PPAR ResearchVolume 2012 (2012), Article ID 269751, 16 pagesdoi:10.1155/2012/269751

Research Article

AS601245, an Anti-Inflammatory JNK Inhibitor, and Clofibrate Have a Synergistic Effect in Inducing Cell Responses and in Affecting the Gene Expression Profile in CaCo-2 Colon Cancer Cells

Angelo Cerbone,¹ Cristina Toaldo,² Stefania Pizzimenti,² Piergiorgio Pettazzoni,² Chiara Dianzani,³ Rosalba Minelli,³ Eric Ciamporcero,² Guglielmo Roma,¹ Mario Umberto Dianzani,² Roberto Canaparo,⁴ Carlo Ferretti,⁴ and Giuseppina Barrera²

¹MerckSerono Ivrea, Istituto di Ricerche Biomediche “A. Marxer”, RBM S.p.A., 10010 Colleretto Giacosa, Italy²Department of Medicine and Experimental Oncology, Section of General Pathology, University of Turin, 10125 Turin, Italy³Department of Anatomy, Pharmacology and Forensic Medicine, Section of Pharmacology and Pharmacognosy, University of Turin,10125 Turin, Italy⁴Department of Anatomy, Pharmacology, and Forensic Medicine, Section of Pharmacology and Experimental Therapy, University of Turin, 10125 Turin, Italy

Received 2 August 2011; Revised 29 October 2011; Accepted 1 November 2011

Academic Editor: J. Reddy

Copyright © 2012 Angelo Cerbone et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract.

PPARαs are nuclear receptors highly expressed in colon cells. They can be activated by the fibrates (clofibrate, ciprofibrate etc.) used to treat hyperlipidemia. Since PPARα transcriptional activity can be negatively regulated by JNK, the inhibition of JNK activity could increase the effectiveness of PPARα ligands. We analysed the effects of AS601245 (a JNK inhibitor) and clofibrate alone or in association, on proliferation, apoptosis, differentiation and the gene expression profile of CaCo-2 human colon cancer cells. Proliferation was inhibited in a dose-dependent way by clofibrate and AS601245. Combined treatment synergistically reduced cell proliferation, cyclin D1 and PCNA expression and induced apoptosis and differentiation. Reduction of cell proliferation, accompanied by the modulation of p21 expression was observed in HepG2 cells, also. Gene expression analysis revealed that some genes were highly modulated by the combined treatment and 28 genes containing PPRE were up-regulated, while clofibrate alone was ineffective. Moreover, STAT3 signalling was strongly reduced by combined treatment. After combined treatment, the binding of PPARα to PPRE increased and paralleled with the expression of the PPAR coactivator MED1. Results demonstrate that combined treatment increases the effectiveness of both compounds and suggest a positive interaction between PPARα ligands and anti-inflammatory agents in humans.

1. Introduction

PPARs are ligand-activated transcription factors belonging to the nuclear receptor superfamily. Three molecular forms of PPAR have been identified, namely, PPARα, PPARβ/δ, and PPARγ, and all involved in many different biological processes [1]. PPARα is the predominant PPAR subtype highly expressed in liver, heart, proximal tubules of kidney cortex, skeletal muscle, intestinal mucosa, and in brown adipose tissues that are metabolically very active [2].

Endogenous ligands with high specificity for PPARα are long-chain unsaturated fatty acids and fatty acid derivatives [3, 4]. Fibrates, which are hypolipidemic drugs used in the treatment of hyperlipidemia, are among the group of synthetic ligands, which are the most important agonists of PPARα.

Since PPARα is expressed in the digestive tract and mainly localized in the intestinal mucosa in the small intestine and in the colon, it has been proposed that a physiological role of the receptor may be to sense the total flux of dietary fatty acids in key tissues [5]. Colon epithelial cells can be physiologically exposed not only to fatty acids but also to hypolipidemic drugs such as fibrates, all PPARα agonists. For this reason, there is particular interest to study the effect of PPARα ligands in colon cancer cells.

Less is known about the role of PPARα in human tumors. Generally, activation of this PPAR by agonists causes inhibition of tumor cell growth [6, 7]. In contrast, in liver murine cell models, Wy-14,643, clofibrate, ciprofibrate, and DEHP were inducers of c-fos, c-jun, junB egr-1, and NUP475 [8]. Indeed, PPARα has been widely employed in hepatocarcinogenesis protocols for rodents [9, 10]. However, in human cell models, PPAR ligands downregulate oncogenes and upregulate proapoptotic genes also [11, 12]. In particular, the proapoptotic role of PPARα ligands has been outlined by a recent review [13].

Beside ligand induction, PPARα activity can be regulated by JNK and p38 mitogen-activated protein kinase (MAPK) phosphorylation. The p38 MAPK phosphorylates the A/B domain of PPARα and enhances its ligand-dependent transcriptional activity [14]. On the contrary, the activation of ERK-MAPK decreases PPARα activity [15]. By inhibiting Rho A, a component of Rho family proteins, which regulate the JNK and the p38 MAPK cascades, cerivastatin stimulates PPARα transcriptional activity by reducing its phosphorylation [16].

AS601245[1,3-Benzothiazol-2-yl-(2-{[2-(3-pyridinyl)ethyl]amino}-4-pyrimidinyl) acetonitrile; JNK inhibitor V] has been selected as a potent and selective JNK inhibitor with anti-inflammatory properties [17]. In the present work, we intend to assess its effect on clofibrate action in colon cancer cells. In particular, we examined the effects of AS601245 and clofibrate, alone or in association, on apoptosis, differentiation, and PPRE binding activity of PPARα in CaCo-2 human colon cancer cells and analysed, through microarray analysis (Affymetrix GeneChip), the gene expression pattern in control and drug-treated cells. Moreover, since the liver is the major target organ expressing PPARα, to assess whether combined treatment could produce some toxic effects in liver cells, we tested, through MTT analysis, the acute toxicity of the both substances and the effect of single and combined treatments on cell proliferation and proliferation-related gene expressions in HepG2 human hepatic cells.

2. Materials and Methods

2.1. Cell Culture and Treatments

CaCo-2 and HepG2 cells, obtained from European Collection of Cell Cultures (ECACC), were cultured at 37°C in a humidified atmosphere of 5% CO₂-air. For all experiments, cells, from 1 to 10 passages, were used. Cells were grown in D-MEM medium supplemented with 10% fetal bovine serum (HyClone, Italy), 2 mM glutamine, 1% nonessential amino acids solution and 1% antibiotic mixture (penicillin streptomycin) (Sigma, Milano, Italy).

Treatments with clofibrate and AS601245[1,3-benzothiazol-2-yl-(2-{[2-(3-pyridinyl)ethyl]amino}-4-pyrimidinyl) acetonitrile; JNK inhibitor V] (SPRI, Geneva, Switzerland) were performed by suspending the drugs in DMSO. The concentration of vehicle in culture did not exceed 1%. Moreover, cultures, treated with 1% DMSO alone, were performed to exclude the vehicle’s effects.

2.2. Cell Proliferation and Viability

CaCo-2 cell proliferation was evaluated by using the kit “CellTiter-Glo Luminescent Cell Viability Assay” (Promega, Milano, Italy). This highly sensitive assay detects the luminescence released by the metabolically active cells. Quantification of luminescence was expressed as RLU (relative light unit). For the proliferation experiments, treatments were performed by adding the drugs (at different concentrations) to the CaCo-2 cells seeded at about 4,000 cells/well in a 96-well plate. HepG2 cell proliferation was analysed through the MTT method. Briefly, 1500 cells/well were seeded in 200 μL of serum-supplemented media and the following day treated with the drugs. 20 μL of 5 mg/mL thiazolyl blue tetrazolium bromide (M2128-SIGMA Aldrich) was subsequently added to the cells and removed 2 hours later. 100 μL of DMSO was added to the cells, and the absorbance was recorded at 570 nm through a 96 well plate ELISA reader. Viability was evaluated through Trypan blue (T8154 SIGMA Aldrich) exclusion test.

2.3. Detection of Apoptosis

Apoptosis was evaluated, 24 and 48 hours after the treatments, by using a Kit Caspase-GLO 3/7 Assay (Promega, Milano, Italy) and confirmed by TUNEL test. The Caspase-GLO 3/7 assay determines the amount of caspase 3 and 7 cleavage of the luminogenic substrate resulting in luciferase reaction and production of light. The TUNEL method from Promega (Milano, Italy) consists of the terminal deoxynucleotidyl transferase-mediated nick-end labelling of FITC-conjugated deoxyuridine triphosphate. Incorporated fluorescein was detected using a fluorescence microscope (Leitz, Dialux 20, Oberkochen, Germany). The number of apoptotic cells was determined by counting the percentage of green fluorescence-positive cells. At least, 100 cells were counted for each experiment. CaCo-2 cells treated with 10 mM butyrate were used as positive control of apoptosis.

2.4. Detection of Differentiated Cells

Differentiation was determined by counting the dome formation in the control or treated cells. Dome formation, which can be attributed to ion and water transport across polarized epithelial cells [18], was quantified in confluent CaCo-2 monolayers using inverted light microscopy and expressed as the number of domes per square centimetre. Domes were recognised as a cohesive group of approximately 30 cells or more that were in a different plane of view compared to cells attached to the culture plate.

Preliminary experiments demonstrated that results obtained by dome count were similar to those obtained with two other methods (transepithelial electrical resistance (TEER) determination and phosphates alkaline assay) (data not shown). CaCo-2 cells treated with 2 mM sodium butyrate (Sigma, Milano, Italy) were used as a positive control.

2.5. RNA Extraction and Array Hybridization

Total RNA from 3 biological replicates of each treatment was isolated using TRIzol reagent (Invitrogen, Milano, Italy). Samples were treated with DNase in order to avoid any genomic contamination. The quality of the resulting RNA was determined by using the Agilent 2100 Bioanalyzer (Agilent Technologies), and RNA content was normalized by using the Thermo Scientific NanoDrop ND-1000 spectrophotometer. RNA samples of each replicate were analyzed by using Affymetrix GeneChip Human Genome U133A plus 2.0 chips (Affymetrix).

GCOS software version 1.2 (Affymetrix) was used to define the probe cell and to calculate the intensity for each cell. CEL files generated were analyzed for the overall data quality using R/Bioconductor. Then, they were processed into the Rosetta Resolver dataset for data normalization, generation of expression values, and statistical analysis. Expression values of all treatment groups were obtained as a ratio versus the negative control (1% DMSO).

Differential analyses between pairs of groups were performed with 1-way ANOVA followed by the Benjamini-Hochberg multiple testing correction (False Discovery Rate-FDR cut-off of 1%) and a Student-Newman-Keuls post hoc analysis. Finally, differentially expressed genes were analysed in Ingenuity Pathway Analysis software version 7.5 (Ingenuity Systems, http://www.ingenuity.com/).

2.6. Real-Time RT-PCR

We selected 4 genes that had shown an approximately 2-fold change in expression for further study by RT-PCR in a separate experiment. Two of these (GANAB and IL6ST) were found to be increased in Affymetrix analysis, whereas the other two were found to be decreased (FGFR2 and CCNG). Total RNA was reverse transcribed into cDNA in a 20 μL reaction using the TaqMan High Capacity cDNA Reverse Transcription Kit provided by Applied Biosystems. 500 ng of total RNA was used as the starting material from each sample. For each Real-Time PCR reaction, the reverse transcribed sample was used as a template. Target mRNA was quantified using an ABI 7900 HT Fast real-time PCR system (Applied Biosystems). Primers were purchased from Applied Biosystems: GANAB (glucosidase, alpha; neutral AB, Hs00929274_m1), IL6ST (interleukin 6 signal transducer (gp130, oncostatin M receptor, Hs00174360_m1), CCNG (cyclin G2, Hs00171119_m1), and FGFR2 (fibroblast growth factor receptor 2, Hs01552926_m1). The TaqMan probes were labelled with a 5′ reporter dye (FAM, 6-carboxyfluorescein) and a 3′ quencher dye (TAMRA, 6-carboxytetramethylrhodamine). Real-time PCR reactions were carried out in triplicate. Data were analyzed by the ABI Sequence Detection System (SDS) software using the relative quantification. The fold changes are determined by the ΔΔCt method as described in Applied Biosystems User Bulletin no. 2.

2.7. DNA-Binding Activity of PPARα

The PPARα binding activity assay was performed by using Trans-AM ELISA-based kit from Active Motif (Carlsbad, CA, USA) according to the manufacturer’s protocol. Briefly, cell extracts were incubated in a 96-well plate coated with an oligonucleotide containing the PPRE motif (5′-AACTAGGTCAAAGGTCA-3′). PPAR contained in nuclear extract, specifically bound to the immobilized oligonucleotide, was detected by using an antibody anti-PPARα (clone H-98, from Santa Cruz Biotechnology) followed by a secondary HRP- (horseradish-peroxidase-) conjugated antibody (Bio-Rad Laboratories) in an ELISA-like assay.

2.8. Western Blot Analysis

Total extracts were prepared by lysis in a buffer containing Tris-HCl buffer, pH 7.4, 150 mM NaCl, 5 mM EDTA, 1% Nonidet P-40, 1 mM sodium orthovanadate, 1 mM phenylmethylsulfonyl fluoride, and 0.05% aprotinin. Insoluble proteins were discarded by high-speed centrifugation at 4°C. Protein concentration in the supernatant was measured in triplicate using a commercially available assay (Bio-Rad Laboratories, Segrate, Italy).

All proteins were separated by SDS-polyacrylamide gel and electroblotted on nitrocellulose membrane (Bio-Rad Laboratories, Segrate, Italy). Membranes were blocked overnight at 4°C in Tris buffered saline (TBS) containing 5% milk plus 0.5% Tween 20 and then incubated at room temperature with primary antibodies (anti-P-PPAR alpha (Ser21) from Thermo Scientific; anti-PPAR alpha from Millipore; anti-STAT3 clone F-2, anti-p-STAT3 (Tyr705) clone B-7, anti-PCNA clone FL-261, anticyclin D1 clone A12 from Santa Cruz Biotechnology; anti-p-STAT3 (Ser727) from ThermoScientific; anti-PPARBP (MED1) clone 2A2; anti-β-actin clone AC-1 from Sigma-Aldrich; anti-P-Jun from cell signaling; anti-p21 from Abcam and horseradish-peroxidase-conjugated secondary antibodies (Bio-Rad Laboratories, Segrate, Italy). Detection was carried out by enhanced chemiluminescence (ECL) according to the manufacturer’s protocol (Amersham-Pharmacia Biotech, Italy, Cologno Monzese, Italy).

Densitometric analysis was performed by using a software program (Multi-Analyst, version 1.1, Bio-Rad Laboratories, Segrate, Italy). All results were standardized using the signal obtained with β-actin.

2.9. Statistical Analysis

The 2-way ANOVA was performed in the proliferation, apoptosis, differentiation, and PPRE binding assays.

3. Results

3.1. Growth of Clofibrate and AS601245-Treated Cells

Both clofibrate and AS601245 were able to inhibit CaCo-2 cell proliferation in a dose-dependent way (Figures 1(a) and 1(b)). To evaluate the efficacy on cell growth of the combination of clofibrate and AS601245, we chose doses able to reduce cell proliferation by 20% (IC20) after 48 hours of treatment. These doses were 5 μM clofibrate (IC 20 : 5 ± 0.4) and 0.1 μM AS601245 (IC 20 : ). Combined treatment significantly reduced cell growth after 72 and 96 hours from the treatment (Figure 1(c)). The treatment with two compounds synergistically reduced the cell growth after 72 hours, whereas, after 96 hours, the reduction is less pronounced. The doses of 5 μM clofibrate, 0.1 μM AS601245, and the combined treatment with these doses were used for all the subsequent experiments.

(a)

(b)

(c)

Figure 1: Caco-2 cell proliferation. (a) Growth of Caco-2 cells treated with clofibrate at the indicated concentrations (from 1 to 50 μM) and at different times; (b) growth of Caco-2 cells treated with AS601245 at the indicated concentrations (from 0,1 to 10 μM) and at different times; (c) growth of Caco-2 cells treated with 5 μM clofibrate, 0,1 μM AS601245, and the association of these two compounds (Clofi + AS601245). Cell proliferation was detected by measuring the luminescence released by the metabolically active cells. The values expressed in RLU (relative light units) are the means ± SD of three separate experiments. Variance analysis: *, ** versus control.

3.2. Proliferation-Related Genes Expressions

Since the reduction of proliferation can be accompanied by the modulation of specific genes, we determined the expression of proliferating cell nuclear antigen (PCNA), cyclin D1 and p21, in CaCo-2 cells. Moreover, we found that AS601245 at the concentration of 0.1 μM was able to inhibit Jun phosphorylation in CaCo-2 cells. In Figure 2(a), the analysis of P-Jun expression revealed that the amount of P-Jun protein was reduced in cells treated with 0.1 μM AS601245. A similar result was observed in cells treated with AS601245 plus clofibrate.

(a)

(b)

(c)

(d)

Figure 2: Proliferation-related protein expressions. (a) Determination of 0.1 μM AS601245 effect in reducing P-Jun expression; (b) time course of PCNA expression in CaCo-2 cells treated with 5 μM clofibrate, 0.1 μM AS601245, and the association of these two compounds (Clofi + AS601245); (c) time course of cyclin D1 expression in CaCo-2 cells treated with 5 μM clofibrate, 0.1 μM AS601245, and the association of these two compounds (Clofi + AS601245); (d) time course of p21 expression in CaCo-2 cells treated with 5 μM clofibrate, 0.1 μM AS601245, and the association of these two compounds (Clofi + AS601245). Graphics represent the relative quantification of protein products performed by densitometric scanning. Data were normalized by using the β-actin signal, expressed as arbitrary densitometric units, and are the mean ± SD of three separate experiments from three different preparations for each condition. Variance analysis: *, ** versus control.

The PCNA expression was reduced in CaCo-2 cells only after 72 hours from the treatments with clofibrate, AS601245, and their combination (Figure 2(b)). Cyclin D1 expression was induced by clofibrate 48 hours from the treatment, but, in the following hours, its expression decreased particularly in combined treatment (Figure 2(c)). Finally, p21 expression did not vary significantly after the treatments (Figure 2(d)).

3.3. Apoptosis and Differentiation after AS601245 and Clofibrate Treatments

Apoptosis detection is reported in Figure 3. Both clofibrate and AS601245 were unable to induce apoptosis when added separately to CaCo-2 cells. Conversely, the association of these two compounds induced a significant increase in caspase 3/7 activity, at 24 and 48 hours after the combined treatments. After 48 hours from the combined treatment, the caspase 3/7 activity was about 4-fold higher than that detected in the control cells. These results were confirmed by using TUNEL test (data not shown).

Figure 3: Induction of apoptosis. Induction of apoptosis in CaCo-2 cells treated with 5 μM clofibrate, 0.1 μM AS601245, and the association of these two compounds (Clofi + AS601245). Apoptosis was evaluated at 0, 24, and 48 hours after the treatments, by measuring caspase 3/7 activity. 20 mM butyrate was used as a positive control. Results normalized to the respective control value for each experimental time is the mean ± SD of three separate experiments from three different preparations for each condition. Variance analysis: ** versus control.

Differentiation of CaCo-2 cells was induced by 0.1 μM AS601245 at 48 hours after the treatment, whereas clofibrate alone did not increase the Dome number (Figure 4). Combined treatment increased the Dome number after 24 hours and caused a greater induction of differentiation compared to single treatments, after 48 hours (an increase of about 5-fold with respect to the control value).

Figure 4: Induction of differentiation. Differentiation of CaCo-2 cells treated with 5 μM clofibrate, 0.1 μM AS601245, and the association of these two compounds (Clofi + AS601245). Cell differentiation was evaluated at 24 and 48 hours after the start of treatments, by measuring dome formation. 2 mM butyrate was used as a positive control. Results, expressed as number of domes per cm², are the mean ± SD of three separate experiments from three different preparations for each condition. Variance analysis: *, ** versus control; $$, versus clofibrate-treated cells; # versus AS601245-treated cells. The picture represents a microscopic image of domes.

3.4. Microarray Analysis of Gene Expression in CaCo-2 Cells

To analyze whether the cell responses to the treatments with 5 μM clofibrate, 0.1 μM AS601245, or with both substances were a consequence of a specific gene pathway modulation, we performed microarray analysis by using the Affymetrix GeneChip platform, 24 hours after the treatments. The complete list of the genes modulated by clofibrate, AS601245, and by the combined treatment is reported in the supplementary data (See Table A in Supplementary Material available online at doi:10.1155/2012/269751). To confirm results obtained by microarray analysis, real time-PCR of 4 selected genes (2 upregulated and 2 downregulated) was performed. Results, reported in supplementary data (Table B), indicated that the up or down fold changes obtained by microarray analysis were similar to those obtained in real-time PCR. Some discrepancies were found only for FGFR2 and CCNG that did not change in clofibrate treated cells, if evaluated by microarray analysis, whereas they were decreased by about −1.5-fold, if analysed by real-time PCR. The supplementary data (Table C) also indicates the genes affected by clofibrate, by AS601245, and by the combined treatment with clofibrate and AS601245, arranged with respect to the relative biological functions and listed on the basis of the value. The genes mainly affected by clofibrate, which modulated a limited group of genes, belonged to the “cancer,” “cellular development,” and “gene expression” groups. AS601245 modulated genes belonging to “cancer,” “cell cycle,” “genetic disorders,” and “cell death” groups. The combined treatments affected mainly genes belonging to “cancer” and “genetic disorder” functions.

The Venn diagram (Figure 5) shows that clofibrate modulated 182 genes, AS601245 modulated 2855 genes, and the combined treatments modulated 848 genes. Among the genes affected by clofibrate alone or AS601245 alone, 161 were common in both of the two groups. The combined treatment affected 108 genes which were present in both the clofibrate and AS601245 groups and 260 genes which were not affected by either clofibrate or AS601245 alone. Among these 260 genes, 65 only were downregulated by the combined treatment, whereas 195 genes were upregulated.

Figure 5: Microarray analysis of gene expression. Venn diagram derived from microarray analysis of gene expression in CaCo-2 cells treated with 5 μM clofibrate, 0.1 μM AS601245, and the association of these two compounds (Clofi + AS601245) at 24 hours. The diagram shows the number of genes modulated by the treatments.

The top ten genes changed the most by the clofibrate treatment, with respect to 1% DMSO treated cells, are reported in Table 1. Clofibrate treatment (Table 1(a)) mainly increased the expression of the GANAB gene (3.8-fold change) which encodes glucosidase alpha, the ATF6B gene which encoded a transcription factor belonging the unfolded protein response (UPR) pathway during ER stress [19, 20], and some genes, belonging to “cancer” function (DLST, IL6ST, MEX3d). Among genes downregulated by clofibrate, the major part belonged mainly to functional groups: “cancer” (STIP1, HNRNPA1, VIL1, and CDH1) and “cellular assembly and organization” (CLASP1 and MACF1).

Table 1: Top ten genesb.

(a) Clofibrate

Gene ID
Gene name
Fold change

GANAB*
Glucosidase, alpha; neutral AB
+3.8

ATF6B
Activating transcription factor 6 beta
+2.8

SETD5
SET domain containing 5
+2.6

NFAT5
Nuclear factor of activated T cells 5, tonicity-responsive
+2.5

DLST
Dihydrolipoamide S-succinyltransferase (E2 component of 2-oxoglutarate complex)
+2.3

IL6ST
Interleukin 6 signal transducer (gp130, oncostatin M receptor)
+2.1

HNRNPA0
Heterogeneous nuclear ribonucleoprotein A0
+2.0

MEX3D
Mex-3 homolog D (C. elegans)
+1.6

CTSZ
Cathepsin Z
+1.5

STIP 1
Stress-induced phosphoprotein 1
−3.1

CLASP 1
Cytoplasmic linker-associated protein 1
−3.1

MACF 1
Microtubule-actin cross-linking factor 1
−2.9

COPA
Coatomer protein complex, subunit alpha
−2.7

HNRNPA1
Heterogeneous nuclear ribonucleoprotein A1
−2.6

SPSB2
SplA/ryanodine receptor domain and SOCS box containing 2
−2.3

TSR1
TSR1, 20S rRNA accumulation, homolog (S. cerevisiae)
−2.3

VIL1*
Villin 1
−2.3

CDH1
Cadherin 1, type 1, E-cadherin (epithelial)
−2.2

CRTAP
Cartilage-associated protein
−2.2

(b) AS601245

Gene ID
Gene name
Fold change

CYP1A1
Cytochrome P450, family 1, subfamily A, polypeptide 1
+5.3

AP3D1
Adaptor-related protein complex 3, delta 1 subunit
+3.6

NFAT5
Nuclear factor of activated T cells 5, tonicity-responsive
+3.1

BMP2K
Bone morphogenetic protein 2 inducible kinase
+2.9

DLST
Dihydrolipoamide S-succinyltransferase (E2 component of 2-oxoglutarate complex)
+2.8

IL6ST
Interleukin 6 signal transducer (gp130, oncostatin M receptor)
+2.8

FAM76B
Family with sequence similarity 76, member B
+2.4

MGA
MAX gene associated
+2.4

THRAP3
Thyroid hormone receptor-associated protein 3
+2.4

GANAB
Glucosidase, alpha; neutral AB
+2.3

RPS27A
Ribosomal protein S27a
−4.2

HNRNPA1
Heterogeneous nuclear ribonucleoprotein A1
−4.1

WDR33
WD repeat domain 33
−3.9

EPN1
Epsin 1
−3.7

KLC2
Kinesin light chain 2
−3.6

STIP1
Stress-induced phosphoprotein 1
−3.6

SEPT9
Septin 9
−3.4

TFDP1
Transcription factor Dp-1
−3.1

LAD1
Ladinin 1
−3.1

CABIN 1
Calcineurin-binding protein 1
−3.1

(c) Clofibrate + AS601245

Gene ID
Gene name
Fold change

CYP1A1
Cytochrome P450, family 1, subfamily A, polypeptide 1
+7.5

IL6ST
Interleukin 6 signal transducer (gp130, oncostatin M receptor)
+6.4

AP3D1
Adaptor-related protein complex 3, delta 1 subunit
+5.1

WASF2
WAS protein family, member 2
+4.1

VAPB
VAMP- (vesicle-associated membrane-protein-)associated protein B and C
+3.9

NFAT5*
Nuclear factor of activated T cells 5, tonicity-responsive
+3.8

THRA
Thyroid hormone receptor, alpha (erythroblastic leukemia viral (v-erb-a) oncogene homolog, avian)
+3.6

GANAB*
Glucosidase, alpha; neutral AB
+3.6

BDP1
B double prime 1, subunit of RNA polymerase III transcription initiation factor IIIB
+3.4

SMARCC1
SWI/SNF related, matrix associated, actin-dependent regulator of chromatin, subfamily c, member 1
+3.2

TRUB1
TruB pseudouridine (psi) synthase homolog 1 (E. coli)
−4.4

HNRNPA1
Heterogeneous nuclear ribonucleoprotein A1
−3.9

SLC39A14
Solute carrier family 39 (zinc transporter), member 14
−3.6

NXT2
Nuclear transport factor-2-like export factor 2
−3.4

MALAT1
Metastasis-associated lung adenocarcinoma transcript 1 (nonprotein coding)
−3.2

LARP5
La ribonucleoprotein domain family, member 5
−3.0

FGB
Fibrinogen beta chain
−2.8

ACTC1
Actin, alpha, cardiac muscle 1
−2.8

TFRC
Transferrin receptor (p90, CD71)
−2.8

RPS27A
Ribosomal protein S27a
−2.7

bThe top ten genes upregulated and downregulated the most by 5 μM Clofibrate (Table 1(a)), 0.1 μM AS601245 (Table 1(b)), and combined treatment (Table 1(c)) with respect to DMSO-treated Caco-2 cells at 24 h.

The genes modulated by the treatments with AS601245 are indicated in Table 1(b). In this case, the gene most upregulated was CYP1A1 (5.3 fold change). The other genes upregulated belonged mainly to the “cancer” and cell death functions (NFAT5, BMO2K, DLST, IL6ST, FAM76B, and MGA). The downregulated genes belonged mainly to the “cancer” biofunction (RPS27A, HNRNPA1, STIP1, and TFDP1).

The top ten genes affected the most by the combined treatment with clofibrate and AS601245 are reported in Table 1(c). Among the genes upregulated by the combined treatment, 6 were upregulated by treatments with the single substances also. CYP1A1 was increased by 7.5-fold, whereas AS601245 alone induced its expression by 5.3-fold. IL6ST was induced by clofibrate (2.0 fold), by AS601245 (2.5-fold change), and, more intensively, by the combined treatment (6.5-fold change). AP3D1 was increased (3.6-fold change) in AS601245 treated cells and with an even greater increase (5.0-fold change) in cells treated with both compounds.

NFAT5 and GANAB genes remained almost unchanged in combined treatment. Finally, SMRCC1 gene expression was increased in AS601245-treated cells by a 2.0-fold change (Table B) and by a 3.1-fold change in cells treated with both substances. The resting genes (WASF2, VAPB, THRA, and BDP1) were not affected in cells treated with a single compound, whereas they were highly increased in cells treated with both substances. Among the downregulated genes, four genes which were unaffected by single treatments (TRUB1, NXT2, FGB, and ACTC1) reached the top ten positions in the combined treatment.

Other genes downregulated with the combined treatment were downregulated also, to a lesser extent, in clofibrate- and AS601245-treated cells (MALAT1, LARP5, and TFRC) or in only AS601245-treated cells (SLC39A14). Finally, two genes were downregulated by a single treatment with AS601245 more than by the combined treatment (HNRNPA1 and RPS27A).

We postulated that the inhibition of JNK could increase the affinity of activated PPARα for the PPRE sequences. For this reason, we investigated, among the genes activated by clofibrate, by AS601245, and by the combined treatment, the genes having PPRE sequences by using the genomewide library of high-confidence predicted PPAR target genes as published by Lemay and collaborators [21] (Table 2). It is noteworthy that, among the genes upregulated by the clofibrate 24 hours after the treatment, none had the PPRE putative sequence in the promoter, indicating that the clofibrate, at this concentration, was not able to induce PPARα binding to PPRE containing genes. After treatment with AS601245 and clofibrate, the number of activated genes, containing PPRE sequences, greatly increased (28 genes were upregulated).

Table 2: Upregulated genes containing PPRE sequencesb.

Gene ID
Gene name
Fold change

Clofibrate
None

AS601245
CYP1A1
Cytochrome P450, family 1, subfamily A, polypeptide 1
5.3

ITGB
Integrin, beta 1 (fibronectin receptor, beta polypeptide, antigen CD29 includes MDF2, MSK12)
2.9

Clofibrate +  601245
AMFR
Autocrine motility factor receptor
2.3

ANKRD12
Ankyrin repeat domain 11
2.2

CASP2
Caspase 2, apoptosis-related cysteine peptidase
2.7

CBX5
Chromobox homolog 5 (HP1 alpha homolog, Drosophila)
1.4

CCND1
Cyclin D1
1.9

CYP1A1
Cytochrome P450, family 1, subfamily A, polypeptide 1
7.5

DDX17
DEAD (Asp-Glu-Ala-Asp) box polypeptide 17

DST
Dystonin
1.8

DUSP6
Dual specificity phosphatase 6
2.2

EHBP1
EH domain-binding protein 1
2.4

EWSR1
Ewing sarcoma breakpoint region 1
1.8

FOSL1
FOS-like antigen 1
1.7

LMCD
LIM and cysteine-rich domains 1
1.8

MARCKS
MARCKS-like 1
2.5

MCAM
Melanoma cell adhesion molecule
1.6

MLL3
Myeloid/lymphoid or mixed-lineage leukemia 3
2.7

NR2F2
Nuclear receptor subfamily 2, group F, member 2
2.4

PCYOX1
Prenylcysteine oxidase 1
1.3

RBM8A
RNA-binding motif protein 8A
2.5

SPEN
Spen homolog, transcriptional regulator (Drosophila)
2.2

TBL1XR1
Transducin (beta)-like 1 X-linked receptor 1
2.5

TTC3
Tetratricopeptide repeat domain 32
1.8

USP47
Ubiquitin specific peptidase 47
1.7

ZNF281
Zinc finger protein 281
1.5

ZNF294
Ring finger protein 160
1.9

bThe genes harbouring PPRE sequences among the upregulated genes by treatment with 5 μM clofibrate, 0.1 μM AS601245, and combined treatment versus DMSO-treated Caco-2 cells at 24 h.

3.4.1. Effect of Clofibrate and AS601245 Treatments on PPARα Binding to PPRE and Med1 Expression

Since microarray analysis indicated that clofibrate alone did not induce expression of genes containing PPRE sequences, whereas the treatment with AS601245 and clofibrate does, we examined, through Elisa assay, the binding of nuclear protein extracts from control cells and cells treated with clofibrate alone, AS601245 alone, and combined treatment with clofibrate and AS601245, to PPRE sequences. Figure 6(a), indicates that 5 μM clofibrate and 0.1 μM AS601245 alone did not increase the PPRE binding, whereas the PPRE binding activity was increased in cells treated with 50 μM clofibrate and, more intensively, in cells treated with 5 μM clofibrate and 0.1 μM AS601245. This increase in binding activity is not linked to the variation of PPARα phosphorylation in serine 21, as demonstrated by the western blot analysis with an anti-phospho-PPAR alpha antibody (data not shown). However, microarray analysis revealed that the PPAR alpha activator, MED1, was increased in combined treated cells, only. To verify if this increase corresponded to an increase in MED1 protein, we analyzed, by Western Blot, the expression of MED1. Results confirmed that MED1 protein was doubled in cells treated with both compounds (Figure 6(b)); moreover, its concentration was increased in cells treated with 50 μM clofibrate also. To assess whether the increase of MED1 expression was maintained in the following days in cells exposed to combined treatment, we performed a time-course analysis of MED1 expression. The results confirmed that the increase of MED1 expression was evident until 72 hours after combined treatment (Figure 6(c)). Among the genes, bearing PPRE sequences in their promoter and activated 24 hours after combined treatment, cyclin D1 has been found. We demonstrated that cyclin D1 expression was increased 24 hours after treatment with 50 μM clofibrate and 5 μM clofibrate plus 0.1 μM AS601245. These variations of cyclin D1 expression at 24 hours were similar to those observed for MED1 expression. (Figure 6(d)).

(a)

(b)

(c)

(d)

Figure 6: PPRE binding activity and Western Blot analysis of Med1 and cyclin D1. (a) PPRE binding activity of PPARα. Results represent the absorbance, detected at 450 nm, subtracted from the control value, and are the mean ± SD of three separate experiments from three different preparations for each condition; (b) Western Blot analysis of Med1 protein detected in CaCo-2 cells treated with 5 μM and 50 μM clofibrate (Clofi), 0.1 μM AS1245, and 5 μM clofibrate plus 0.1 μM AS601245 (Clofi + AS601245), collected at 24 hours after the treatment; (c) Western Blot analysis of Med1 protein detected in CaCo-2 cells treated with 5 μM clofibrate, 0.1 μM AS1245, and 5 μM clofibrate plus 0.1 μM AS601245 (Clofi + AS), collected at 24, 48, and 72 hours after the treatment; (d) Western Blot analysis of cyclin D1 detected in CaCo-2 cells treated with 5 μM and 50 μM clofibrate (Clofi), 0.1 μM AS1245, and 5 μM Clofibrate plus 0.1 μM AS601245 (Clofi + AS601245), collected at 24 hours after the treatment. Graphics represent the relative quantification of protein products performed by densitometric scanning. Data were normalized by using the β-actin signal, expressed as arbitrary densitometric units, and are the mean ± SD of three separate experiments from three different preparations for each condition. Variance analysis: *, ** versus control.

3.5. Analysis of JAK/STAT Signalling

The most important gene, modulated by combined treatment, was IL6ST (also called gp130).

This protein is the receptor for IL-6 cytokine. The binding induces the dimerization of gp130 chains resulting in activation of Janus kinases (JAKs). JAKs phosphorylate gp130, leading to the activation and phosphorylation of the STAT1 and STAT3 transcription factors [22, 23]. Although both transcription factors can be involved in gp130 downstream signalling, it has been demonstrated that STAT3 is necessary for the growth of colorectal cancer in mice [24, 25]. For these reasons, we analysed in colon cancer cells the expression of STAT3 protein and the phosphorylation of STAT3 after clofibrate and AS601245 treatments (Figures 7(a), 7(b), 7(c) and 7(d)). STAT 3 expression did not vary after the treatments, and the amount of serine-phosphorylated STAT3 did not vary either. Interestingly, the amount of tyrosine-phosphorylated STAT3 is strongly decreased after treatments with the highest concentration of AS601245 and in particular after combined treatment, which induced a synergistic decrease of phosphorylation.

(a)

(b)

(c)

(d)

Figure 7: Analysis of JAK/STAT signalling. Western Blot analysis of STAT3 (a), P-STAT3 (Ser727) (b), and P-STAT3 (Tyr705) (c) proteins levels analyzed in CaCo-2 cells treated with clofibrate (Clofi) alone, AS601245 alone at the indicated concentrations, and combined treatment with 5 μM clofibrate and 0,1 μM AS601245 (Clofi + AS) and collected at 24 hours after the treatment. Graphics represent the relative quantification of protein products performed by densitometric scanning. Data were normalized by using the β-actin signal and expressed as arbitrary densitometric units. (d) Graphics represent the normalization of the protein level of P-STAT3 (Tyr705) by using STAT3 signal. Results are the mean ± SD of three separate experiments from three different preparations for each condition. Variance analysis: *, ** versus control.

3.6. Effects of AS601245 and Clofibrate in HepG2 Cells

Since fibrates and other drugs are principally metabolized in liver, we tested the toxic effect of 5 μM clofibrate, 0.1 μM AS601245, and the association of the two substances in a liver cell line: the HepG2 cells, which has been demonstrated to be responsive to hepatotoxic compounds [26]. Acute toxicity was evaluated with the MTT test, performed 2 hours after the chemical additions. The amount of viable cells was determined by using the trypan blue dye exclusion test also. Results confirmed that 5 μM clofibrate, 0.1 μM AS601245, and the combined treatment with the two substances did not cause acute toxicity in HepG2 cells (data not shown). In this cell line, the effect of clofibrate, AS601245, and combined treatment in inhibiting cell proliferation was been evaluated (Figure 8(a)). All treatments reduced cell proliferation starting from 48 hours after the beginning of experiments, and the inhibitory effect reached the maximum at 72 hours. No significant differences were found between the three different treatments. Since the reduction of proliferation can be dependent on the modulation of specific gene expression, we tested PCNA, cyclin D1, and p21 proliferation-related protein expression, 24 hours after the treatments. PCNA and cyclin D1 expression did not change after the treatments (Figures 8(b) and 8(d)). On the contrary, p21 expression, which did not change after the treatments in CaCo-2 cells, was upregulated by clofibrate, AS601245, and combined treatment in HepG2 cells (Figure 8(c)).

(a)

(b)

(c)

(d)

Figure 8: Effect of clofibrate and AS601245 in HepG-2 human liver cells. (a) Growth of HepG-2 cells treated with 5 μM clofibrate, 0,1 μM AS601245, and the association of these two compounds (Clofi + AS601245); (b) Western Blot analysis of PCNA detected in CaCo-2 cells treated with 5 μM clofibrate, 0.1 μM AS1245, and 5 μM clofibrate plus 0.1 μM AS601245 (Clofi + AS601245), collected at 24 hours after the treatment; (c) Western Blot analysis of p21, detected in CaCo-2 cells treated with 5 μM clofibrate, 0.1 μM AS1245, and 5 μM clofibrate plus 0.1 μM AS601245 (Clofi+AS601245), collected at 24 hours after the treatment; (d) Western Blot analysis of cyclin D1 detected in CaCo-2 cells treated with 5 μM clofibrate, 0.1 μM AS1245, and 5 μM clofibrate plus 0.1 μM AS601245 (Clofi + AS601245), collected at 24 hours after the treatment. Graphics represent the relative quantification of protein products performed by densitometric scanning. Data were normalized by using the β-actin signal, expressed as arbitrary densitometric units, and are the mean ± SD of three separate experiments from three different preparations for each condition. Variance analysis: *, ** versus control.

4. Discussion

Results obtained demonstrated that the combined treatment with clofibrate and AS601245 inhibits proliferation and downregulated the expression of two proliferation-related proteins, PCNA and cyclin D1, 72 hours after the treatment of CaCO-2 human colon cells. Caspase activities and TUNEL test demonstrated that apoptosis increased significantly only in cells treated with both compounds, whereas apoptosis was not induced by such compounds, added separately. The proapoptotic action of PPAR ligands has been reported in many in vitro studies performed in some cancer cell lines [27, 28]. However, at the concentration used in this study, clofibrate alone did not induce a significant increase of caspase activity in CaCo-2 cells. AS601245 was ineffective too, although it modulated the expression of about 511 genes belonging to the “cell death” group. On the other hand, the JNK inhibition can elicit cellular responses, which range from apoptosis induction to increased survival, depending on the stimuli and the cell type [29]. Since the combined treatment only was able to induce apoptosis, we paid particular attention to genes, involved in the apoptotic pathway, which were unaffected or slightly modulated after the treatment with a single compound and highly modulated by the combined treatment. Among the top ten genes highly modulated by the combined treatment, the THRA gene, which codifies for the thyroid hormone receptor, has been shown to be related to the apoptosis induction of hematopoietic progenitor cells [30]. Several other genes, up- or downregulated by the combined treatment only, were involved in apoptosis induction. For example, CASP2 (caspase 2, +2.8-fold change) and KLF6 (Kruppel like factor 6, +1.5 fold change) [31, 32] were upregulated, whereas ARHGEF7 (Rho guanine nucleotide exchange factor-GEF7) [33] and RAB23 (member Ras oncogene family) were down regulated by a 1.9- and 2.2-fold change, respectively (Table A).

However, the most important change in gene expression, after combined treatment regards the IL6ST gene, which was induced about 6 fold, 24 hours after the treatment, as demonstrated by affymetric analysis and confirmed by RT-PCR. IL6ST (or gp130) is a universal signal transducing receptor for all IL-6 family cytokines [34]. The role played by IL-6 signalling in mediating tumour growth is equivocal [35], in certain tumour cells, it inhibits proliferation, whereas, in “in vivo” models, it stimulates cell growth. Moreover, the significance of an increase of gp130 expression also is controversial: on one hand, it may indicate an increase in the response to the IL-6 family cytokine stimuli, on the other hand, the soluble form signalling receptor subunit gp130, which is generated by differential splicing, is the natural inhibitor of IL-6 trans-signalling responses [35]. We analyzed the downstream signalling of gp130, through the analysis of STAT3 phosphorylation. STAT3 is constitutively active in most tumor cells but not in normal cells. Phosphorylation of STAT3 at tyrosine 705 leads to its dimerization, nuclear translocation, DNA binding, and gene transcription. The phosphorylation of STAT3 at serine 727 may regulate its activity negatively or positively [36]. AS601245 and, at higher level, the combined treatment reduced STAT3 phosphorylation at tyrosine 705, indicating a strong inhibition of STA3-induced gene transcription. STAT3 regulates the expression of genes that mediate survival and proliferation and can be involved in apoptosis induction and in reduction of cell proliferation caused by combined treatment. Interestingly, AS601245 alone reduced in a dose-dependent way STAT3 phosphorylation. This result is in agreement with the work by Kim et al. [37] demonstrating that a JNK inhibitor negatively correlated with the viability of cancer cells and reduced STAT3 activity.

As far as it regards differentiation induction, clofibrate alone did not increase differentiation of CaCo-2 cells. AS601245 is more effective than clofibrate in inducing differentiation, and it shows a synergistic effect when added together with clofibrate. As well as for the apoptosis induction, the action of JNK in differentiation is controversial. Ding and collaborators demonstrated that differentiation is associated with increased JNK activity and c-Jun phosphorylation [38]. In agreement with these findings, inhibition of JNK has been shown to attenuate intestinal cell differentiation [39]. On the contrary, other authors demonstrated that the MAP kinase pathway inhibitor U0126, in combination with butyrate, promotes differentiation in some colon cancer cell lines [40]. Our results demonstrated that AS601245, at 24 hours, did not increase the number of Domes, whereas, after 48 hours, differentiation induction was evident. Moreover, the addition of AS601245 to clofibrate increased the differentiation of CaCo-2 cells both at 24 and 48 hours.

By analysing the expression profile of the genes involved in this pathway, we found some genes affected by AS601245, which were further modulated by the association of these two compounds (Table A). A role, in the differentiation-process, may be played by the MGA gene, activated by 2.361-fold in AS601245-treated cells and by 3.089-fold in cells treated with AS601245 and clofibrate. This gene codifies a member of MAD family proteins belonging to the Max/Mad network which is involved in the control of various aspects of cell behaviour, including proliferation, differentiation, and apoptosis [41].

Clofibrate alone, at the concentration of 5 μM, did not activate genes containing PPRE sequences, probably because of its low concentration. However, when added together with AS601245, 28 genes containing putative PPRE sequences were upregulated. This datum is in agreement with the hypothesis of an increase of PPAR transcriptional activity after JNK inhibition [42] and is further sustained by the results obtained in PPRE binding activity, which demonstrated a strong increase in DNA binding of cells treated with both AS601245 and clofibrate. The gene expression profile revealed that the expression of the PPARα activator MED1 was increased by 1.8-fold in cells treated with both compounds only. MED1 (also referred as PBP/TRAP220/DRIP205) was shown as a critical component of the TRAP/DRIP/ARC/Mediator complex [43] which facilitates interaction of ligand-activated PPAR with RNA polymerase and the general basal transcription machinery to enhance the transcription of a specific set of genes [44–46]. Western Blot analysis confirmed the increase of MED1 protein in cells treated with 5 μM clofibrate plus 0.1 μM AS691245. This increase remained elevated in the cells treated with both compounds until 72 hours after the treatment. Moreover, an increase of MED1 expression occurred even in 50 μM clofibrate-treated cells. These results paralleled with the increase of PPRE binding activity and may suggest that MED1 expression was involved in increasing the number of genes, containing PPRE sequences, activated by combined treatment. According to this hypothesis, we demonstrated that the expression of cyclin D1 protein, codified by a gene containing PPRE sequences that was upregulated after combined treatment, was increased, not only after combined treatment, but also after treatment with 50 μM clofibrate.

The experiments performed in HepG2 cells showed that the single and combined treatment did not induce hepatotoxicity in human liver cells. Moreover, the analysis of the effect of these compounds on HepG2 cells proliferation indicated that there was no synergistic effect between clofibrate and AS601245. In this cell line, the pattern of proliferation-related protein expression was different from that detected in CaCO-2 cells. Indeed, in HepG-2 cells, the p21 expression was increased in clofibrate, AS601245 and clofibrate plus AS601245, treated cells. This result may be related to the fact that HepG2 cells have a wild-type p53 gene [47], whereas, in CaCo-2 cells, p53 is not expressed [48].

5. Conclusions

Taken together, our data demonstrate the effectiveness of combined treatments with PPARα agonists and a JNK inhibitor in inducing apoptosis, differentiation, and PPRE binding activity in colon cancer cells and support the data suggesting a positive interaction between PPARα ligands and anti-inflammatory agents in humans [49, 50]. The positive interaction originates from the modulation of several signalling pathways which were affected by the association of clofibrate and AS601245.

Authors’ Contribution

A. Cerbone and C. Toaldo contributed equally to this paper.

Acknowledgment

This work was supported by grants from Regione Piemonte and Università degli Studi di Torino (GB).

References

T. Lemberger, B. Desvergne, and W. Wahli, “Peroxisome proliferator-activated receptors: a nuclear receptor signaling pathway in lipid physiology,” Annual Review of Cell and Developmental Biology, vol. 12, pp. 335–363, 1996.

F. Beck, S. Plummer, P. V. Senior, S. Byrne, S. Green, and W. J. Brammar, “The ontogeny of peroxisome-proliferator-activated receptor gene expression in the mouse and rat,” Proceedings of the Royal Society B, vol. 247, no. 1319, pp. 83–87, 1992.

S. A. Kliewer, S. S. Sundseth, S. A. Jones et al., “Fatty acids and eicosanoids regulate gene expression through direct interactions with peroxisome proliferator-activated receptors α and γ,” Proceedings of the National Academy of Sciences of the United States of America, vol. 94, no. 9, pp. 4318–4323, 1997.

B. M. Forman, J. Chen, and R. M. Evans, “Hypolipidemic drugs, polyunsaturated fatty acids, and eicosanoids are ligands for peroxisome proliferator-activated receptors α and δ,” Proceedings of the National Academy of Sciences of the United States of America, vol. 94, no. 9, pp. 4312–4317, 1997.

S. Cuzzocrea, R. Di Paola, E. Mazzon et al., “Role of endogenous and exogenous ligands for the peroxisome proliferators activated receptors alpha (PPAR-α) in the development of inflammatory bowel disease in mice,” Laboratory Investigation, vol. 84, no. 12, pp. 1643–1654, 2004.

D. Panigrahy, A. Kaipainen, S. Huang et al., “PPARα agonist fenofibrate suppresses tumor growth through direct and indirect angiogenesis inhibition,” Proceedings of the National Academy of Sciences of the United States of America, vol. 105, no. 3, pp. 985–990, 2008.

Z. Strakova, P. Mavrogianis, X. Meng et al., “In vivo infusion of interleukin-1β and chorionic gonadotropin induces endometrial changes that mimic early pregnancy events in the baboon,” Endocrinology, vol. 146, no. 9, pp. 4097–4104, 2005.

B. J. Ledwith, T. E. Johnson, L. K. Wagner et al., “Growth regulation by peroxisome proliferators: opposing activities in early and late G1,” Cancer Research, vol. 56, no. 14, pp. 3257–3264, 1996.

M. S. Rao and J. K. Reddy, “Hepatocarcinogenesis of peroxisome proliferators,” Annals of the New York Academy of Sciences, vol. 804, pp. 573–587, 1996.

S. Dzhekova-Stojkova, J. Bogdanska, and Z. Stojkova, “Peroxisome proliferators: their biological and toxicological effects,” Clinical Chemistry and Laboratory Medicine, vol. 39, no. 6, pp. 468–474, 2001.

S. Laurora, S. Pizzimenti, F. Briatore et al., “Peroxisome proliferator-activated receptor ligands affect growth-related gene expression in human leukemic cells,” Journal of Pharmacology and Experimental Therapeutics, vol. 305, no. 3, pp. 932–942, 2003.

A. Cerbone, C. Toaldo, S. Laurora et al., “4-Hydroxynonenal and PPARγ ligands affect proliferation, differentiation, and apoptosis in colon cancer cells,” Free Radical Biology and Medicine, vol. 42, no. 11, pp. 1661–1670, 2007.

F. Penna, G. Bonelli, F. M. Baccino, and P. Costelli, “Cytotoxic properties of clofibrate and other peroxisome proliferators: relevance to cancer progression,” Current Medicinal Chemistry, vol. 17, no. 4, pp. 309–320, 2010.

P. M. Barger, A. C. Browning, A. N. Garner, and D. P. Kelly, “p38 mitogen-activated protein kinase activates peroxisome proliferator-activated receptor α: a potential role in the cardiac metabolic stress response,” Journal of Biological Chemistry, vol. 276, no. 48, pp. 44495–44501, 2001.

K. A. Burns and J. P. Vanden Heuvel, “Modulation of PPAR activity via phosphorylation,” Biochimica et Biophysica Acta, vol. 1771, no. 8, pp. 952–960, 2007.

G. Martin, H. Duezm, C. Blanquart et al., “Statin-induced inhibition of the Rho-signaling pathway activates PPARalpha and induces HDL apoA-I,” Journal of Clinical Investigation, vol. 107, no. 11, pp. 1423–1432, 2001.

C. Ferrandi, R. Ballerio, P. Gaillard et al., “Inhibition of c-Jun N-terminal kinase decreases cardiomyocyte apoptosis and infarct size after myocardial ischemia and reperfusion in anaesthetized rats,” The British Journal of Pharmacology, vol. 142, no. 6, pp. 953–960, 2004.

M. J. Ramond, M. Martinot-Peignoux, and S. Erlinger, “Dome formation in the human colon carcinoma cell line Caco-2 in culture. Influence of ouabain and permeable supports,” Biology of the Cell, vol. 54, no. 1, pp. 89–92, 1985.

M. A. McGuckin, R. D. Eri, I. Das, R. Lourie, and T. H. Florin, “ER stress and the unfolded protein response in intestinal inflammation,” The American Journal of Physiology, Gastrointestinal and Liver Physiology, vol. 298, no. 6, pp. 820–832, 2010.

C. Zang, H. Liu, J. Bertz et al., “Induction of endoplasmic reticulum stress response by TZD18, a novel dual ligand for peroxisome proliferator-activated receptor α/γ, in human breast cancer cells,” Molecular Cancer Therapeutics, vol. 8, no. 8, pp. 2296–2307, 2009.

D. G. Lemay and D. H. Hwang, “Genome-wide identification of peroxisome proliferator response elements using integrated computational genomics,” Journal of Lipid Research, vol. 47, no. 7, pp. 1583–1587, 2006.

P. C. Heinrich, I. Behrmann, G. Muller-Newen, F. Schaper, and L. Graeve, “Interleukin-6-type cytokine signalling through the gp130/Jak/STAT pathway,” Biochemical Journal, vol. 334, no. 2, pp. 297–314, 1998.

P. C. Heinrich, I. Behrmann, S. Haan, H. M. Hermanns, G. Müller-Newen, and F. Schaper, “Principles of interleukin (IL)-6-type cytokine signalling and its regulation,” Biochemical Journal, vol. 374, no. 1, pp. 1–20, 2003.

S. Grivennikov, E. Karin, J. Terzic et al., “IL-6 and Stat3 are required for survival of intestinal epithelial cells and development of colitis-associated cancer,” Cancer Cell, vol. 15, no. 2, pp. 103–113, 2009.

J. Bollrath, T. J. Phesse, V. A. von Burstin et al., “gp130-mediated Stat3 activation in enterocytes regulates cell survival and cell-cycle progression during colitis-associated tumorigenesis,” Cancer Cell, vol. 15, no. 2, pp. 91–102, 2009.

A. van Summeren, J. Renes, F. G. Bouwman et al., “Proteomics investigations of drug-induced hepatotoxicity in HepG2 cells,” Toxicological Sciences, vol. 120, no. 1, pp. 109–122, 2011.

F. Penna, P. Reffo, G. Muzio et al., “Mechanisms of clofibrate-induced apoptosis in Yoshida AH-130 hepatoma cells,” Biochemical Pharmacology, vol. 77, no. 2, pp. 169–176, 2009.

G. Muzio, M. Maggiora, M. Oraldi, A. Trombetta, and R. A. Canuto, “PPARα and PP2A are involved in the proapoptotic effect of conjugated linoleic acid on human hepatoma cell line SK-HEP-1,” International Journal of Cancer, vol. 121, no. 11, pp. 2395–2401, 2007.

E. F. Wagner and A. R. Nebreda, “Signal integration by JNK and p38 MAPK pathways in cancer development,” Nature Reviews Cancer, vol. 9, no. 8, pp. 537–549, 2009.

O. Gandrillon, N. Ferrand, J. J. Michaille, L. Roze, M. H. Zile, and J. Samarut, “c-erbAα/T3R and RARs control commitment of hematopoietic self-renewing progenitor cells to apoptosis or differentiation and are antagonized by the v-erbA oncogene,” Oncogene, vol. 9, no. 3, pp. 749–758, 1994.

V. Stoka, B. Turk, S. L. Schendel et al., “Lysosomal protease pathways to apoptosis: cleavage of Bid, not pro-caspases, is the most likely route,” Journal of Biological Chemistry, vol. 276, no. 5, pp. 3149–3157, 2001.

S. Kremer-Tal, G. Narla, Y. Chen et al., “Downregulation of KLF6 is an early event in hepatocarcinogenesis, and stimulates proliferation while reducing differentiation,” Journal of Hepatology, vol. 46, no. 6, pp. 645–654, 2007.

Y. H. Hsu, W. L. Lin, Y. T. Hou et al., “Podocalyxin EBP50 ezrin molecular complex enhances the metastatic potential of renal cell carcinoma through recruiting Rac1 guanine nucleotide exchange factor ARHGEF7,” The American Journal of Pathology, vol. 176, no. 6, pp. 3050–3061, 2010.

H. Knupfer and R. Preiss, “Significance of interleukin-6 (IL-6) in breast cancer (review),” Breast Cancer Research and Treatment, vol. 102, no. 2, pp. 129–135, 2007.

S. Rose-John, K. Mitsuyama, S. Matsumoto, W. M. Thaiss, and J. Scheller, “Interleukin-6 trans-signaling and colonic cancer associated with inflammatory bowel disease,” Current Pharmaceutical Design, vol. 15, no. 18, pp. 2095–2103, 2009.

B. B. Aggarwal, A. B. Kunnumakkara, K. B. Harikumar et al., “Signal transducer and activator of transcription-3, inflammation, and cancer: how intimate is the relationship?” Annals of the New York Academy of Sciences, vol. 1171, pp. 59–76, 2009.

J. H. Kim, S. C. Lee, J. Ro, H. S. Kang, H. S. Kim, and S. Yoon, “Jnk signaling pathway-mediated regulation of Stat3 activation is linked to the development of doxorubicin resistance in cancer cell lines,” Biochemical Pharmacology, vol. 79, no. 3, pp. 373–380, 2010.

Q. Ding, Q. Wang, and B. M. Evers, “Alterations of MAPK activities associated with intestinal cell differentiation,” Biochemical and Biophysical Research Communications, vol. 284, no. 2, pp. 282–288, 2001.

M. A. Lea, C. Ibeh, N. Shah, and M. P. Moyer, “Induction of differentiation of colon cancer cells by combined inhibition of kinases and histone deacetylase,” Anticancer Research, vol. 27, no. 2, pp. 741–748, 2007.

A. Orchel, Z. Dzierzewicz, B. Parfiniewicz, L. Weģlarz, and T. Wilczok, “Butyrate-induced differentiation of colon cancer cells is PKC and JNK dependent,” Digestive Diseases and Sciences, vol. 50, no. 3, pp. 490–498, 2005.

S. Rottmann and B. Lüscher, “The Mad side of the Max network: antagonizing the function of Myc and more,” Current Topics in Microbiology and Immunology, vol. 302, pp. 63–122, 2006.

C. Diradourian, J. Girard, and J. P. Pégorier, “Phosphorylation of PPARs: from molecular characterization to physiological relevance,” Biochimie, vol. 87, no. 1, pp. 33–38, 2005.

C. Rachez, B. D. Lemon, Z. Suldan et al., “Ligand-dependent transcription activation by nuclear receptors requires the DRIP complex,” Nature, vol. 398, no. 6730, pp. 824–828, 1999.

M. R. Dotson, C. X. Yuan, R. G. Roeder et al., “Structural organization of yeast and mammalian mediator complexes,” Proceedings of the National Academy of Sciences of the United States of America, vol. 97, no. 26, pp. 14307–14310, 2000.

C. K. Glass and M. G. Rosenfeld, “The coregulator exchange in transcriptional functions of nuclear receptors,” Genes and Development, vol. 14, no. 2, pp. 121–141, 2000.

Y. Shang, X. Hu, J. DiRenzo, M. A. Lazar, and M. Brown, “Cofactor dynamics and sufficiency in estrogen receptor-regulated transcription,” Cell, vol. 103, no. 6, pp. 843–852, 2000.

A. Sharma, A. S. Meena, and M. K. Bhat, “Hyperthermia-associated carboplatin resistance: differential role of p53, HSF1 and Hsp70 in hepatoma cells,” Cancer Science, vol. 101, no. 5, pp. 1186–1193, 2010.

R. M. Ray, S. Bhattacharya, and L. R. Johnson, “Mdm2 inhibition induces apoptosis in p53 deficient human colon cancer cells by activating p73- and E2F1-mediated expression of PUMA and Siva-1,” Apoptosis, vol. 16, no. 1, pp. 35–44, 2011.

I. Avis, A. Martínez, J. Tauler et al., “Inhibitors of the arachidonic acid pathway and peroxisome proliferator-activated receptor ligands have superadditive effects on lung cancer growth inhibition,” Cancer Research, vol. 65, no. 10, pp. 4181–4190, 2005.

J. M. Lehmann, J. M. Lenhard, B. B. Oliver, G. M. Ringold, and S. A. Kliewer, “Peroxisome proliferator-activated receptors α and γ are activated by indomethacin and other non-steroidal anti-inflammatory drugs,” Journal of Biological Chemistry, vol. 272, no. 6, pp. 3406–3410, 1997.