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There is growing evidence that aminobisphosphonates like ibandronate show anticancer activity by an unknown mechanism. Biochemically, they prevent posttranslational isoprenylation of small GTPases, thus inhibiting their activity. In tumor cells, activated RAS-GTPase, the founding member of the gene family, down-regulates the expression of the pro-apoptotic gene FAS via epigenetic DNA-methylation by DNMT1. We compared ibandronate treatment in neoplastic human U-2 osteosarcoma and in mouse CCL-51 breast cancer cells as well as in the immortalized non-neoplastic MC3T3-E1 osteoblastic cells. Ibandronate attenuated cell proliferation in all cell lines tested. In the neoplastic cells we found up-regulation of caspases suggesting apoptosis. Further we found stimulation of FAS-expression as a result of epigenetic DNA demethylation that was due to down-regulation of DNMT1, which was rescued by re-isoprenylation by both geranylgeranyl-pyrophosphate and farnesylpyrophosphate. In contrast, ibandronate did not affect FAS and DNMT1 expression in MC3T3-E1 non-neoplastic cells. Data suggest that bisphosphonates via modulation of the activity of small-GTPases induce apoptosis in neoplastic cells by DNA-CpG-demethylation and stimulation of FAS-expression. In conclusion the shown epigenetic mechanism underlying the anti-neoplastic activity of farnesyl-transferase-inhibition, also explains the clinical success of other drugs, which target this pathway.
The 3rd generation of aminobisphosphonates like alendronate, risedronate, zoledronic acid, ibandronate and other compounds affect bone resorption of osteoclasts by inhibiting isoprenylation of the small GTP-binding proteins and are therefore used as anti-resorptive treatment of osteoporosis. Additionally to their effects on bone, there is growing evidence for an anticancer activity of these drugs [1–8]. However, the mechanisms involved in these effects remain poorly understood.
Biochemically, aminobisphosphonates act principally by inhibiting farnesyl pyrophosphate (FPP) synthase – an enzyme of the mevalonate pathway – thereby preventing the post-translational modification (prenylation) of small guanosine triphosphate (GTP)-binding proteins (small-GTPases) that is essential for their function. Because small GTP-binding proteins modulate nearly every cellular activity, it is clear that functional inhibition from members of this protein family influences growth and differentiation of normal cells as well as of tumor cells [3,5,7,9–11].
The founding members of the large family of small-GTPases are the three RAS-proteins, HRAS, NRAS and KRAS. Activation of the RAS/RAF/MEK/ERK pathway, for instance by mutation of the involved GTPases or their regulating members, is responsible for the development of a plethora of cancers [12–14] and targeting this pathway seems to be a promising strategy in tumor therapy [15,16]. The RAS/RAF/MEK/ERK pathway activates DNA-methylation processes [17–19]. Epigenetic processes include histone modifications and methylation of CpGs (cytosine-guanosine dinucleotides) on the DNA, especially on gene promoters. Changes of the methylation state of gene promoters lead to alteration in gene expression patterns. This influences cellular differentiation and apoptosis and thus tumor formation (for review see Refs. [19–22]). DNA methylation dependent inactivation of tumor suppressor genes like cell cycle inhibitors (e.g. CDKN1A, CDKN1B, CDKN2A, CDKN2B) and LOX (lysyl oxidase) as well of the pro-apoptotic gene FAS (TNF receptor superfamily, member 6) is often observed during development of neoplastic diseases. Promoter CpG-hypermethylation of these genes was found in colon cancers , prostate carcinomas [24–26], breast cancers [27–29] or hematologic malignancies [30–33]. Consequently, several DNA demethylating agents were developed and are now in use as anti neoplastic drugs to reactivate genes such as FAS which plays a key role in immortality of cancer stem cells .
It has recently been shown that activated RAS prevents cellular apoptosis by epigenetic inhibition of Fas expression through stimulation of the RAF/MEK/MAPK1 pathway with subsequent Fas promoter methylation via DNMT1 (DNA-(cytosine-5-)-methyltransferase 1), an enzyme responsible for CpG methylation during cell replication . Similarly, in osteoblasts, extracellular matrix (collagen type I) preserves CpG-methylation of the Fas promoter via MAPK1 and DNMT1, thus preventing apoptosis of proliferating osteoblasts . Although, utmost efforts have been spent to clarify the relevance and the regulation of cytosine methylation for physiological and pathological development, only few progresses have been made until now. The involvement of RAS and other small GTP-binding proteins in bisphosphonates’ activity and the knowledge of apoptotic effects on bone cells, also of bisphosphonates of the 3rd generation [1,4,6,7,35–37], suggest that these drugs could modulate CpG-methylation of gene promoters.
Here, we demonstrate that the aminobisphosphonate ibandronate modulates the DNA methylation status of the FAS promoter by influencing the isoprenylate pathway in human U-2 osteosarcoma (OS) cells and CCL-51 cells, a murine mammary gland tumor cell line, but not in non-neoplastic immortalized MC3T3-E1 cells. Treatment with ibandronate leads to re-expression of FAS and to increased activity of apoptosis-associated caspases in the tumor cell lines. Knock down of FAS mRNA expression by siRNA technique largely re-establishes cell viability in ibandronate treated neoplastic U-2 OS cells. Our data suggest that epigenetic mechanisms play a key role in the apoptotic activity of bisphosphonates, and possibly many of their effects on cellular physiology including systemic changes within an organism.
MC3T3-E1 cells, a clonal pre-osteoblastic cell line derived from newborn mouse calvaria (kindly donated by Dr. Kumegawa, Meikai University, Department of Oral Anatomy, Sakado, Japan) and the human osteosarcoma cell line U-2 OS were cultured in alpha-minimum essential medium (α-MEM; Biochrom, Berlin, Germany) supplemented with 50 μg/mL ascorbic acid (Sigma–Aldrich, St. Louis, MO), 5% fetal calf serum (Biochrom), and 10 μg/mL gentamycin (Sigma–Aldrich). CCL-51 cells, a murine mammary gland tumor cell line, were cultured in eagle minimum essential medium (EMEM, Sigma–Aldrich) supplemented with 292 μg/mL l-glutamine, 10% fetal calf serum and 10 μg/mL gentamycin. All cells were cultured in humidified air under 5% CO2 at 37 °C. For propagation, cells were subcultured twice a week using 0.001% pronase E (Roche, Mannheim, Germany) and 0.02% EDTA in Ca2+- and Mg2+-free phosphate-buffered saline (PBS) before achieving confluence. To prevent a potential phenotypic drift during repeated sub-cultures, the cells were not used for more than 4 weeks after thawing. For experiments, cells were seeded in culture dishes at a density of 20,000/cm2 as untreated controls or treated with the indicated compounds at times and concentrations specified. Ibandronate, geranylgeranyl-pyrophosphate (GGPP) and farnesyl-pyrophosphate (FPP) were purchased from Sigma-Aldrich. Ibandronate was dissolved in water and aliquots were frozen at −20 °C.
To assess cell metabolic activity, a commercially available, MTT similar assay (EZ4U; Biomedica, Vienna, Austria) was used. For this purpose, the cell lines were incubated with increasing concentrations of ibandronate (1–50 μM for MC3T3-E1 and U-2 OS cells or 1–200 μM for CCL-51 cells). After a comparable doubling time for all three cell lines the assay was performed following the protocol of the supplier.
Cells were seeded in 24 multi-well culture dishes at a density of 20,000/cm2 and were either left untreated (controls) or treated with ibandronate, GGPP and FPP at the indicated concentrations for 72 h. Thereafter, cells were detached with 0.001% pronase E and the number of viable cells was assessed with Casy cell counter (Schaerfe Systems, Germany). Each experiment was performed in quadruplicate and experiments were carried out twice.
Caspase 3/7 and caspase 8 activities were measured by using the Caspase-Glo 3/7 and Caspase-Glo 8 assay Kit (Promega, Corp., Madison, WI) following manufactures instructions. Briefly, after treatments, cells were lysed and substrate cleavage by caspases was measured by the generated luminescent signal with a 96 multi-well luminometer (Glomax, Promega). Each experiment was performed in quintuplicate and experiments were carried out twice.
DNA and RNA were extracted using a DNA/RNA Isolation Kit (Qiagen, Hilden, Germany) following manufacturers instructions. cDNA was synthesized from 0.5 μg RNA using the 1st Strand cDNA Synthesis Kit (Roche) as described by the supplier. The obtained cDNA was subjected to PCR amplification with a real-time cycler using FastStart SYBR-Green Master Mix (Roche) for the genes Fas and Dnmt1 (primers are shown in Table 1). The qRT-PCR was performed with 45 cycles composed of 30 s denaturation at 95 °C, 30 s annealing at the indicated temperature (Table 1) and 30 s extension at 72 °C after 10 min of initial denaturation at 95 °C. For normalization of the expression we used the 18S RNA TaqMan probe (4319413E, Applied Biosystems, Forster City, CA) in the respective master mix according to the suppliers suggested conditions (Applied Biosystems). All PCRs were performed in triplicate and expression was evaluated using the comparative quantitation method . For each of the three time independent biological replicates, the triplicate results of the qRT-PCR were averaged and this mean value was treated as a single statistical unit.
For FAS depletion by siRNA, U-2 OS cells were seeded at 20,000 cells/cm2 in a 48-multi-well plate and transfected with 100 nM of a mixture of two FAS siRNAs (SASI_Hs01 00079050, SASI_Hs01_00079052, Sigma–Aldrich) by electroporation using the Neon Transfection System (Invitrogen) following supplier's protocol. Next day cells were treated with 7.2 μM ibandronate (EC50). After 72 h of incubation, cell metabolic activity was measured with the EZ4U assay as described above. Furthermore to control FAS mRNA and protein knockdown, cells were seeded in a six-multi well plate or 5 cm petri dish at 20,000 cells/cm2 and transfected with the FAS siRNA as described above. 96 h after transfection mRNA or protein was isolated as described above and below and FAS mRNA and protein expression was measured by qRT-PCR and immune-blot, respectively.
For whole cell protein extraction, cells were washed twice with PBS, scraped in SDS sample buffer (2% SDS, 100 mM β-mercaptoethanol, 125 mM Tris–HCl, pH 6.8) heated at 95 °C for 5 min and sonicated for further 5 min. To divide cell proteins into cytosolic and membrane fractions, cells were detached from culture vessels washed with PBS and incubated in hypotonic buffer (10 mM HEPES pH 7.8, 1.5 mM MgCl2, 10 mM KCl, 0.5 mM DTT, 0.2 mM PMSF) for 10 min on ice. Then, cells were broken by 20 strokes in a Dounce homogenizator and suspensions were centrifuged at 3300 × g for 20 min at 4 °C. Supernatants were centrifuged for another 30 min at 15,000 × g at 4 °C and the supernatants thus obtained were saved as cytosolic fraction. The pellets were dissolved in SDS sample buffer constituting the membrane fraction. Protein content was measured with Coomassie protein assay (Thermo Fisher Scientific, Waltham, MA) or with bicinchoninic acid assay (Sigma–Aldrich) for the SDS extracts. For immune-blotting 30 μg of protein extracts for RAS and FAS or 50 μg of protein extracts for DNMT1 were fractionated on 12%, 10% or 8% SDS-PAGE, respectively. Following SDS-gel electrophoresis, the proteins were transferred to nitrocellulose filters (Millipore) and blocked overnight with 10% blocking reagent (Roche Applied Science, Mannheim, Germany) in TN Buffer (50 mM Tris, 125 mM NaCl, pH 8). Subsequently, the filters were incubated for 1 h at room temperature with an antibody against DNMT1 (K-18, Santa Cruz Biotechnology, Santa Cruz, CA), against FAS and against RAS (610197 and 610002, BD Transduction Laboratories™) all diluted 1:200 in blocking buffer. Afterwards, filters were washed three times with immune blot wash buffer (TN buffer containing 0.01% Tween) and incubated for an additional hour with an anti-goat IgG HRP-labeled secondary antibody (Sigma–Aldrich) diluted 1:160,000 in blocking buffer or with an anti-mouse IgG/anti-rabbit IgG horseradish peroxidase (HRP)-labeled secondary antibody (Roche) diluted 1:10,000 in the blocking buffer, respectively. Finally, the blots were washed again three times with immune-blot washing buffer before detection of light emission with the BM chemiluminescence immune blotting kit (Roche Applied Science) as described by the supplier. Chemiluminescence was measured with an image acquisition system (Vilber-Lourmat, France).
Cell fractionation was controlled by immunoblotting using antibodies against integrin-β5 (ITGB5, H-96, Santa Cruz Biotechnology, Santa Cruz, CA) for the membrane and mitogen-activated protein kinase 4 (MAPK4, Transduction Laboratories, BD, Franklin Lakes, NY) for the cytosolic fraction (Suppl. Fig. 3).
Supplementary data associated with this article can be found, in the online version, at http://dx.doi.org/10.1016/j.bcp.2012.10.016.
To analyze Fas promoter 5-methylcytosine levels, appropriate fragments of the targeted promoter regions were generated by digestion of 1 μg of genomic DNA with 20 U of the CpG methylation insensitive restriction enzymes MboII (Promega) or PstI (Fermentas, St. Leon-Rot, Germany) (for the murine or for the human Fas gene, respectively) for 1 h at 37 °C from cells cultured for 24, 48 and 72 h with 50 μM ibandronate in the medium. Subsequently, the enzyme was heat inactivated at 65 °C for 20 min. The Fas promoter region was selected as shown before . In brief, in the murine cell lines two CpG rich regions were analyzed, the first at 2.6 kb and the second starting at 30 bp upstream from the Fas transcriptional start site (TSS) [17,19]. In the human osteosarcoma cell line, a CpG rich region of the proximal FAS promoter region was analyzed . This fragment spanned from 79 bp upstream from the TSS into 359 bp of the first exon and showed an overall CpG content above 50%. PstI digestion generated a suitable fragment of 942 bp covering the CpG rich region. After digestion, DNA was purified using a commercially available PCR clean-up kit following the supplier's instructions. In the next step methylated DNA fragments were captured using the “MethylMiner Methylated DNA Enrichment Kit” (Invitrogen). In brief, methylated DNA was captured by methyl-CpG binding domain protein 2 (MBD2) coupled to magnetic beads to separate the modified from the non-modified DNA fractions. DNA was eluted from the magnetic beads with 200 μL of 2 M NaCl solution as single fraction independent from the CpG methylation density and concentrated by ethanol precipitation. Finally, the mean methylation status of the fragments was determined by amplifying the fragments by quantitative real-time PCR. Amplification ratios of the bound (methylated) DNA fraction to unbound (unmethylated) DNA fraction were calculated (for primer design see Table 1).
For this purpose, cells were treated with 50 μM ibandronate for 72 h. Subsequently, chromatin cross-linking, cell lysis, chromatin sharing, DNMT1 immune precipitation and DNA clean up were performed with the ChampionChip one-day kit (SABiosciences, Hilden, Germany) following manufacturer's instructions. Thereby, chromatin from untreated as well as from ibandronate treated cells was incubated overnight on a rotor at 4 °C with 4 μg of anti-DNMT1 antibody (K-18, Santa Cruz Biotechnology, Santa Cruz, CA) or with 4 μg of non-immune serum as negative control. Before immune precipitation, 1% (10 μL) of the chromatin was saved and stored at 4 °C for further use as reference. DNMT1 binding on appropriate FAS promoter regions was measured by qRT-PCR (for ChIP-FAS promoter primers see Table 1). For quantitation of the qRT-PCR values, for each sample, DNA signal of the DNMT1-precipitated chromatin was normalized to the unprecipitated chromatin.
Statistical analyses were performed either with ANOVA or with Student's t-test using Prism 4.03 (GraphPad Software, San Diego, CA), P ≤ 0.05 was considered as significant. The data of the experiments are presented as means ± standard deviation (SD).
After 72 h of treatment, ibandronate attenuated cell multiplication in all cell lines tested, although with different half maximal effective concentrations (EC50, Fig. 1A–C). Using a MTT-like assay to assess cell viability/proliferation, in the bone related cells MC3T3-E1 (Fig. 1A) and U-2 OS (Fig. 1B), ibandronate showed a comparable half maximal effect (EC50) with 6.8 μM (95% c.i.: 6.00–7.67 μM) and 7.21 μM (95% c.i.: 5.90–8.79 μM), respectively, while the CCL-51 cells (Fig. 1C) were less sensitive with an EC50 of 14.4 μM (95% c.i.: 14.0–14.9 μM). Using cell counting only approximate similarities were found for the three cell-lines. This may be explained by the strong changes in cell morphology after ibandronate treatment, which makes it difficult to determine, if a cell is still viable (Suppl. Fig. 1A–C).
Supplementary data associated with this article can be found, in the online version, at http://dx.doi.org/10.1016/j.bcp.2012.10.016.
In MC3T3-E1 cells, caspase 8 and particularly caspase 3/7 activities were reduced after 72 h of ibandronate treatment in a concentration dependent manner showing significance at 20 μM for caspase 3/7 and at 100 μM for caspase 8 (Fig. 1D). An opposite effect was seen in the two tumor cell lines analyzed: caspase 8 as well as caspase 3/7 activities were significantly increased after 72 h of ibandronate treatment in human U-2 OS osteosarcoma cells (Fig. 1E) as well as in murine CCL-51 breast tumor cells (Fig. 1F).
In line with the effects observed on caspase activities, ibandronate failed to significantly regulate the mRNA expression of the pro-apoptotic gene Fas in MC3T3-E1 cells at any time (Fig. 2A) and after 72 h at any concentration tested (Fig. 2B). In contrast, already after 24 h of treatment, FAS mRNA expression was strongly induced in U-2 OS cells (Fig. 2C) and after 48 h in CCL-51 cells (Fig. 2E). This stimulation was dose dependent but showed significance only at concentrations of 100 μM in U-2 OS cells (Fig. 2D) or higher than 20 μM in CCL-51 cells (Fig. 2F).
To demonstrate the role of FAS in ibandronate induced apoptosis, U-2 OS cells were transfected with FAS siRNA by electroporation and cell viability/proliferation was measured with the MTT-like assay (Fig. 3A). In ibandronate treated cells, a difference of 19.2% in down regulation of cell viability/proliferation was measured between electroporation of unexposed and electroporation of exposed cells, which suggest that electroporation makes cells more sensitive to ibandronate. This assumption is supported by a similar effect found by transfection of the control siRNA. Transfection of FAS siRNA recovered cell viability/proliferation to a large extent (87%), suggesting that a second, minor process is involved in down-regulation of cell viability/proliferation too. FAS knock down by siRNA was controlled by FAS mRNA expression (Suppl. Fig. 2).
Supplementary data associated with this article can be found, in the online version, at http://dx.doi.org/10.1016/j.bcp.2012.10.016.
Translation of the FAS mRNA expression to the protein level is demonstrated in Fig. 3B. Protein extracts isolated from FAS siRNA transfected cells, which were either left untreated or treated with ibandronate for 72 h, were subjected to immune-blotting and probed with an anti-FAS antibody. Similarly to mRNA regulation, when compared to controls, ibandronate up regulated FAS protein expression. FAS siRNA transfected cells, however, showed no significant difference to controls, neither untreated nor ibandronate treated.
Similar to Fas expression, ibandronate failed to affect Dnmt1 expression in MC3T3-E1 cells at any time (Fig. 4A) and after 72 h at any concentration (Fig. 4B) tested. However, Dnmt1 expression was clearly down regulated in both tumor cell lines. In U-2 OS cells this effect was already visible after 24 h (Fig. 4C), while in CCL-51 cells significance was reached after 72 h of treatment with 50 μM ibandronate (Fig. 4E). At this time, in U-2 OS cells, DNMT1 expression was already strongly down regulated at 20 μM ibandronate in culture medium (Fig. 4D) whereby a comparable effect was reached at 100 μM ibandronate for CCL-51 cells (Fig. 4F). Fig. 6G and H compares the effect of 72 h of treatment with 50 μM ibandronate on DNMT1 protein expression by immune blot analysis in the three cell lines studied.
72 h after seeding, in MC3T3-E1 cells basal Fas promoter methylation was considerably lower as in the two neoplastic cell lines (Table 2). Furthermore, in MC3T3-E1 cells, 72 h of 50 μM ibandronate treatment failed to significantly affect DNMT1 binding on Fas promoter (Fig. 5A). After 72 h, in U-2 OS cells (Fig. 5C) as well as in CCL-51 cells (Fig. 5E) treatment with ibandronate significantly reduced binding of DNMT1 to the FAS promoter.
Reduced binding of DNMT1 to the Fas promoter suggested changes in DNA methylation, which was evaluated by comparing the concentration of methyl-cytosines vs. unmethylated cytosines in the promoter. While as expected, no change in the methylation status of the Fas promoter in MC3T3-E1 cells was found (Fig. 5B), ibandronate significantly reduced the methyl-cytosine concentration of the Fas promoter in U-2 OS already after 24 h (Fig. 5D) and after 48 h in CCL-51 cells (Fig. 5F).
Bisphosphonates inhibit the activities of the enzymes farnesyl- and geranylgeranyl-diphosphate synthase, which cause disruption of small-GTPases prenylation thus altering their sub-cellular distribution. Cells were either left untreated or treated with ibandronate. Thereafter, proteins of the membrane as well as of cytoplasmatic fraction were isolated and subjected to immune blotting. As shown in Fig. 6A, in MC3T3-E1 cells RAS was primarily localized in the cytoplasm and, therefore, ibandronate did not affect RAS localization in this cell-line. In U-2 OS cells (Fig. 6B) as well as in CCL-51 cells (Fig. 6C) RAS was primarily localized in cell membranes. After exposure to 50 μM ibandronate for 72 h, in both cell lines a clear shift in RAS localization from the cell membranes to cytoplasm was seen (Fig. 6B and C).
Cell fractionation was controlled by immune blotting of integrin-β5 for the membrane and mitogen-activated protein kinase 4 for the cytosolic fraction (Suppl. Fig. 3).
Inhibition of prenylation of small-GTPases by bisphosphonates can be rescued by parallel treatment with the substrate FPP for RAS or GGPP for the other modified small-GTPases.
As already shown in Fig. 1 and Supplemental Fig. 1, treatment of MC3T3-E1 cells with 50 μM ibandronate reduced the cell number by about 90%. After the same culture time 10 μM GGPP by itself attenuated cell multiplication by about 50% and could only partially rescue the effect of ibandronate on these cells (Fig. 7A). In U-2 OS cells 50 μM ibandronate significantly reduced cell multiplication. Although GGPP itself reduced cell multiplication by about 25%, it could rescue the effect caused by ibandronate (Fig. 7B). Similarly, in CCL-51 cells GGPP could rescue ibandronate attenuated cell multiplication but, differentially, did only marginally influence cell multiplication (Fig. 7C). In MC3T3-E1 cells neither ibandronate nor GGPP influenced Fas expression (Fig. 7D). Again, in both other studied cell lines ibandronate induced FAS expression. GGPP alone had no significant effect on FAS expression, but down regulated ibandronate induced FAS expression in both U-2 OS (Fig. 7E) as well as in CCL-51 cell lines (Fig. 7F). Regarding DNMT1 expression, again all three treatments (ibandronate, GGPP or combination of both) showed no effect in MC3T3-E1 cells (Fig. 7G). However in both tumor cell lines, ibandronate, as expected, down regulated expression of DNMT1. GGPP counteracted this effect and had no effect when administered singularly (Fig. 7H and I). This supports our hypothesis that small-GTPases induce DNMT1 expression is inhibited by bisphosphonates leading to promoter demethylation and FAS expression.
Next we tested the effects of FPP (40 μM) on cell multiplication (Fig. 8). In the immortalized MC3T3-E1 cell line (Fig. 8A), FPP reduced cell number to 63%, in U-2 OS cells to 71% (Fig. 8B) while it did not affect this parameter in CCL-51 cells (Fig. 8C). However, in contrast to GGPP, FPP could not rescue the down-regulation of cell multiplication by ibandronate (Fig. 8A–C). The effects of FPP on FAS expression were comparable to that of GGPP: no significant effects in MC3T3-E1 cells (Fig. 8D), while in both neoplastic cell lines (Fig. 8E and F) 40 μM FPP rescued the ibandronate mediated up-regulation of FAS. Comparable effects were also found on DNMT1 expression with no effects in MC3T3-E1 cells (Fig. 8G), while in U-2 OS FPP rescued the down-regulation of DNMT1 expression by ibandronate (Fig. 8H). Differentially, FPP did not change the attenuation of Dnmt1 expression in CCL-51 cells (Fig. 8I). FPP alone did not affect DNMT1 expression in any one of these cell lines.
A growing body of evidence attributes an anti-tumorigenic capacity to bisphosphonates. Several studies have shown that in patients affected by diverse malignances, bisphosphonate therapies show a positive outcome with regard to tumor growth and metastatic activity [40–46]. However, the mechanisms underlying those effects remain poorly understood.
By activation, the Ras superfamily of small GTPases attaches to cellular membranes and, among many other cell regulatory functions, promotes cell proliferation, differentiation and survival [12,16,47]. Aminobisphosphonates exert their pharmacologic activity by inhibiting the mevalonate pathway. By this way, these drugs prevent prenylation of small-GTPases as well as their attachment to the cellular membranes and thereby their function [5,7,48]. While the apoptotic impact of simple bisphosphonates (clodronate and etidronate) can be considered as secured, the mode of action of aminobisphosphonates on cells is not as clear [9,11,49,50]. Initially, J774 macrophages have been considered as a model of aminobisphosphonates’ action because this cell line matched the order of potency of the diverse bisphosphonates for inhibiting bone resorption and inducing apoptosis [7,51–53]. However using primary rabbit or human derived osteoclasts, it has been demonstrated that inhibition of bone resorption by bisphosphonates does not require osteoclast apoptosis [54–56]. Taking into account that J744 are lymphoma-derived tumorigenic cells  one can conclude that bisphosphonates act in tumor cells in a different way as compared to normal osteoclasts.
This is in accordance with the findings in this study, where in non neoplastic immortalized mouse preosteoblastic MC3T3-E1 cells, ibandronate attenuated cell multiplication by down-regulation of the cell cycle as suggested by decreased expression of cyclins Ccn2a and Ccn2d (not shown). Moreover, down-regulation of caspase 3/7 and caspase 8 in MC3T3-E1 cells assigned to aminobisphosphonates an anti-apoptotic activity as found in MLO-Y4 osteocytes  while in tumorigenic RAW 264.7 macrophages most bisphosphonates induced apoptosis . In primary human osteoblasts at concentrations higher than 10−7 M zoledronate dose dependently reduced cell proliferation, although, at the highest concentration apoptosis was found as well . Treatment of fetal immortalized osteoblasts with pamidronate and zoledronate resulted in a dose dependent down-regulation of cell proliferation with increased differentiation . However, increased cell proliferation of human primary trabecular bone cells  and of human bone marrow stromal cells by alendronate and risedronate has been reported as well . Summarizing these findings, in normal mesenchymal bone cells, bisphosphonates decrease proliferation but apoptosis was found only at very high concentrations, while in tumorigenic cells amino-bisphosphonates induce apoptosis.
Here we show that treatment of tumor cell lines with ibandronate down regulated genes of the DNA CpG-methylation apparatus (Dnmt1, Dnmt3b, Hells), which resulted in reduced binding of DNMT1 at the promoter of FAS in both tumor cell lines. Absence of the DNA-methyltransferases at the promoter results in reduced CpG-methylation of the promoter during further cell divisions, which is followed by increased expression of the gene [63–65]. Increased expression of FAS is followed by increased activity of caspase 3/7 and caspase 8, which is a classical sign of apoptosis. Interestingly, no change of FAS methylation status and of Fas expression was found in non-neoplastic MC3T3-E1 cells. The very low basal methylation level of Fas promoter in these cells can explain this fact. We have recently demonstrated that culturing these cells on culture dishes that are not covered by collagen results in down-regulation of DNMT1 and HELLS followed by demethylation of the Fas promoter and increased expression of the gene .
Small-GTPases play a central role in bisphosphonates’ activity. These drugs inhibit the activity of the enzymes, which are responsible for synthesis of FPP and GGPP, which are transferred to the amino acids motif CAAX anchoring of the small-GTPases to the cell membrane, which is a prerequisite for their action. Effects of bisphosphonates on small-GTPases mediated signal transduction can be rescued by co-treatment with GGPP or FPP, where in general FPP rescues RAS-activity and GGPP the activity of the RHO- and RAB-family [66,67]. Again, transformed cell lines behaved differentially; in CCL-51 and U-2 OS, GGPP rescued ibandronate attenuated cell multiplication, up regulated DNMT1 and, consequently, down regulated FAS expression. GGPP, however, could not rescue the immortalized non-neoplastic cell line MC3T3-E1 from the effects of ibandronate. We found no down-regulation of Dnmt1 and no up-regulation of Fas. Moreover, GGPP alone significantly decreased cell multiplication as well. GGPP is the posttranslational modifier of the RHO- and RAB-small-GTPases. Recently, it has been demonstrated that inhibition of prenylation by bisphosphonates rather activates than inactivates the RHO family of small-GTPases including RAC, CDC42 and RHO . Interestingly, osteoblast-restricted Rac1 deletion leads to defective bone acquisition in vivo and knockdown impairs growth and induces apoptosis in the osteoblast cell line OP9 . These data suggest that GGPP increases interaction of RAC1 with cellular membranes, which results in reduced activated RAC1 leading to decreased proliferation and increased apoptosis.
A down-regulation of cell multiplication was also found in mesenchymal MC3T3-E1 and U-2 OS cells by FPP but not in the neoplastic cell line resulting from an epithelial tumor. Down-regulation of cell multiplication by FPP suggests the involvement of RAS. After translation, FAS is farnesylated and transported to the endoplasmatic reticulum where it is prepared for palmitoylation and forwarded to the Golgi-membranes. This initiates a cycle of traffic to and from the plasma membranes, where it is activated [13,16]. Higher cellular concentrations of FPP could influence the equilibrium of this cycle and therefore alter differentiation, proliferation and apoptosis rate.
Unlike GGPP, FPP could not rescue down-regulation of cell multiplication by ibandronate in U-2 OS and CCL-51. This suggests that RHO- and RAB-small-GTPases are responsible for ibandronate's effect on this parameter. This is surprising because in U-2 OS, FPP canceled the effect on DNMT1 expression and inhibited up-regulation of FAS. An explanation is down-regulation of the cell cycle by ibandronate via down-regulation of cyclins and a possible up-regulation of cell cycle inhibitors [68–71]. From the rescue-experiments one can conclude that ibandronate inhibits cell multiplication by decreasing cell cycling and by increasing apoptosis. Apart from apoptosis a second process was also suggested by transfection of FAS siRNA, which could not completely recover ibandronate's down-regulation of cell viability/proliferation. However, this experiment strengthens our hypothesis that up-regulation of FAS is responsible for induction of apoptosis via caspases and confirms recent data obtained from HMC1 mast cell leukemia cells that were treated with demethylating drugs .
Although FPP and GGPP differentially influenced cell multiplication, unexpectedly, except for Dnmt1 expression in CCL-51, no differences were found in rescuing FAS and DNMT1 expression; both isoprenoids could recover the effects of ibandronate, which is in line with recent findings that both isoprenoids are able to recover bisphosphonates-induced apoptosis. There are several possible explanations for this finding . Bisphosphonates are, with some exceptions [72,73], inhibitors of FPP-synthase but not of the GGPP-synthase. Therefore, when cells were treated with FPP some of the compounds will be converted to GGPP, which will modify and rescue RHO-family small-GTPases as well, at least partially . Recently, it has been demonstrated that in presence of inhibition of farnesyltransferase, geranylgeranylation occurs instead of farnesylation of KRAS4A,B and NRAS but not for HRAS. Moreover, geranylgeranyltransferase can use FPP as substrate as well to modify proteins of the RHO-family [74–80]. As bisphosphonates deplete both FPP and GGPP, raising the concentration of one of the isoprenoids by addition, modification with the “wrong” modifier may occur. These facts may support a critical view on the implication of the rescue experiments, so that no unambiguous assignment of a small-GTPase can be made. Even though the presented results clearly demonstrate the involvement of small-GTPases in the epigenetic DNA methylation process and FAS mediated apoptosis, a detailed analysis of the large family of small-GTPases will be necessary to unravel the mechanism.
Taken together, our experiments support the common knowledge that more members of the group of small-GTPases are involved in the regulation of cell multiplication and apoptosis and suggest a different mode of action of bisphosphonates in non-transformed vs. neoplastic cell lines, as supported by previous findings [10,81].
As already mentioned above, most tumors or transformed neoplastic cells are characterized by an activated RAS/MAPK pathway [13–15], which results in methylation of cytosines in the promoter of tumor suppressor genes and of the pro-apoptotic FAS gene [12,24,30,32,33,82,83]. Both tumor cell lines, however, have a highly methylated FAS promoter, and therefore, an inhibited FAS expression. This suggests that RAS must be activated and attached to the cell membrane to enable bisphosphonates to display their epigenetic activity. Ibandronate, as demonstrated by immune-blotting, prevented RAS from attachment to membranes and translocated the protein into the cytoplasm; no change was found in MC3T3-E1 cells indicating that RAS is not attached to membranes, and therefore not or only marginally active, as generally found in normal, growth factor-unstimulated cells [47,84]. Our results could explain why tumor cells react differentially in response to bisphosphonates when compared with normal cells. It should be emphasized again that activation RAS/MAPK pathway seems to be a prerequisite for bisphosphonates’ action in tumor cells. Featuring the RAS/MAPK pathway is well founded by the fact that epigenetic silencing of the Fas promoter is a consequence from the signaling cascade of this pathway [17,39]. However, results of this study suggest that in addition to RAS, other members of small-GTPases must be involved in regulation of FAS promoter methylation as well. Differences in responses to ibandronate of the epithelial CCL-51 cells compared to the mesenchymal cells suggest involvement of RAC1, a gene that has been found important for osteoblastic proliferation, differentiation and apoptosis . The use of specific inhibitors of small-GTPases will help to clarify the mechanism of the selective epigenetic activation of FAS and other epigenetic silenced tumor suppressor genes [8,15]. It should be emphasized that other inhibitors of small-GTPases may demonstrate epigenetic mechanisms as well.
A recent publication has demonstrated that bisphosphonate pulse treatment differentially affects mesenchymal stem cells . Passive demethylation of a gene promoter needs at least one or two cell cycles. Short treatment of cells will activate promoter demethylation, which then will be inherited to the daughter cells, where apoptotic factors could further activate the demethylated FAS gene.
Methylation of tumor suppressor genes is a common mechanism in tumor development. Loss of hormone responsiveness in breast and prostate cancer as well as in leukemias may contribute to increased mortality that often happens by CpG-methylation of promoter DNA [25,26,28,29,85,86] and drugs decreasing CpG-methylation are promising for future treatment of such tumors. Our findings could possibly explain some contradictory results in clinical trials using bisphosphonates combined with an adjuvant endocrine therapy [40,87]; only a subgroup of patients with an epigenetic inactivated estrogen receptor ESR1 seems to respond to this therapy via RAS/MAPK pathway.
In summary, we demonstrated that ibandronate is an epigenetically active drug. In tumor cells it inhibits activated RAS and down-regulates DNMT1 expression. This leads to demethylation of CpGs in the FAS promoter resulting in activation of FAS transcription. Subsequently apoptosis is induced in the affected neoplastic cells. In contrast, ibandronate does not exert these effects in non-neoplastic (immortalized) cell lines.
Epigenetic mechanisms play an important role in multiple physiological and pathological processes . Besides their use as antiresorptive treatment for osteoporosis, bisphosphonates as epigenetically active drugs with the potential to re-activate pro-apoptotic genes, could gain a consolidated role in antitumor treatment.
The authors state that they have no conflicts of interest.
This study was supported by the Fonds zur Foerderung der Wissenschaftlichen Forschung (FWF; The Austrian Science Fund) Project P24370-B19, the Medical Scientific Fund of the Mayor of the City of Vienna (Project 2565), the WGKK (Social Health Insurance Vienna), and the AUVA (Austrian Social Insurance for Occupational Risks).