria from the cytosol. The translocated Bax
induces an increase of mitochondrial membrane permeabilization and cytochrome c
release [94]. In the recent report provided further details for the action mechanism
of SP600125 on the ER and mitochondrial functions [95]. Considering these reports,
the action of SP600125 used in our study should be revised carefully. There is still a
possibility that results would be changing by the concentrations or timing of
SP600125 when it was treated with γ-T3 (Fig.2.2.5). Further studies are needed
that concentrate on more efficient upstream signals leading to the JNK activation
as well and this notion remains to be tested.
Caspase are the final effectors of both extrinsic and intrinsic apoptosis,
52
therefore it is expected that interfering with their function impairs these pathway
leading to a survival advantage for cancer cells and indeed caspase alterations are
not rare in a variety of tumors [96]. It has been demonstrated those two pathways
through which the caspase family proteases can be activated: one is the death
signal-induced, death receptor-mediated pathway; the other is the stress-induced,
mitochondrion-mediated pathway [97]. Typically, the death receptor-initiated
pathway involved activation of initiator caspase 8, which in turn activates caspase 3
[97]. In addition, caspase 3 and caspase 9 as well as caspase generated truncated
Bid that triggers cytochome c release [98]. There is a report that when the caspase
12 activity was inhibited by Z-ATAD-FMK, the mitochondria dependent activation
of caspase 9 and caspase 3 was not provoked to a sufficient level required for
subsequent activation of caspase 8 in Jurkat T cells [99]. On the other hand, in all
MM cell lines, Z-VAD-FMK 10 µM resulted no significant effect on
sorafenib-mediated cell killing whereas the caspase inhibitor did potently inhibit
the cytotoxicity of TRAIL in those cell lines sensitive to TRAIL [100]. Therefore,
they didn’t significantly affect the synergistic cell growth inhibition of γ-T3 and
statin that needed to explore the molecular mechanisms of ER stress.
53
2.4 Summary
γ-T3 increased ER stress markers; GRP78 and CHOP but not caspase 4.
γ-T3 induced growth inhibition was slightly blocked by salubrinal, a protector
of ER stress related apoptosis in MSTO cells.
γ-T3 and statin (ATV) combination up-regulated JNK activation but it had
almost no effect on their synergistic growth inhibitory effect.
Caspase 8 and caspase 9 inhibitors did not significantly change cell
cytotoxicity induced by γ-T3 and statin (ATV, SMV).
54
Conclusion
In this study, we analyzed that treatment effect of γ-T3 and statin exhibited a
synergistic effect against human malignant mesothelioma cells in vitro.
In Chapter1, synergistic effect of combined treatment with gamma-tocotrienol and
statin on human malignant mesothelioma cells was revealed.
γ-T3 and statin exhibited a synergistic effect against human MM cells by
complimentary and synergetic mechanism; inhibition of the MVL pathway
including HMGR and the following MAPK signaling (induced by both γ-T3 and
statin), and caspase 3 activation (induced by statin). Whether caspase 3 activation
was derived from MVL pathway or not had not been confirmed yet. In this study,
stains were used at 6.25 μM when combined with γ-T3. It still seems a little bit high
concentration in consideration of previous clinical tolerance of statin [37], however,
there is a possibility that lower than 6.25 μM concentration of statins combined
with high concentration of γ-T3 (more than 20 μM) could work effectively since γ-T3
is assumed to be safe. Moreover, our combination use of γ-T3 and statin has shown
not only cytostatic effect but also cytotoxicity, as shown sub-G1 increase and caspase
3 activation.
In Chapter2, it was revealed that endoplasmic reticulum stress seemed to be
involved with the combination effect of γ-T3 and statin.
Our work found that the expression levels of GRP78 and CHOP were
unchanged by treatment with ATV or SMV alone (Fig. 2.2.1a and b). It indicates
that statins in the present study did not affect ER stress, and also that statins did
not inhibit γ-T3 induced ER stress which might lead the following apoptosis. Then
we used ER stress factors such as JNK and caspase family members, caspase 8 and
caspase 9 which are reported to be related with ER stress, although they didn’t
significantly affect the synergistic cell growth inhibition of γ-T3 and statin.
Therefore, the downstream apoptotic pathway of ER stress mediated cell death is
still unclear.
Taken together, current research shows that γ-T3 synergistically enhances the
anti-proliferative effect of statins on MM cells via mevalonate pathway, and
promotes apoptosis via ER stress signal and intrinsic apoptosis pathway, in which
55
one the vital inducer could be caspase 3 (Fig. D). Overall, the combination of γ-T3
and statins could be useful for MM therapy and functions in a complementary style.
These findings suggest that a combination treatment may cause significant
inhibition of cancer cell growth, which will help to overcome the resistance of MM to
current chemotherapies. The distinct molecular targets of this combined therapy
should be explored in further detail.
56
Fig. D Mechanism scheme of “γ-T3 + statins”. Bold arrows indicate each effects
induced by γ-T3, statins, and γ-T3 + statins, respectively which have shown in this
study.
Caspase 9
Caspase 8
57
References
[1] A. Jemal, F. Bray, MM. Center, J. Ferlay, E. Ward, D. Forman, Global cancer
statistics. CA CANCER J CLIN. 61, 2011, 69–90.
[2] R. Lozano, Global and regional mortality from 235 causes of death for 20 age
groups in 1990 and 2010: a systematic analysis for the Global Burden of
Disease Study 2010. Lancet. 380, 2012, 2095–2128.
[3] Cancer, World Health Organization. Retrieved 5 January 2011.
[4] B.V. Robinson, A.W. Musk and R.A. Lake, Malignant mesothelioma, Lancet
2005, 397–408.
[5] J. Peto, A. Decarli, C. La Vecchia, F. Levi and E. Negri, The European
mesothelioma epidemic, Br. J. Cancer 79, 1999, 666–672.
[6] J. Peto, J.T. Hodgson, F.E. Matthews and J.R. Jones, Continuing increase in
mesothelioma mortality in Britain, Lancet 345, 1995, 535–539.
[7] T. Murayama, K. Takahashi, Y. Natori and N. Kurumatani, Estimation of
future mortality from pleural malignant mesothelioma in Japan based on an
age-cohort model, Am. J. Ind. Med. 49, 2006, 1–7.
[8] V. Delgermaa, K. Takahashi, E.K. Park, G.V. Le, T. Hara and T. Sorahan,
Global mesothelioma deaths reported to the World Health Organization
between 1994 and, Bull. World Health Organ. 89, 2011, 716–724.
[9] M.S. Kanarek, Mesothelioma from chrysotile asbestos: update, Ann. Epidemiol.
21, 2011, 688–697.
[10] C. Riganti, S. Orecchia, F. Silvagno, G. Pescarmona and P.G. Betta, Asbestos
induces nitric oxide synthesis in mesothelioma cells via Rho signaling
inhibition, Am. J. Respir. Cell Mol. Biol. 36, 2007, 746–756.
58
[11] S. Yoshitaka Molecular pathogenesis of malignant mesothelioma,
Carcinogenesis. 34, 2013, 1413–1419.
[12] A. Scherpereel , P. Astoul , P. Baas , T. Berghmans, Guidelines of the
European Respiratory Society and the European Society of Thoracic
Surgeons for the management of malignant pleural mesothelioma. Eur
Respir J. 35, 2010, 479–495.
[13] W.S. Bruce, M.D. Robinson, A.L. Richard, Advance in malignant
mesothelioma, N ENGL J MED 353, 2005, 1591–1603.
[14] V. Izzi , L. Masuelli , I. Tresoldi , C. Foti , A. Modesti , R. Bei . Immunity and
malignant mesothelioma: From mesothelial cell damage to tumor
development and immune response-based therapies, Cancer Letters. 322,
2012, 18–34.
[15] AL. Cleaver , K. Bhamidipaty , B. Wylie , T. Connor , C. Robinson, Long-term
exposure of mesothelial cells to SV40 and asbestos leads to malignant
transformation and chemotherapy resistance. Carcinogenesis. 2013, 1–24.
[16] A. Baldi, AM. Groeger, V. Esposito, R. Cassandro, Expression of p21 in SV40
large T antigen positive human pleural mesothelioma: relationship with
survival, Thorax. 57, 2002, 353–356.
[17] C. Maneglod, J. Symanowsky, U. Gatzemeier, M. Reck, J. Von Pawel,
Second-line (post-study) chemotherapy received by patients treated in the
phase III trial of pemetrexed plus cisplatin versus cisplatin alone in
malignant pleural mesothelioma. Annals Oncology, 16, 2005, 923–927.
[18] K.J. Whittle, P.J. Dunphy and J.F. Pennock, The isolation and properties of
delta-tocotrienol from Hevea latex, Biochem. J. 100, 1966, 138–145.
[19] R.S. Wong and A.K. Radhakrishnan, Tocotrienol research: past into present,
Nutr. Rev. 70, 2012, 483–490.
[20] V.B. Wali, S.V. Bachawal and P.W. Sylvester, Endoplasmic reticulum stress
59
mediates gamma-tocotrienol-induced apoptosis in mammary tumor cells,
Apoptosis 14, 2009, 1366–1377.
[21] V.B. Wali and P.W. Sylvester, Synergistic antiproliferative effects of
gamma-tocotrienol and statin treatment on mammary tumor cells, Lipids 42,
2007, 1113–1123.
[22] M. Berbéea, Q. Fua, M. Boermaa, J. Wanga, K.S. Kumarb and M.
Hauer-Jensena, Gamma-Tocotrienol ameliorates intestinal radiation injury
and reduces vascular oxidative stress after total-body irradiation by an
HMG-CoA reductasedependent mechanism, Radiat. Res. 171, 2009, 596–605.
[23] K.S. Ahn, G. Sethi, K. Krishnan and B.B. Aggarwal, Gamma-tocotrienol
inhibits nuclear factor-kappaB signaling pathway through inhibition of
receptor-interacting protein and TAK1 leading to suppression of
antiapoptotic gene products and potentiation of apoptosis, J. Biol. Chem. 282,
2007, 809–820.
[24] Q. Jiang, X. Rao, C.Y. Kim, H. Freiser, Q. Zhang, Z. Jiang and G. Li,
Gamma-tocotrienol induces apoptosis and autophagy in prostate cancer cells
by increasing intracellular dihydrosphingosine and dihydroceramide, Int. J.
Cancer 130, 2012, 685–693.
[25] S.U. Luk, W.N. Yap, Y.T. Chiu, D.T. Lee, S. Ma, T.K. Lee, R.S. Vasireddy,
Y.C. Wong, Y.P. Ching, C. Nelson, Y.L. Yap and M.T. Ling,
Gamma-tocotrienol as an effective agent in targeting prostate cancer stem
cell-like population, Int. J. Cancer 128, 2011, 2182–2191.
[26] A. Gopalan, W. Yu, B.G. Sanders and K. Kline, Eliminating drug resistant
breast cancer stem-like cells with combination of simvastatin and
gamma-tocotrienol, Cancer Lett. 328, 2013, 285–296.
[27] Z. Yang, H. Xiao, H. Jin, P.T. Koo, D.J. Tsang and C.S. Yang, Synergistic
actions of atorvastatin with gamma-tocotrienol and celecoxib against human
colon cancer HT29 and HCT116 cells, Int. J. Cancer 126, 2010, 852–863.
60
[28] M. Sakai, M. Okabe, H. Tachibana and K. Yamada, Apoptosis induction by
gamma-tocotrienol in human hepatoma Hep3B cells, J. Nutr. Biochem. 17,
2006, 672–676.
[29] C. Skogastierna, M. Johansson, P. Parini, M. Eriksson, L.C. Eriksson, L.
Ekstrom and L. Bjorkhem-Bergman, Statins inhibit expression of thioredoxin
reductase 1 in rat and human liver and reduce tumour development, Biochem.
Biophys. Res. Commun. 417, 2012, 1046–1051.
[30] T.J. Wilt, H.E. Bloomfield, R. MacDonald, D. Nelson, I. Rutks, M. Ho, G.
Larsen, A. McCall, S. Pineros and A. Sales, Effectiveness of statin therapy in
adults with coronary heart disease, Arch. Intern. Med. 164, 2004, 1427–1436.
[31] P. Lochhead and A.T. Chan, Statins and colorectal cancer, Clin.
Gastroenterol. Hepatol. 11, 2013, 109–118.
[32] W.W. Wong, J. Dimitroulakos, M.D. Minden and L.Z. Penn, HMG-CoA
reductase inhibitors and the malignant cell: the statin family of drugs as
triggers of tumor-specific apoptosis, Leukemia 16, 2002, 508–519.
[33] M. Osmak, Statins and cancer: current and future prospects, Cancer Lett.
324, 2012, 1–12.
[34] J.W. Jukema, C.P. Cannon, A.J. de Craen, R.G. Westendorp and S. Trompet,
The controversies of statin therapy: weighing the evidence, J. Am. Coll.
Cardiol. 60, 2012, 875–881.
[35] K. Undela, V. Srikanth and D. Bansal, Statin use and risk of breast cancer: a
meta-analysis of observational studies, Breast Cancer Res. Treat. 135, 2012,
261–269.
[36] X. Cui, Y. Xie, M. Chen, J. Li, X. Liao, J. Shen, M. Shi, W. Li, H. Zheng and B.
Jiang, Statin use and risk of pancreatic cancer: a meta-analysis, Cancer
Causes Control 23, 2012, 1099–1111.
[37] A. Thibault, D. Samid, A.C. Tompkins, W.D. Figg, M.R. Cooper, R.J. Hohl, J.
61
Trepel, B. Liang, N. Patronas, D.J. Venzon, E. Reed and C.E. Myers, Phase I
study of lovastatin, an inhibitor of the mevalonate pathway, in patients with
cancer, Clin. Cancer Res. 2, 1996, 483–491.
[38] C. Xu, B. Bailly-Maitre, J.C. Reed, endoplasmic reticulum stress: cell life and
death decisions, J Clin Invest. 115, 2005, 2656–2664.
[39] S. L. Amy, M. H. Linda, ER Stress and Cancer, Cancer Biology & Therapy. 5,
2006, 721–722.
[40] C. Koumenis, C. Naczki, M. Koritzinsky, S. Rastani, A. Diehl, N. Sonenberg,
A. Koromilas, B.G. Wouters, Regulation of protein synthesis by hypoxia via
activation of the endoplasmic reticulum kinase PERK and phosphorylation of
the translation initiation factor eIF2alpha, Mol. Cell. Biol. 22 (2002)
7405–7416.
[41] M. Moenner, O. Pluquet, M. Bouchecareilh, E. Chevet, Integrated
Endoplasmic Reticulum Stress Responses in Cancer, Cancer Res. 67, 2007,
10631–10634.
[42] S. Aznar and J.C. Lacal, Rho signals to cell growth and apoptosis, Cancer
Lett. 165, 2001, 1–10.
[43] P.W. Sylvester, Synergistic anticancer effects of combined gamma-tocotrienol
with statin or receptor tyrosine kinase inhibitor treatment, Genes Nutr. 7,
2012, 63–74.
[44] V.B. Wali, S.V. Bachawal and P.W. Sylvester, Suppression in mevalonate
synthesis mediates antitumor effects of combined statin and
gamma-tocotrienol treatment, Lipids 44, 2009, 925–934.
[45] H. Mo and C.E. Elson, Studies of the isoprenoid-mediated inhibition of
mevalonate synthesis applied to cancer chemotherapy and chemoprevention,
Exp. Biol. Med. (Maywood) 229, 2004, 567–585.
[46] H.K. Lim, P.V. Asharani and M.P. Hande, Enhanced genotoxicity of silver
62
nanoparticles in DNA repair deficient Mammalian cells, Front. Genet, 3,
2012, 104.
[47] Y. Sekido, Genomic abnormalities and signal transduction dysregulation in
malignant mesothelioma cells, Cancer Sci. 101, 2010, 1–6.
[48] S. Tomek, S. Emri, K. Krejcy and C. Manegold, Chemotherapy for malignant
pleural mesothelioma: past results and recent developments, Br. J. Cancer 88,
2003, 167–174.
[49] F. Vandermeers, P. Hubert, P. Delvenne, C. Mascaux, B. Grigoriu, A. Burny,
A. Scherpereel and L. Willems, Valproate, in combination with pemetrexed
and cisplatin, provides additional efficacy to the treatment of malignant
mesothelioma, Clin. Cancer Res. 15, 2009, 2818–2828.
[50] K. Nakashima, N. Virgona, M. Miyazawa, T. Watanabe and T. Yano, The
tocotrienol-rich fraction from rice bran enhances cisplatin-induced
cytotoxicity in human mesothelioma H28 cells, Phytother. Res. 24, 2010,
1317–1321.
[51] S.K. Park, B.G. Sanders and K. Kline, Tocotrienols induce apoptosis in breast
cancer cell lines via an endoplasmic reticulum stress-dependent increase in
extrinsic death receptor signaling, Breast Cancer Res. Treat. 124, 2010,
361–375.
[52] V.B. Wali, S.V. Bachawal and P.W. Sylvester, Combined treatment of
gamma-tocotrienol with statins induce mammary tumor cell cycle arrest in
G1, Exp. Biol. Med. (Maywood) 234, 2009, 639–650.
[53] W. Sun, W. Xu, H. Liu, J. Liu, Q. Wang, J. Zhou, F. Dong and B. Chen,
Gamma-Tocotrienol induces mitochondria-mediated apoptosis in human
gastric adenocarcinoma SGC-7901 cells, J. Nutr. Biochem. 20, 2009, 276–284.
[54] I.G. Berthold, H.K. Berthold, H. Gylling, M. Hallikainen, E. Giannakidou, S.
Stier, Y. Ko, D. Patel, A.K. Soutar, U. Seedorf, C.S. Mantzoros, J. Plat and W.
Krone, Effects of ezetimibe and/or simvastatin on LDL receptor protein
63
expressionand on LDL receptor and HMG-CoA reductase gene expression: a
randomized trial in healthy men, Atherosclerosis 198, 2008, 198–207.
[55] M. Rudling, B. Angelin, L. Ståhle, E. Reihnér, S. Sahlin, H. Olivecrona, I.
Björkhem and C. Einarsson, Regulation of hepatic low-density lipoprotein
receptor, 3-hydroxy-3-methylglutaryl coenzyme A reductase, and cholesterol
7alphahydroxylase mRNAs in human liver, J. Clin. Endocrinol. Metab. 87,
2002, 4307–4313.
[56] B.L. Song and R.A. DeBose-Boyd, Insig-dependent ubiquitination and
degradation of 3-hydroxy-3-methylglutaryl coenzyme a reductase stimulated
by delta- and gamma-tocotrienols, J. Biol. Chem. 281, 2006, 25054–25061.
[57] D.H. Wong, J.A. Villanueva, A.B. Cress, A. Sokalska, I. Ortega and A.J.
Duleba, Resveratrol inhibits the mevalonate pathway and potentiates the
antiproliferative effects of simvastatin in rat theca-interstitial cells, Fertil.
Steril. 96, 2011, 1252–1258.
[58] Y.S. Lin, J. Park, J.W. De Schutter, X.F. Huang, A.M. Berghuis, M. Sebag
and Y.S. Tsantrizos, Design and synthesis of active site inhibitors of the
human farnesyl pyrophosphate synthase: apoptosis and inhibition of ERK
phosphorylation in multiple myeloma cells, J. Med. Chem. 55, 2012,
3201–3215.
[59] M. Weis, C. Heeschen, A.J. Glassford and J.P. Cooke, Statins have biphasic
effects on angiogenesis, Circulation 105, 2002, 739–745.
[60] K. Sawada, K. Morishige, M. Tahara, R. Kawagishi, Y. Ikebuchi, K. Tasaka
and Y. Murata, Alendronate inhibits lysophosphatidic acid-induced migration
of human ovarian cancer cells by attenuating the activation of rho, Cancer
Res. 62, 2002, 6015–6020.
[61] D.A. Altomare, H. You, G.H. Xiao, M.E. Ramos-Nino, K.L. Skele, A. De
Rienzo, S.C. Jhanwar, B.T. Mossman, A.B. Kane and J.R. Testa, Human and
mouse mesotheliomas exhibit elevated AKT/PKB activity, which can be
targeted pharmacologically to inhibit tumor cell growth, Oncogene 24, 2005,
64
6080–6089.
[62] A. Mathy, P. Baas, O. Dalesio and N. van Zandwijk, Limited efficacy of
imatinib mesylate in malignant mesothelioma: a phase II trial, Lung Cancer
50, 2005, 83–86.
[63] S.J. Heo, K.N. Kim, W.J. Yoon, C. Oh, Y.U. Choi, A. Affan, Y.J. Lee, H.S. Lee
and D.H. Kang, Chromene induces apoptosis via caspase-3 activation in
human leukemia HL-60 cells, Food Chem. Toxicol. 49, 2011, 1998–2004.
[64] H. Sato, H. Iwata, Y. Takano, R. Yamada, H. Okuzawa, Y. Nagashima, K.
Yamaura, K. Ueno and T. Yano, Enhanced effect of connexin 43 on
cisplatin-induced cytotoxicity in mesothelioma cells, J. Pharmacol. Sci. 110,
2009, 466–475.
[65] K. Takahashi and G. Loo, Disruption of mitochondria during
tocotrienol-induced apoptosis in MDA-MB-231 human breast cancer cells,
Biochem. Pharmacol. 67, 2004, 315–324.
[66] Y. Soini, K. Kahlos, R. Sormunen, M. Säily, P. Mäntymaa, P. Koistinen, P.
Pääkkö and V. Kinnula, Activation and relocalization of caspase 3 during the
apoptotic cascade of human mesothelioma cells, APMIS 113, 2005, 426–435.
[67] I. Mohiuddin, X. Cao, B. Fang, M. Nishizaki and W.R. Smythe, Significant
augmentation of pro-apoptotic gene therapy by pharmacologic bcl-xl
down-regulation in mesothelioma, Cancer Gene Ther. 8, 2001, 547–554.
[68] X. Cao, C. Rodarte, L. Zhang, C.D. Morgan, J. Littlejohn and W.R. Smythe,
Bcl2/bcl-xL inhibitor engenders apoptosis and increases chemosensitivity in
mesothelioma, Cancer Biol. Ther. 6, 2007, 246–252.
[69] J.H. Stewart, D.M. Nguyen, G.A. Chen and D.S. Schrumpp, Induction of
apoptosis in malignant pleuralmesothelioma cells by activation of Fas
(Apo-1/CD95) death-signal pathway, J. Thorac. Cardiovasc. Surg. 23, 2002,
295–302.
65
[70] M. Kitamura, Endoplasmic reticulum stress and unfolded protein response in
renal pathophysiology: Janus faces. Am J Physiol Renal Physiol. 295, 2008,
323–334.
[71] A.D. Garg, A. Kaczmarek, O. Krysko, P. Vandenabeele, D.V. Krysko, P.
Agostinis, ER stress-induced inflammation: does it aid or impede disease
progression?, Trends Mol Med. 18, 2012, 589–98.
[72] H.L. Pahl, Signal transduction from the endoplasmic reticulum to the cell
nucleus. Physiol Rev. 79, 1999, 683–701.
[73] G. Jing, J.J. Wang, S.X. Zhang, ER stress and apoptosis: a new mechanism
for retinal cell death. Exp Diabetes Res. 2012, 2012, 1–11.
[74] L. Moretti, Y.I. Cha, K.J. Niermann, B. Lu, Switch between apoptosis and
autophagy: radiation-induced endoplasmic reticulum stress?, Cell Cycle. 6,
2007, 793–798.
[75] H. Urra, E. Dufey, F. Lisbona, D. Rojas-Rivera, C, Hetz, When ER stress
reaches a dead end, Biochim Biophys Acta. 1833, 2013, 3507–3517.
[76] Y. Chen, F. Brandizzi, IRE1: ER stress sensor and cell fate executor. Trends
Cell Biol. 23, 2013, 547–55.
[77] C.L. Liu, X. Li, G.L. Hu, R.J. Li, Y.Y. He, W. Zhong, S. Li, K.L. He, L.L. Wang,
Salubrinal protects against tunicamycin and hypoxia induced cardiomyocyte
apoptosis via the PERK-eIF2α signaling pathway, J Geriatr Cardiol. 9, 2012,
258–268.
[78] M. Moenner, O. Pluquet and M. Bouchecareilh, Integrated endoplasmic
reticulum stress responses in cancer, Cancer Res. 67, 2007, 10631–10634.
[79] G.P. Meares, A.A. Zmijewska and R.S. Jope, HSP105 interacts with GRP78
and GSK3 and promotes ER stress-induced caspase-3 activation, Cell. Signal.
20, 2008, 347–358.
66
[80] H.Y. Tsai, Y.F. Yang, A.T. Wu, C.J. Yang, Y.P. Liu, Y.H. Jan, C.H. Lee, Y.W.
Hsiao, C.T. Yeh, C.N. Shen, P.J. Lu, M.S. Huang and M. Hsiao, Endoplasmic
reticulum ribosome-binding protein 1 (RRBP1) overexpression is frequently
found in lung cancer patients and alleviates intracellular stress-induced
apoptosis through the enhancement of GRP78, Oncogene 2013, 1–11, (epub
ahead of print).
[81] D. Patacsil, A.T. Tran, Y.S. Cho, S. Suy, F. Saenz, I. Malyukova, H. Ressom,
S.P. Collins, R. Clarke and D. Kumar, Gamma-tocotrienol induced apoptosis
is associated with unfolded protein response in human breast cancer cells, J.
Nutr. Biochem. 23, 2012, 93–100.
[82] T. Nakagawa, H. Zhu, N. Morishima, E. Li, J. Xu, B.A. Yankner and J. Yuan,
Caspase-12 mediates endoplasmic-reticulum-specific apoptosis and
cytotoxicity by amyloid-beta, Nature 403, 2000, 98–103.
[83] M. Boyce, K.F. Bryant, C. Jousse, K. Long, H.P. Harding, A selective
Inhibitor of eIF2a dephosphorylation protects cells from ER stress, SCIENCE.
307, 2005, 935–939.
[84] T. Hosoi, A. Kume, K. Otani, T. Oba, K. Ozawa, A unique modulator of
endoplasmic reticulum stress-signalling pathways: the novel pharmacological
properties of amiloride in glial cells, Br. J. Pharmacol. 159, 2010, 428–437.
[85] M.A. Bogoyevitch, The isoform-specific functions of the c-Jun N-terminal
Kinases (JNKs): differences revealed by gene targeting, BioEssays 28, 2006,
923–934.
[86] H. Zhu, H. Zhu, S. Xiao, H. Sun, C. Xie, Y, Ma, Activation and crosstalk
between the endoplasmic reticulum road and JNK pathway in
ischemia-reperfusion brain injury, Acta Neurochir (Wien). 154, 2012,
1197–203.
[87] M. Koyuturk, M. Ersoz, N. Altiok, Simvastatin induces apoptosis in human
breast cancer cells: p53 and estrogen receptor independent pathway
requiring signalling through JNK, Cancer Lett. 250, 2007, 220–228.
67
[88] A. Gopalan, W. Yu, Q. Jiang, Y. Jang, B.G. Sanders, K. Kline, Involvement
of de novo ceramide synthesis in gamma-tocopherol and
gamma-tocotrienol-induced apoptosis in human breast cancer cells. Mol Nutr
Food Res. 56, 2012, 1803–1811.
[89] M.K. Jung, Y.K. Houh, S. Ha, Y. Yang, D. Kim, T.S. Kim, S.R. Yoon, S.I.
Bang, B.J. Cho, W.J. Lee, H. Park, D. Cho, Recombinant Erdr1 suppresses
the migration and invasion ability of human gastric cancer cells, SNU-216,
through the JNK pathway, Immunol Lett. 150, 2013, 145–151.
[90] S. Win, T.A. Than, J.C. Fernandez-Checa, N. Kaplowitz, JNK interaction
with Sab mediates ER stress induced inhibition of mitochondrial respiration
and cell death, Cell Death and Disease, 5, 2014, e989.
[91] J.H. Lin, P. Walter, T.S. Yen, Endoplasmic reticulum stress in disease
pathogenesis, Annu Rev Pathol. 3, 2008, 399–425.
[92] S.S. Anand, M. Maruthi, P.P. Babu, The specific, reversible JNK inhibitor
SP600125 improves survivability and attenuates neuronal cell death in
experimental cerebral malaria (ECM), Parasitol Res. 112, 2013, 1959–66.
[93] D.O. Moon, M.O. Kim, Y.H. Choi, N.D. Kim, J.H. Chang, G.Y. Kim, Bcl-2
overexpression attenuates SP600125-induced apoptosis in human leukemia
U937 cells, Cancer Lett. 264, 2008, 316–325.
[94] Y. Murakami, E. Aizu-Yokota, Y. Sonoda, S. Ohta, T. Kasahara, Suppression
of endoplasmic reticulum stress-induced caspase activation and cell death by
the overexpression of Bcl-xL or Bcl-2, J Biochem. 141, 2007, 401–410.
[95] P. Yenki, F. Khodagholi, F. Shaerzadeh, Inhibition of phosphorylation of JNK
suppresses Aβ-induced ER stress and upregulates prosurvival mitochondrial
proteins in rat hippocampus, J Mol Neurosci. 49, 2013, 262–269.
[96] B. Favaloro, N. Allocati, V. Graziano, C. Di Ilio, V. De Laurenzi, Role of
apoptosis in disease, Aging (Albany NY). 4, 2012, 330–349.
68
[97] T.J. Fan, L.H. Han, R.S. Cong, J. Liang, Caspase family proteases and
apoptosis, Acta Biochim Biophys Sin (Shanghai). 37, 2005, 719–727.
[98] A. Jimbo, E. Fujita, Y. Kouroku, J. Ohnishi, N. Inohara, K. Kuida, K.
Sakamaki, S. Yonehara, ER stress induces caspase-8 activation, stimulating
cytochrome c release and caspase-9 activation, Experimental Cell Research,
283, 2003, 156–166.
[99] S. M. Kim, H. S. Park, D. Y. Jun, H. J. Woo, M. H. Woo, C. H. Yang, Y. H.
Kim, Mollugin induces apoptosis in human Jurkat T cells through
endoplasmic reticulum stress-mediated activation of JNK and caspase-12 and
subsequent activation of mitochondria-dependent caspase cascade regulated
by Bcl-xL, Toxicology and Applied Pharmacology, 241, 2009, 210–220.
[100] S.I. Katz, L. Zhou, G. Chao, C.D. Smith, T. Ferrara, W. Wang, D.T. Dicker,
W.S. El-Deiry, Sorafenib inhibits ERK1/2 and MCL-1(L) phosphorylation
levels resulting in caspase-independent cell death in malignant pleural
mesothelioma, Cancer Biol Ther. 8, 2009, 2406–2416.
69
List of publication
Guligena Tuerdi, Saki Ichinomiya, Hiromi Sato, Sana Siddig, Eriko Suwa, Hiroki Iwata,
Tomohiro Yano, Koichi Ueno. Synergistic effect of combined treatment with
gamma-tocotrienol and statin on human malignant mesothelioma cells. Cancer Letters,
2013, 339(1), 116-127.
70
Acknowledgements
First and foremost, I would like to express my sincere gratitude and appreciation
to my supervisor, Professor Koichi Ueno for his continues guidance and support
during my studies. Many thanks for his continuous discussions and encouragement.
Many thanks for his efforts in reviewing and correcting this thesis manuscript.
Second, I would like my teacher, Assistant Professor Hiromi Sato whose useful
suggestions, incisive comments and constructive criticism have contributed greatly
to the completion of this thesis. She devotes a considerable portion of her time to
reading my manuscripts. Her tremendous assistance in developing the framework
for analysis and in having gone through the draft versions of this thesis several
times as well as her great care in life deserve more thanks than I can find words to
express.
After that, I am also greatly indebted to all my teachers who have helped me
directly and indirectly in my studies. Any progress that I have made is the result of
their profound concern and selfless devotion. Among them the following require
mentioning: Associate Professor Katsunori Yamaura, Professor Toshihiko Toida,
and Professor Rena Kasimu.
Then, I would like to thank deeply to Department of Geriatric Pharmacology and
Therapeutics laboratory mates and friends companionship and assistance especially
Ph.D. Eriko Suwa.
Last but not least, I would like to deepest thanks go to my beloved family for their
encouragement and support which have been rendered to me throughout my study
in Japan. They have reminded me that what I do would been important. When I am
feeling down or stressed out their listening to me helped me a lot. My parents are
my proud of my life.
71
Examiners
This thesis for the doctorate in pharmaceutical sciences was examined by the
following referees authorized by the Graduated School of Pharmaceutical Sciences
Chiba University, Japan.
Professor of Chiba University (Graduate School of Pharmaceutical Sciences)
Nobunori Sato, Ph.D. (Pharm. Sci) ~Chief examiner~
Professor of Chiba University (Graduate School of Pharmaceutical Sciences)
Hiroyuki Takano, M.D. & Ph.D.
Professor of Chiba University (Graduate School of Pharmaceutical Sciences)
Yuko Sekine, Ph.D. (Pharm. Sci)