Background
Fanconi anemia (FA) is a rare recessive disorder, characterized by congenital skeletal abnormalities, progressive bone marrow failure and an increased cancer susceptibility [
1]. The disease is caused by bi-allelic mutations in one of 13 FA genes, all of which have now been identified [
2]. The FA genes appear to act in a common pathway of DNA damage signalling and DNA remodelling, distal parts of which interact with regulators of cell cycle control and DNA repair, especially the repair of DNA interstrand-crosslinks.
There are three consecutive compartments of the FA pathway [
3]. The proximal compartment consists of eight FA proteins (A, B, C, E, F, G, L, and M), which form a nuclear FA core complex upon activation. This complex functions as an E3 ligase and mediates the monoubiquitination of FANCD2 [
4], which represents the central FA pathway protein. FANCI also becomes monoubiquitinated during this process [
5,
6] and cooperates with FANCD2 in the ID (FANC
I/FANC
D 2) complex [
7,
8]. The activated proteins of the ID complex subsequently co-localize with proteins of the distal FA pathway compartment (FANCD1/BRCA2, FANCN, and FANCJ) and with other DNA-repair proteins such as RAD51 at sites of DNA-damage. Cells having a defect in one of the proximal FA core complex genes are deficient in FANCD2/FANCI monoubiquitination and FANCD2/FANCI nuclear focus formation. Similarly, cells having a defect in one of the distal FA pathway genes
FANCD1 or
FANCN are deficient in RAD51 focus formation [
8‐
12]. Cells with a defect in one of the ID complex proteins lack the respective protein and are defective in monoubiquitination of the other. Thus, inactivation of the FA pathway can comprehensively be identified at the cellular level by assays detecting FANCD2 monoubiquitination and FANCD2/RAD51 focus formation.
FA pathway inactivation occurs sporadically in a variety of tumor types of non-FA patients, suggesting a role of the FA genes in tumor suppression or maintenance of genomic stability among the general population. Distal FA pathway inactivation via mutations in
FANCD1 occurs in familial cases of breast (2-25%) [
13] and ovarian cancer (2-6%) [
14], in familial cases of pancreatic cancer (17%) [
15] and in sporadic cancers of various tumor entities [
16‐
18]. In comparison, genetic inactivation of the proximal FA pathway appears to occur infrequently in tumors among the general population and has, in terms of GI cancers, yet only been reported in pancreatic cancer, where it was associated with rare mutations in
FANCC or
FANCG [
19,
20]. In addition, germline mutations of
FANCC might contribute to the tumorigenesis or tumor progression of pancreatic cancer [
20‐
22]. Finally, epigenetic inactivation of the proximal FA pathway via hypermethylation of
FANCF has been reported in a variety of tumor entities [
23‐
27], but its significance is not yet well understood [
28,
29].
Unlike the setting in FA patients, FA pathway-deficient tumors arising in patients of the general population harbor the FA gene defect exclusively in the tumor cells, whereas stroma and all other non-malignant cells lack the defect, thus representing a tumor-specific, absolute biochemical difference [
30]. As FA pathway-deficient cells are hypersensitive to ICL-agents and PARP inhibitors, FA pathway inactivation in tumors represents a promising target for rational, genotype-based anticancer therapy [
31‐
38].
The prevalence of FA pathway defects has not yet been systematically investigated in GI cancer. We assessed proximal and distal FA pathway function in 48 cell lines derived from gastric, pancreatic, colorectal, hepatocellular and cholangiocellular carcinomas applying assays for FANCD2 monoubiquitination and FANCD2/RAD51 focus formation [
39]. We newly identified a single cell line, HuH-7, derived from a hepatocellular carcinoma (HCC), which exhibited a proximal FA pathway defect, ascribable to genetic
FANCC inactivation. When compared to four other HCC cell lines, HuH-7 cells exhibited an increased sensitivity towards ICL-agents, which was reversible in these cells by genetic correction through
FANCC overexpression. Our data represent the first evidence for genetic inactivation of the proximal FA pathway in HCC and further support the assumption that genetic inactivation of the proximal FA pathway is a rare event in solid tumors among the general population.
Discussion
We report here the identification and functional characterization of an inactivating nonsense
FANCC mutation in the HCC cell line HuH-7. This cell line was established from a well-differentiated HCC of a 57 year-old Japanese male patient [
42], displays an aneuploid phenotype with an average number of 60 chromosomes, and is negative for HBV and HCV [
43,
44]. To our knowledge, this is the first evidence of genetic inactivation of the proximal FA pathway in a GI tumor entity other than pancreatic cancer.
The identified
FANCC nonsense mutation c.553C > T, p.R185X in HuH-7 represents a known FA mutation, first described by Gibson et al. [
45]. Interestingly, non-splice site nonsense mutations can cause exon-skipping through aberrant splicing [
46], and accordingly, the c.553C > T mutation has been reported to cause partial transcriptional skipping of exon 6 of
FANCC in an FA patient [
45], a mechanism confirmed for HuH-7 in our study.
Unfortunately, no matched non-malignant tissue is available for HuH-7, precluding definitive genomic copy number analyses in regard to whether the identified
FANCC mutation represents a homo- or hemizygous mutation in this cell line. However, according to copy number analyses by the Sanger Institute (Cambridge, UK) using high-density single nucleotide polymorphism (SNP) arrays (SNP 6.0) [
47], HuH-7 harbors three nearly identical copies of the chromosomal arm 9q, where
FANCC is located at 9q22.3, as evidenced by virtually exclusive homozygosity of all SNPs assessed on 9q. According to proposed evaluation models for the identification of LOH events where no matching normal tissue is available, these data are strongly suggestive (although not definitely evidentiary) of allelic loss of one copy of chromosome 9q including the non-mutated
FANCC allele in the original tumor (or its precursor cells), followed by repeated duplication of the remaining chromosome 9q, including the mutated
FANCC allele, later on [
48‐
50]. Typical recurrent numerical chromosomal aberrations in HCC include losses on 1p, 4q, 8p, 13q, 16q, and 17p and gains on 1q, 8q, 16p and 20q [
51]. Although chromosome 9 is rarely clonally altered on the cytogenetic level in HCC, LOH has been reported for several regions on chromosome 9 including the loci of the
FANCC (9q22.3) and the
FANCG (9p13) genes [
52].
FA pathway defects in tumors require bi-allelic inactivation of one of at least 13 FA genes. On the one hand, these bi-allelic mutations could both be inherited, as applies to tumors occurring in FA-patients. On the other hand, mono-allelic germline mutations of distal FA pathway genes, such as
FANCD1,
FANCN or
FANCJ, confer low to medium penetrance susceptibility for breast/ovarian cancer [
12,
13,
53] and, as applies to
FANCD1 and
FANCN, also for pancreatic cancer [
15,
54‐
57]. In addition, inherited mono-allelic mutations of proximal FA pathway genes have been associated with the predisposition for or the accelerated development of certain tumors [
21,
54,
55,
58]. In particular, germline mutations of
FANCC have been described in pancreatic cancer, associated with LOH in the tumor [
21,
22]. However, germline and somatic changes in
FANCC and
FANCG may have comparatively low penetrance for pancreatic cancer [
55], which is supported by studies investigating germline mutations of upstream FA pathway genes in sporadic, yet FA-typical tumors among the general population [
59]. Nevertheless, as the
FANCC mutation in HuH-7 reported in our study represents an established FA mutation and was therefore most likely present in the germline of the patient in mono-allelic form, our data might indicate an increased risk for the development of HCC in individuals of the general population harboring this or other
FANCC mutations.
The occurrence of an FA-associated
FANCC mutation in HCC could also denote a tissue-specific susceptibility for the development of HCC in FA patients; The majority of solid malignancies seen in FA patients consists of head and neck or gynaecologic carcinomas (5.3%), as reported in a large meta-analysis of 1300 cases [
60], but also 2.8% of all FA patients developed liver tumors. These tumors manifested at a significantly younger age than other solid malignancies (median age: 13 years for liver tumors as compared to 26 years for other solid malignancies). In fact, the cumulative probability of liver tumors in FA patients has been estimated to be 46% by age 50 [
60]. However, the significance of these data regarding a potential liver-specific cancer susceptibility of FA patients is complicated by the observation that many liver tumors do not proceed to malignancy during the life span of FA patients [
60,
61]. In addition, there appears to be a strong association between androgen therapy, which is frequently used for the treatment of bone marrow failure in FA, and the occurrence of liver tumors [
60‐
63]. Nevertheless, HCC represented the majority (58%) of tumors of 36 FA patients with androgen-related liver tumors in one study [
61]. Thus, the association of FA with HCC could be attributable both to the primary tumorigenic effects of FA pathway inactivation in hepatocytes, as well as to potential secondary, amplifying or accelerating effects of androgen therapy in FA patients.
We demonstrated that HCC cells having an inactivated FA pathway display the classic cellular FA phenotype, including a specific hypersensitivity towards ICL-agents, illustrated in HuH-7 by a pronounced cell cycle arrest in G2 upon treatment with MMC at low concentrations and a strongly decreased proliferation rate as compared to a panel of non-isogenic HCC lines. Importantly, this ICL-hypersensitivity phenotype was reversed using an isogenic HuH-7 model of exogenous
FANCC expression, confirming that ICL-hypersensitivity in these cells was attributable specifically to inactivation of
FANCC. Of note however, IC50-ratios between
FANCC-deficient and
FANCC-proficient cells were partly smaller in the isogenic model than could have been expected from our results using the non-isogenic model. This observation could be attributable to FA pathway-independent ICL-sensitivity differences among the non-isogenic HCC cell lines, but could also provide further support for our previous hypothesis that constitutive exogenous
FANCC over-expression does not completely substitute for physiologically regulated, endogenous
FANCC expression [
37,
38].
It is well established that systemic chemotherapy lacks effectiveness in unselected HCC patients [
64,
65] and HCC are therefore considered largely chemoresistant, at least partially explaining the poor prognosis of this tumor entity [
66]. Accordingly, guidelines are currently lacking also regarding the choice of chemotherapeutic agent to use in transarterial chemoembolization (TACE), one of the major treatment modalities for non-surgical patients at advanced HCC stages [
67]. Our data indicate that non-FA patients having a FA-deficient HCC might predictably benefit from treatment using ICL-agents. Consequently, assessment of FA pathway function in HCC could facilitate individualized therapeutic approaches, using genotype-based patient stratification in regard to both systemic chemotherapy and TACE.
To get an estimate of the prevalence of
FANCC inactivation in HCC, we sequenced cDNA derived from 18 surgical HCC tissue specimens to screen for genetic
FANCC inactivation. We further screened these samples for hypermethylation of the
FANCC promoter region and for lack of
FANCC mRNA expression, as epigenetic
FANCC inactivation has previously been reported in acute leukaemia and breast cancer [
68,
69]. Additionally, we included
FANCG and
FANCF in these analyses, as
FANCG represents another proximal FA gene that has been described to be mutated in GI cancer, specifically in pancreatic cancer [
20,
22], while
FANCF has been reported to be epigenetically inactivated in various tumor types [
23‐
25,
27]. On the genetic level, we found no further inactivating alterations, especially no evidence for complete homozygous gene deletions, inactivating point mutations, small deletions or insertions, in
FANCC,
FANCG or
FANCF, respectively. The detected
FANCG variant c.20C > T, p.S7F has been reported in an FA patient of the complementation group G in addition to pathogenic
FANCG mutations [
70]. There is no information available on the nature of the c.643C > A, p.Q215K variant in
FANCG. However, LOH or a second sequence variant was not detected in that tumor either. Additionally, since only two to three overlapping PCR reactions were used to amplify the complete coding sequences of
FANCC,
FANCG and
FANCF, respectively, most potential large intragenic deletions would have been detected. However, this mechanism of proximal FA gene inactivation occurs almost exclusively in
FANCA, whereas it appears to be extremely rare in
FANCC and has not at all been described in
FANCG [
20,
71‐
73]. On the epigenetic level, we found no evidence for hypermethylation of
FANCC,
FANCG or
FANCF in any of the 18 samples. Consistently,
FANCC,
FANCG and
FANCF were expressed in all samples on the mRNA level.
Our negative screening results for proximal FA pathway inactivation in HCC were not unexpected, as a hypothetical high prevalence should have become evident earlier during clinical trials - manifesting as a selective chemosensitivity of the majority of HCC towards ICL-agents. Nevertheless, the lack of FA mutations in 18 HCC does not rule out rare occurrences of proximal FA pathway inactivation in HCC and is consistent with previous reports on the low prevalence of proximal FA pathway inactivation in various tumor entities among the general population [
20‐
22,
26,
29,
68]. Future studies applying a higher sample number are required to definitely determine the prevalence of FA pathway inactivation in HCC.
Materials and methods
Cell lines, culture conditions and HCC tissue samples
Cell lines PL3, PL5, PL8, PL11 and PL45 were kindly provided by S.E. Kern (Johns Hopkins University, Baltimore, Maryland). Cell lines AZ-521, CoGa-5, CoGa-5L, Coga-12, HCA-7, Isreco 1, MKN7, MKN45, NCl-N87 and L3.6pl were kindly donated by C.J. Bruns, M. Gerhard, F.T. Kolligs and M. Ogris (Technical University and Ludwig-Maximilians-University, Munich, Germany). The remaining cell lines were purchased from the European Collection of Cell Cultures (Sigma-Aldrich, Munich, Germany) or the American Type Culture Collection (LGC Standards, Wesel, Germany). RKO cells harboring an engineered disruption of the
FANCG or
FANCC gene have been described [
36]. Cells were grown in DMEM supplemented with 10% fetal calf serum, L-glutamine and penicillin/streptomycin (PAA, Cölbe, Germany). The 18 HCC tissue samples were a kind gift of the Human Tissue and Cell Research-Trust (HTCR, Regensburg, Germany) and originated from HCCs that where surgically removed at the Ludwig-Maximilians-University (Munich, Germany).
Immunoblotting
Cells were treated with MMC (Sigma) at 100 nM for 24 h or left untreated. Consecutively, cells were lysed and protein extracts boiled and loaded on 6% polyacrylamide gels. After electrophoresis, proteins were transferred to PVDF membranes, which were blocked for 1 h in TBS-Triton X-100/2% milk before the primary antibody was applied overnight at 4°C (1:1000; anti-FANCD2 H-300, Santa Cruz Biotechnology, Heidelberg, Germany; anti-FANCC ab5065, Abcam, Cambridge, UK). HA-tagged FANCC was detected using an anti-HA antibody (1:1000; 12CA5, Santa Cruz). Antibodies directed against anti-RAD50 (1:5000; 13B3, GeneTex, San Antonio, TX), anti-p84 (1:1000; ab487, Abcam), anti-CUL1 (1:1000; 2H4C9, Invitrogen, Karlsruhe, Germany) or anti-β-ACTIN (1:10.000; AC-15, Sigma) served as loading controls. The membranes were washed and stained with anti-rabbit or anti-mouse HRP-conjugated antibodies (1:2000 to 1:10.000; GE Healthcare, Freiburg, Germany). Enhanced chemo-luminescence was elicited using SuperSignal West Pico substrate (Thermo Scientific, Schwerte, Germany) according to the manufacturer's instructions.
Experiments were performed as described before [
74]. In brief, cells were grown on coverslips until ~80% confluency and were exposed to ionizing γ-radiation (IR) at 15 Gy using a cesium-137 irradiator. After incubation for 6 h, the cells were fixed using 3.7% formaldehyde and -20°C methanol. The cells were permeabilized using Triton X-100 and incubated in blocking buffer (PBS +2% bovine serum albumin +0.5% Triton X-100) for 30 min. Consecutively, the cells were labelled using antibodies against FANCD2 (FI-17) or RAD51 (H-92) (Santa Cruz), respectively, for 2 h at room temperature. After washing, Alexa 488 goat anti-mouse or anti-rabbit antibody (Invitrogen) was applied for 1.5 h. Nuclei were counterstained using Hoechst 33342 (Roche Diagnostics, Mannheim, Germany), mounted and analyzed using a fluorescence microscope and Axiovision Software (Carl Zeiss AG; Oberkochen, Germany). The settings were kept identical for all samples.
Gene complementation studies
For FA complementation group determination, the cell line HuH-7 was transduced with retroviral constructs containing full-length cDNAs of
FANCA,
FANCB,
FANCC,
FANCE,
FANCF,
FANCG or
FANCL and analyzed for cell cycle arrest upon treatment with MMC and for restoration of FANCD2 monoubiquitination, as previously described [
26]. For isogenic studies, HuH-7 cells were stably transduced with either HA-tagged pMSCV-
FANCC (HuH-7/
FANCC) or the corresponding pMSCV empty control vector (HuH-7/ev).
gDNA sequencing
High molecular weight genomic DNA was prepared using a salting-out technique. Amplification of the
FANCC exons was performed using published primer sets [
75]. PCR products were purified using the GFX PCR DNA and Gel Band Purification kit (GE Healthcare). DNA sequencing of PCR products was performed using ABI-PRISM big-dye terminator chemistry on the ABI 310 instrument (Applied Biosystems, Darmstadt, Germany).
mRNA expression analyses and cDNA sequencing
Total RNA was extracted from surgical HCC tissues or cell lines using the NucleoSpin RNAII-Kit (Macherey-Nagel, Düren, Germany). RNA was reverse-transcribed using SuperScriptII reverse transcriptase (Invitrogen) and cDNA synthesized. Aberrant splicing of
FANCC was determined by RT-PCR using the following primer pairs: Fwd 5'-ACTGCCCAAACTGCTGAAG-3' and Rev 5'-GTTCAGACGCTAATGATAAAACCA-3' (spanning the first non-coding exon to coding exon 5), Fwd 5'-TTCTGGACAATCAAAACTTAACTCC-3' and Rev 5'-GCTGCTGCTTCTGGACATT-3' (spanning the coding exons 3 to 13), Fwd 5'-GTAGTCTG CCTCTGGCTTCG-3' and Rev 5'-TTGAGGAGAAGGTGCCTGAT-3' (spanning the coding exons 7 to 13). Expression of
FANCC,
FANCF and
FANCG mRNA was validated by RT-PCR as described previously [
76]. For sequencing of the complete coding regions of
FANCC,
FANCF and
FANCG, respectively, the corresponding cDNAs were amplified in two (
FANCF) or three (
FANCC and
FANCG) overlapping PCR reactions (primer sets available on request). Amplified products were sequenced using an ABI-Prism 3100-Avant Sequencer (Applied Biosystems) and sequence changes confirmed at the genomic level by gDNA sequencing. Reference genomic and cDNA sequences of the FA genes are available in the Fanconi Anemia Mutation Database [
77].
Cell proliferation assays
The assays were performed over a broad range of concentrations covering 100% to 0% cell survival. 1,500-2,000 cells/well were plated in 96-well plates, allowed to adhere, and treated. Following incubation for 6 d, the cells were washed, lysed in 100 μl H2O, and 0.5% Picogreen (Molecular Probes, Invitrogen) was added. Fluorescence was measured (Cytofluor Series 4000, Applied Biosystems) and growth inhibition calculated as compared to the untreated control samples. Three independent experiments were performed per agent, with each data point reflecting triplicate wells. Error bars represent standard error of the mean (SEM) from three experiments.
Cell cycle analyses
Cells were seeded in 12-well plates and treated in duplicate for 48 h using various MMC concentrations (ranging from 25 to 200 nM) or were left untreated. The cells were fixed, stained with propidium iodide, and the DNA content per cell was measured using flow cytometry (FACSCalibur, Becton Dickinson, Heidelberg, Germany). The data were analyzed using CELLQuest Pro software (Becton Dickinson). Alternatively, unfixed cells were stained with DAPI at a final concentration of 1 μg/ml in a buffer containing 154 mM NaCl, 1 mM CaCl2, 0.5 mM MgCl2, 0.1 M TRIS, 0.2% BSA, and 0.1% NP40 for 30 min in the dark. Univariate flow histograms were recorded on an analytical, triple-laser equipped flow cytometer (LSRII, Becton Dickinson) using UV excitation of the DAPI dye. The resulting cell cycle distributions reflecting cellular DNA content were quantified using the MPLUS AV software package (Phoenix Flow Systems, San Diego, CA).
HpaII restriction enzyme methylation analysis
PCR-based HpaII-restriction assays were performed as described previously [
23]. Transcriptional silencing through CpG hypermethylation was analyzed using published primer sets for
FANCF [
23] and
FANCC [
69], respectively. Primers used for
FANCG were 5'-GAGTGCAATGGCACGATG-3' (forward) and 5'-GCATGCTGGGAGTCGTAGTA-3' (reverse). CpGenome universal methylated or unmethylated DNA (Chemicon - Millipore, Schwalbach am Taunus, Germany), respectively, were used as controls.
Competing interests
The authors declare that they have no competing interests.
Authors' contributions
AP was involved in study design, acquisition, analysis and interpretation of most of the data and drafted the manuscript. KN and DS carried out the complementation studies and parts of the genomic sequencing. UP, AZ, BT and DM performed and interpreted most of the immunoblotting assays. UP and AZ further performed and interpreted drug sensitivity assays and AZ additionally performed parts of the genomic sequencing. AR, EDT and AZ performed and interpreted the FACS analyses. SO performed immunoblotting, immunofluorescence and interpreted the nuclear focus formation assays. BT and FB engineered the stably transduced HuH-7 pMSCV lines. GUD provided and analyzed cholangiocellular carcinoma cell lines. WET provided the HCC tumor specimens. HH provided the retroviral constructs. EDT, CS, BG and DS participated in the conception and the design of the study or provided important intellectual content. EG conceived the project, coordinated the experiments, directed the analysis and interpretation of the data and wrote the final manuscript. All authors read and approved the final manuscript.