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The application of methylation specific electrophoresis (MSE) to DNA methylation analysis of the 5' CpG island of mucin in cancer cells
© Yokoyama et al; licensee BioMed Central Ltd. 2012
Received: 29 June 2011
Accepted: 14 February 2012
Published: 14 February 2012
Methylation of CpG sites in genomic DNA plays an important role in gene regulation and especially in gene silencing. We have reported mechanisms of epigenetic regulation for expression of mucins, which are markers of malignancy potential and early detection of human neoplasms. Epigenetic changes in promoter regions appear to be the first step in expression of mucins. Thus, detection of promoter methylation status is important for early diagnosis of cancer, monitoring of tumor behavior, and evaluating the response of tumors to targeted therapy. However, conventional analytical methods for DNA methylation require a large amount of DNA and have low sensitivity.
Here, we report a modified version of the bisulfite-DGGE (denaturing gradient gel electrophoresis) using a nested PCR approach. We designated this method as methylation specific electrophoresis (MSE). The MSE method is comprised of the following steps: (a) bisulfite treatment of genomic DNA, (b) amplification of the target DNA by a nested PCR approach and (c) applying to DGGE. To examine whether the MSE method is able to analyze DNA methylation of mucin genes in various samples, we apply it to DNA obtained from state cell lines, ethanol-fixed colonic crypts and human pancreatic juices.
The MSE method greatly decreases the amount of input DNA. The lower detection limit for distinguishing different methylation status is < 0.1% and the detectable minimum amount of DNA is 20 pg, which can be obtained from only a few cells. We also show that MSE can be used for analysis of challenging samples such as human isolated colonic crypts or human pancreatic juices, from which only a small amount of DNA can be extracted.
The MSE method can provide a qualitative information of methylated sequence profile. The MSE method allows sensitive and specific analysis of the DNA methylation pattern of almost any block of multiple CpG sites. The MSE method can be applied to analysis of DNA methylation status in many different clinical samples, and this may facilitate identification of new risk markers.
The gene expression profile of a cancer specimen is a valuable source of biological information that has potential clinical utility . However, RNA or DNA of a sufficient quality and quantity for analysis may not be recoverable from clinical samples. Methylation of CpG sites in genomic DNA plays an important role in gene regulation, especially in gene silencing, and the promoter region of a transcribed gene is generally hypomethylated. Mechanisms of epigenetic regulation for expression of various mucins (MUC1, MUC2, MUC3A, MUC4, MUC5AC and MUC17) are reported [2–10]. Furthermore, abnormal epigenetic changes appear to be early "seeds of methylation" that precede detection of genetic mutations [11, 12]. Thus, a method for detecting alteration of methylation status could be a valuable tool for early diagnosis of cancer, monitoring of tumor behavior, and assessing the response of tumors to targeted therapy.
To resolve this issue, we developed a modified version of the bisulfite-denaturing gradient gel electrophoresis (DGGE)  which used a nested PCR approach to increase the sensitivity of detection of DNA methylation pattern, since the DGGE can detect disparity of single mutation in the same size PCR product. We designated this method as methylation specific electrophoresis (MSE). The MSE method allows sensitive and specific analysis of the DNA methylation pattern of almost any block of multiple CpG sites. We applied this method to analyze the DNA methylation patterns of promoter regions of various mucins in 12 cancer cell lines. In addition, we examined the DNA methylation patterns of the promoter region of MUC1 in samples of human isolated colonic crypts, and also examined human pancreatic juices collected from the patients with pancreatic ductal adenocarcinoma (PDAC) having a very poor prognosis and from the patients with intraductal papillary mucinous neoplasm (IPMN) having a favorable prognosis.
Human pancreatic carcinoma cell lines HPAF II, BxPC3, PANC1; human breast cancer cell lines MCF-7, T-47D, MDA-MB-453; and human colon adenocarcinoma cell lines Caco2 and LS174T were obtained from American Type Culture Collection. HPAF II, MCF-7, LS174T, and Caco2 cells were cultured in Eagle's MEM (Sigma-Aldrich), PANC1 cells were cultured in DMEM (Sigma-Aldrich), BxPC3 and T-47D cells were cultured in RPMI 1640 (Sigma-Aldrich), and MDA-MB-453 cells were cultured in Leibovitz's L-15 medium (Invitrogen, Carlsbad, CA, USA). All media were supplemented with 10% fetal bovine serum (Invitrogen, Carlsbad, CA, USA), 100 U/ml penicillin (Sigma-Aldrich) and 100 μg/ml streptomycin (Sigma-Aldrich).
Isolation of human colonic crypts
Fresh normal and tumor tissue samples were obtained from colorectal carcinoma specimens that were obtained surgically at Iwate Medical College Hospital. Normal colonic mucosa was taken from an area distant from the tumor. The tumor samples were obtained from the tumor-rich area of carcinomas. Crypt isolation from the normal and neoplastic mucosa was performed as previously reported [20–22]. Briefly, fresh normal mucosae and tumors were minced with a razor into minute pieces and then incubated at 37°C for 30 minutes in calcium- and magnesium-free Hanks' balanced salt solution (CMF) containing 30 mmol/L ethylene-diaminetetraacetic acid (EDTA). Following this procedure, the tissue was stirred in CMF for 30-40 minutes. Normal and neoplastic glands were separated from the lamina propria mucosa or fibrous stroma. The isolated crypts were immediately fixed in 70% ethanol and stored at 4°C until used for DNA and RNA extraction, and were also embedded in paraffin for immunohistochemical staining. All studies using human materials in this article were approved by the ethical committees of Kagoshima University hospital and other hospitals.
After completion of endoscopic retrograde pancreatography, pancreatic juice was collected using endoscopic nasopancreatic drainage (ENPD) or pancreatic stenting in 2 patients with PDAC and 5 patients with IPMN at Osaka Medical College Hospital . Collection of the samples was approved by the ethical committee of the hospital and informed consent was obtained from each patient. All studies using human materials in this article were approved by the ethical committees of Kagoshima University hospital and other hospitals.
Extraction and quantification of mRNA
Extraction of RNA
Total RNA was extracted from the cell lines, human colonic crypts and pancreatic juices using a RNeasy Mini kit (QIAGEN, Chuo-ku, Tokyo, Japan). Total RNA of 1 μg was then reverse transcribed with a High Capacity RNA-to-cDNA Kit (Applied Biosystems, Foster City, CA, USA).
Real time PCR assay
For quantification of MUC1 mRNA in the ethanol-fixed isolated crypts from human colonic normal mucosa and carcinoma lesions, the real time PCR assay was performed as described previously . The primers and probes were designed and synthesized by Applied Biosystems. The product number of the Target Assay Mix used for MUC1 was Hs00410317. Human glyceraldehyde-3-phosphate dehydrogenase (GAPDH; product number 4310884E) was used to calibrate the original concentration of mRNA; i.e., the concentration of mRNA in the cell was defined as the ratio of target mRNA copies versus GAPDH mRNA copies. In this analysis, data from three separate experiments were averaged.
For confirmation of gene expression level in cell lines, semiquantitative RT-PCR were performed using a Fast Cycling PCR kit (QIAGEN, Japan). The RT-PCR products were subjected to electrophoresis on 1% agarose gel. Differentially expressed genes were detected using the primer pairs (shown in Additional file 1: Table S1).
Extraction of DNA and bisulfite modification
DNA from cell lines, ethanol-fixed human crypt sections, and pancreatic juice samples was extracted using a DNeasy Tissue System (QIAGEN, Chuo-ku, Tokyo, Japan). Bisulfite modification of the genomic DNA was carried out using an Epitect Bisulfite Kit (QIAGEN, Chuo-ku, Tokyo, Japan).
Preparation of the samples for MSE method
Synthetic oligonucleotides used in MSE and conventional bisulfite-DGGE
A. The nested PCR primer set
B. The target PCR primer set
5'-[GC CLAMP] AGGAGAGAAAAGGGTGATTAG -3'
Preparation of the samples
Information of PCR product size and primer location
A. The nested PCR primer set
-219 bp to -200 bp
+156 bp to +137 bp
-460 bp to -441 bp
-200 bp to -219 bp
-478 bp to -418 bp
+17 bp to -6 bp
-249 bp to -228 bp
-30 bp to -11 bp
-3960 bp to -3941 bp
-3511 bp to -3530 bp
-383 bp to -361 bp
+203 bp to +180 bp
B. The target PCR primer set
-124 bp to -15 bp
+42 bp to +23 bp
-437 bp to -418 bp
-222 bp to -241 bp
-321 bp to -302 bp
-10 bp to -31 bp
-194 bp to -173 bp
-59 bp to -38 bp
-3842 bp to -3823 bp
-3658 bp to -3677 bp
-200 bp to -181 bp
+72 bp to +53 bp
Denaturing gradient gel electrophoresis (DGGE)
After the PCR, DGGE was performed as described by Schäfer and Muyzer  using the D-Code system (Bio-Rad Laboratories, Hercules, CA, USA). Electrophoresis was performed with 1-mm thick 10% polyacrylamide gels (ratio of acrylamide to bisacrylamide, 40:1) submerged in 1Χ TAE buffer (40 mM Tris, 40 mM acetic acid, 1 mM EDTA, pH 7.5) at a constant temperature of 60°C. PCR products in amounts ranging from 5 μl were applied to the individual lanes on the gel. The electrophoresis conditions for the target gene fragment were 14 h at 70 V in a linear denaturant gradient (MUC1, 30%-40%; MUC2, 25%-35%; MUC3A, 25%-35%; MUC4, 25%-45%; MUC5AC, 30%-40%; MUC17, 35%-45%). After electrophoresis, the gels were incubated for 30 min in Milli-Q water containing GelRed (dilution 1:10000) (Biotium, Hayward, CA, USA) and photographed using AE-6905 N (ATTO). The emission intensity of the band was measured using Image J (NIH).
Conventional bisulfite-DGGE for comparison
In the conventional bisulfite-DGGE method, the bisulfite treated DNA was amplified using the target primer sets (Table 1B). PCR parameters were as above, except that the annealing temperatures for the MUC1, MUC2, MUC3A, MUC4, MUC5AC and MUC17 reactions were 53, 51, 52, 57, 62 and 53°C respectively. Information on each PCR product size and each primer location is shown in Table 2B. All steps of PCR were performed using a Fast Cycling PCR kit (QIAGEN, Japan). After the PCR, these products were applied to DGGE.
MUC1 protein expression was assessed by immunohistochemistry using an anti-MUC1 monoclonal antibody (MAb) clone 014E (Mab MUC1-014E), which was developed by Yonezawa et al. , in ethanol-fixed paraffin-embedded 4-μm sections of the isolated human normal and neoplastic crypts. Immunohistochemistry was performed by the immunoperoxidase method as follows. Antigen retrieval was performed using CC1 antigen retrieval buffer (Ventana Medical Systems, Tucson, AZ, USA) for all sections. Following incubation with MAb MUC1-014E (diluted 1:5) in phosphate-buffered saline (PBS, pH 7.4) with 0.1% bovine serum albumin, sections were stained on a Benchmark XT automated slide stainer using a diaminobenzidine detection kit (Ventana Medical Systems).
Results and discussion
MSE approach for MUC1 promoter region
We examined the characteristics of the MSE approach for MUC1 using cell lines in which the DNA methylation status of the MUC1 promoter region has been precisely defined . First, we made controls of fully methylated and unmethylated DNA. The completely fully methylated control DNA was prepared by the treatment using methyltransferase (Sss I) on DNA from Caco2 which has the highest methylation status in the cell lines examined in the previous MassARRAY analysis (Additional file 2: Table S2) . Similarly, the fully unmethylated control DNA was prepared by PCR for the MUC1 promoter region on DNA from T-47D which has the lowest methylation status in the cell lines examined in the previous MassARRAY analysis (Additional file 2: Table S2) . The bisulfite-sequencing analyses for the fully methylated and unmethylated controls showed clearly defined methylated and unmethylated sequence (Additional file 3: Table S3). The MSE analyses for the fully methylated and unmethylated controls showed clearly defined methylated and unmethylated bands (Additional file 4: Figure S1). This electrophoretic migration distance depends on mutation (cytosine vs. thymine) in the target sequence, but not on the PCR product size. Thus, the "methylated sequence" carrying many cytosines shows higher mobility than the "un-methylated sequence" carrying many thymines which are converted from cytosines by the bisulfite treatment. For this reason, the more a band migrates, the higher the band is methylated. In addition, the multiple bands indicate a mix of various patterns of methylated CpG sequences. This method provides information on the degree of methylation status by the migration distance of bands and the variation of methylated sequences by the numbers of bands, although it does not provides the individual CpG methylation ratio.
Sensitivity of MSE in MUC1 promoter region analysis
Resolution of MSE in MUC1 promoter region analysis
Next, we analyzed DNA derived from BxPC3 (tendency for lower methylation of the MUC1 promoter region) and Panc1 (tendency for higher methylation of the MUC1 promoter region) (Figure 2B, upper panel). These 2 cell lines has heterogeneity of methylated CpG sequence pattern . Thus, BxPC3 shows various bands which are inclined toward the hypomethylated side. Similarly, Panc1 shows various bands which are inclined toward the hypermethylated side. Aggerholm et al demonstrated a correlation exists between the band migration and the number of methylated sites in a denaturing gradient gel . In addition, we tested MSE on a mixture of DNA derived from BxPC3 and Panc1 (Figure 2B, upper panel). We found that the emission intensity of the band for the hypo-methylated MUC1 promoter was directly proportional to the contamination ratio of hypo-methylated cells (R2 = 0.993; Figure 2B, lower panel). MSE can accurately detect a methylation target at a level of 0.1%. These results indicate that MSE can detect 3 abnormal cells (un-methylated MUC1 promoter) in 3000 normal (methylated MUC1 promoter) cells. We have shown that MSE is not only highly specific and sensitive, but that it also can rapidly detect biologically relevant information in patient samples. In contrast, Li et al. suggested that an optimized MSP assay was unable to detect methylated templates when the fraction of methylated fragments was < 6.2% in parallel assays . MSE provides significant advantages over the conventional bisulfite-DGGE since MSE requires only 200 pg of DNA of low quality, making it suitable for small biopsies, ethanol-fixed tissue, and clinical fluid samples.
Application of MSE for promoter regions of various mucins
Application of MSE for human samples
To our knowledge, there is no report describing this intuitive modification of the bisulfite-DGGE method. Nobody could show the diagnostic usefulness of DNA methylation status of mucin genes for pancreatic juices. Interestingly, in the pancreatic juice analysis, the electrophoresis band pattern of MSE revealed a significant difference of degree of methylation status in the promoter region of MUC1, MUC2 or MUC4 between PDAC with a very poor prognosis and IPMN with a favorable prognosis. A further study is needed to clarify the biological significance of this observation, but the lower methylation in PDAC compared to IPMN may provide an approach for early diagnosis of pancreatic neoplasm.
The MSE method can provide a qualitative information of methylated sequence profile. The MSE method is a simple, sensitive, and specific method for determining the DNA methylation status of almost any CpG island. Here, we have shown that MSE can be used to analyze ethanol-fixed samples (human colonic crypts) and human fluid samples (human pancreatic juice). Thus, MSE can be applied to analysis of DNA methylation in many different clinical samples, and this may facilitate identification of new risk markers.
This work was supported by Princess Takamastu Cancer Research Fund (11-24319) (S. Yonezawa); by Scientific Research on Priority Areas 20014022 and Scientific Research (B) 23390085 (S. Yonezawa) and Scientific Research (C) 20590399 (M. Higashi) grants from the Ministry of Education, Science, Sports, Culture and Technology, Japan; by an International Educational Research Support Project for Islands, Environment and Medicine (S. Yokoyama); by a JSPS Fellowship Grant-in-Aid (no. 239349) (S. Kitamoto); by a Pancreas Reserch Foundation of Japan (S. Yokoyama) and by the Kodama Memorial Foundation, Japan (S. Yokoyama & M. Higashi). The authors thank Ms. Yukari Nishimura and Ms. Sayuri Yoshimura for their excellent technical assistance.
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