3-D DNA methylation phenotypes correlate with cytotoxicity levels in prostate and liver cancer cell models
BMC Pharmacology and Toxicology volume 14, Article number: 11 (2013)
The spatial organization of the genome is being evaluated as a novel indicator of toxicity in conjunction with drug-induced global DNA hypomethylation and concurrent chromatin reorganization. 3D quantitative DNA methylation imaging (3D-qDMI) was applied as a cell-by-cell high-throughput approach to investigate this matter by assessing genome topology through represented immunofluorescent nuclear distribution patterns of 5-methylcytosine (MeC) and global DNA (4,6-diamidino-2-phenylindole = DAPI) in labeled nuclei.
Differential progression of global DNA hypomethylation was studied by comparatively dosing zebularine (ZEB) and 5-azacytidine (AZA). Treated and untreated (control) human prostate and liver cancer cells were subjected to confocal scanning microscopy and dedicated 3D image analysis for the following features: differential nuclear MeC/DAPI load and codistribution patterns, cell similarity based on these patterns, and corresponding differences in the topology of low-intensity MeC (LIM) and low in intensity DAPI (LID) sites.
Both agents generated a high fraction of similar MeC phenotypes across applied concentrations. ZEB exerted similar effects at 10–100-fold higher drug concentrations than its AZA analogue: concentration-dependent progression of global cytosine demethylation, validated by measuring differential MeC levels in repeat sequences using MethyLight, and the concurrent increase in nuclear LIM densities correlated with cellular growth reduction and cytotoxicity.
3D-qDMI demonstrated the capability of quantitating dose-dependent drug-induced spatial progression of DNA demethylation in cell nuclei, independent from interphase cell-cycle stages and in conjunction with cytotoxicity. The results support the notion of DNA methylation topology being considered as a potential indicator of causal impacts on chromatin distribution with a conceivable application in epigenetic drug toxicology.
DNA methylation is a crucial epigenetic modification of the human genome beyond the DNA sequence level that is involved in regulating many cellular processes. Cancer cells frequently exhibit abnormally high levels of DNA methylation in gene-specific CpG-rich promoter regions[2–5]. Furthermore, DNA methylation also occurs at non-CpG islands within the major part of the genome known as heterochromatin[6, 7], which plays a key role in nuclear architecture and genome stability[8–10]. It is now clear that DNA hypomethylation in human cancer is also very frequent and affects more cytosine residues than does DNA hypermethylation, accounting for a net loss of 5-methylcytosine (global DNA hypomethylation), as observed in many cancers[11–14]. The reversible nature of epigenetic imbalances in various types of cancers constitutes an attractive therapeutic target. The goal of epigenetic therapy in cancer is the reprogramming of aberrant cells towards normal phenotypes. In this regard, the drug discovery field has so far been mostly focusing on screening the effect of candidate agents on the levels of molecular cell signaling and metabolism. However, in recent years of the post-genomic era, chromatin conformation and the higher–order genome organization, which set the framework for the global orchestration as well the locus-specific regulation of gene expression in the human cell nucleus[15–18], are gaining more attention in therapy; the reason being that these functional structures can become affected as a consequence of epigenetic interference by chromatin-modifying agents such as inhibitors of DNA methylation.
Catalytic DNA methyltransferase (DNMT) inhibitors have been so far categorized into two classes: nucleoside analogues and non-nucleoside analogues. The two nucleoside analogues, 5-azacytidine (AZA, Vidaza™) and 5-aza-2′-deoxycytidine (decitabine, Dacogen™) are the most advanced in their category, having received US Federal Drug Agency (FDA) approval for their use in treating myelodysplastic syndrome (MDS) and hematopoietic malignancies[21, 22]. Zebularine (ZEB) or 1-β-D-ribofuranosyl-2(1H)-pyrimidone has recently emerged as a new DNMT inhibitor (DNMTi), with properties that makes it a potential drug candidate for oral administration: (i) stability at pH ranges between 1.0 and 7.0 in aqueous solutions, (ii) far less toxicity than AZA and decitabine to cultured cells, and (iii) no detectable toxicity in a T-cell lymphoma mouse model[23–27].
The specific mechanism of DNA methylation alterations induced by azacytidine nucleoside analogues is complex and not fully understood. Azacytidine is thought to form a stable covalent bond with DNMTs after its incorporation into genomic DNA, thereby trapping the enzyme and sequestering it from transferring methyl groups to other regions of the genome[28–30]. Such a passive mechanism of DNA demethylation as a result of exposure to DNMTi has been proposed and is thought to progress with several cell divisions, after which DNMT levels increase and specific gene regions show re-methylation. Azacytidine treatment of cells also was shown to induce degradation of DNMT1 via the ubiquitin-activating proteosomal pathway, as well as p53-mediated cell cycle arrest and DNA repair. Chromatin packaging and organization are altered in cells treated with azacytidine. Nucleosome depletion of symmetrically demethylated gene loci have been demonstrated after drug treatment. However, it should be noted that there are additional reports indicating that genomic regions with AZA DNA-DNMT adducts are improperly packaged and transcriptional activation can only occur with DNA repair and recruitment of other protein factors[34, 35].
To date, differential DNA methylation analysis has been quantitatively performed mostly by means of molecular approaches including electrophoretic, chromatographic, PCR-based, array-based, and sequencing technologies[36, 37]. Furthermore, evidences indicate that DNMTi also influence repressive histone marks leading to changes in nucleosome positioning[33, 34]. Hence, a novel nucleosome footprinting assay was developed, which takes advantage of improvements in these technologies and focuses on the characterization of locus-specific as well as genome-wide chromatin conformation with respect to DNA methylation on a single molecule level[38, 39]. Such an analytical tool can be used to characterize the differential chromatin states and changes thereof that can occur under drug influence and would benefit therapeutic design: as demethylating drugs may, in addition to their physiologic role, also affect chromatin architecture and related gene expression programs in cells[40–47]. The structure and function of the human genome are so intricately intertwined that understanding its regulation requires viewing the genome as a dynamic three-dimensional entity that emerges from iterations of dynamic folding of the primary chromatin structure, the so-called nucleosomal array: also considering the mass of heterochromatin that is largely repressed and condensed through DNA methylation and histone-tail modifications, which are perturbed in complex diseases[17, 18]. The immunodeficiency, centromere instability and facial anomalies (ICF) syndrome is a classic example, in which normally highly compacted juxtacentromeric satellite DNA is found hypomethylated and decondensed in chromosomes 1 and 16. Therefore, the higher genome organization of DNA provides an additional layer of cell-specific information that could render itself valuable in the evaluation of drug action, as it has potential to be translated into high-throughput and cost-efficient pre-clinical genotoxicity assays. In this sense, little is known about the spatial progression of DNA hypomethylation in cell nuclei in response to DNMTi. The analysis of global nuclear DNA methylation patterns could provide a useful means in assessing said epigenetic effect of this class and possibly other classes of drugs in a large number of single cells, as the underlying molecular processes may involve large-scale chromatin reorganization visible by light microscopy[40–44, 49–51]. Recently introduced, 3D-qDMI, can measure DNA methylation changes in situ, through the differential analysis of relevant nuclear structures that are represented by methylated CpG-dinucleotides (MeC) and global DNA[40–42] (Figure1). Our analyses revealed significant differences in image patterns of MeC and heterochromatin-derived signals between untreated AtT20 mouse pituitary tumor cells and a subpopulation of these cells treated with AZA, which has been reported to change DNA methylation patterns on a genomic scale. Furthermore, the recently upgraded methodology was able to monitor the dual effect of demethylating agents in human cancer cells: (a) a global decrease in MeC content, and (b) the subsequent reorganization of highly compact heterochromatic regions of the genome as reflected by a significant decrease of DAPI intensity in the relevant nuclear areas. The effects resulted in LIM and LID sites, whose distributions can be mapped within cell nuclei. This approach supports profiling at single-cell level, and provides a rapid display of cell-specific DNA methylation (MeC) phenotypes that is related to drug response in targeted cells. Initial results obtained with 3D-qDMI indicated towards the relatively gentle effect of zebularine on the genome, an observation that is concordant with reported studies based on molecular profiling. Initial proof-of-principle analyses focusing more on technology development were restricted to the application of one concentration per epigenetic drug. Here we report on the first-time probing of the 3D-qDMI system’s utility in a dose-dependent manner: by administration of a larger concentration range of the relatively more gentle nucleoside zebularine in comparison to its extensively characterized more aggressive analogue 5-azacytidine[23–27, 53, 54]. The notion was to follow a more gradual DNA demethylation effect of the agents on 5-methylcytosine topology, along with cytotoxicity evaluations, in the two in vitro models, DU145 prostate cancer cells and Huh-7 hepatocarcinoma cells, which have known sensitivity to both drugs[55–59].
Cell culture and drug treatment
DU145 human prostate cancer cells were obtained from American Tissue Culture Collection (catalog number HTB-81, ATCC). The vendor certifies authentication of cells using a variety of techniques such as short tandem repeat (STR) analysis and cytogenetic analyses (G-banding, fluorescence in situ hybridization). Huh-7 cells were a gift from Dr. Vaithilingaraja Arumugaswami (Cedars-Sinai Medical Center, Los Angeles, CA). The cells were propagated for less than six months after receipt and resuscitation. Cells were grown in Dulbecco’s modified Eagle’s medium (DMEM, Cellgro) supplemented with 10% newborn calf serum, and 1% antibiotic/antimycotic (1000 units/ml penicillin G sodium, 10 mg/ml streptomycin sulfate) (Gemini Bio-Products), in 5% CO2, 37°C. Cells were plated at 1 × 105 cells onto coverslips in multi-well plates in replicates, and allowed to attach for 24 hours. For dose dependency assay, wells were divided into two groups: (i) control populations that were not treated for 72 hours, and (ii) populations of cells treated with two different drugs at different concentrations for 72 hours: 0.5 μM, 1 μM, 2.5 μM, 5 μM, 10 μM and 20 μM of 5-azacytidine (Sigma-Aldrich), and 8 μM, 40 μM, 200 μM, 500 μM and 1000 μM of zebularine (Sigma-Aldrich), all in DMEM. For all cells, drug concentrations were freshly prepared prior to administration, and the drug-medium mixture was changed every 24 hours. Subsequently, cells were partially fixed for immunofluorescence and partially harvested for cytotoxicity testing by flow cytometry.
DU145 prostate cancer cells were arrested in G0/G1 and G2-phases following previously established protocols[60, 61]. Briefly, cells were seeded onto glass coverslips at a concentration of 105 cells/ml for immunofluorescence staining and subsequent imaging via confocal microscopy. A parallel set of cultures (at the same concentration) was maintained in culture flasks, for flow cytometry. All cells were first allowed to attach and grow for 24 hours in regular proliferative medium (DMEM/10% FBS/1% penicillin/1% streptomycin), which was then replaced by serum-deprived DMEM for 72 hours, followed by a recovery period of 4 hours, in which cells were maintained again in regular proliferative medium. G0/G1 populations were partially fixed at this point for use in either immunocytochemistry or FACS. The remainder cultures were processed for a double-thymidine block to enrich cells in G2-phase: (i) first blocking with deoxythymidine (Sigma) at 2 mM for 18 hours, (ii) recovery in regular proliferative medium for 12 hours to escape S-phase, (iii) second blocking with 2 mM deoxythymidine for another 18 hours, and (iv) second recovery in regular proliferative medium for 8 hours, to release cells into G2. At this point G2-cells were fixed for further experimentation. Enrichment efficiency was checked by propidium iodide (PI) staining of cells and nuclear DNA content analysis, following standard protocols as previously described in Wong et al.: cells were fixed in 70% ethanol/PBS and maintained for at least 4 hours at 4°C; then incubated in 5 μg/ml PI (Sigma) for 30 minutes at 37°C immediately prior to flow cytometry with a FACScan (Becton Dickinson). FACS data were analyzed using the ModFit LT program (Verity Software House, Topsham, ME, USA).
Induction of apoptosis and cell viability was analyzed in cells that were treated as replicates in parallel to cells that were subsequently analyzed by immunofluorescence. For that purpose, 2×105 cells/ml were stained with Annexin V (7-AAD) and PI, respectively. In essence, trypsinated cells from parallel wells were processed with the Annexin V-FITC Apoptosis Detection Kit I (BD Biosciences). Cells (1×105) were incubated for 15 minutes at room temperature with 7-AAD and PI in a total volume of 510 μl comprised of 5 μl of each of the fluorescent dyes, each and 500 μl of 1X binding buffer. Controls with unstained cells and cells stained with either dye alone were used for FACS setup. Samples were analyzed at emission wavelengths of 530 nm (for Annexin V-FITC) and 650 nm (for PI) using FACScan. The fluorescence of 104 cells was acquired and analyzed with CellQuest software (Becton Dickinson).
Immunofluorescence and image acquisition
In order to preserve the three-dimensional structure, cells cultured on glass coverslips in 12-well microplates (Costar, Corning) were fixed with 4% paraformaldehyde/phosphate buffered saline (PBS) (Sigma-Aldrich) and processed for immunofluorescence as previously described. The following antibody sets were used: a monoclonal mouse anti-5-MeC antibody (Clone 33D3, Aviva Systems Biology, San Diego, CA) together with an Alexa488-conjugated polyclonal donkey anti-mouse IgG (H + L) (Invitrogen), and a polyclonal rabbit anti-H3K9me3 antibody (Active Motif) together with an Alexa647-conjugated chicken anti-rabbit IgG (H + L) (Invitrogen). All specimens were counterstained with DAPI. Specimens were imaged by a confocal laser-scanning microscope (TCS SP5 X Supercontinuum, Leica Microsystems Inc.) that allows for any excitation line within the continuous range of 470 to 670 nm, in 1 nm increments. The system was additionally equipped with a 405 nm diode laser line for excitation of DAPI fluorescence. Serial optical sections were collected at increments of 200–300 nm with a Plan-Apo 63X 1.3 glycerol immersion lens (pinhole size was 1.0 Airy unit). To avoid bleed-through, the imaging of each channel was performed sequentially. The typical image size was 2048 × 2048, with a respective voxel size of 116 nm × 116 nm × 230.5 nm (x, y, and z axes), and resolution was 12 bits per pixel in all channels. Fluorescence intensity of MeC-signals and DAPI-signals from optical two-dimensional sections were recorded into separate 3D channels. Raw images were obtained as Leica Image Format (lif) and offline-converted to a series of TIFFs for downstream image analysis.
3D image analysis
Image analysis was performed in three main steps, as comprehensively described in[43, 44]: 1) image segmentation resulting in the delineation of a 3D shell for each individual nucleus; 2) extraction of MeC and DAPI signal intensity distributions within each 3D shell; 3) assessment of cell population heterogeneity through 2D histograms of MeC versus DAPI distribution patterns, utilizing K-L divergence, and 4) the mapping of LIMs and LIDs within individual nuclei. A newly added analytical component for this study was the calculation of mean intensity of MeC signals. Images in each two-channel 3D stack were acquired under nearly identical conditions and modality settings, and so the drift of the settings during acquisition is considered minimal and can be neglected. For codistribution analysis, the MeC and DAPI signals were mapped as respective 2D scatter plots, and following the Kullback–Leibler (KL) divergences were calculated between individual 2D plots (nuclei) and the reference 2D plot (cumulative plot from all nuclei in one drug/concentration experiment). Based on the KL value, cells were categorized as: similar KL G ∈ [0, 0.5), likely similar KL G ∈ [0.5, 2), unlikely similar KL G ∈ [2, 4.5), and dissimilar KL G ∈ [4.5, ∞) in order to evaluate a ratio of similar and dissimilar cells. For localization of resulting LIM and LID sites, the nuclei were analyzed by an algorithm introduced in. Briefly, segmented nuclei were eroded at a constant voxel rate of 1.32 μm × 1.3 μm × 0.25 μm, and MeC and DAPI signals were recorded as integrated intensity values within each nuclear shell. Then, local densities of LIM and LID sites as well as LIM and LID profiles were determined for each nuclear shell as the subset of voxels within a defined intensity range between two thresholds measured separately for each channel (MeC and DAPI): tbcg is the threshold value for the background, and tQ, which separates high-amplitude from low-amplitude intensities, as explicitly described in. All analytical findings related to image processing including numerical results, MeC/DAPI codistribution patterns, individual and combined MeC/DAPI images, LIM/LID outputs of cells were exported by means of a graphical user interface to text or graphics files respectively for further statistical analyzes. A built-in pseudo-coloring of KL divergence, and LIM and LID site shading was superimposed onto original images to facilitate visual reading and evaluation of experimental data.
Antibody specificity and sensitivity test
The specificity and sensitivity of the applied anti-5-methylcytosine antibody used in this study was assessed with a test-microarray as shown in Figure2. Antibody testing was performed by an immunofluorescence assay utilizing a custom made spotted microarray (Full Moon Biosystems) comprising multiple copies of two synthesized 24-mer oligonucleotide probes that were immobilized onto glass microscopic slides: 5′-TCGTTTTTTTTTTTTTTTTTTCGT-3′ (C-oligo) (MWG Biotech), and its counterpart 5′-TmeCGTTTTTTTTTTTTTTTTTTmeCGT-3′ (MeC-oligo) (Biopolymers-Thermo Scientific), in which the two cytosine molecules were replaced by methylcytosine. Immunofluorescence was performed with the primary anti-methylcytosine antibody and the Alexa488 conjugated secondary antibody, and alternatively a Cy3-conjugated goat anti-mouse IgG1, using a denaturing step with hydrochloric acid, a blocking step with 3% BSA in PBS, and stringency washes as described for the in situ immunofluorescence assay above. Fluorescence detection was performed comparatively at 5 microns resolution with a microarray scanner (G2565BA, Agilent Technologies) equipped with a helium-neon laser (633 nm) to excite Cy3, and the above-mentioned confocal microscope with a Plan-Apo 10X 0.7 lens.
MethyLight assay for repetitive elements
MethyLight assays for measuring DNA methylation content of Alu, Satα and Sat2 repeat sequences were performed as previously described by Weisenberger et al.. Briefly, genomic DNA was extracted from harvested Huh-7 cells and 1 μg of genomic DNA was converted with bisulfite and recovered using the Zymo EZ DNA methylation kit (Zymo Research, Irvine, CA), as recommended by the manufacturer. Aliquots of the bisulfite-converted DNAs were used in separate MethyLight assays as previously described. MethyLight data specific for the three types of repetitive elements were expressed as percent of methylated reference (PMR).
Zebularine exerts a comparably lower degree of cytotoxicity than 5-azacytidine
We evaluated cultured DU145 prostate cancer cells and Huh-7 hepatocellular carcinoma cell lines for imaging-based DNA methylation analysis using the 3D-qDMI system to determine DNA methylation phenotypes of cells after 5-zacytidine and zebularine administration. These drugs have been used with a variety of cancer cell lines, including DU145 and Huh-7 cells, and described as being compatible to a large extent with cell viability and cell division[25, 40, 53–59]. The azanucleoside drug concentrations applied here were in the range as previously reported by investigations utilizing molecular nucleic acids-based assays.
For cytotoxicity analysis, we tested cells that were cultured in parallel to those used for imaging-based DNA methylation analysis. Cytotoxicity analysis was divided into an initial cell counting with an aliquot of trypsinized cells, followed by staining of the remainder of the cells with Annexin V and propidium iodide, and subsequent flow cytometry. Zebularine was administered at molar concentrations (8–1000 μM) that were one to two orders of magnitude higher than AZA (0.5–20 μM) with comparable cytotoxic effects (Figure3A,3B). Therefore, ZEB can be categorized as an agent with a much lower cytotoxic potential. This has also been described in previous reports[23, 27]. In more detail, flow cytometry revealed a higher sensitivity of DU145 for ZEB compared to Huh-7 cells: IC10 and IC50 of ZEB were 8 μM and 500 μM, respectively for DU145 versus 200 μM and 1000 μM for Huh-7. In the case of AZA we experienced fewer discrepancies: IC10 was 0.5 μM for both cell types and IC50 was measured at 10 μM for DU145 and 5 μM for Huh-7. A greater than two-fold increase of the apoptotic fraction (Annexin V-positive) for AZA-treated cells of both types was detected at 2.5 μM, and for ZEB-treated DU145 cells at 200 μM, whereas same effects were registered in Huh-7 cells at 1000 μM (Figures3C and3D). For the comparative analysis of the two drugs at different concentrations, 2.5 × 105 cells were initially seeded onto coverslips. After 72 hours we recorded a tripling of naïve cells and only a doubling for both cell types at the drugs’ IC10 levels. Analogously, at IC50 ZEB-treated cells did not show any population growth, whereas AZA-treated cells showed significant reduction of their populations: Huh-7 cells were reduced to 50% and DU145 cells even to 10% of their original confluency. The results underline the ability of ZEB to reduce proliferation at higher doses without acting discernibly cytotoxic as demonstrated by AZA.
High variation in DNA demethylation and differential drug sensitivity revealed by cell-by-cell imaging
Untreated cells as well as cells treated separately with AZA and ZEB were automatically imaged from different areas of each coverslip. Imaged sub-populations were batch-processed off-line using 3D-qDMI software. We evaluated drug action by measuring two parameters on a per-cell basis: (i) the 5-methylcytosine load of nuclei, which we refer to as the mean intensity of the MeC signal (I MeC), and (ii) the nuclear topology of the MeC versus DAPI signals. The number of cells that we could extract the MeC-specific signals from depended on the cytotoxicity level of the drugs: resulting in a certain density of intact cells for each drug type, and subsequently the number of analyzable nuclei per image frame. We determined I MeC across all resulting nuclei for each drug type. Figure4 illustrates relevant statistics in naïve cells and each of the treated populations. The mean intensity was evaluated by a two-sample Kolmogorov-Smirnov test run for the experiments with each combination of drug and cell line. In DU145 (ZEB) cells, a significant difference was observed between all distributions of I MeC, except for the 200 μM dose that was not significantly different from 40 μM and 500 μM. In DU145, cells treated with AZA the distributions of I MeC for untreated and 0.5 μM were not significantly different. Also, no significant difference was observed between 10 μM and 20 μM in Huh-7 (AZA) cells, as well as between untreated and 8 μM dose, and the three highest concentrations in Huh-7 (ZEB) cells. The significance level in each test (β) was determined by Bonferroni correction (β = α/n) for α = 0.05, n = 6 or 7 for ZEB and AZA treatments, respectively.
The experimental results confirm the hypomethylating effect of both drugs; the increase of drug concentration causes a progressive loss of globally measured MeC-specific signal in nuclei (I MeC) and a decrease of I MeC spread (Figure4). Interestingly, AZA, at the highest concentration applied (20 μM), reduced the I MeC stronger in Huh-7 cells (88%) than in DU145 cells (75%), whereas ZEB at the highest concentration (1000 μM) reduced I MeC in DU145 cells at 72% versus 50% in Huh-7 cells, on average. However, when comparing global DNA methylation of cell nuclei at the equitoxic levels, ZEB showed a much stronger DNA hypomethylation effect than its nucleoside analogue at IC10 — 15% versus 5% for DU145 and 43% versus 18% for Huh-7 — then a milder effect at IC50: 54% versus 69% for DU145 and 50% versus 80% for Huh-7 cells. These results are in agreement with previous studies[24, 26, 54], and underline the less toxic effect of zebularine on cells and the milder nature of the drug when compared to AZA. In other words, AZA-treatment in both cell lines showed an approximate reduction of I MeC at 63% between IC10 and IC50 concentrations, whereas the I MeC reduction leap was significantly different between ZEB-treated cells: I MeC ≈ 39% for DU145 and only 7% for Huh-7 cells. The data indicate that if DNA hypomethylation effects would be influencing cytotoxicity, dose–response may vary for different drugs in different cells.
Dose-dependent topological progression of DNA hypomethylation correlates with cytotoxicity
The analysis of the MeC/DAPI codistribution showed a high fraction of cells with pooled all similar categories in response to both drugs for all concentrations (Figure4). ZEB-treated populations contained ≥ 90% similar cells, compared with AZA-treated populations with an average ≥ 85% and a slight tendency to drop for DU145 cells at 0.5 μM and 10 μM (82% and 79%, respectively). The cell population heterogeneity analysis was performed with an average total cell number of n = 300. Figure5 displays normalized proportions of the two resultant categories of cells, and example MeC/DAPI codistributions are presented in Figure6.
The effect of the drugs can be perceived as a reduction in the MeC signal, with a similar effect in both cell systems, when compared to nuclei of untreated cells. In case of each drug, we observed a dose-dependent reduction of the MeC-specific signal. At lower drug concentrations (ZEB: 8 μM and 40 μM; AZA: 0.5 μM and 1 μM) the nucleus still shows significant DNA methylation in its periphery, which becomes hypomethylated at medium to higher drug doses (ZEB: 200–1000 μM, AZA: 5–20 μM). This is accompanied by a decrease of DNA methylation at interior nuclear regions, gradually affecting also DAPI-dense areas that are attributed to heterochromatin. Zebularine at the 1000 μM dose shows extremely strong hypomethylation in the entire nuclear space, including a large portion of heterochromatin in the nuclear interior (Figure5). In comparison, AZA shows similar effects already at 5 μM (data not shown). These observations support our findings presented in Figure3. The visual impressions of DNA hypomethylation in response to drug type and concentration were confirmed by quantitation of MeC and DAPI signal codistributions in the respective nuclei and displayed as accompanying scatter plots (Figure6).
In addition to AZA-treatments, a subset of Huh-7 cells was separately stained for covisualizing differential spatial distribution of histone H3 lysine 9 trimethylation (H3K9me3) and global DNA. H3K9me3 is associated with heterochromatin and is involved in the recruitment and binding of heterochromatin protein 1 (HP1), with subsequent chromatin condensation and compaction[66, 67]. Therefore, we monitored this marker in sample cells to specifically record changes in higher-order heterochromatin organization in conjunction with AZA drug application (Figure7). Our findings show a high degree of colocalization between the H3K9me3 and DAPI signals in untreated cells and cells treated with the entire spectrum of applied AZA concentrations. Therefore, one can assume that DAPI signals could be utilized as a surrogate marker for visualizing changes of global heterochromatin organization. Furthermore, it is conceivable that a reduction in H3K9me3 could lead to local DNA decondensation as extensively reported elsewhere[10, 68]. These findings support our topologic approach in using DAPI signals as a convenient way of reporting changes in heterochromatin organization and distribution, extensively discussed in previous works[43, 44]: as we found that DAPI staining is compatible with the hydrochloric acid-treatment conditions of fixed cells we applied for MeC-signal retrieval without any detectable obscuring of both signals.
To further emboss the differential spatial distribution of global DNA and its methylated portion, we focused on the changes in the localization of LIMs and LIDs, as subsets of nuclear signals that represent hypomethylated sites and areas of lower DNA density in naïve and treated cells. As illustrated in Figure8, both LIM and LID sites in the untreated cells have a rim-like localization at or close to the nuclear border (LIM 0.5 = 0.80–0.85, and LID 0.5 = 0.85) for both cell types after zebularine treatment, while only 15–20% of LIMs were located in nuclei. In cells comparatively treated with ZEB and AZA, the nuclei showed an increased portion of interior LIM and LID sites after treatment with each drug. The increase in LIM sites is correlated with the increase in ZEB concentration: on average the LIM-portion in DU145/Huh-7 is raised to ~30%/~40% at 8 μM, ~40%/~40% at 40 μM, ~45%/~50% at 200 μM, 50%/60% at 500 μM, and ~55%/~65% at 1000 μM, respectively. In comparison, the LID-portion in the nuclear interior significantly expanded at lower ZEB concentrations: up to 50% at 8 μM for DU145 and 40% at 40 μM for Huh-7, but did not significantly change beyond this concentration in either cell type. In AZA-treated cells the change for LIDs was very similar, however, LIM sites increased up to 60% on average as can be inferred from the subset of data displayed for the equitoxic drug concentrations in Figure9. For the two drugs, the responding distributions of LIM and LID sites are quite similar between equitoxic concentrations with a slight difference of IC50 for DU145 cells. Interestingly in this context, LID distributions did not vary substantially compared to LIM distributions between IC10 and IC50 concentrations. From these results we glean that an increase of global DNA hypomethylation can be traced in a dose-dependent manner. However, a significant concurrent reorganization of the genome based on changes in DAPI densities occurs already at the lower applied drug concentrations, and does not seem to become stronger at concentrations that are 25–100-fold higher. Therefore, the differential LIM and LID topology supplements the MeC/DAPI codistribution findings described in Figure6. The respective diagrams of the cells show a flattening of MeC/DAPI codistribution and the increase of LIM sites concurrent with increasing dosage. Stronger hypomethylating effects at higher concentrations of AZA or ZEB were not accompanied by an additional increase of LID sites. Also, the increase in LIM distribution towards higher LIM densities reflects the spatial progression of DNA hypomethylation, which seems to positively correlate with drug-based cytotoxicity.
MeC/DAPI codistribution patterns are independent from cell cycle interphases
Interphase cells are largely divided into two prominent groups based on their cell cycle stage: G0/G1-phase and G2-phase, differing in DNA content. Compared to haploid G1-cells diploid G2-cells normally contain two copies of the genome after having undergone the intermediate S-phase, in which DNA is replicated. Therefore, we investigated the possibility of existing differences in MeC/DAPI distribution patterns between these two cell cycle phases. DU145 cells were synchronized in culture and arrested in G0/G1 and G2-phases. Cell stage-enriched populations were processed for immunofluorescence and 3-D imaging. We found that synchronized cell populations were comprised of an absolute majority of cells in interphase, as most of the barely attached and round metaphase cells are usually lost during the early synchronization steps (Figures10A and10B). Utilizing 3D-qDMI, we did not detect any significant differences for MeC/DAPI codistribution patterns between the two major cell cycle phases. Sample signatures of selected (similar) G1 and G2-cells with a low KL-value that represent typical global nuclear MeC phenotypes are shown in Figure10 (C–F), and demonstrate similar codistribution patterns seen for untreated DU145 cells (Figure5). Based on these results, we conclude that significant changes in MeC/DAPI patterns detected by 3D-qDMI are a result of drug action and not influenced by eventual cell cycle phase variability.
In comparison, when analyzing DNA methylation and DAPI loads of nuclei in synchronized cell populations, we found that the amplitude of the respective mean intensities I MeC and I DAPI has nearly doubled in G2 versus G0/G1 phase. However, the distribution of these two values shows a large spread in both phases (Figure11). This fact demonstrates that although we could measure general load trends that most probably correlate with the doubling of the genome between G1 and G2 phases, overall mean intensities of global DNA and total MeC content can drastically vary, even between synchronized cells; therefore making it difficult to distinguish between their natural variation and strictly drug-induced changes. On the contrary, when MeC/DAPI codistribution data of the same G1 and G2 arrested cells were combined, the computationally merged population presented a high degree of homogeneity, as calculated by KL-divergence measurement. This confirms the high similarity between the MeC phenotypes of cells from the two different populations, and emphasizes on the robustness of MeC/DAPI patterns in evaluating drug-induced effects on nuclear DNA methylation topology.
Analysis of DNA methylation levels in repeat sequences correlates with imaging results
For comparative analysis of differential DNA methylation loads and to verify the quantitative accuracy of 3D-qDMI, Huh-7 cells were subjected to AZA treatment under the same conditions (concentrations and exposure times) as for cells interrogated by image and flow cytometry, and analyzed using MethyLight technology, a real-time PCR based DNA methylation assay. MethyLight assays measuring DNA methylation of repetitive element sequences have been previously described as accurate surrogates for quantitating global DNA methylation levels. Using this technique, we measured DNA methylation levels in the three of the most prevalent and highly methylated human repeat sequences: the short interspersed nuclear element (SINE) Alu sequences that are highly abundant in the human genome, as well as the pericentromeric Sat2 and the centromeric Satα, which both belong to constitutive heterochromatin. The choice of said targets was based on the facts that DNA hypomethylation of these sequences can lead to local chromatin decondensation and genomic instability, which have been well characterized in diverse cancers and other types of complex traits such as ICF syndrome[8, 13, 48]. Also, these repetitive elements have been shown to become hypomethylated after exposure to DNMTi[12–14, 69]. The molecular assay revealed that DNA methylation levels in all three classes of repetitive elements showed similar trends and were in strong agreement with results observed for global DNA methylation with 3D-qDMI: the untreated cells record the highest level of MeC content with a gradual decline as the drug concentration increases, and a re-increase of DNA methylation for the 20 μM AZA dose. We believe that because of the purportedly extensive damage to cell integrity at the 20 μM AZA concentration, the more methylated (possibly drug-resistant) cells may have selectively survived (Figure12). This was observed with microscopic imaging, in which the cell populations were significantly reduced compared to lower drug doses and contained larger numbers of highly methylated cells, which were excluded as outliers in 3D-qDMI analysis.
In order to draw direct comparisons between image-derived data and molecular sequenced-based results a correlation coefficient was calculated between in situ global DNA methylation levels, i.e. normalized MeC mean intensities of analyzed Huh-7 cells (obtained by 3D-qDMI, Figure4) and DNA methylation levels measured (normalized PMR values) for each class of repeat sequence across AZA concentrations up to the 10 μM dose, as shown in Table1. The comparison resulted in high correlations between the outcome of the two platforms, the highest being for the interspersed Alu sequences (R = 0.96), followed by pericentromeric Sat2 and centromeric Satα (R = 0.89 and 0.86, respectively).
Epigenetic drugs including DNA methyltransferase inhibitors, which are meant to correct for DNA methylation imbalances in cells, constitute promising therapeutic approaches in the battle against cancer. The FDA-approved azanucleotides 5-azacytidine and decitabine are already administered to patients with hematologic neoplasias. Zebularine has emerged as a new member of this type of agents that has shown potentials for long-term oral applications, as a result of systematic comparative analyses[23–27, 70, 71]. However, most of the assessments have been performed utilizing molecular methods that reveal precise information regarding CpG methylation profiles of non-repetitive sequences, but are currently costly and time-consuming, if not challenged, when applied in a cell-by-cell mode. Nevertheless, we believe that analysis of cultured cell models at single-cell resolution is necessary to obtain a more global and cell systemic picture of drug action and efficacy in the search for new drugs as well as the epigenetic evaluation of existing drugs. Thus, high-content and high-throughput analyses, which have been supported by recent advancements in imaging technology and computational capacities, offer valuable means for rapid and cost-effective cellular phenotyping in drug screening. Furthermore, the vast majority of studies so far have been focusing on assessing the hypomethylating potential of drugs on selected gene promoters in combination with cell viability testing for drug cytotoxicity and genotoxicity. However, hypomethylating agents can also perturb the epigenetic regulation of chromatin conformation, thus having an impact on the higher-order genome organization and nuclear architecture that regulate genome integrity and gene expression. We were interested in tracking the progression and extent of such global structural changes, also in correlation with drug cytotoxicity to additionally elaborate on the verification of the 3D-qDMI system’s utility for the therapeutic field. Towards this end, we have conducted a comparative cell-by-cell evaluation of zebularine and its extensively characterized isoform 5-azacytidine based on their effects on global nuclear DNA and its higher-order organization in the cell nucleus. For the purpose of generating comparable topological data, we chose human cell culture models that have rendered themselves as sensitive to both agents, as well as cell culture conditions and drug doses that have been used previously in comprehensive studies to explore differential changes on the level of DNA methylation for targeted single-copy CpG sites. Our study includes standard viability testing for measuring cytotoxicity and upgraded 3D-qDMI for evaluating the demethylation effects on two levels: (i) changes in the load of nuclear MeC (I MeC), and (ii) alterations in the spatial codistribution of MeC and global DNA, including condensed heterochromatin regions that are represented by bright DAPI areas in the nuclei of cells. Our cytotoxicity data as well as the results of our topologic approach are strongly concordant with data presented by other investigators[23, 25, 26, 73–75]. Drug response efficacy, as judged by the degree of spatial nuclear MeC/DAPI patterns, was comparably high for the two drugs across all concentrations.
In terms of cytotoxicity, we found that the Huh-7 hepatocarcinoma cells reacted more sensitively to zebularine than the prostate cancer cells. Nevertheless, for both cell types, zebularine elicited similar cytotoxicity levels at doses that were one to two orders of magnitude higher than for 5-azacytidine, thus can be considered as much less cytotoxic at near-equimolar concentrations. The results are in accordance with data from other investigations that have probed the two agents in various other cancer cell models such as bladder (T24), colon (HCT-116), ovarian (A2780 and HEY) and breast (MBA-MD-231 and MCF-7) cancer cell lines, as well as in acute myeloid leukemia cells (AML 193)[23, 25, 73–75]. Investigations addressing the chemistry behind this phenomenon have led to cumulative evidence indicating the formation of a permanent covalent bond between human as well as selected bacterial DNMTs and 5-azacytidine that can trap the enzyme in a suicide complex (triggering apoptosis). In comparison, only a stable but no permanent covalent bond has been proven between zebularine and the same DNMTs, which would allow the enzymes’ release after binding in vitro as well as in vivo. This may explain why higher concentrations of zebularine are necessary for similar levels of global DNA hypomethylation in cell nuclei and its lower cytotoxicity (at equimolar concentrations), compared with AZA[76, 77].
Furthermore, we observed that the increase in cytotoxicity correlates with global 5-methylcytosine levels, especially the extent of DNA hypomethylation at DAPI-positive heterochromatic sites as revealed by 3D-qDMI through scatter plotting of MeC/DAPI codistribution. This was also true for AZA-treated cells (data not shown). Along the same lines, when localizing low-intensity MeC and DAPI sites in the same nuclei, we could map the gradual increase in LIMs from the nuclear periphery into the more interior parts of the nuclei. However, we experienced that a strong level of LID increase within the nuclei interior was already seen at the lower zebularine concentration (8–40 μM), compared to naïve cells, which did not significantly change up to the highest concentration applied (1000 μM). These LID-patterns were very similar to the one in AZA-treated cells (Figure8), in which the majority of LIDs were found to be located in the nuclear periphery. These conclusions are drawn from images of cells with seemingly intact nuclear envelope. In fact, for drug concentrations ≥5 μM for 5-azacytidine and ≥500 μM for zebularine, a large number of cells were found to present DAPI and MeC signals outside of their nuclei, leading to the assumption that the drugs had also affected the nuclear envelope and caused DNA leakage. In these cells the respective LID curves were located below the diagonal of the graphs (not shown). Due to the cytotoxic effect induced by high drug concentrations, such cells were not included in our further analyses.
Therefore we cannot exclude any contribution of topological changes of gDNA/heterochromatin to cytotoxicity. On the contrary, we assume that global DNA demethylation may lead to both DNA hypomethylation as well as gDNA reorganization, which are bilateral and together could lead to cellular decline. Although, our data here suggest that cytotoxicity is more fine-correlated with DNA hypomethylation than with bulk DNA reorganization. However, it may also be possible that only local gDNA rearrangements occurred under the conditions applied in our study. The latter effect is conceivable from the increase of LIMs in nuclear areas that harbor heterochromatin: as a significant LIM increase was detected for cells already at low zebularine doses, a compounding of both DNA demethylation effects may have triggered cellular disruption. Figure6 underlines the fact that 5-azacytidine has equivalent effects at concentrations that are much lower than of zebularine.
The mode of action of azanucleosides is quite complex. Cytosine hypomethylation by azanucleosides, including zebularine, has been extensively reported to reactivate tumor suppressor genes and apoptosis-related genes[79–81] but also the relaxation of highly compacted chromatin that can be seen as a loss of gDNA (DAPI) signal per voxel[43, 44], as chromatin conformation is linked to DNA methylation and its bilateral relationship to histone tail modifications. Therefore, we believe that cell-by-cell topological analysis as used in our approach, i.e. the topology of LIMs and LIDs in combination with the display of differential MeC/DAPI colocalization patterns shows a potential to serve as a valuable indicator for the observed phenomena: cytotoxicity-correlated global DNA hypomethylation and DNA reorganization, as consequences of drug effects. For the selected combinations of cell types and agents, the measurement of mean MeC signal (I MeC) — a derivative of DNA methylation load, across all imaged cells — corresponded well with the level of cytotoxicity (Figure4). However, for the majority of cases I MeC presented a relatively high standard deviation, whereas for the same cell populations we observed a low fraction of dissimilar cells in terms of MeC/gDNA distribution (Figure5). The discrepancy between the two signatures becomes more plausible with the analysis of synchronized DU145 cells: high similarity was measured between G0/G1-cells and G2-cells in MeC/DAPI codistribution (Figure10). On the contrary, individual intensity values for global 5-methylcytosine (MeC) and overall DNA (DAPI) nearly doubled between G0/G1-phase and G2-phase as expected, although with a large spread in both signal distributions indicating high signal variability even in synchronized cells (Figure11). Based on these findings, we believe that signatures based on spatial MeC/DAPI codistribution are more robust in MeC-phenotyping of cells than simply measuring DNA methylation loads, as they can better distinguish between drug-induced demethylation effects and the variation of methylation among individual cells. In combination with K-L divergence measurement, such a cell-by-cell cross-examination as performed with 3D-qDMI can provide structure-based quantities for studying epigenetic drug response.
Finally, in order to test the quantitative accuracy of 3D-qDMI a comparative analysis was performed utilizing MethyLight assays that have been specifically designed for and proven to measure differential levels of DNA methylation in repeat sequences such as Alu, Sat2, and Satα with high confidence. These sequences are highly methylated in human cells and also represent a significant portion of their genomes. Therefore, they have been proven to serve as surrogates for measuring the global content of 5-methylcytosine in cells. Our comparative analyses revealed a significantly high degree of correlation between the outcomes of the two methods. We chose MethyLight as a validated technique over high-pressure liquid chromatography (HPLC), used as a standard method for measuring global DNA methylation: as the latter method requires significantly more input DNA (5–10 μg).
We conclude that the results of our work strongly support the idea of utilizing the spatial higher-order genome organization as a sentinel for drug-induced toxicity effects in liaison with global DNA hypomethylation. In particular, nuclear DNA methylation distribution patterns have proven to serve as an indicator of topological changes of the genome that could perturb spatial interactions of genomic loci and subsequent expression programs leading to cytotoxicity in treated cells. This is quite conceivable as it has been observed that DNA hypomethylation after treatment with DNMTi can be accompanied by additional changes in histone-tail modifications and nucleosome depletion that decrease DNA-repressive mechanisms and support a more open chromatin conformation[83–86], an effect that we could reconcile with 3D image analysis for H3K9me3. A decrease in this repressive and compacting chromatin landmark with increasing doses of 5-azacytidine correlates well with a decrease in gDNA signal, and could be interpreted as chromatin decondensation (Figure7). These downstream effects remain to be evaluated by determining the underlying molecular effects of possible cellular reprogramming, including the degree of heterochromatin demethylation. Especially, the loss of global DNA methylation at heterochromatic areas of the genome that harbor highly repetitive DNA sequences such as highly abundant Alu repeats, transposable long interspersed nuclear elements (LINEs) and satellite DNAs can be associated with multiple risks towards genome instability[8, 88]; through an adverse reorganization of the genome with side effects, such as transcriptional activation of oncogenes, activation of latent retrotransposons, chromosomal instability, and telomere elongation of chromosomes[11, 89–92]. More specifically, Satα and Sat2 DNA hypomethylation may favor centromeric and pericentromeric instability, respectively. Alu retroelements, if left unchecked, would insert throughout the genome into non-coding and coding regions. The result would be mutations, and activation of oncogenes: spontaneous insertion of an Alu element causes nearby promoters to be hypomethylated, increasing gene expression[93, 94]. Diseases directly associated with Alu insertion into coding regions include neurofibromatosis, haemophilia, agammaglobulinaemia, leukemia, breast cancer and ovarian cancer. Any malignancy caused by Alu insertion is both heritable along somatic cell lines as well as in the germline. This concern has been recently strengthened by observations, in which specific genomic areas were found to become re-methylated during a following DNA replication step after initial drug-induced demethylation; as a possible mechanism to protect these sequences from permanent hypomethylation. The study showed that exposure of cancer cells to agents such as 5-azacytidine and decitabine preferentially led to demethylation of CpGs not located in CpG-islands, whereas island-associated CpGs became preferentially re-methylated, suggesting that CG-dinucleotides in repetitive elements could become more persistently hypomethylated than gene-associated CGs.
In light of these observations, it appears reasonable to point out the necessity of new assays and complementary bioinformatics for detecting unwanted genomic-scale adverse effects such as heterochromatin reorganization, that could be used as endpoints in the cytotoxic and genotoxic risk assessment of already existing demethylating drugs and next-generation chromatin-targeting agents under development. Recent advancements in cellular imaging and computational image analysis have made it feasible for large volumes of images from thousands of cells to be analyzed in relatively short amount of time at substantially lower costs. Imaging-based cytomics also enables the quantification of spatial and temporal distribution of molecules and cellular components within their native environment, which can boost understanding drug activity at the cell systemic level. Within this context, MeC phenotyping appears to provide a valuable technology, and further investigations will be crucial to evaluate its performance for a broader spectrum of epigenetic drugs in cytotoxicity and eventually genotoxicity testing. Hence, the combination of 3D-qDMI with comparative techniques that provide genome-wide sequence-specific MeC-profiles and detail concurrent changes in chromatin conformation could lead to validation of MeC phenotypes in assessment of drug-induced chromatin states. A variety of impressive high-resolution sequencing-based techniques have recently become available such as NOMe-Seq, which provides nucleosome positioning landscapes; chromosome conformation capture (3C) methodology and its whole-genomic version Hi-C, which map the 3D architecture of the genome by proximity-based ligation and subsequent next-generation sequencing[98, 99]; a related method called chromatin interaction analysis using paired-end tag sequencing (ChIA–PET), and newer attempts that focus on increasing the sensitivity of chromatin immunoprecipitation-based assays towards single-cell analysis. For example: the correlation of chromatin textures derived from MeC patterns with matching nucleosome depleted regions and proximity-ligation profiles can lead to the identification of MeC phenotypes indicative of risky and genotoxic drug effects.
Cedars-Sinai Medical Center
Fetal bovine serum
- IC10 :
Inhibitory concentration at which 10% of cells are nonviable.
Jaenisch R, Bird A: Epigenetic regulation of gene expression: how the genome integrates intrinsic and environmental signals. Nat Genet. 2003, 33: 245-254. 10.1038/ng1089.
Jones PA, Baylin SB: The epigenomics of cancer. Cell. 2007, 128: 683-692. 10.1016/j.cell.2007.01.029.
Herman JG, Baylin SB: Gene silencing in cancer is associated with promoter hypermethylation. N Engl J Med. 2003, 349: 2042-2054. 10.1056/NEJMra023075.
Esteller M: Epigenetics in cancer. N Engl J Med. 2008, 358: 1148-1159. 10.1056/NEJMra072067.
Costello JF, Frühwald MC, Smiraglia DJ, Rush LJ, Robertson GP, Gao X, Wright FA, Feramisco JD, Peltomäki P, Lang JC, Schuller DE, Yu L, Bloomfield CD, Caligiuri MA, Yates A, Nishikawa R, Su Huang H, Petrelli NJ, Zhang X, O’Dorisio MS, Held WA, Cavenee WK, Plass C: Aberrant CpG-island methylation has non-random and tumour-type-specific patterns. Nat Genet. 2000, 24: 132-138. 10.1038/72785.
Ehrlich M, Gama-Sosa MA, Huang LH, Midgett RM, Kuo KC, McCune RA, Gehrke C: Amount and distribution of 5-methylcytosine in human DNA from different types of tissues of cells. Nucleic Acids Res. 1982, 10: 2709-2721. 10.1093/nar/10.8.2709.
Gardiner-Garden M, Frommer M: CpG islands in vertebrate genomes. J Mol Biol. 1987, 196: 261-282. 10.1016/0022-2836(87)90689-9.
Ehrlich M: DNA Hypomethylation in cancer cells. Epigenomics. 2009, 1: 239-259. 10.2217/epi.09.33.
Puitri EL, Robertson KD: Epigenetic mechanisms and genome stability. Clin Epigenetics. 2011, 2: 299-314. 10.1007/s13148-010-0017-z.
Peng JC, Karpen GH: Epigenetic regulation of heterochromatic stability. Curr Opin Genet Dev. 2008, 18: 204-211. 10.1016/j.gde.2008.01.021.
Feinberg AP, Vogelstein B: Hypomethylation distinguishes genes of some human cancers from their normal counterparts. Nature. 1983, 301: 89-92. 10.1038/301089a0.
Gama-Sosa MA, Slagel VA, Trewyn RW, Oxenhandler R, Kuo KC, Kuo KC, Gehrke CW, Ehrlich M: The 5-methylcytosine content of DNA from human tumors. Nucleic Acid Res. 1983, 11: 6883-6894. 10.1093/nar/11.19.6883.
Ehrlich M: NA hypomethylation and cancer. DNA Alterations in Cancer: Genetic and Epigenetic Changes. Edited by: Ehrlich M. 2000, Natick, MA: Eaton Publishing, 273-291.
Dunn BK: Hypomethylation: one side of a larger picture. Ann N Y Acad Sci. 2003, 983: 28-42. 10.1111/j.1749-6632.2003.tb05960.x.
Fraser P, Bickmore W: Nuclear organization of the genome and the potential for gene regulation. Nature. 2007, 447: 413-417. 10.1038/nature05916.
Deal RB, Henikoff S: Capturing the dynamic epigenome. Genome Biol. 2010, 11: 218-10.1186/gb-2010-11-10-218.
Misteli T: Higher-order genome organization in human disease. Cold Spring Harb Perspect Biol. 2010, 2: a000794-10.1101/cshperspect.a000794.
Li G, Reinberg D: Chromatin higher-order structures and gene regulation. Curr Opin Genet Dev. 2011, 21: 175-186. 10.1016/j.gde.2011.01.022.
Tajbakhsh J: DNA methylation topology: potential of a chromatin landmark for epigenetic drug toxicology. Epigenomics. 2011, 3: 761-770. 10.2217/epi.11.101.
Yoo CB, Jones PA: Epigenetic therapy of cancer: past, present and future. Nat Rev Drug Discov. 2006, 5: 37-50. 10.1038/nrd1930.
Gore SD, Jones C, Kirkpatrick P: Decitabine. Nat Rev Drug Discov. 2006, 5: 891-892. 10.1038/nrd2180.
Issa JP, Kantarjian H: 5-azacytidine. Nat Rev Drug Discov. 2005, S6-S7. Suppl
Cheng JC, Matsen CB, Gonzales FA, Ye W, Greer S, Marquez VE, Jones PA, Selker EU: Inhibition of DNA methylation and reactivation of silenced genes by zebularine. J Natl Cancer Inst. 2003, 95: 399-409. 10.1093/jnci/95.5.399.
Yoo CB, Cheng JC, Jones PA: Zebularine: a new drug for epigenetic therapy. Biochem Soc Trans. 2004, 32: 910-912. 10.1042/BST0320910.
Marquez VE, Kelley JA, Agbaria R, Ben-Kasus T, Cheng JC, Yoo CB, Jones PA: Zebularine: a unique molecule for an epigenetically based strategy in cancer chemotherapy. Ann N Y Acad Sci. 2005, 1058: 246-254. 10.1196/annals.1359.037.
Herranz M, Martín-Caballero J, Fraga MF, Ruiz-Cabello J, Flores JM, Desco M, Marquez V, Esteller M: The novel DNA methylation inhibitor zebularine is effective against the development of murine T-cell lymphoma. Blood. 2006, 107: 1174-1177.
Stresemann C, Bokelmann I, Mahlknecht U, Lyko F: 5-azacytidine causes complex DNA methylation responses in myeloid leukemia. Mol Cancer Ther. 2008, 7: 2998-3005. 10.1158/1535-7163.MCT-08-0411.
Santi DV, Norment A, Garrett CE: Covalent bond formation between a DNA-cytosine methyltransferase and DNA containing 5-azacytosine. Proc Natl Acad Sci USA. 1984, 81: 6993-6997. 10.1073/pnas.81.22.6993.
Bender CM, Gonzalgo ML, Gonzales FA, Nguyen CT, Robertson KD, Jones PA: Roles of Cell Division and Gene Transcription in the Methylation of CpG Islands. Mol Cell Biol. 1999, 19: 6690-6698.
Weisenberger DJ, Velicescu M, Cheng JC, Gonzales FA, Liang G, Jones PA: Role of the DNA Methyltransferase Variant DNMT3b3 in DNA Methylation. Mol Cancer Res. 2004, 2: 62-72.
Ghoshal K, Datta J, Majumder S, Bai S, Kutay H, Motiwala T, Jacob ST: 5-Aza-Deoxycytidine Induces Selective Degradation of DNA Methyltransferase 1 by a Proteasomal Pathway That Requires the KEN Box, Bromo-Adjacent Homology Domain, and Nuclear Localization Signal. Mol Cell Biol. 2005, 25: 4727-4741. 10.1128/MCB.25.11.4727-4741.2005.
Zhu WG, Hileman T, Ke Y, Wang P, Lu S, Duan W, Dai Z, Tong T, Villalona-Calero MA, Plass C, Otterson GA: 5-aza-2′-deoxycytidine activates the p53/p21Waf1/Cip1 pathway to inhibit cell proliferation. J Biol Chem. 2004, 279: 15161-15166. 10.1074/jbc.M311703200.
Yang X, Noushmehr H, Han H, Andreu-Vieyra C, Liang G, Jones PA: Gene reactivation by 5-aza-2′-deoxycytidine-induced demethylation requires SRCAP-mediated H2A.Z insertion to establish nucleosome depleted regions. PLoS Genet. 2012, 8: e1002604-10.1371/journal.pgen.1002604.
Patra SK, Patra A, Rizzi F, Ghosh TC, Bettuzzi S: Demethylation of (Cytosine-5-C-methyl) DNA and regulation of transcription in the epigenetic pathways of cancer development. Cancer Metastasis Rev. 2008, 27: 315-334. 10.1007/s10555-008-9118-y.
Patra SK, Bettuzzi S: Epigenetic DNA-(cytosine-5-carbon) modifications: 5-aza-2′-deoxycytidine and DNA-demethylation. Biochemistry (Mosc). 2009, 74: 613-619. 10.1134/S0006297909060042.
Ammerpohl O, Martin-Subero JI, Richter J, Vater I, Siebert R: Hunting for the 5th base: Techniques for analyzing DNA methylation. Biochim Biophys Acta. 2009, 1790: 847-862. 10.1016/j.bbagen.2009.02.001.
Laird PW: Principles and challenges of genome-wide DNA methylation analysis. Nat Rev Genet. 2010, 11: 191-203.
Fatemi M, Pao MM, Jeong S, Gal-Yam EN, Egger G, Weisenberger DJ, Jones PA: Footprinting of mammalian promoters: use of a CpG DNA methyltransferase revealing nucleosome positions at a single molecule level. Nucleic Acids Res. 2005, 33: e176-10.1093/nar/gni180.
Kelly TK, Liu Y, Lay FD, Liang G, Berman BP, Jones PA: Genome-wide mapping of nucleosome positioning and DNA methylation within individual DNA molecules. Genome Res. 2012, 22: 2497-2506. 10.1101/gr.143008.112.
Haaf T: The effects of 5-azacytidine and 5-azadeoxycytidine on chromosome structure and function: implications for methylation-associated cellular processes. Pharmacol Ther. 1995, 65: 19-46. 10.1016/0163-7258(94)00053-6.
De Capoa A, Menendez F, Poggesi I, Giancotti P, Grappelli C, Marotta MR, Di Leandro M, Reynaud C, Niveleau A: Cytological evidence for 5-azacytidine-induced demethylation of the heterochromatic regions of human chromosomes. Chromosome Res. 1996, 4: 271-276. 10.1007/BF02263676.
Tajbakhsh J, Wawrowsky KA, Gertych A, Bar-Nur O, Vishnevsky E, Lindsley EH, Farkas DL: Characterization of tumor cells and stem cells by differential nuclear methylation imaging. Imaging, Manipulation, and Analysis of Biomolecules, Cells, and Tissues. Proceedings of the SPIE: 19–24 January 2008. Edited by: Farkas DL DL, Nicolau DV, Robert C, Leif RC. 2008, San Jose, CA: SPIE Publications, 6859F1-6859F10.
Gertych A, Wawrowsky KA, Lindsley E, Vishnevsky E, Farkas DL, Tajbakhsh J: Automated quantification of DNA demethylation effects in cells via 3D mapping of nuclear signatures and population homogeneity assessment. Cytometry A. 2009, 75: 569-583.
Gertych A, Farkas DL, Tajbakhsh J: Measuring topology of low-intensity DNA methylation sites for high-throughput assessment of epigenetic drug-induced effects in cancer cells. Exp Cell Res. 2010, 316: 3150-3160. 10.1016/j.yexcr.2010.08.013.
Szyf M: Epigenetics, DNA methylation, and chromatin modifying drugs. Annu Rev Pharmacol Toxicol. 2009, 49: 243-263. 10.1146/annurev-pharmtox-061008-103102.
Tajbakhsh J, Gertych A, Farkas DL: Utilizing nuclear DNA methylation patterns in cell-based assays for epigenetic drug screening. Drug Discovery World. 2010, 27-35. spring edition
Tong WG, Wierda WG, Lin E, Kuang SQ, Bekele BN, Estrov Z, Wei Y, Yang H, Keating MJ, Garcia-Manero G: Genome-wide DNA methylation profiling of chronic lymphocytic leukemia allows identification of epigenetically repressed molecular pathways with clinical impact. Epigenetics. 2010, 5: 499-508. 10.4161/epi.5.6.12179.
Ehrlich M: DNA hypomethylation, cancer, the immunodeficiency, centromeric region instability, facial anomalies syndrome and chromosomal rearrangements. J Nutr. 2002, 132: 2424S-2429S.
Espada J, Esteller M: Epigenetic control of nuclear architecture. Cell Mol Life Sci. 2007, 64: 449-457. 10.1007/s00018-007-6358-x.
Santos AP, Abranches R, Stoger E, Beven A, Viegas W, Shaw PJ: The architecture of interphase chromosomes and gene positioning are altered by changes in DNA methylation and histone acetylation. J Cell Sci. 2002, 115: 4597-4605. 10.1242/jcs.00160.
Gilbert N, Thomson I, Boyle S, Allan J, Ramsahoye B, Bickmore WA: DNA methylation affects nuclear organization, histone modifications, and linker histone binding but not chromatin compaction. J Cell Biol. 2007, 177: 401-411. 10.1083/jcb.200607133.
Christman JK: 5-azacytidine and 5-aza-2′-deoxycytidine as inhibitors of DNA methylation: mechanistic studies and their implications for cancer therapy. Oncogene. 2002, 21: 5483-5495. 10.1038/sj.onc.1205699.
Stresemann C, Brueckner B, Musch T, Stopper H, Lyko F: Functional diversity of DNA methyltransferase inhibitors in human cancer cell lines. Cancer Res. 2006, 66: 2794-2800. 10.1158/0008-5472.CAN-05-2821.
Dote H, Cerna D, Burgan WE, Carter DJ, Cerra MA, Hollingshead MG, Camphausen K, Tofilon PJ: Enhancement of in vitro and in vivo tumor cell radiosensitivity by the DNA methylation inhibitor zebularine. Clin Cancer Res. 2005, 11: 4571-4579. 10.1158/1078-0432.CCR-05-0050.
Schwarze SR, Fu VX, Desotelle JA, Kenowski ML, Jarrard DF: The identification of senescence-specific genes during the induction of senescence in prostate cancer cells. Neoplasia. 2005, 7: 816-823. 10.1593/neo.05250.
Ewald J, Desotelle J, Almassi N, Jarrard D: Drug-induced senescence bystander proliferation in prostate cancer cells in vitro and in vivo. Br J Cancer. 2008, 98: 1244-1249. 10.1038/sj.bjc.6604288.
Patra A, Deb M, Dahiya R, Patra SK: 5-Aza-2′-deoxycytidine stress response and apoptosis in prostate cancer. Clin Epigenetics. 2011, 2: 339-348. 10.1007/s13148-010-0019-x.
Venturelli S, Armeanu S, Pathil A, Hsieh CJ, Weiss TS, Vonthein R, Wehrmann M, Gregor M, Lauer UM, Bitzer M: Epigenetic combination therapy as a tumor-selective treatment approach for hepatocellular carcinoma. Cancer. 2007, 109: 2132-2141. 10.1002/cncr.22652.
Andersen JB, Factor VM, Marquardt JU, Raggi C, Lee YH, Seo D, Conner EA, Thorgeirsson SS: An integrated genomic and epigenomic approach predicts therapeutic response to zebularine in human liver cancer. Sci Transl Med. 2010, 2: 54ra77-10.1126/scitranslmed.3001338.
Heinemann L, Simpson GR, Annels NE, Vile R, Melcher A, Prestwich R, Harrington KJ, Pandha HS: The effect of cell cycle synchronization on tumor sensitivity to reovirus oncolysis. Mol Ther. 2010, 18: 2085-2093. 10.1038/mt.2010.189.
Whitfield ML, Zheng LX, Baldwin A, Ohta T, Hurt MM, Marzluff WF: Stem-loop binding protein, the protein that binds the 3′ end of histone mRNA, is cell cycle regulated by both translational and posttranslational mechanisms. Mol Cell Biol. 2000, 20: 4188-4198. 10.1128/MCB.20.12.4188-4198.2000.
Wong C, Stearns T: Mammalian cells lack checkpoints for tetraploidy, aberrant centrosome number, and cytokinesis failure. BMC Cell Biol. 2005, 6: 6-10.1186/1471-2121-6-6.
van Engeland M, Nieland LJ, Ramaekers FC, Schutte B, Reutelingsperger CP: Annexin V-affinity assay: a review on an apoptosis detection system based on phosphatidylserine exposure. Cytometry. 1998, 31: 1-9. 10.1002/(SICI)1097-0320(19980101)31:1<1::AID-CYTO1>3.0.CO;2-R.
Tajbakhsh J, Gertych A: Three-dimensional quantitative DNA methylation imaging for chromatin texture analysis in pharmacoepigenomics and toxicoepigenomics. Epigenomics: From Chromatin Biology to Therapeutics. Edited by: Appasani K. 2012, Cambridge, UK: Cambridge University Press, 273-
Weisenberger DJ, Campan M, Long TI, Kim M, Woods C, Fiala E, Ehrlich M, Laird PW: Analysis of repetitive element DNA methylation by MethyLight. Nucleic Acids Res. 2005, 33: 6823-6836. 10.1093/nar/gki987.
Cowell IG, Aucott R, Mahadevaiah SK, Burgoyne PS, Huskisson N, Bongiorni S, Prantera G, Fanti L, Pimpinelli S, Wu R, Gilbert DM, Shi W, Fundele R, Morrison H, Jeppesen P, Singh PB: Heterochromatin, HP1 and methylation at lysine 9 of histone H3 in animals. Chromosoma. 2002, 111: 22-36. 10.1007/s00412-002-0182-8.
Lachner M, O’Carroll D, Rea S, Mechtler K, Jenuwein T: Methylation of histone H3 lysine 9 creates a binding site for HP1 proteins. Nature. 2001, 410: 116-120. 10.1038/35065132.
Peng JC, Karpen GH: Heterochromatic genome stability requires regulators of histone H3 K9 methylation. PLoS Genet. 2009, 5: e1000435-10.1371/journal.pgen.1000435.
Shvachko LP: Alterations of constitutive pericentromeric heterochromatin in lymphocytes of cancer patients and lymphocytes exposed to 5-azacytidine is associated with hypomethylation. Exp Oncol. 2008, 30: 230-234.
Chiam K, Centenera MM, Butler LM, Tilley WD, Bianco-Miotto T: GSTP1 DNA methylation and expression status is indicative of 5-aza-2′-deoxycytidine efficacy in human prostate cancer cells. PLoS One. 2011, 6: e25634-10.1371/journal.pone.0025634.
Chen M, Shabashvili D, Nawab A, Yang SX, Dyer LM, Brown KD, Hollingshead M, Hunter KW, Kaye FJ, Hochwald SN, Marquez VE, Steeg P, Zajac-Kaye M: DNA methyltransferase inhibitor, zebularine, delays tumor growth and induces apoptosis in a genetically engineered mouse model of breast cancer. Mol Cancer Ther. 2012, 11: 370-382. 10.1158/1535-7163.MCT-11-0458.
Lang P, Yeow K, Nichols A, Scheer A: Cellular imaging in drug discovery. Nat Rev Drug Discov. 2006, 5: 343-356. 10.1038/nrd2008.
Cheng JC, Weisenberger DJ, Gonzales FA, Liang G, Xu GL, Hu YG, Marquez VE, Jones PA: Continuous zebularine treatment effectively sustains demethylation in human bladder cancer cells. Mol Cell Biol. 2004, 24: 1270-1278. 10.1128/MCB.24.3.1270-1278.2004.
Scott SA, Lakshimikuttysamma A, Sheridan DP, Sanche SE, Geyer CR, Hu YG, Marquez VE, Jones PA: Zebularine inhibits human acute myeloid leukemia cell growth in vitro in association with p15INK4B demethylation and reexpression. Exp Hematol. 2007, 35: 263-273. 10.1016/j.exphem.2006.10.005.
Billam M, Sobolewski MD, Davidson NE: Effects of a novel DNA methyltransferase inhibitor zebularine on human breast cancer cells. Breast Cancer Res Treat. 2010, 120: 581-592. 10.1007/s10549-009-0420-3.
van Bemmel DM, Brank AS, Eritja R, Marquez VE, Christman JK: DNA (Cytosine-C5) methyltransferase inhibition by oligodeoxyribonucleotides containing 2-(1H)-pyrimidinone (zebularine aglycon) at the enzymatic target site. Biochem Pharmacol. 2009, 78: 633-641. 10.1016/j.bcp.2009.05.017.
Champion C, Guianvarc’h D, Sénamaud-Beaufort C, Jurkowska RZ, Jeltsch A, Ponger L, Arimondo PB, Guieysse-Peugeot AL: Mechanistic insights on the inhibition of c5 DNA methyltransferases by zebularine. PLoS One. 2010, 5: e12388-10.1371/journal.pone.0012388.
Stresemann C, Lyko F: Modes of action of the DNA methyltransferase inhibitors 5-azacytidine and decitabine. Int J Cancer. 2008, 123: 8-13. 10.1002/ijc.23607.
Huang J, Plass C, Gerhauser C: Cancer chemoprevention by targeting the epigenome. Curr Drug Targets. 2011, 12: 1925-1956. 10.2174/138945011798184155.
Khan R, Schmidt-Mende J, Karimi M, Gogvadze V, Hassan M, Ekström TJ, Zhivotovsky B, Hellström-Lindberg E: Hypomethylation and apoptosis in 5-azacytidine-treated myeloid cells. Exp Hematol. 2008, 36: 149-157. 10.1016/j.exphem.2007.10.002.
Ruiz-Magaña MJ, Rodríguez-Vargas JM, Morales JC, Saldivia MA, Schulze-Osthoff K, Ruiz-Ruiz C: The DNA methyltransferase inhibitors zebularine and decitabine induce mitochondria-mediated apoptosis and DNA damage in p53 mutant leukemic T cells. Int J Cancer. 2012, 130: 1195-1207. 10.1002/ijc.26107.
D’Alessio AC, Szyf M: Epigenetic tête-à-tête: the bilateral relationship between chromatin modifications and DNA methylation. Biochem Cell Biol. 2006, 84: 463-476. 10.1139/o06-090.
Nguyen CT, Weisenberger DJ, Velicescu M, Gonzales FA, Lin JC, Liang G, Jones PA: Histone H3-lysine 9 methylation is associated with aberrant gene silencing in cancer cells and is rapidly reversed by 5-aza-2′-deoxycytidine. Cancer Res. 2002, 62: 6456-6461.
Lin JC, Jeong S, Liang G, Takai D, Fatemi M, Tsai YC, Egger G, Gal-Yam EN, Jones PA: Role of nucleosomal occupancy in the epigenetic silencing of the MLH1 CpG island. Cancer Cell. 2007, 12: 432-444. 10.1016/j.ccr.2007.10.014.
Komashko VM, Farnham PJ: 5-azacytidine treatment reorganizes genomic histone modification patterns. Epigenetics. 2010, 5: 229-240. 10.4161/epi.5.3.11409.
Si J, Boumber YA, Shu J, Qin T, Ahmed S, He R, Jelinek J, Issa JP: Chromatin remodeling is required for gene reactivation after decitabine-mediated DNA hypomethylation. Cancer Res. 2010, 70: 6968-6977. 10.1158/0008-5472.CAN-09-4474.
Csoka AB, Szyf M: Epigenetic side-effects of common pharmaceuticals: a potential new field in medicine and pharmacology. Med Hypotheses. 2009, 73: 770-780. 10.1016/j.mehy.2008.10.039.
Gaudet F, Hodgson JG, Eden A, Jackson-Grusby L, Dausman J, Gray JW, Leonhardt H, Jaenisch R: Induction of tumors in mice by genomic hypomethylation. Science. 2003, 300: 489-492. 10.1126/science.1083558.
Holliday R, Pugh JE: DNA modification mechanisms and gene activity during development. Science. 1975, 187: 226-232. 10.1126/science.1111098.
Bestor TH, Tycko B: Creation of genomic methylation patterns. Nat Genet. 1996, 12: 363-367. 10.1038/ng0496-363.
Ehrlich M: DNA methylation in cancer: too much, but also too little. Oncogene. 2002, 21: 5400-5413. 10.1038/sj.onc.1205651.
Vera E, Canela A, Fraga MF, Esteller M, Blasco MA: Epigenetic regulation of telomeres in human cancer. Oncogene. 2008, 27: 6817-6833. 10.1038/onc.2008.289.
Feltus FA, Lee EK, Costello JF, Plass C, Vertino PM: DNA motifs associated with aberrant CpG island methylation. Genomics. 2006, 87: 5728-5729.
Kang MI, Rhyu MG, Kim YH, Jung YC, Hong SJ, Cho CS, Kim HS: The length of CpG islands is associated with the distribution of Alu and L1 retroelements. Genomics. 2006, 87: 580-590. 10.1016/j.ygeno.2006.01.002.
Deininger PL, Batzer MA: Alu repeats and human disease. Mol Genet Metab. 1999, 67: 183-193. 10.1006/mgme.1999.2864.
Hagemann S, Heil O, Lyko F, Brueckner B: 5-azacytidine and decitabine induce gene-specific and non-random DNA demethylation in human cancer cell lines. PLoS One. 2011, 6: e17388-10.1371/journal.pone.0017388.
Tárnok A: Cytomics for discovering drugs. Cytometry A. 2010, 77: 1-2.
Dostie J, Richmond TA, Arnaout RR, Selzer RA, Lee WL, Honan TA, Rubio ED, Krumm A, Lamb J, Nusbaum C, Green RD, Dekker J: Chromosome conformation capture carbon copy (5C): a massively parallel solution for mapping interactions between genomic elements. Genome Res. 2006, 16: 1299-1309. 10.1101/gr.5571506.
Lieberman-Aiden E, van Berkum NL, Williams L, Imakaev M, Ragoczy T, Telling A, Amit I, Lajoie BR, Sabo PJ, Dorschner MO, Sandstrom R, Bernstein B, Bender MA, Groudine M, Gnirke A, Stamatoyannopoulos J, Mirny LA, Lander ES, Dekker J: Comprehensive mapping of long-range interactions reveals folding principles of the human genome. Science. 2009, 326: 289-293. 10.1126/science.1181369.
Fullwood MJ, Fullwood MJ, Liu MH, Pan YF, Liu J, Xu H, Mohamed YB, Orlov YL, Velkov S, Ho A, Mei PH, Chew EG, Huang PY, Welboren WJ, Han Y, Ooi HS, Ariyaratne PN, Vega VB, Luo Y, Tan PY, Choy PY, Wansa KD, Zhao B, Lim KS, Leow SC, Yow JS, Joseph R, Li H, Desai KV, Thomsen JS: An oestrogen-receptor-a-bound human chromatin interactome. Nature. 2009, 462: 58-64. 10.1038/nature08497.
Goren A, Ozsolak F, Shoresh N, Ku M, Adli M, Hart C, Gymrek M, Zuk O, Regev A, Milos PM, Bernstein BE: Chromatin profiling by directly sequencing small quantities of immunoprecipitated DNA. Nat Methods. 2010, 7: 47-49. 10.1038/nmeth.1404.
The pre-publication history for this paper can be accessed here:http://www.biomedcentral.com/2050-6511/14/11/prepub
We thank Patricia Lin (CSMC Research Flow Cytometry Core) for helping us with flow cytometry and Vaithilingaraja Arumugaswami (CSMC) for Huh-7 cells. This work was supported by the DOD-CDMRP Award W81XWH-10-1-0939 (to JT), the NIH grant 1R21CA143618-01A1 (to AG), and institutional grants from the Department of Surgery at CSMC.
The authors declare that they have no competing interests.
JT designed and conducted the study, and performed all drug experiments. JHO contributed with cell synchronization assays. KAW performed imaging. AG and JT conceptualized image analyses. AG contributed analytical software tools. AG and JT performed image and statistical data analysis. JT wrote the manuscript together with AG. DJW was in charge of the comparative MethyLight assays and helped with manuscript revision. All authors read and approved the final manuscript.
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Gertych, A., Oh, J.H., Wawrowsky, K.A. et al. 3-D DNA methylation phenotypes correlate with cytotoxicity levels in prostate and liver cancer cell models. BMC Pharmacol Toxicol 14, 11 (2013). https://doi.org/10.1186/2050-6511-14-11
- DNA methylation phenotype
- Chromatin distribution
- High-throughput cell assay
- 3D image analysis
- Repetitive element
- Epigenetic drug