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Review

Modulation of Telomerase Activity in Cancer Cells by Dietary Compounds: A Review

by
Takahiro Eitsuka
1,*,
Kiyotaka Nakagawa
1,
Shunji Kato
1,
Junya Ito
1,
Yurika Otoki
1,
Soo Takasu
1,
Naoki Shimizu
1,
Takumi Takahashi
1 and
Teruo Miyazawa
2,3
1
Food & Biodynamic Chemistry Laboratory, Graduate School of Agricultural Science, Tohoku University, Sendai 980-0845, Japan
2
Food and Biotechnology Innovation Project, New Industry Creation Hatchery Center (NICHe), Tohoku University, Sendai 980-8579, Japan
3
Food and Health Science Research Unit, Graduate School of Agricultural Science, Tohoku University, Sendai 980-0845, Japan
*
Author to whom correspondence should be addressed.
Int. J. Mol. Sci. 2018, 19(2), 478; https://doi.org/10.3390/ijms19020478
Submission received: 31 December 2017 / Revised: 25 January 2018 / Accepted: 1 February 2018 / Published: 6 February 2018
(This article belongs to the Special Issue Role of Telomeres and Telomerase in Cancer and Aging)
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Abstract

:
Telomerase is expressed in ~90% of human cancer cell lines and tumor specimens, whereas its enzymatic activity is not detectable in most human somatic cells, suggesting that telomerase represents a highly attractive target for selective cancer treatment. Accordingly, various classes of telomerase inhibitors have been screened and developed in recent years. We and other researchers have successfully found that some dietary compounds can modulate telomerase activity in cancer cells. Telomerase inhibitors derived from food are subdivided into two groups: one group directly blocks the enzymatic activity of telomerase (e.g., catechin and sulfoquinovosyldiacylglycerol), and the other downregulates the expression of human telomerase reverse transcriptase (hTERT), the catalytic subunit of human telomerase, via signal transduction pathways (e.g., retinoic acid and tocotrienol). In contrast, a few dietary components, including genistein and glycated lipid, induce cellular telomerase activity in several types of cancer cells, suggesting that they may be involved in tumor progression. This review summarizes the current knowledge about the effects of dietary factors on telomerase regulation in cancer cells and discusses their molecular mechanisms of action.

Graphical Abstract

1. Introduction

Telomeres cap the ends of linear chromosomes and maintain chromosomal stability by preventing end-to-end fusion and degradation [1]. In mammals, telomeres are composed of 5′-TTAGGG-3′ tandem base pair repeats followed by a 3′ G-rich single-stranded overhang. Because conventional DNA polymerases cannot completely replicate the 3′ end of lagging strands owing to the end-replication problem, telomeres shorten by ~50–200 bases with each round of cell division [2]. Eventually, telomeres reach a critical length and cells enter replicative senescence (the so-called Hayflick limit). Human telomerase, a ribonucleoprotein enzyme, elongates the 3′ end of telomeres by adding the tandem arrays of TTAGGG repeats [3]. Telomerase is expressed in ~90% of cancer cells and tumor tissues [4], indicating that the addition of telomeric DNA by telomerase contributes to the infinite proliferation of cancer cells. The tumor cells without telomerase activity utilize a unique mechanism of telomere maintenance termed alternative lengthening of telomeres to keep dividing without limits [5]. In most somatic cells, this enzymatic activity is not detectable [4]. Thus, normal cells have a limited ability to proliferate. On the other hand, germ cells [6] and self-renewing tissues (e.g., the ovary [4], intestinal epithelium [7], and hematopoietic stem cells [8]) possess telomerase activity.
Human telomerase is essentially composed of two subunits: human telomerase RNA component (hTR; also known as hTERC) and human telomerase reverse transcriptase (hTERT). hTR contains an RNA template complementary to the 3′ overhang of telomeres [9]. hTERT acts as the catalytic subunit that adds telomeric DNA to the 3′ overhang [10,11]. Besides, some telomerase-associated proteins such as dyskerin, NOP10, NHP2, and GAR1 have been reported to contribute to proper telomerase function in vivo [12]. Although hTR and telomerase-associated proteins are ubiquitously expressed in all human cells, hTERT is expressed only in telomerase-positive cells and tissues. The expression level of hTERT mRNA highly correlates with cellular telomerase activity [13], suggesting that hTERT is a critical determinant of telomerase activity. Thus, it is important to understand the mechanism underlying hTERT regulation in order to take advantage of telomerase for cancer diagnosis and treatment.
The 5′ promoter region of hTERT has been cloned [14,15,16], and several transcription factors, including c-Myc, Sp1, activating enhancer-binding protein-2 (AP-2), hypoxia-inducible factor 1 (HIF-1), ETS, estrogen receptor (ER), E2F, activator protein 1 (AP-1), vitamin D receptor (VDR) in complex with retinoid X receptor (RXR), p53, Wilms’ tumor 1 (WT1), myeloid zinc finger protein 2 (MZF-2), and CCCTC-binding factor (CTCF), have been found to modulate the transcriptional activity of the hTERT promoter (Figure 1) [17]. Among these transcription factors, c-Myc plays a pivotal role in hTERT mRNA expression. c-Myc can recognize and bind to the E-box consensus sequence (5′-CACGTG-3′) in the target gene promoter. The hTERT promoter contains two E-box sites located at positions −165 and +44 relative to the transcription start site (+1 position). The expression of c-myc mRNA is highly related to the expression of hTERT mRNA [18]. Treatment with antisense c-myc oligonucleotides downregulates c-myc and hTERT expression in human leukemic cells, thus leading to the suppression of cellular telomerase activity [19]. The above findings clearly indicate that c-Myc acts as a crucial signaling factor in the regulation of hTERT transcription.
Epigenetic modifications (i.e., DNA methylation, histone modifications, and noncoding RNA) alter the recruitment of transcription factors and chromatin structure, thereby affecting gene expression [20]. DNA methylation is catalyzed by DNA methyltransferases (DNMTs) through the addition of a methyl group at the C-5 position of cytosine. These enzymes include DNMT1, DNMT3A, and DNMT3B; DNMT1 participates in the methylation of hemimethylated DNA to maintain the methylation status of daughter strands after the replication process, whereas DNMT3A and DNMT3B are responsible for de novo DNA methylation [21]. The cytosine methylation generally occurs in cytosine–guanine (CG) clusters (referred to as CpG islands). The methyl group in CpG islands is thought to directly block DNA recognition and binding by several transcription factors, meaning that CpG methylation is involved in gene silencing. The hTERT promoter contains many CpG sites, but most CpG islands in this promoter are surprisingly hypermethylated (especially from position −650 to −150 relative to the transcription start site) in telomerase-positive cancer cell lines [22]. Such hypermethylation of the hTERT promoter abrogates binding of transcriptional repressors, such as CTCF and E2F. In fact, treatment of cancer cells with 5-aza-2′-deoxycytidine, a DNA methylation inhibitor, allows CTCF to bind to the hTERT promoter and to repress hTERT expression (Figure 2) [23]. Thus, CpG hypermethylation of the hTERT promoter in tumor cells is intended in part to block binding of the transcriptional repressor, thereby increasing the transcription of the hTERT gene.
Histone modifications such as acetylation, methylation, phosphorylation, and ubiquitination participate in changes of chromatin structure, leading to altered gene transcription [24]. For instance, histone acetylation is mediated by histone acetyltransferases (HATs), which add an acetyl group to a lysine residue within a histone tail. The presence of acetylated lysine in the histone tail attenuates the interaction between histones and DNA, eliciting a relaxed chromatin structure thereby permitting access of transcription factors to the DNA and, therefore, promoting a transcriptionally active gene status. In contrast, histone deacetylases (HDACs) can remove the acetyl group and cause chromatin condensation and gene silencing. Some researchers have shown that trichostatin A (TSA), an HDAC inhibitor, induces hTERT mRNA expression and telomerase activity in a Mad- and Sp1-dependent manner in normal cells [25,26] but has no effect on cancer cells, such as human fibrosarcoma (HT-1080) and cervical cancer (HeLa and C33A) cell lines. In contrast, hTERT transcription and telomerase activity are suppressed by treatment with TSA in prostate cancer [27], leukemia [28], and brain cancer cells [29]. Choi et al. [30] revealed that TSA downregulates DNMT1 and causes demethylation of a CTCF-binding site in the hTERT promoter, resulting in repression of hTERT expression in HCT116 colorectal cancer cells. These results suggest that the effects of TSA on hTERT transcription depend on cell type. In addition to histone acetylation, hTERT expression is governed by histone methylation. SET and MYND domain-containing protein 3 (SMYD3) is a lysine 4 on histone 3 (H3K4)-specific dimethyl transferase and trimethyl transferase. SMYD3 binds to a specific DNA sequence (5′-CCCTCC-3′) in the promoter region of hTERT, facilitates dimethylation or trimethylation of H3K4, and activates hTERT transcription [31].
Noncoding RNAs perform key functions in epigenetic regulation. MicroRNAs (miRNAs), one of the largest families of noncoding RNAs, are ~23 nucleotides long [32]. They can post-transcriptionally downregulate or degrade their target mRNAs by binding to the recognition sites in the 3′ untranslated region (3′UTR) of their specific mRNA, thus acting as repressors of gene expression. Multiple types of miRNAs have been shown to target hTERT mRNA, thereby reducing proliferation of cells derived from neuroblastoma [33], anaplastic thyroid carcinoma [34], gastric cancer [35,36], cervical cancer [37], head and neck squamous cell carcinoma [38], ovarian cancer [39], and breast cancer (Table 1) [40]. These observations indicate that the epigenetic regulation of DNA methylation, histone modifications, and noncoding RNAs markedly contribute to hTERT gene expression.
Telomerase activity in cancer cells is also regulated by promoter mutations and rearrangements of hTERT. Point mutations in the hTERT promoter can generate new consensus motifs for transcription factors [41]. Structural rearrangements of hTERT bring the enhancers close to the hTERT promoter [42]. Therefore, mutations and rearrangements of hTERT participate in the upregulation of hTERT expression.
To date, we and other groups have found that several dietary compounds can regulate telomerase activity in cancer cells. Telomerase inhibitors derived from food are subdivided into two groups: one group interacts with telomerase and directly blocks its enzymatic activity, and the other downregulates the expression of hTERT via signal transduction pathways. On the other hand, a few dietary components upregulate cellular telomerase activity in several types of cancer cells, implying that they may be involved in tumor progression. This review summarizes the current knowledge about the effects of food factors on telomerase activity in cancer cells and discusses their molecular mechanisms of action.

2. Inhibition of Telomerase Activity by Dietary Components

2.1. Retinoic Acid

Vitamin A (also known as retinol) is a fat-soluble vitamin necessary for embryonic development, organ formation, immune function, and vision [43]. Retinol is converted to retinal by alcohol dehydrogenase in the body, and retinal can be altered to retinoic acid by retinaldehyde dehydrogenase. Retinoic acid, particularly all-trans retinoic acid (RA; Figure 3A), participates in the regulation of cell growth and differentiation [44]. One in vivo study showed that telomerase activity is reduced during stem cell maturation in embryonic development [45], suggesting that the suppression of telomerase may be linked to cell differentiation. Sharma et al. [46] investigated the effect of differentiation inducers, including dimethyl sulfoxide and RA (1 µM), on telomerase activity in HL-60 human leukemia cells, and demonstrated that both inducers decrease this enzymatic activity. These agents do not directly inhibit this activity at all. Furthermore, treatment of SW480 colon carcinoma cells with these inducers does not cause cell differentiation and has no effect on telomerase activity. Love et al. [47] showed that 2 µM RA induces differentiation of HL-60 cells and attenuation of hTERT expression via epigenetic regulation. Treatment with RA leads to hypoacetylation and hypermethylation of the hTERT promoter by altering DNMT expression. These results [46,47] indicate that telomerase inhibition takes place in response to the differentiation status. In contrast, Pendino et al. [48,49] reported that RA can downregulate telomerase independently of cell differentiation. In maturation-resistant NB4 acute promyelocytic leukemia cells, the reduction in telomerase activity by RA stems from the downregulation of hTERT mRNA expression through activation of retinoic acid receptor (RAR) and RXR [49]. However, 1 nM RA elicits telomerase activity and decreases p16INK4A expression, therefore extending the lifespan of normal human oral keratinocytes, while 100 nM RA does not influence the cellular senescence [50]. It is noteworthy that the very low concentration of RA (1 nM) has the characteristic effect on the proliferative capacity of normal keratinocytes.

2.2. Vitamin D3

This vitamin is made in the skin from 7-dehydrocholesterol during exposure to ultraviolet sunlight. Vitamin D3 is metabolized by cytochrome P450 (CYP) enzymes such as 27A1 and CYP2R1 in the liver and is then converted to 1α,25-dihydroxyvitamin D3 (1α,25(OH)2VD3; Figure 3B), the physiologically active form of vitamin D3, by CYP27B1 in the kidneys [51]. 1α,25(OH)2VD3 is essential for bone remodeling, immunity, insulin secretion, and blood pressure regulation [52]. In addition to these beneficial effects, 1α,25(OH)2VD3 acts as a differentiation inducer as well as RA does. Treatment with 1α,25(OH)2VD3, therefore, drives the differentiation of HL-60 cells and suppresses telomerase activity [46]. Most physiological functions of 1α,25(OH)2VD3 are mediated by a nuclear transcription factor, VDR [53]. 1α,25(OH)2VD3 binds to VDR and promotes the interaction with its heterodimer partner, RXR, that is activated by 9-cis-retinoic acid. The VDR–RXR complex binds to a specific DNA sequence called a vitamin D response element (VDRE; there are several versions), initiating the transcription of target genes. Because the promoter region of hTERT contains a VDRE, Ikeda et al. [54] examined the influence of 1α,25(OH)2VD3 and 9-cis-retinoic acid on telomerase activity. Although treating PC3 human prostate cancer cells with a single treatment of 1α,25(OH)2VD3 or 9-cis-retinoic acid (10 nM each) did not inhibit telomerase, the combination of 1α,25(OH)2VD3 and 9-cis-retinoic acid reduced the enzymatic activity via direct interaction of the heterodimer of VDR and RXR with the VDRE. Significant suppression of tumor growth in nude mice inoculated with PC3 cells was observed after intraperitoneal injections of both 1α,25(OH)2VD3 (5 ng/mouse) and 9-cis-retinoic acid (5 ng/mouse) at 3-day intervals. Kasiappan et al. [55] provided direct evidence for the involvement of a miRNA, miR-498, in the downregulation of hTERT through VDR. 1α,25(OH)2VD3 (100 nM) causes the formation of the VDR–RXR heterodimer and its binding to a VDRE located in the 5′ regulatory region of the miR-498 gene in OVCAR3 human ovarian cancer cell line. miR-498 binds to the complementary sequence in the 3′UTR of hTERT mRNA, thereby leading to its breakdown. These findings imply that VDR plays a unique role in telomerase inhibition by 1α,25(OH)2VD3.

2.3. Polyphenols

These are a major group of phytochemicals present in fruits, vegetables, and beverages, with over 8000 phenolic structures currently identified [56].
The predominant polyphenols in green tea include (−)-epicatechin, (−)-epicatechin-3-gallate, (−)-epigallocatechin, and (−)-epigallocatechin-3-gallate (EGCG; Figure 3C), the last of which accounts for approximately 50% of the total phenolic content of green tea extract [57]. Naasani et al. [58] revealed that a physiological concentration of catechin (~1 μM), particularly EGCG, directly inhibits telomerase activity. An analysis of inhibition kinetics by means of a Dixon plot showed that EGCG is a competitive inhibitor relative to a telomerase substrate primer, indicating that EGCG competitively interacts with the substrate-binding site of telomerase. Prolonged treatment with 15 μM EGCG drives telomere shortening in U937 monoblastoid leukemia cells and HT29 adenocarcinoma cells and eventually induces senescence-associated β-galactosidase activity, a biomarker of cellular aging. Oral administration of EGCG (1.2 mg/mouse per day) significantly reduces tumor size in nude mice carrying an HCT-L1 (human colon carcinoma cells) xenograft [59]. In addition to direct inhibition of telomerase enzymatic activity, (−)-epigallocatechin and EGCG (20–40 μM) repress telomerase via downregulation of hTERT mRNA [60]. Berletch et al. [61] revealed that 100 μM EGCG causes demethylation of hTERT promoter and binding of E2F-1, an hTERT repressor, to the target promoter in MCF-7 breast cancer cells. Furthermore, Min et al. [62] showed that the decrease in hTERT mRNA expression by EGCG in HCT116 human colon cancer cells is driven by increased binding of CTCF to the hTERT core promoter region via downregulation of DNMT1 expression. Two mechanisms for DNMT inhibition by EGCG have been proposed: EGCG inhibits DNMT activity via direct binding to the catalytic site [63]; alternatively, the suppression of DNMT mRNA expression is implicated in the p21WAF1–p300–DNMT axis [62,64]. Therefore, the transcriptional repression of hTERT is primarily due to epigenetic regulation by EGCG.
Curcumin (Figure 3D) is a major component of turmeric and is commonly consumed as a spice in Asian countries. Curcumin affects several signaling molecules, thus exerting physiological effects such as antioxidant, anti-inflammatory, anticancer, and neuroprotective [65]. Ramachandran et al. [66] revealed that treatment with 50–100 μM curcumin decreases telomerase activity and hTERT mRNA expression in MCF-7 cells but does not influence c-myc mRNA. This result means that curcumin downregulates telomerase through a c-Myc–independent pathway. Heat shock protein 90 (Hsp90), a molecular chaperone, performs essential functions in the folding and maturation of its substrate proteins, and p23 is a co-chaperone that stabilizes Hsp90-substrate protein complexes. Hsp90 and p23 can bind to hTERT and promote its proper assembly with hTR [67]. Lee and Chung [68] discovered that curcumin disrupts the binding of p23 to hTERT, attenuating nuclear translocation of the hTERT protein and thereby inhibiting telomerase activity. Khaw et al. [69] demonstrated that curcumin prevents telomerase activity and hTERT expression and found that prolonged treatment (15 days) causes telomere shortening in brain tumor cells.
Genistein (Figure 3E), an isoflavone found abundantly in soy, has protective effects against cancer, obesity, osteoporosis, and inflammation [70]. Some reports have proven that phosphorylation of the hTERT subunit by the Akt kinase [71] and protein kinase C (PKC) [72] augments telomerase activity, indicating that telomerase can be controlled by post-translational modifications. Jagadeesh et al. [73] reported that 10–100 μM genistein reduces telomerase activity in DU-145 and PC-3 prostate cancer cells not only by decreasing hTERT expression through downregulation of c-myc but also by dephosphorylation of hTERT through Akt inhibition. Li et al. [74] revealed that treatment of MCF-7 cells with 50–100 μM genistein inhibits DNMT expression and causes hypomethylation of the E2F-1 recognition sequence in the hTERT promoter, thus leading to increased binding of E2F-1 to its promoter and therefore repressing hTERT and telomerase activity.
Resveratrol (Figure 3F), which is contained in grapes, red wine, peanuts, and some berries, possesses preventive effects against cancer, cardiovascular diseases, and neurodegenerative disorders [75]. Lanzilli et al. [76] found that resveratrol reduces telomerase activity and the nuclear protein levels of hTERT in MCF-7 cells. Pterostilbene, a dimethyl ether analog of resveratrol, has telomerase-inhibitory properties [77]. Kala et al. [78] showed that a combination of resveratrol (15 μM) and pterostilbene (5 μM) decreases hTERT expression through sirtuin 1 (SIRT1) and DNMT inhibition in HCC1806 breast cancer cells. The knockdown of SIRT1, a nicotinamide adenine dinucleotide-dependent deacetylase, represses hTERT mRNA expression, suggesting the involvement of SIRT1 in hTERT regulation.

2.4. Ceramide

This compound (Figure 3G) consists of sphingosine, a long-chain amino alcohol, linked to a fatty acid via an amide bond, and plays a major part in the metabolism of sphingolipids. Ceramide is used as a substrate to generate more complex sphingolipids (such as sphingomyelin and glycosphingolipids, which are essential components of the cell membrane) while being a degradation product of complex sphingolipid molecules [79]. Ceramide can regulate various cellular phenomena, including cell proliferation, death, migration, and senescence [80]. Inhibitory effects of ceramide on telomerase in A549 human lung adenocarcinoma cells have been extensively investigated by Ogretmen et al. [81,82,83,84,85]. For example, treatment with 20 μM C6-ceramide suppresses cellular telomerase activity and causes shortening of telomere length, whereas 20 μM dihydro-C6-ceramide shows no inhibition [81,82]. Overexpression of sphingomyelinase, the enzyme responsible for the conversion of sphingomyelin to ceramide, significantly decreases telomerase activity. Moreover, overexpression of glucosylceramide synthase, which converts ceramide to glucosylceramide, attenuates the inhibitory effects of C6-ceramide on telomerase. These findings suggest that telomerase inhibition is specific to ceramide, but not to other sphingolipids. Ceramide represses telomerase activity via decreased hTERT mRNA expression by rapid degradation of the c-Myc protein [83]. Wooten and Ogretmen [84] revealed that downregulation of hTERT mRNA by ceramide is mediated by Sp1 and Sp3 (transcription factors of the Sp1 family)-dependent regulation of hTERT transcription. Ceramide treatment elicits deacetylation of Sp3 and histone H3 at an hTERT promoter site, thereby preventing the transcription of hTERT [85].

2.5. Sulfoquinovosyldiacylglycerol (SQDG)

The photosynthetic membranes of higher plants contain abundant glyceroglycolipids, including SQDG (Figure 3H), monogalactosyldiacylglycerol (MGDG), and digalactosyldiacylglycerol (DGDG) [86]. SQDG possesses a unique sulfoquinovose headgroup, a derivative of glucose with a sulfonate group, and exerts anticancer effects [87]. We demonstrated that SQDG directly inhibits telomerase activity with 50% inhibition at 22 μM, whereas MGDG and DGDG have no effect even at concentrations of 100 μM [88]. Eicosapentaenoic acid (EPA), one of SQDG components, inhibits this enzymatic activity too, suggesting that the structure of the sulfate group and fatty acid of SQDG is essential for the inhibitory action on telomerase activity.

2.6. Fatty Acids

Fatty acids are a fundamental component of dietary lipids. Among polyunsaturated fatty acids, the n-3 and n-6 fatty acids are distinguished by the positions of double bonds with respect to the methyl end of the acyl chain. For example, in n-3 fatty acids, the first double bond is located at the third carbon atom from the methyl end. Both n-3 and n-6 fatty acids are important constituents of cell membrane lipids and therefore influence cell membrane properties such as fluidity, flexibility, and membrane-bound enzymatic activities [89]. In addition to the structural functions, n-3 and n-6 fatty acids can act as precursors of bioactive lipid mediators [90]. Long-chain n-3 fatty acids such as EPA (Figure 3I) and docosahexaenoic acid (DHA) have protective effects against inflammation, cancer, cardiovascular disease, and dementia [91]. We found that fatty acids (C18–C22) directly inhibit telomerase activity [92]. IC50 (the concentration causing 50% inhibition of the telomerase activity) values are listed in Table 2, indicating that the inhibitory potency of fatty acids increases with the number of double bonds, and that cis-fatty acids possess higher inhibitory activities than trans-isomers do. Accordingly, polyunsaturated fatty acids such as EPA and DHA can strongly prevent telomerase enzymatic activity. A Lineweaver–Burk plot revealed that EPA is a competitive inhibitor relative to the telomerase substrate primer, implying that fatty acids may interact with the primer-binding site of telomerase. Besides, we demonstrated that physiological concentrations of EPA and DHA (≤50 μM) downregulate hTERT and c-myc mRNA via PKC inhibition, thereby repressing telomerase activity. Our results indicate that fatty acids, especially EPA and DHA, not only directly inhibit the enzymatic activity of telomerase but also downregulate telomerase at the transcriptional level.

2.7. Tocotrienol

Vitamin E forms can be categorized into two groups: tocopherol (Toc) and tocotrienol (T3), based on their structural difference in the isoprenoid-derived hydrophobic tail (Figure 3J). Both Toc and T3 have four forms: α-, β-, γ-, and δ-isomers. Toc is contained in a variety of foods (e.g., nuts, whole grains, and common vegetable oils). In contrast, T3 is present at low levels in most plants but annatto, palm, and rice bran oils are richer sources of T3 [93]. T3 has a broad range of beneficial activities, including antioxidative, antitumor, antidiabetic, anti-inflammatory, cardioprotective, and neuroprotective properties [94]. These bioactivities of T3 are superior to those of Toc because incorporation of T3 into the lipid bilayer of the cell membrane is more effective than that of Toc [95]. We revealed that 5–20 μM T3, particularly β- and δ-isomers, dose-dependently suppresses telomerase activity in DLD-1 human colorectal adenocarcinoma cells, and the inhibitory potency of δ-T3 is stronger than that of the β-isomer [96]. On the other hand, Toc (α-, β-, γ-, and δ-isomers) exerts only negligible inhibition of telomerase. The reduction in cellular telomerase activity by T3 is due to downregulation of hTERT and c-myc mRNA through PKC inhibition. Furthermore, ferulic acid, a potent phenolic antioxidant abundant in rice bran oil, potentiates the anticancer effects of T3 [97]. Co-treatment with T3 and ferulic acid therefore synergistically decrease telomerase and hTERT expression [98,99].

2.8. Sulforaphane

This compound (Figure 3K) is a sulfur-containing isothiocyanate derivative present in cruciferous vegetables such as broccoli, broccoli sprouts, and cauliflower. Sulforaphane exerts powerful anticancer activity via apoptosis induction, suppression of cell cycle progression, angiogenesis inhibition, and anti-inflammatory action [100]. Moon et al. [101] found that 10–20 μM sulforaphane suppresses telomerase activity in Hep3B human hepatoma cells. The reduction in telomerase activity is mediated by downregulation of hTERT mRNA via c-Myc suppression, as well as dephosphorylation of hTERT through Akt inhibition. Meeran et al. [102] reported that treatment of breast cancer cells (MCF-7 and MDA-MB-231) with sulforaphane causes demethylation of the hTERT promoter via DNMT inhibition, thereby facilitating the binding of CTCF to the promoter site and attenuating hTERT expression and telomerase activity.

3. Telomerase Induction in Cancer Cells by Dietary Factors

3.1. Genistein

As described above, genistein in the pharmacological concentration range (10–100 μM) reduces telomerase activity. Because physiological concentrations of genistein are estimated to be <2 μM, Chau et al. [103] investigated the effect of genistein on telomerase at concentrations of ≤1 μM. As a result, physiologically achievable concentrations of genistein augmented telomerase activity and hTERT mRNA expression in DU-145 cells. Of note, TRAMP mice—a popular transgenic mouse model of prostate cancer—fed a diet containing genistein (250 mg/kg diet) from 12 to 20 weeks of age demonstrated a threefold increase in prostate weight as compared with the control group. Moreover, significant elevation of telomerase activity was observed in the prostate tissue of TRAMP mice consuming the genistein-supplemented diet. This study raised the possibility that physiological concentrations of genistein may have adverse effects on patients with prostate cancer.

3.2. A Glycated Lipid

Maillard reactions may contribute to food deterioration and the pathogenesis of diabetes. Our research group found that phosphatidylethanolamine (PE) reacts with glucose to form a PE-linked Amadori product (Amadori-PE; Figure 3L) [104]. Amadori-PE is present in some foods (e.g., infant formula and chocolate) [105] and, moreover, crucially participates in the development of diabetic complications [106]. Several epidemiological studies have shown that type 2 diabetes significantly raises cancer risk [107]. Nevertheless, little is known about the molecular mechanism underlying the involvement of diabetes in tumor development. We, therefore, examined the link between Amadori-PE and tumor progression, with an emphasis on telomerase activity. Physiological concentrations of Amadori-PE (1–5 μM: plasma concentrations of this lipid in diabetic patients) increased telomerase activity in PANC-1 human pancreatic carcinoma cells by upregulating hTERT mRNA expression through the induction of c-myc [108]. A similar phenomenon was observed in other cancer cells (MIA PaCa-2 human pancreatic carcinoma, HepG2 human hepatoma, and DLD-1). This finding provides experimental evidence for a unique role of lipid glycation in the relation between diabetes and cancer.

4. Conclusions

Establishment of the method for the sensitive detection of telomerase activity, namely, the telomeric repeat amplification protocol (TRAP) assay [4], in 1994 enabled screening for telomerase inhibitors, as well as the diagnosis of cancer by means of telomerase. Since then, numerous types of telomerase inhibitors have been identified and developed. Examples of such inhibitors include reverse transcriptase inhibitors (e.g., 3′-azido-3′-deoxythymidine triphosphate [109]), hTR antisense oligonucleotides (e.g., imetelstat [110]), G-quadruplex stabilizers (for instance, TMPyP4 [111]), synthetic compounds from random screening (e.g., BIBR1532 [112]), and HSP90 inhibitors (such as geldanamycin [113]). Among these inhibitors, imetelstat is a potent agent specific to telomerase. Imetelstat can bind with high affinity to hTR, thus blocking the interaction between telomerase and telomere DNA. Recent phase II trials uncovered a clinical benefit of imetelstat for patients with myeloproliferative disorders [114,115].
As mentioned above, several dietary components (i.e., RA, 1α,25(OH)2VD3, polyphenols, ceramide, SQDG, fatty acids, tocotrienol, and sulforaphane) inhibit telomerase by directly blocking the enzymatic activity and/or by decreasing hTERT expression. Most telomerase inhibitors derived from food factors have been evaluated only in cell culture experiments. To date, a few studies have focused on the in vivo efficacy of these inhibitors [54,59]. Orally administered EGCG suppresses tumor size and shortens telomere length in tumor tissue [59], indicating that EGCG exhibits the telomerase-inhibitory effect in vivo. The in vivo anticancer efficacy of 1α,25(OH)2VD3 combined with 9-cis-retinoic acid has been examined only by tumor volume measurement [54]. It is unclear whether the tumor suppressive effect of 1α,25(OH)2VD3 and 9-cis-retinoic acid is mediated through telomerase inhibition since VDR-RXR can affect diverse growth-regulatory signaling pathways [116]. The evaluation of telomerase activity, telomere length, hTERT expression, or their combination, as well as tumor size measurement, would be necessary to determine the in vivo effectiveness of telomerase inhibitors. In contrast to the chemically synthesized inhibitors such as imetelstat, a human trial targeting telomerase using dietary compounds has never been conducted. A clinical application of dietary factors to cancer treatment is highly attractive because they are nontoxic to healthy cells at physiological concentrations. Prior to initiating human clinical trials, further animal experiments should be performed to investigate their potential applications in cancer treatment and prevention. On the other hand, genistein and Amadori-PE induce telomerase activity in cancer cells. Telomerase activity levels in tumor cells positively correlate with an aggressive tumor phenotype [117]. Overexpression of hTERT induces cell proliferation via upregulation of growth-controlling genes and promotes cell survival by apoptosis suppression [118,119]. Therefore, telomerase activation by genistein and Amadori-PE may be relevant to cancer progression.
The TRAP assay is highly sensitive but tends to generate several extra bands, raising the possibility that the potency of telomerase inhibitors may be inappropriately evaluated [120]. However, this assay has been applied by many research groups [46,55,58,66,73,76,81,101,103]. Thus, some modified TRAP assays have been reported with improved specificity and reliability [121]. Tatematsu et al. [122] developed a stretch PCR method that achieves quantitative evaluation by the addition of extra tag sequences to the 5′-ends of the forward and reverse PCR primers, and we and some researchers have utilized this method [54,88,92,96,98,108]. On the other hand, treatment with EGCG [58], curcumin [69], and ceramide [82] leads to telomere shortening in cancer cells. Multiple methods have been developed for telomere length analysis, including terminal restriction fragment (TRF) analysis, real-time PCR, single telomere length analysis, and quantitative fluorescence in situ hybridization [123]. Among these methods, TRF analysis is widely used [58,69,82] and is often regarded as the gold standard.
A more detailed understanding of the mechanisms underlying telomerase regulation will be necessary for the identification of novel telomerase inhibitors. Further studies, with special emphasis on in vivo experiments, are needed to apply dietary compounds to cancer treatment and prevention.

Acknowledgments

Some of the work presented in this review was partly supported by a grant from The Tojuro Iijima Foundation for Food Science and Technology, and JSPS KAKENHI Grant Numbers 19780105, 25450185, 17K07803.

Author Contributions

Takahiro Eitsuka wrote the manuscript; Kiyotaka Nakagawa, Shunji Kato, Junya Ito, Yurika Otoki, Soo Takasu, Naoki Shimizu, Takumi Takahashi, and Teruo Miyazawa revised the manuscript.

Conflicts of Interest

The authors declare no conflict of interest.

Abbreviations

hTRhuman telomerase RNA component
hTERThuman telomerase reverse transcriptase
AP-2activating enhancer-binding protein-2
HIF-1hypoxia-inducible factor 1
ERestrogen receptor
AP-1activator protein 1
VDRvitamin D receptor
RXRretinoid X receptor
WT1Wilms’ tumor 1
MZF-2myeloid zinc finger protein 2
CTCFCCCTC-binding factor
DNMTDNA methyltransferase
HAThistone acetyltransferase
HDAChistone deacetylase
TSAtrichostatin A
SMYD3SET and MYND domain-containing protein 3
H3K4lysine 4 on histone 3
miRNAmicroRNA
3′UTR3′ untranslated region
RAall-trans retinoic acid
RARretinoic acid receptor
CYPcytochrome P450
1α,25(OH)2VD31α,25-dihydroxyvitamin D3
VDREvitamin D response element
EGCG(−)-epigallocatechin-3-gallate
Hsp90heat shock protein 90
PKCprotein kinase C
SIRT1sirtuin 1
SQDGSulfoquinovosyldiacylglycerol
MGDGmonogalactosyldiacylglycerol
DGDGdigalactosyldiacylglycerol
EPAeicosapentaenoic acid
DHAdocosahexaenoic acid
Toctocopherol
T3tocotrienol
PEphosphatidylethanolamine
Amadori-PEphosphatidylethanolamine-linked Amadori product
TRAPtelomeric repeat amplification protocol

References

  1. McEachern, M.J.; Krauskopf, A.; Blackburn, E.H. Telomeres and their control. Annu. Rev. Genet. 2000, 34, 331–358. [Google Scholar] [CrossRef] [PubMed]
  2. Levy, M.Z.; Allsopp, R.C.; Futcher, A.B.; Greider, C.W.; Harley, C.B. Telomere end-replication problem and cell aging. J. Mol. Biol. 1992, 225, 951–960. [Google Scholar] [CrossRef]
  3. Morin, G.B. The human telomere terminal transferase enzyme is a ribonucleoprotein that synthesizes TTAGGG repeats. Cell 1989, 59, 521–529. [Google Scholar] [CrossRef]
  4. Kim, N.W.; Piatyszek, M.A.; Prowse, K.R.; Harley, C.B.; West, M.D.; Ho, P.L.; Coviello, G.M.; Wright, W.E.; Weinrich, S.L.; Shay, J.W. Specific association of human telomerase activity with immortal cells and cancers. Science 1994, 266, 2011–2015. [Google Scholar] [CrossRef] [PubMed]
  5. Bryan, T.M.; Englezou, A.; Gupta, J.; Bacchetti, S.; Reddel, R.R. Telomere elongation in immortal human cells without detectable telomerase activity. EMBO J. 1995, 14, 4240–4248. [Google Scholar] [PubMed]
  6. Collins, K.; Mitchell, J.R. Telomerase in the human organism. Oncogene 2002, 21, 564–579. [Google Scholar] [CrossRef] [PubMed]
  7. Hiyama, E.; Tatsumoto, N.; Kodama, T.; Hiyama, K.; Shay, J.; Yokoyama, T. Telomerase activity in human intestine. Int. J. Oncol. 1996, 9, 453–458. [Google Scholar] [CrossRef] [PubMed]
  8. Yui, J.; Chiu, C.P.; Lansdorp, P.M. Telomerase activity in candidate stem cells from fetal liver and adult bone marrow. Blood 1998, 91, 3255–3262. [Google Scholar] [PubMed]
  9. Feng, J.; Funk, W.D.; Wang, S.S.; Weinrich, S.L.; Avilion, A.A.; Chiu, C.P.; Adams, R.R.; Chang, E.; Allsopp, R.C.; Yu, J.; et al. The RNA component of human telomerase. Science 1995, 269, 1236–1241. [Google Scholar] [CrossRef] [PubMed]
  10. Nakamura, T.M.; Morin, G.B.; Chapman, K.B.; Weinrich, S.L.; Andrews, W.H.; Lingner, J.; Harley, C.B.; Cech, T.R. Telomerase catalytic subunit homologs from fission yeast and human. Science 1997, 277, 955–959. [Google Scholar] [CrossRef] [PubMed]
  11. Meyerson, M.; Counter, C.M.; Eaton, E.N.; Ellisen, L.W.; Steiner, P.; Caddle, S.D.; Ziaugra, L.; Beijersbergen, R.L.; Davidoff, M.J.; Liu, Q.; et al. hEST2, the putative human telomerase catalytic subunit gene, is up-regulated in tumor cells and during immortalization. Cell 1997, 90, 785–795. [Google Scholar] [CrossRef]
  12. Arndt, G.M.; MacKenzie, K.L. New prospects for targeting telomerase beyond the telomere. Nat. Rev. Cancer 2016, 16, 508–524. [Google Scholar] [CrossRef] [PubMed]
  13. Takakura, M.; Kyo, S.; Kanaya, T.; Tanaka, M.; Inoue, M. Expression of human telomerase subunits and correlation with telomerase activity in cervical cancer. Cancer Res. 1998, 58, 1558–1561. [Google Scholar] [PubMed]
  14. Cong, Y.S.; Wen, J.; Bacchetti, S. The human telomerase catalytic subunit hTERT: Organization of the gene and characterization of the promoter. Hum. Mol. Genet. 1999, 8, 137–142. [Google Scholar] [CrossRef]
  15. Takakura, M.; Kyo, S.; Kanaya, T.; Hirano, H.; Takeda, J.; Yutsudo, M.; Inoue, M. Cloning of human telomerase catalytic subunit (hTERT) gene promoter and identification of proximal promoter sequences essential for transcriptional activation in immortalized and cancer cells. Cancer Res. 1999, 59, 551–557. [Google Scholar] [PubMed]
  16. Horikawa, I.; Cable, P.L.; Afshari, C.; Barrett, J.C. Cloning and characterization of the promoter region of human telomerase reverse transcriptase gene. Cancer Res. 1999, 59, 826–830. [Google Scholar] [PubMed]
  17. Kyo, S.; Takakura, M.; Fujiwara, T.; Inoue, M. Understanding and exploiting hTERT promoter regulation for diagnosis and treatment of human cancers. Cancer Sci. 2008, 99, 1528–1538. [Google Scholar] [CrossRef] [PubMed]
  18. Wu, K.J.; Grandori, C.; Amacker, M.; Simon-Vermot, N.; Polack, A.; Lingner, J.; Dalla-Favera, R. Direct activation of TERT transcription by c-MYC. Nat. Genet. 1999, 21, 220–224. [Google Scholar] [CrossRef] [PubMed]
  19. Fujimoto, K.; Takahashi, M. Telomerase activity in human leukemic cell lines is inhibited by antisense pentadecadeoxynucleotides targeted against c-myc mRNA. Biochem. Biophys. Res. Commun. 1997, 241, 775–781. [Google Scholar] [CrossRef] [PubMed]
  20. Egger, G.; Liang, G.; Aparicio, A.; Jones, P.A. Epigenetics in human disease and prospects for epigenetic therapy. Nature 2004, 429, 457–463. [Google Scholar] [CrossRef] [PubMed]
  21. Jair, K.W.; Bachman, K.E.; Suzuki, H.; Ting, A.H.; Rhee, I.; Yen, R.W.; Baylin, S.B.; Schuebel, K.E. De novo CpG island methylation in human cancer cells. Cancer Res. 2006, 66, 682–692. [Google Scholar] [CrossRef] [PubMed]
  22. Zinn, R.L.; Pruitt, K.; Eguchi, S.; Baylin, S.B.; Herman, J.G. hTERT is expressed in cancer cell lines despite promoter DNA methylation by preservation of unmethylated DNA and active chromatin around the transcription start site. Cancer Res. 2007, 67, 194–201. [Google Scholar] [CrossRef] [PubMed]
  23. Renaud, S.; Loukinov, D.; Abdullaev, Z.; Guilleret, I.; Bosman, F.T.; Lobanenkov, V.; Benhattar, J. Dual role of DNA methylation inside and outside of CTCF-binding regions in the transcriptional regulation of the telomerase hTERT gene. Nucleic Acids Res. 2007, 35, 1245–1256. [Google Scholar] [CrossRef] [PubMed]
  24. Jenuwein, T.; Allis, C.D. Translating the histone code. Science 2001, 293, 1074–1080. [Google Scholar] [CrossRef] [PubMed]
  25. Cong, Y.S.; Bacchetti, S. Histone deacetylation is involved in the transcriptional repression of hTERT in normal human cells. J. Biol. Chem. 2000, 275, 35665–35668. [Google Scholar] [CrossRef] [PubMed]
  26. Takakura, M.; Kyo, S.; Sowa, Y.; Wang, Z.; Yatabe, N.; Maida, Y.; Tanaka, M.; Inoue, M. Telomerase activation by histone deacetylase inhibitor in normal cells. Nucleic Acids Res. 2001, 29, 3006–3011. [Google Scholar] [CrossRef] [PubMed]
  27. Suenaga, M.; Soda, H.; Oka, M.; Yamaguchi, A.; Nakatomi, K.; Shiozawa, K.; Kawabata, S.; Kasai, T.; Yamada, Y.; Kamihira, S.; et al. Histone deacetylase inhibitors suppress telomerase reverse transcriptase mRNA expression in prostate cancer cells. Int. J. Cancer 2002, 97, 621–625. [Google Scholar] [CrossRef] [PubMed]
  28. Woo, H.J.; Lee, S.J.; Choi, B.T.; Park, Y.M.; Choi, Y.H. Induction of apoptosis and inhibition of telomerase activity by trichostatin A, a histone deacetylase inhibitor, in human leukemic U937 cells. Exp. Mol. Pathol. 2007, 82, 77–84. [Google Scholar] [CrossRef] [PubMed]
  29. Khaw, A.K.; Silasudjana, M.; Banerjee, B.; Suzuki, M.; Baskar, R.; Hande, M.P. Inhibition of telomerase activity and human telomerase reverse transcriptase gene expression by histone deacetylase inhibitor in human brain cancer cells. Mutat. Res. 2007, 625, 134–144. [Google Scholar] [CrossRef] [PubMed]
  30. Choi, J.H.; Min, N.Y.; Park, J.; Kim, J.H.; Park, S.H.; Ko, Y.J.; Kang, Y.; Moon, Y.J.; Rhee, S.; Ham, S.W.; et al. TSA-induced DNMT1 down-regulation represses hTERT expression via recruiting CTCF into demethylated core promoter region of hTERT in HCT116. Biochem. Biophys. Res. Commun. 2010, 391, 449–454. [Google Scholar] [CrossRef] [PubMed]
  31. Liu, C.; Fang, X.; Ge, Z.; Jalink, M.; Kyo, S.; Björkholm, M.; Gruber, A.; Sjöberg, J.; Xu, D. The telomerase reverse transcriptase (hTERT) gene is a direct target of the histone methyltransferase SMYD3. Cancer Res. 2007, 67, 2626–2631. [Google Scholar] [CrossRef] [PubMed]
  32. Bartel, D.P. MicroRNAs: Target recognition and regulatory functions. Cell 2009, 36, 215–233. [Google Scholar] [CrossRef] [PubMed]
  33. Chakrabarti, M.; Banik, N.L.; Ray, S.K. miR-138 overexpression is more powerful than hTERT knockdown to potentiate apigenin for apoptosis in neuroblastoma in vitro and in vivo. Exp. Cell Res. 2013, 319, 1575–1585. [Google Scholar] [CrossRef] [PubMed]
  34. Mitomo, S.; Maesawa, C.; Ogasawara, S.; Iwaya, T.; Shibazaki, M.; Yashima-Abo, A.; Kotani, K.; Oikawa, H.; Sakurai, E.; Izutsu, N.; et al. Downregulation of miR-138 is associated with overexpression of human telomerase reverse transcriptase protein in human anaplastic thyroid carcinoma cell lines. Cancer Sci. 2008, 99, 280–286. [Google Scholar] [CrossRef] [PubMed]
  35. Chen, L.; Lü, M.H.; Zhang, D.; Hao, N.B.; Fan, Y.H.; Wu, Y.Y.; Wang, S.M.; Xie, R.; Fang, D.C.; Zhang, H.; Hu, C.J.; et al. miR-1207-5p and miR-1266 suppress gastric cancer growth and invasion by targeting telomerase reverse transcriptase. Cell Death Dis. 2014, 5, e1034. [Google Scholar] [CrossRef] [PubMed]
  36. Zhang, D.; Xiao, Y.F.; Zhang, J.W.; Xie, R.; Hu, C.J.; Tang, B.; Wang, S.M.; Wu, Y.Y.; Hao, N.B.; Yang, S.M. miR-1182 attenuates gastric cancer proliferation and metastasis by targeting the open reading frame of hTERT. Cancer Lett. 2015, 360, 151–159. [Google Scholar] [CrossRef] [PubMed]
  37. Zhao, Q.; Zhai, Y.X.; Liu, H.Q.; Shi, Y.A.; Li, X.B. MicroRNA-491-5p suppresses cervical cancer cell growth by targeting hTERT. Oncol. Rep. 2015, 34, 979–986. [Google Scholar] [CrossRef] [PubMed]
  38. Li, J.; Lei, H.; Xu, Y.; Tao, Z.Z. miR-512-5p suppresses tumor growth by targeting hTERT in telomerase positive head and neck squamous cell carcinoma in vitro and in vivo. PLoS ONE 2015, 10, e0135265. [Google Scholar] [CrossRef] [PubMed]
  39. Bai, L.; Wang, H.; Wang, A.H.; Zhang, L.Y.; Bai, J. MicroRNA-532 and microRNA-3064 inhibit cell proliferation and invasion by acting as direct regulators of human telomerase reverse transcriptase in ovarian cancer. PLoS ONE 2017, 12, e0173912. [Google Scholar] [CrossRef] [PubMed]
  40. Dinami, R.; Buemi, V.; Sestito, R.; Zappone, A.; Ciani, Y.; Mano, M.; Petti, E.; Sacconi, A.; Blandino, G.; Giacca, M.; et al. Epigenetic silencing of miR-296 and miR-512 ensures hTERT dependent apoptosis protection and telomere maintenance in basal-type breast cancer cells. Oncotarget 2017, 8, 95674–95691. [Google Scholar] [CrossRef] [PubMed]
  41. Akincilar, S.C.; Unal, B.; Tergaonkar, V. Reactivation of telomerase in cancer. Cell. Mol. Life Sci. 2016, 73, 1659–1670. [Google Scholar] [CrossRef] [PubMed]
  42. Barthel, F.P.; Wei, W.; Tang, M.; Martinez-Ledesma, E.; Hu, X.; Amin, S.B.; Akdemir, K.C.; Seth, S.; Song, X.; Wang, Q.; et al. Systematic analysis of telomere length and somatic alterations in 31 cancer types. Nat. Genet. 2017, 49, 349–357. [Google Scholar] [CrossRef] [PubMed]
  43. Theodosiou, M.; Laudet, V.; Schubert, M. From carrot to clinic: An overview of the retinoic acid signaling pathway. Cell. Mol. Life Sci. 2010, 67, 1423–1445. [Google Scholar] [CrossRef] [PubMed]
  44. Dragnev, K.H.; Rigas, J.R.; Dmitrovsky, E. The retinoids and cancer prevention mechanisms. Oncologist 2000, 5, 361–368. [Google Scholar] [CrossRef] [PubMed]
  45. Martín-Rivera, L.; Herrera, E.; Albar, J.P.; Blasco, M.A. Expression of mouse telomerase catalytic subunit in embryos and adult tissues. Proc. Natl. Acad. Sci. USA 1998, 95, 10471–10476. [Google Scholar] [CrossRef] [PubMed]
  46. Sharma, H.W.; Sokoloski, J.A.; Perez, J.R.; Maltese, J.Y.; Sartorelli, A.C.; Stein, C.A.; Nichols, G.; Khaled, Z.; Telang, N.T.; Narayanan, R. Differentiation of immortal cells inhibits telomerase activity. Proc. Natl. Acad. Sci. USA 1995, 92, 12343–12346. [Google Scholar] [CrossRef] [PubMed]
  47. Love, W.K.; Berletch, J.B.; Andrews, L.G.; Tollefsbol, T.O. Epigenetic regulation of telomerase in retinoid-induced differentiation of human leukemia cells. Int. J. Oncol. 2008, 32, 625–631. [Google Scholar] [CrossRef] [PubMed]
  48. Pendino, F.; Flexor, M.; Delhommeau, F.; Buet, D.; Lanotte, M.; Segal-Bendirdjian, E. Retinoids down-regulate telomerase and telomere length in a pathway distinct from leukemia cell differentiation. Proc. Natl. Acad. Sci. USA 2001, 98, 6662–6667. [Google Scholar] [CrossRef] [PubMed]
  49. Pendino, F.; Dudognon, C.; Delhommeau, F.; Sahraoui, T.; Flexor, M.; Bennaceur-Griscelli, A.; Lanotte, M.; Ségal-Bendirdjian, E. Retinoic acid receptor alpha and retinoid-X receptor-specific agonists synergistically target telomerase expression and induce tumor cell death. Oncogene 2003, 22, 9142–9150. [Google Scholar] [CrossRef] [PubMed]
  50. You, Y.O.; Lee, G.; Min, B.M. Retinoic acid extends the in vitro life span of normal human oral keratinocytes by decreasing p16(INK4A) expression and maintaining telomerase activity. Biochem. Biophys. Res. Commun. 2000, 268, 268–274. [Google Scholar] [CrossRef] [PubMed]
  51. Bikle, D.D. Vitamin D metabolism, mechanism of action, and clinical applications. Chem. Biol. 2014, 21, 319–329. [Google Scholar] [CrossRef] [PubMed]
  52. Holick, M.F. Vitamin D: Importance in the prevention of cancers, type 1 diabetes, heart disease, and osteoporosis. Am. J. Clin. Nutr. 2004, 79, 362–371. [Google Scholar] [CrossRef] [PubMed]
  53. Sutton, A.L.; MacDonald, P.N. Vitamin D: More than a “bone-a-fide” hormone. Mol. Endocrinol. 2003, 17, 777–791. [Google Scholar] [CrossRef] [PubMed]
  54. Ikeda, N.; Uemura, H.; Ishiguro, H.; Hori, M.; Hosaka, M.; Kyo, S.; Miyamoto, K.; Takeda, E.; Kubota, Y. Combination treatment with 1alpha,25-dihydroxyvitamin D3 and 9-cis-retinoic acid directly inhibits human telomerase reverse transcriptase transcription in prostate cancer cells. Mol. Cancer Ther. 2003, 2, 739–746. [Google Scholar] [PubMed]
  55. Kasiappan, R.; Shen, Z.; Tse, A.K.; Jinwal, U.; Tang, J.; Lungchukiet, P.; Sun, Y.; Kruk, P.; Nicosia, S.V.; Zhang, X.; et al. 1,25-Dihydroxyvitamin D3 suppresses telomerase expression and human cancer growth through microRNA-498. J. Biol. Chem. 2012, 287, 41297–41309. [Google Scholar] [CrossRef] [PubMed]
  56. Han, X.; Shen, T.; Lou, H. Dietary Polyphenols and Their Biological Significance. Int. J. Mol. Sci. 2007, 8, 950–988. [Google Scholar] [CrossRef]
  57. Lin, J.K.; Liang, Y.C. Cancer chemoprevention by tea polyphenols. Proc. Natl. Sci. Counc. Repub. China B 2000, 24, 1–13. [Google Scholar] [PubMed]
  58. Naasani, I.; Seimiya, H.; Tsuruo, T. Telomerase inhibition, telomere shortening, and senescence of cancer cells by tea catechins. Biochem. Biophys. Res. Commun. 1998, 249, 391–396. [Google Scholar] [CrossRef] [PubMed]
  59. Naasani, I.; Oh-Hashi, F.; Oh-Hara, T.; Feng, W.Y.; Johnston, J.; Chan, K.; Tsuruo, T. Blocking telomerase by dietary polyphenols is a major mechanism for limiting the growth of human cancer cells in vitro and in vivo. Cancer Res. 2003, 63, 824–830. [Google Scholar] [PubMed]
  60. Lin, S.C.; Li, W.C.; Shih, J.W.; Hong, K.F.; Pan, Y.R.; Lin, J.J. The tea polyphenols EGCG and EGC repress mRNA expression of human telomerase reverse transcriptase (hTERT) in carcinoma cells. Cancer Lett. 2006, 236, 80–88. [Google Scholar] [CrossRef] [PubMed]
  61. Berletch, J.B.; Liu, C.; Love, W.K.; Andrews, L.G.; Katiyar, S.K.; Tollefsbol, T.O. Epigenetic and genetic mechanisms contribute to telomerase inhibition by EGCG. J. Cell Biochem. 2008, 103, 509–519. [Google Scholar] [CrossRef] [PubMed]
  62. Min, N.Y.; Kim, J.H.; Choi, J.H.; Liang, W.; Ko, Y.J.; Rhee, S.; Bang, H.; Ham, S.W.; Park, A.J.; Lee, K.H. Selective death of cancer cells by preferential induction of reactive oxygen species in response to (−)-epigallocatechin-3-gallate. Biochem. Biophys. Res. Commun. 2012, 421, 91–97. [Google Scholar] [CrossRef] [PubMed]
  63. Fang, M.Z.; Wang, Y.; Ai, N.; Hou, Z.; Sun, Y.; Lu, H.; Welsh, W.; Yang, C.S. Tea polyphenol (−)-epigallocatechin-3-gallate inhibits DNA methyltransferase and reactivates methylation-silenced genes in cancer cell lines. Cancer Res. 2003, 15, 7563–7570. [Google Scholar]
  64. Tan, H.H.; Porter, A.G. p21WAF1 negatively regulates DNMT1 expression in mammalian cells. Biochem. Biophys. Res. Commun. 2009, 382, 171–176. [Google Scholar] [CrossRef] [PubMed]
  65. Gupta, S.C.; Kismali, G.; Aggarwal, B.B. Curcumin, a component of turmeric: From farm to pharmacy. Biofactors 2013, 39, 2–13. [Google Scholar] [CrossRef] [PubMed]
  66. Ramachandran, C.; Fonseca, H.B.; Jhabvala, P.; Escalon, E.A.; Melnick, S.J. Curcumin inhibits telomerase activity through human telomerase reverse transcritpase in MCF-7 breast cancer cell line. Cancer Lett. 2002, 184, 1–6. [Google Scholar] [CrossRef]
  67. Forsythe, H.L.; Jarvis, J.L.; Turner, J.W.; Elmore, L.W.; Holt, S.E. Stable association of hsp90 and p23, but Not hsp70, with active human telomerase. J. Biol. Chem. 2001, 276, 15571–15574. [Google Scholar] [CrossRef] [PubMed]
  68. Lee, J.H.; Chung, I.K. Curcumin inhibits nuclear localization of telomerase by dissociating the Hsp90 co-chaperone p23 from hTERT. Cancer Lett. 2010, 290, 76–86. [Google Scholar] [CrossRef] [PubMed]
  69. Khaw, A.K.; Hande, M.P.; Kalthur, G.; Hande, M.P. Curcumin inhibits telomerase and induces telomere shortening and apoptosis in brain tumour cells. J. Cell Biochem. 2013, 114, 1257–1270. [Google Scholar] [CrossRef] [PubMed]
  70. Mukund, V.; Mukund, D.; Sharma, V.; Mannarapu, M.; Alam, A. Genistein: Its role in metabolic diseases and cancer. Crit. Rev. Oncol. Hematol. 2017, 119, 13–22. [Google Scholar]
  71. Kang, S.S.; Kwon, T.; Kwon, D.Y.; Do, S.I. Akt protein kinase enhances human telomerase activity through phosphorylation of telomerase reverse transcriptase subunit. J. Biol. Chem. 1999, 274, 13085–13090. [Google Scholar] [CrossRef] [PubMed]
  72. Kim, Y.W.; Hur, S.Y.; Kim, T.E.; Lee, J.M.; Namkoong, S.E.; Ki, I.K.; Kim, J.W. Protein kinase C modulates telomerase activity in human cervical cancer cells. Exp. Mol. Med. 2001, 33, 156–163. [Google Scholar] [CrossRef] [PubMed]
  73. Jagadeesh, S.; Kyo, S.; Banerjee, P.P. Genistein represses telomerase activity via both transcriptional and posttranslational mechanisms in human prostate cancer cells. Cancer Res. 2006, 66, 2107–2115. [Google Scholar] [CrossRef] [PubMed]
  74. Li, Y.; Liu, L.; Andrews, L.G.; Tollefsbol, T.O. Genistein depletes telomerase activity through cross-talk between genetic and epigenetic mechanisms. Int. J. Cancer 2009, 125, 286–296. [Google Scholar] [CrossRef] [PubMed]
  75. Rauf, A.; Imran, M.; Suleria, H.A.R.; Ahmad, B.; Peters, D.G.; Mubarak, M.S. A comprehensive review of the health perspectives of resveratrol. Food Funct. 2017, 8, 4284–4305. [Google Scholar] [CrossRef] [PubMed]
  76. Lanzilli, G.; Fuggetta, M.P.; Tricarico, M.; Cottarelli, A.; Serafino, A.; Falchetti, R.; Ravagnan, G.; Turriziani, M.; Adamo, R.; Franzese, O.; et al. Resveratrol down-regulates the growth and telomerase activity of breast cancer cells in vitro. Int. J. Oncol. 2006, 28, 641–648. [Google Scholar] [CrossRef] [PubMed]
  77. Tippani, R.; Prakhya, L.J.; Porika, M.; Sirisha, K.; Abbagani, S.; Thammidala, C. Pterostilbene as a potential novel telomerase inhibitor: Molecular docking studies and its in vitro evaluation. Curr. Pharm. Biotechnol. 2014, 14, 1027–1035. [Google Scholar] [CrossRef] [PubMed]
  78. Kala, R.; Shah, H.N.; Martin, S.L.; Tollefsbol, T.O. Epigenetic-based combinatorial resveratrol and pterostilbene alters DNA damage response by affecting SIRT1 and DNMT enzyme expression, including SIRT1-dependent γ-H2AX and telomerase regulation in triple-negative breast cancer. BMC Cancer 2015, 15, 672. [Google Scholar] [CrossRef] [PubMed]
  79. Ogretmen, B.; Hannun, Y.A. Biologically active sphingolipids in cancer pathogenesis and treatment. Nat. Rev. Cancer. 2004, 4, 604–616. [Google Scholar] [CrossRef] [PubMed]
  80. Saddoughi, S.A.; Ogretmen, B. Diverse functions of ceramide in cancer cell death and proliferation. Adv. Cancer Res. 2013, 117, 37–58. [Google Scholar] [PubMed]
  81. Ogretmen, B.; Schady, D.; Usta, J.; Wood, R.; Kraveka, J.M.; Luberto, C.; Birbes, H.; Hannun, Y.A.; Obeid, L.M. Role of ceramide in mediating the inhibition of telomerase activity in A549 human lung adenocarcinoma cells. J. Biol. Chem. 2001, 276, 24901–24910. [Google Scholar] [CrossRef] [PubMed]
  82. Sundararaj, K.P.; Wood, R.E.; Ponnusamy, S.; Salas, A.M.; Szulc, Z.; Bielawska, A.; Obeid, L.M.; Hannun, Y.A.; Ogretmen, B. Rapid shortening of telomere length in response to ceramide involves the inhibition of telomere binding activity of nuclear glyceraldehyde-3-phosphate dehydrogenase. J. Biol. Chem. 2004, 279, 6152–6162. [Google Scholar] [CrossRef] [PubMed]
  83. Ogretmen, B.; Kraveka, J.M.; Schady, D.; Usta, J.; Hannun, Y.A.; Obeid, L.M. Molecular mechanisms of ceramide-mediated telomerase inhibition in the A549 human lung adenocarcinoma cell line. J. Biol. Chem. 2001, 276, 32506–32514. [Google Scholar] [CrossRef] [PubMed]
  84. Wooten, L.G.; Ogretmen, B. Sp1/Sp3-dependent regulation of human telomerase reverse transcriptase promoter activity by the bioactive sphingolipid ceramide. J. Biol. Chem. 2005, 280, 28867–28876. [Google Scholar] [CrossRef] [PubMed]
  85. Wooten-Blanks, L.G.; Song, P.; Senkal, C.E.; Ogretmen, B. Mechanisms of ceramide-mediated repression of the human telomerase reverse transcriptase promoter via deacetylation of Sp3 by histone deacetylase 1. FASEB J. 2007, 21, 3386–3397. [Google Scholar] [CrossRef] [PubMed]
  86. Bishop, D.G.; Sparace, S.A.; Mudd, J.B. Biosynthesis of sulfoquinovosyldiacylglycerol in higher plants: The origin of the diacylglycerol moiety. Arch. Biochem. Biophys. 1985, 240, 851–858. [Google Scholar] [CrossRef]
  87. Sahara, H.; Ishikawa, M.; Takahashi, N.; Ohtani, S.; Sato, N.; Gasa, S.; Akino, T.; Kikuchi, K. In vivo anti-tumour effect of 3′-sulphonoquinovosyl 1′-monoacylglyceride isolated from sea urchin (Strongylocentrotus intermedius) intestine. Br. J. Cancer. 1997, 75, 324–332. [Google Scholar] [CrossRef] [PubMed]
  88. Eitsuka, T.; Nakagawa, K.; Igarashi, M.; Miyazawa, T. Telomerase inhibition by sulfoquinovosyldiacylglycerol from edible purple laver (Porphyra yezoensis). Cancer Lett. 2004, 212, 15–20. [Google Scholar] [CrossRef] [PubMed]
  89. Stillwell, W.; Wassall, S.R. Docosahexaenoic acid: Membrane properties of a unique fatty acid. Chem. Phys. Lipids 2003, 126, 1–27. [Google Scholar] [CrossRef]
  90. Bannenberg, G.; Serhan, C.N. Specialized pro-resolving lipid mediators in the inflammatory response: An update. Biochim. Biophys. Acta 2010, 1801, 1260–1273. [Google Scholar] [CrossRef] [PubMed]
  91. Sampath, H.; Ntambi, J.M. Polyunsaturated fatty acid regulation of gene expression. Nutr. Rev. 2004, 62, 333–339. [Google Scholar] [CrossRef] [PubMed]
  92. Eitsuka, T.; Nakagawa, K.; Suzuki, T.; Miyazawa, T. Polyunsaturated fatty acids inhibit telomerase activity in DLD-1 human colorectal adenocarcinoma cells: A dual mechanism approach. Biochim. Biophys. Acta 2005, 1737, 1–10. [Google Scholar] [CrossRef] [PubMed]
  93. Packer, L.; Weber, S.U.; Rimbach, G. Molecular aspects of alpha-tocotrienol antioxidant action and cell signalling. J. Nutr. 2001, 131, 369S–373S. [Google Scholar] [CrossRef] [PubMed]
  94. Aggarwal, B.B.; Sundaram, C.; Prasad, S.; Kannappan, R. Tocotrienols, the vitamin E of the 21st century: Its potential against cancer and other chronic diseases. Biochem. Pharmacol. 2010, 80, 1613–1631. [Google Scholar] [CrossRef] [PubMed]
  95. Suzuki, Y.J.; Tsuchiya, M.; Wassall, S.R.; Choo, Y.M.; Govil, G.; Kagan, V.E.; Packer, L. Structural and dynamic membrane properties of alpha-tocopherol and alpha-tocotrienol: Implication to the molecular mechanism of their antioxidant potency. Biochemistry 1993, 32, 10692–10699. [Google Scholar] [CrossRef] [PubMed]
  96. Eitsuka, T.; Nakagawa, K.; Miyazawa, T. Down-regulation of telomerase activity in DLD-1 human colorectal adenocarcinoma cells by tocotrienol. Biochem. Biophys. Res. Commun. 2006, 348, 170–175. [Google Scholar] [CrossRef] [PubMed]
  97. Eitsuka, T.; Tatewaki, N.; Nishida, H.; Kurata, T.; Nakagawa, K.; Miyazawa, T. Synergistic inhibition of cancer cell proliferation with a combination of δ-tocotrienol and ferulic acid. Biochem. Biophys. Res. Commun. 2014, 453, 606–611. [Google Scholar] [CrossRef] [PubMed]
  98. Eitsuka, T.; Tatewaki, N.; Nishida, H.; Nakagawa, K.; Miyazawa, T. A combination of δ-tocotrienol and ferulic acid synergistically inhibits telomerase activity in DLD-1 human colorectal adenocarcinoma cells. J. Nutr. Sci. Vitaminol. 2016, 62, 281–287. [Google Scholar] [CrossRef] [PubMed]
  99. Eitsuka, T.; Tatewaki, N.; Nishida, H.; Nakagawa, K.; Miyazawa, T. Synergistic Anticancer Effect of Tocotrienol Combined with Chemotherapeutic Agents or Dietary Components: A Review. Int. J. Mol. Sci. 2016, 17, 1605. [Google Scholar] [CrossRef] [PubMed]
  100. Juge, N.; Mithen, R.F.; Traka, M. Molecular basis for chemoprevention by sulforaphane: A comprehensive review. Cell Mol. Life Sci. 2007, 64, 1105–1127. [Google Scholar] [CrossRef] [PubMed]
  101. Moon, D.O.; Kang, S.H.; Kim, K.C.; Kim, M.O.; Choi, Y.H.; Kim, G.Y. Sulforaphane decreases viability and telomerase activity in hepatocellular carcinoma Hep3B cells through the reactive oxygen species-dependent pathway. Cancer Lett. 2010, 295, 260–266. [Google Scholar] [CrossRef] [PubMed]
  102. Meeran, S.M.; Patel, S.N.; Tollefsbol, T.O. Sulforaphane causes epigenetic repression of hTERT expression in human breast cancer cell lines. PLoS ONE 2010, 5, e11457. [Google Scholar] [CrossRef] [PubMed]
  103. Chau, M.N.; El Touny, L.H.; Jagadeesh, S.; Banerjee, PP. Physiologically achievable concentrations of genistein enhance telomerase activity in prostate cancer cells via the activation of STAT3. Carcinogenesis 2007, 28, 2282–2290. [Google Scholar] [CrossRef] [PubMed]
  104. Oak, J.H.; Nakagawa, K.; Miyazawa, T. Synthetically prepared Aamadori-glycated phosphatidylethanolaminecan trigger lipid peroxidation via free radical reactions. FEBS Lett. 2000, 481, 26–30. [Google Scholar] [CrossRef]
  105. Oak, J.H.; Nakagawa, K.; Miyazawa, T. UV analysis of Amadori-glycated phosphatidylethanolamine in foods and biological samples. J. Lipid Res. 2002, 43, 523–529. [Google Scholar] [PubMed]
  106. Nakagawa, K.; Oak, J.H.; Higuchi, O.; Tsuzuki, T.; Oikawa, S.; Otani, H.; Mune, M.; Cai, H.; Miyazawa, T. Ion-trap tandem mass spectrometric analysis of Amadori-glycated phosphatidylethanolamine in human plasma with or without diabetes. J. Lipid Res. 2005, 46, 2514–2524. [Google Scholar] [CrossRef] [PubMed]
  107. Everhart, J.; Wright, D. Diabetes mellitus as a risk factor for pancreatic cancer. A meta-analysis. JAMA 1995, 273, 1605–1609. [Google Scholar] [CrossRef] [PubMed]
  108. Eitsuka, T.; Nakagawa, K.; Ono, Y.; Tatewaki, N.; Nishida, H.; Kurata, T.; Shoji, N.; Miyazawa, T. Amadori-glycated phosphatidylethanolamine up-regulates telomerase activity in PANC-1 human pancreatic carcinoma cells. FEBS Lett. 2012, 586, 2542–2547. [Google Scholar] [CrossRef] [PubMed]
  109. Pai, R.B.; Pai, S.B.; Kukhanova, M.; Dutschman, G.E.; Guo, X.; Cheng, Y.C. Telomerase from human leukemia cells: Properties and its interaction with deoxynucleoside analogues. Cancer Res. 1998, 58, 1909–1913. [Google Scholar] [PubMed]
  110. Jackson, S.R.; Zhu, C.H.; Paulson, V.; Watkins, L.; Dikmen, Z.G.; Gryaznov, S.M.; Wright, W.E.; Shay, J.W. Antiadhesive effects of GRN163L-an oligonucleotide N3′->P5′ thio-phosphoramidate targeting telomerase. Cancer Res. 2007, 67, 1121–1129. [Google Scholar] [CrossRef] [PubMed]
  111. Wheelhouse, R.T.; Sun, D.; Han, H.; Han, F.X.; Hurley, L.H. Cationic porphyrins as telomerase inhibitors: The interaction of tetra-(N-methyl-4-pyridyl)porphine with quadruplex DNA. J. Am. Chem. Soc. 1998, 120, 3261–3262. [Google Scholar] [CrossRef]
  112. Damm, K.; Hemmann, U.; Garin-Chesa, P.; Hauel, N.; Kauffmann, I.; Priepke, H.; Niestroj, C.; Daiber, C.; Enenkel, B.; Guilliard, B.; et al. A highly selective telomerase inhibitor limiting human cancer cell proliferation. EMBO J. 2001, 20, 6958–6968. [Google Scholar] [CrossRef] [PubMed]
  113. Villa, R.; Folini, M.; Porta, C.D.; Valentini, A.; Pennati, M.; Daidone, M.G.; Zaffaroni, N. Inhibition of telomerase activity by geldanamycin and 17-allylamino, 17-demethoxygeldanamycin in human melanoma cells. Carcinogenesis 2003, 24, 851–859. [Google Scholar] [CrossRef] [PubMed]
  114. Tefferi, A.; Lasho, T.L.; Begna, K.H.; Patnaik, M.M.; Zblewski, D.L.; Finke, C.M.; Laborde, R.R.; Wassie, E.; Schimek, L.; Hanson, C.A.; et al. A Pilot Study of the Telomerase Inhibitor Imetelstat for Myelofibrosis. N. Engl. J. Med. 2015, 373, 908–919. [Google Scholar] [CrossRef] [PubMed]
  115. Baerlocher, G.M.; Oppliger Leibundgut, E.; Ottmann, O.G.; Spitzer, G.; Odenike, O.; McDevitt, M.A.; Röth, A.; Daskalakis, M.; Burington, B.; Stuart, M.; et al. Telomerase Inhibitor Imetelstat in Patients with Essential Thrombocythemia. N. Engl. J. Med. 2015, 373, 920–928. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  116. Campbell, F.C.; Xu, H.; El-Tanani, M.; Crowe, P.; Bingham, V. The yin and yang of vitamin D receptor (VDR) signaling in neoplastic progression: Operational networks and tissue-specific growth control. Biochem. Pharmacol. 2010, 79, 1–9. [Google Scholar] [CrossRef] [PubMed]
  117. Hiyama, E.; Hiyama, K.; Yokoyama, T.; Matsuura, Y.; Piatyszek, M.A.; Shay, J.W. Correlating telomerase activity levels with human neuroblastoma outcomes. Nat. Med. 1995, 1, 249–255. [Google Scholar] [CrossRef] [PubMed]
  118. Smith, L.L.; Coller, H.A.; Roberts, J.M. Telomerase modulates expression of growth-controlling genes and enhances cell proliferation. Nat. Cell Biol. 2003, 5, 474–479. [Google Scholar] [CrossRef] [PubMed]
  119. Gorbunova, V.; Seluanov, A.; Pereira-Smith, O.M. Expression of human telomerase (hTERT) does not prevent stress-induced senescence in normal human fibroblasts but protects the cells from stress-induced apoptosis and necrosis. J. Biol. Chem. 2002, 277, 38540–38549. [Google Scholar] [CrossRef] [PubMed]
  120. Maritz, M.F.; Richards, L.A.; Mackenzie, K.L. Assessment and quantification of telomerase enzyme activity. Methods Mol. Biol. 2013, 965, 215–231. [Google Scholar] [PubMed]
  121. Fajkus, J. Detection of telomerase activity by the TRAP assay and its variants and alternatives. Clin. Chim. Acta 2006, 371, 25–31. [Google Scholar] [CrossRef] [PubMed]
  122. Tatematsu, K.; Nakayama, J.; Danbara, M.; Shionoya, S.; Sato, H.; Omine, M.; Ishikawa, F. A novel quantitative ‘stretch PCR assay’, that detects a dramatic increase in telomerase activity during the progression of myeloid leukemias. Oncogene 1996, 13, 2265–2274. [Google Scholar] [PubMed]
  123. Montpetit, A.J.; Alhareeri, A.A.; Montpetit, M.; Starkweather, A.R.; Elmore, L.W.; Filler, K.; Mohanraj, L.; Burton, C.W.; Menzies, V.S.; Lyon, D.E.; et al. Telomere length: A review of methods for measurement. Nurs. Res. 2014, 63, 289–299. [Google Scholar] [CrossRef] [PubMed]
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Figure 1. Promoter region of hTERT and transcription factors essential for regulating its activity. +1 is the transcription start site; +78 (ATG) is the first codon of the hTERT protein.
Figure 1. Promoter region of hTERT and transcription factors essential for regulating its activity. +1 is the transcription start site; +78 (ATG) is the first codon of the hTERT protein.
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Figure 2. Regulation of hTERT transcription by 5-aza-2′-deoxycytidine. In cancer cells, CTCF recognition sequence in hTERT gene is hypermethylated, thus blocking CTCF binding and inducing hTERT expression. Treatment with 5-aza-2′-deoxycytidine leads to demethylation of hTERT promoter, thereby causing the binding of CTCF to the target site and suppressing hTERT transcription.
Figure 2. Regulation of hTERT transcription by 5-aza-2′-deoxycytidine. In cancer cells, CTCF recognition sequence in hTERT gene is hypermethylated, thus blocking CTCF binding and inducing hTERT expression. Treatment with 5-aza-2′-deoxycytidine leads to demethylation of hTERT promoter, thereby causing the binding of CTCF to the target site and suppressing hTERT transcription.
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Figure 3. Chemical structures of telomerase modulators. (A) All-trans retinoic acid (RA). (B) 1α,25-Dihydroxyvitamin D3 (1α,25(OH)2VD3). (C) (−)-Epigallocatechin-3-gallate (EGCG). (D) Curcumin. (E) Genistein. (F) Resveratrol. (G) Ceramide. R, acyl chain. (H) Sulfoquinovosyldiacylglycerol (SQDG). R1 and R2 indicate acyl chains. (I) Eicosapentaenoic acid (EPA). (J) Tocotrienol (T3) and tocopherol (Toc). (K) Sulforaphane. (L) Phosphatidylethanolamine-linked Amadori product (Amadori-PE). R1 and R2 indicate acyl chains.
Figure 3. Chemical structures of telomerase modulators. (A) All-trans retinoic acid (RA). (B) 1α,25-Dihydroxyvitamin D3 (1α,25(OH)2VD3). (C) (−)-Epigallocatechin-3-gallate (EGCG). (D) Curcumin. (E) Genistein. (F) Resveratrol. (G) Ceramide. R, acyl chain. (H) Sulfoquinovosyldiacylglycerol (SQDG). R1 and R2 indicate acyl chains. (I) Eicosapentaenoic acid (EPA). (J) Tocotrienol (T3) and tocopherol (Toc). (K) Sulforaphane. (L) Phosphatidylethanolamine-linked Amadori product (Amadori-PE). R1 and R2 indicate acyl chains.
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Table
Table 1. hTERT regulation by miRNA.
Table 1. hTERT regulation by miRNA.
Tumor TypemiRNAReference
NeuroblastomamiR-138[33]
Anaplastic thyroid carcinomamiR-138[34]
Gastric cancermiR-1207-5p[35]
miR-1266[35]
miR-1182[36]
Cervical cancermiR-491-5p[37]
Head and neck squamous cell carcinomamiR-512-5p[38]
Ovarian cancermiR-532[39]
miR-3064[39]
Breast cancermiR-296[40]
miR-512[40]
Table
Table 2. IC50 values of various fatty acids.
Table 2. IC50 values of various fatty acids.
Number of Carbon AtomsFatty AcidIC50 (μM) 1
C12Lauric acid [12:0]>100
cis-11-Dodecenoic acid [12:1 Δ11cis]>100
C14Myristic acid [14:0]>100
Myristoleic acid [14:1 Δ9cis]>100
C16Palmitic acid [16:0]>100
Palmitoleic acid [16:1 Δ9cis]25
C18Stearic acid [18:0]>100
Oleic acid [18:1 Δ9cis]35
Vaccenic acid [18:1 Δ11cis]38
Elaidic acid [18:1 Δ9trans]55
trans-Vaccenic acid [18:1 Δ11trans]74
Linoleic acid [18:2 Δ9-12cis]25
Linolelaidic acid [18:2 Δ9-12trans]>50
γ-Linolenic acid [18:3 Δ6-9-12cis]13
α-Linolenic acid [18:2 Δ9-12-15cis]10
C20Arachidic acid [20:0]>100
cis-5-Eicosenoic acid [20:1 Δ5cis]>100
cis-11-Eicosenoic acid [20:1 Δ11cis]>100
trans-11-Eicosenoic acid [20:1 Δ11trans]>100
cis-11-14-Eicosadienoic acid [20:2 Δ11-14cis]70
cis-8-11-14-Eicosatrienoic acid [20:3 Δ8-11-14cis]30
cis-11-14-17-Eicosatrienoic acid [20:3 Δ11-14-17cis]24
Arachidonic acid [20:4 Δ5-8-11-14cis]25
Eicosapentaenoic acid (EPA) [20:5 Δ5-8-11-14-17cis]19
C22cis-13-16-19-Docosatrienoic acid [22:3 Δ13-16-19cis]45
Docosahexaenoic acid (DHA) [22:6 Δ4-7-10-13-16-19cis]5
1 IC50: concentration (μM) causing 50% inhibition of telomerase activity.

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Eitsuka, T.; Nakagawa, K.; Kato, S.; Ito, J.; Otoki, Y.; Takasu, S.; Shimizu, N.; Takahashi, T.; Miyazawa, T. Modulation of Telomerase Activity in Cancer Cells by Dietary Compounds: A Review. Int. J. Mol. Sci. 2018, 19, 478. https://doi.org/10.3390/ijms19020478

AMA Style

Eitsuka T, Nakagawa K, Kato S, Ito J, Otoki Y, Takasu S, Shimizu N, Takahashi T, Miyazawa T. Modulation of Telomerase Activity in Cancer Cells by Dietary Compounds: A Review. International Journal of Molecular Sciences. 2018; 19(2):478. https://doi.org/10.3390/ijms19020478

Chicago/Turabian Style

Eitsuka, Takahiro, Kiyotaka Nakagawa, Shunji Kato, Junya Ito, Yurika Otoki, Soo Takasu, Naoki Shimizu, Takumi Takahashi, and Teruo Miyazawa. 2018. "Modulation of Telomerase Activity in Cancer Cells by Dietary Compounds: A Review" International Journal of Molecular Sciences 19, no. 2: 478. https://doi.org/10.3390/ijms19020478

APA Style

Eitsuka, T., Nakagawa, K., Kato, S., Ito, J., Otoki, Y., Takasu, S., Shimizu, N., Takahashi, T., & Miyazawa, T. (2018). Modulation of Telomerase Activity in Cancer Cells by Dietary Compounds: A Review. International Journal of Molecular Sciences, 19(2), 478. https://doi.org/10.3390/ijms19020478

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