Background
Acute lymphoblastic leukemia (ALL) is the most frequent childhood malignancy and accounts for 75% of pediatric leukemias. Since the 1980s, improved supportive care, precise risk classification, and personalized chemotherapy have increased the cure rate of pediatric ALL to approximately 90% in developed countries [
1]. However, a better understanding of ALL pathogenesis is needed to further improve the cure rate and quality of life. The advent of high-throughput, genome-wide gene expression analysis has provided new insights into leukemogenesis and suggested potential targets for therapy [
2,
3].
CCCTC-binding factor (CTCF) is a highly conserved 11-zinc finger protein that is involved in multiple regulatory functions, including transcriptional activation/repression [
4,
5], chromatin insulation [
6,
7], DNA imprinting [
8,
9], and X chromosome inactivation [
10,
11]. CTCF was first identified and characterized as a transcriptional repressor of the
c-myc gene in chickens, mice, and humans [
5,
12,
13]. Thus, CTCF was considered as a candidate tumor suppressor. However, CTCF also possesses some oncogenic features. CTCF levels are elevated in breast cancer cell lines and tumors and are associated with resistance to apoptosis [
14]. CTCF expression in pediatric leukemia cells has not been investigated.
We previously observed that
CTCF mRNA levels are up-regulated in leukemic cells based on the genome-wide microarray analysis from 100 Chinese pediatric ALL bone marrow samples [
15,
16]. To investigate the biological function of CTCF in pediatric ALL, we analyzed CTCF expression in clinical samples at different stages of disease progression and observed CTCF over-expression in leukemic cells from both newly diagnosed (ND) and relapsed (RE) samples. In addition, the expression of CTCF increased in a similar fashion among the different subtypes of pediatric ALL samples and cell lines. Increased CTCF expression in cancer cells could be anti-apoptotic or promote cell proliferation. Using leukemia cell line Nalm-6, we demonstrated that knock-down of CTCF increased cell apoptosis and decreased cell viability; conversely, over-expression of CTCF rescued cells from apoptosis and enhanced cell proliferation. We next explored the mechanistic basis of CTCF function, which revealed that inhibition of nuclear factor-kappa B (NF-κB) activity down-regulated CTCF expression, whereas activation of the NF-κB pathway restored CTCF expression. Furthermore, inhibition of the NF-κB pathway increased cell apoptosis in a process that was partially rescued by ectopic over-expression of CTCF. To this extent, CTCF may contribute to the pathogenesis of pediatric ALL by acting as an anti-apoptotic factor via the NF-κB pathway. These results indicate that CTCF might serve as a possible therapeutic gene target in future clinical strategies.
Discussion
CTCF functions as an epigenetic regulator and transcription factor that controls gene expression and cell fate. In B cell lymphomas, increased expression of CTCF is associated with down-regulation of c-myc, resulting in cell growth arrest and apoptosis [
20]. Accumulation of CTCF in human K562 myeloid cells leads to growth inhibition and promotion of differentiation into the erythroid lineage [
21]. Ectopic expression of CTCF in many cell types inhibits cell clonogenicity by causing growth retardation without apoptosis [
22]. Sufficient evidence proves that
CTCF could be a tumor suppressor gene. However, other studies have provided evidence contradicting a pro-apoptotic or anti-proliferative role of CTCF. CTCF knock-down triggers apoptosis in breast cancer cells, whereas over-expression of CTCF partially protects cells from Bax-induced apoptosis [
14];
CTCF mRNA knock-down promotes stress-induced apoptosis in human corneal epithelial cells [
23]. These contradictory results led us to investigate the biological function of CTCF in pediatric ALL.
Our previous genome-wide microarray analysis of samples from 100 children with ALL revealed that CTCF mRNA was over-expressed. The present study revealed that the mRNA and protein levels of CTCF are up-regulated in ND samples and return to normal levels in CR samples following chemotherapy, suggesting that CTCF may serve as a promising indicator of disease progression and treatment response.
Although intensive chemotherapy combined with potent supportive care has improved the survival conditions of pediatric ALL patients, the overall cure rate has not significantly increased in recent years. Approximately 20% of patients relapse, a leading factor in treatment failure. Notably, this study revealed CTCF expression signatures associated with disease relapse. A total of 4 relapsed ALL patients were enrolled in this study to observe the changes in CTCF expression during different disease phases. We observed that CTCF expression increased again upon disease relapse but remained at normal levels in the CR samples. This finding indicates that CTCF levels increased as the malignant clones expanded and were detectable for a brief time before disease recurrence. Additional clinical samples should be studied to confirm these findings.
Leukemia is recognized as a progressive, malignant disease caused by distorted differentiation, apoptosis, and proliferation of hematopoietic cells at different stages. The levels of CTCF were elevated rather than decreased in pediatric ALL samples, which is not characteristic of a tumor suppressor and inspired us to further examine this finding. We hypothesized that over-expression of CTCF may protect leukemic cells from apoptotic cell death or promote cancer cell proliferation. As expected, reduced CTCF levels caused apoptotic cell death and proliferative inhibition in leukemic cell lines. These results indicate a possible link between CTCF expression and sensitivity to apoptosis and proliferation. Specifically, increased CTCF levels may be necessary to protect against apoptotic stimuli and promote leukemic cell viability. These findings may be relevant to the potential use of CTCF as a therapeutic target in pediatric ALL because reducing CTCF levels could result in apoptotic cell death and growth inhibition of cancer cells without affecting normal blood cells, although further studies are needed.
CTCF over-expression has been reported to induce apoptosis and growth retardation in various cell types [
20‐
22]. Undoubtedly, our results introduce a controversial role for the tumor suppressor CTCF in apoptosis and proliferation. Cell type, cellular environment, genetic background, and other variables play important roles in the ultimate function of CTCF. The combination of these factors often has conflicting effects, making it difficult to predict the exact functional outcome of any combination. For example, WT-1 [
24‐
27] may behave as either an anti-apoptotic or pro-apoptotic factor in different cellular contexts. Previous study reported such a controversial role of CTCF in breast cancer cells [
14] and human corneal epithelial cells [
23], which strongly support our findings. In this study, we suggest a similar dual role for CTCF in pre-B ALL cells.
Explanation of this complex behavior will require a better understanding of regulatory networks. Increased CTCF levels in leukemic cells may be involved in the development of apoptotic resistance and increased cell proliferation. NF-κB is a multi-component pathway that controls hundreds of genes involved in diverse cellular processes, including cell proliferation, cellular growth, and apoptosis. Dysregulation of the pathway leads to many human diseases, such as cancer [
28]. Here, we demonstrated that changes in NF-κB activation by either a NF-κB-inhibitor or a NF-κB-activator affected
CTCF mRNA and protein expression in leukemic cells, suggesting that CTCF is involved downstream of the NF-κB pathway.
To further explore the functional role of CTCF in the NF-κB pathway, we determined that ectopic over-expression of CTCF effectively rescues Nalm-6 cells from apoptotic death rather than proliferative inhibition, indicating that CTCF is primarily involved in the anti-apoptotic pathway mediated by NF-κB in leukemic cells. However, the ability of CTCF to rescue cells from apoptotic death induced by an NF-κB-inhibitor cannot be explained solely by this pathway. The regulation of cell apoptosis and proliferation by CTCF also involves other pathways, such as the extracellular signal-regulated kinase (Erk) and Akt signaling pathways [
29]. Further studies are needed to clarify the direct and indirect effects of CTCF on this regulation. In addition, several unanswered questions must be addressed, including which NF-κB subtype interacts with CTCF in leukemic cells and which network regulates CTCF involvement in the NF-κB signaling pathway.
Materials and methods
A total of 28 children (7 months to 15 years, median age of 5 years) diagnosed with ALL and treated in the Hematology Oncology Center of Beijing Children’s Hospital between December 2002 and April 2009 were enrolled in this study. Informed consent was obtained from the parents or legal guardians of the patients. A single sample was obtained from a child with immune thrombocytopenic purpura (ITP) as a negative control. The study design followed the Helsinki guidelines and was approved by the Beijing Children’s Hospital Ethics Committee prior to initiating the study.
All patients were diagnosed with ALL using a combination of morphology, immunology, cytogenetics, and molecular biology (MICM). The cytogenetic ALL subtypes were experimentally identified by G-banding karyotype and multiplex nested reverse transcription-polymerase chain reaction (RT-PCR). A total of 29 fusion genes were assessed by RT-PCR, including TEL-AML1, BCR-ABL, E2A-PBX1, MLL-AF4, and SIL-TAL1.
Paired bone marrow (BM) samples from 16 pediatric patients (n = 32) were collected at the time the patient was characterized as newly diagnosed (ND) or in complete remission (CR). From these samples, 10 (n = 20) were randomly selected for quantitative real-time PCR (qRT-PCR) analysis (Table
1). In addition, 8 unpaired BM samples (n = 8) from 4 ND and 4 CR patients were collected. Matched BM samples were also collected from 4 relapsed patients at the time of ND, CR, and relapse (RE) (n = 12). The clinical features of these patients are described in detail in Table
2.
Cell samples, RNA isolation, and qRT-PCR
BM samples were collected in ethylenediaminetetraacetic acid (EDTA) tubes. Mononuclear cells were isolated by Ficoll gradient centrifugation (MD Pacific, Tianjin, China, density: 1.077 g/ml) and cryo-preserved in a -80°C freezer for subsequent experiments. Total RNA from the BM samples and cell lines was extracted using Trizol reagent (Invitrogen, Paisley, UK) and the mirVana™ Protein and RNA Isolation System (Ambion, USA), respectively, according to the manufacturers’ instructions. cDNA was synthesized using random hexamers and Moloney murine leukemia virus reverse transcriptase (Promega, Madison, USA). For BM samples, qRT-PCR was performed with the GenomeLab GeXP Genetic Analysis System (Beckman Coulter, CEQ8000, USA) using the GenomeLab™ GeXP Start Kit (Beckman Coulter, USA). The
GAPDH gene was used as an internal control. The primer sequences were as follows:
CTCF, 5′-AGGTGACACTATAGAATACAGCAGGAGGGTCTGCTATC-3′ and 5′-GTACGACTCACTATAGGGAGTGTGGCTTTTCATGTGACG-3′;
GAPDH, 5′-AGGTGACACTATAGAATAAATCCCATCACCATCTTCCA-3′ and 5′-GTACGACTCACTATAGGGATTCACACCCATGACGAACAT-3′. The qRT-PCR reaction was performed with a starting temperature of 95°C for 10 min, followed by 35 cycles of 30 s at 94°C, 30 s at 55°C, and 1 min at 72°C. Each assay was repeated three times to ensure reproducibility and reliability. For cell lines, real-time PCR was done as described previously [
16]. The threshold cycle (Ct) values for both
CTCF and
GAPDH on each PCR array were used to calculate the fold-changes in mRNA expression. The relative expression level was normalized to the
GAPDH by the method of 2
-∆∆Ct.
Plasmid construction and preparation
The full-length cDNA encoding human CTCF (727 amino acids, NP_006556.1) was cloned into the pEGFP-N2 vector (EcoRI/ApaI digestion), which carries an enhanced-GFP tag; the resulting construct was named pEGFP-N2-CTCF. For the RNA interference (RNAi) experiment, the U6 promoter-driven shRNA expression vector pNeoU6 + 1 and the shRNA plasmid specific for firefly luciferase (sh-luc) were prepared by our lab facility [
30]. Both plasmids contain a GFP tag. The two target sites in the
CTCF mRNA coding regions were sh-CTCF-1 (658–677, ATGTAGATGTGTCTGTCTAC) and sh-CTCF-2 (953–971, TACTCGTCCTCACAAGTGC). These targeted sequences were verified as unique sequences in the human genomic and transcriptional sequence database (NCBI). The plasmids were purified using a Plasmid Mini Kit (Omega, Bio-tek, USA) in accordance with the manufacturer’s instructions.
Generation of antibodies and Western blot
The anti-CTCF polyclonal antibody was generated by injecting the pET28a-CTCF antigen into a rabbit. The pET28a-CTCF antigen was constructed by inserting the N-terminal region of CTCF (amino acids 1–280) into the pET28a expression vector. The antiserum had good specificity and could be used to detect human CTCF by Western blot. The anti-GAPDH antibody was produced by the animal center of our institution [
16].
Samples containing 20 μg of total protein were separated on 8% ~ 12% SDS-PAGE gels according to the different molecular weight and then transferred onto nitrocellulose membranes (Whatman, Germany) in transfer buffer (25 mM Tris-base, 40 mM glycine, and 20% methanol) using a Mini Trans-Blot Cell (BIO-RAD) at 400 mA for 2 h. The membranes were blocked by incubation in 5% nonfat milk in TBS-T (20 mM Tris, 137 mM NaCl, and 0.1% Tween 20) for 1 h at room temperature. Proteins were detected using specific rabbit polyclonal anti-CTCF (1:2,000) or rabbit polyclonal anti-GAPDH (1:5,000) antibodies. After washing with TBS-T, the membranes were incubated with goat anti-rabbit immunoglobulin G secondary antibodies (1:5,000, Pierce, USA) in TBS-T containing 5% nonfat milk for 45 min at room temperature. The proteins were visualized using an enhanced chemiluminescence kit (Amersham, USA).
Cell culture and drug treatment
Nalm-6 is a pre-B ALL cell line with no fusion gene, while Reh is a pre-B ALL cell line with the
TEL-AML1 fusion gene. Jurkat is a T-lineage ALL cell line. Cells were cultured in a modified HyQ RPMI-1640 medium (Hyclone, USA) supplemented with 10% fetal bovine serum (FBS, PAA, USA) in a 5% CO
2 humidified atmosphere at 37°C. In the NF-κB-inhibited drug experiments, the cells were treated with ammonium pyrrolidinedithiocarbamate (PDTC, 100 μM/ml) [
31] or dimethyl sulfoxide (DMSO) for 20 h. In the NF-κB-activated drug experiments, the cells were treated with various concentrations of lipopolysaccharides (LPS, 5 or 10 μg/ml) [
19] for 12 h. The cells were harvested and washed twice with PBS. The cells were incubated on ice for 30 min in 1× cell lysis buffer [20 mM Tris, 50 mM NaCl, 2 mM Na
3VO
4, 10 mM NaF, 1 mM EDTA, 0.1% Triton X-100, and Proteinase Inhibitor Cocktail (Roche)] and then sonicated. Following centrifugation at 4°C for 30 min, the supernatants were frozen at -80°C or used immediately.
Nuclear protein extraction and determination of NF-κB activation
Nuclear proteins (including NF-κB p65) were isolated and analyzed by Western blot. The cells were washed twice with ice-cold PBS and suspended in NE buffer A [10 mM Hepes-NaOH (pH 7.9), 1.5 mM MgCl2, 10 mM KCl, proteinase inhibitor, 1 mM DTT, and 1 mM PMSF]. Intact nuclei were released from the cells by several washes with NE buffer B [NE Buffer A supplemented with 0.3% NP-40]. Nuclear membranes were damaged by adding NE buffer C [12.5% glycerol, 1mMTris-HCl (pH 6.5), 0.1 mM EDTA], followed by three cycles of sonication. A mouse monoclonal anti-p65 antibody (1:2,000, Santa Cruz, USA) was used to analyze the translocation of NF-κB to nuclei by standard Western blot analysis as described above. A rabbit polyclonal anti-histone H3 CT pan antibody (1:5,000, Upstate, USA) and a mouse monoclonal anti-α-tubulin antibody (1:10,000, Sigma, USA) were used as loading controls for nuclear and cytoplasmic proteins, respectively.
Transient transfection, cellular apoptosis, and proliferation assays
In the knock-down and over-expression experiments, the shRNA and over-expressing plasmids were transiently transfected into Nalm-6 cells (2 × 106 seeding density) using the Amaxa Cell Line Nucleofector Kit T and the Nucleofector Device (Lonza, Swiss) according to the manufacturer’s instructions. The cells were incubated for 72 h in 2 ml of antibiotic-free media containing 10% FBS and harvested for apoptosis analysis and Western blot. A total of 1 × 104 cells per well were seeded in a 96-well plate after transfection, with triplicate seedings per clone. Viable cells were counted using the Cell Counting Kit-8 (CCK-8, Dojindo, Japan) assay for 5 days according to the manufacturer’s instructions. All values were normalized to the non-treated cells (sh-luc plasmid and pEFG-N2 vector). For the drug treatment experiments, PDTC or DMSO was added to the Nalm-6 cells to inhibit NF-κB activation 20 h prior to the transfection of pEGFP-N2-CTCF or pEGFP-N2. The cells were harvested for apoptosis analysis and Western blot 48 h after transfection. Cell viability was assessed by CCK-8 analysis as described above.
For the apoptotic assays, GFP-positive cells were sorted and collected by flow cytometry (BD, FACSAria II, USA) to measure the silencing efficiency. The percentages of Annexin V-APC/PI stained (BD, USA) positive and negative cells were analyzed with FlowJo software. Besides, caspase-3 activity in cells was further determined by Western blot using specific mouse monoclonal antibody against caspase-3 (Beyotime Institute of Biotechnology, Nanjing, China), which contains specificities for detecting both procaspase-3 (1:500) and cleaved caspase-3 (1:250).
Semi-quantitative analysis
Western blots were subjected to semi-quantitative analysis using Gel-Pro Analyzer 4.0 software. The relative expression level of CTCF was normalized to the integrated optical density (IOD) of CTCF compared with GAPDH (loading control).
Competing interests
The authors declare that they have no competing interests.
Authors’ contributions
HZ performed cell culture, real-time PCR, cell apoptotic and proliferative assays, drug treatment experiments, pathway exploration, flow cytometry analysis and semi-quantitative analysis; LZ carried out the detection of clinical samples by qRT-PCR and Western blot, performed shRNA plasmids construction, and participated in cell apoptotic assay; Both HZ and LZ were involved in data analysis, drafted the manuscript and contributed equally in this study; HH performed over-expressing plasmids construction and anti-CTCF polyclonal antibody production; SZ carried out the bio-informatics analysis; WZ produced the heat map; XL participated in cell apoptotic assay; XZ and CG collected the clinical ALL samples and performed RNA isolation and cDNA synthesis; MM participated in the detection of clinical samples by qRT-PCR; SB conceived the idea of the study and participated in its design; HZ guided the research, participated in the study design, and revised the manuscript. All authors read and approved the final manuscript.