Table of Contents Author Guidelines Submit a Manuscript
Journal of Oncology
Volume 2012 (2012), Article ID 105949, 17 pages
Review Article

Folate and Colorectal Cancer in Rodents: A Model of DNA Repair Deficiency

Department of Nutrition and Food Science, Wayne State University, 410 W. Warren, 2018 Science Hall, Detroit, MI 48202, USA

Received 28 March 2012; Accepted 7 June 2012

Academic Editor: Julian J. Raffoul

Copyright © 2012 Rita Rosati et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.


Fortification of grains has resulted in a positive public health outcome vis-a-vis reduced incidence of neural tube defects. Whether folate has a correspondingly beneficial effect on other disease outcomes is less clear. A role for dietary folate in the prevention of colorectal cancer has been established through epidemiological data. Experimental data aiming to further elucidate this relationship has been somewhat equivocal. Studies report that folate depletion increases DNA damage, mutagenesis, and chromosomal instability, all suggesting inhibited DNA repair. While these data connecting folate depletion and inhibition of DNA repair are convincing, we also present data demonstrating that genetic inhibition of DNA repair is protective in the development of preneoplastic colon lesions, both when folate is depleted and when it is not. The purpose of this paper is to (1) give an overview of the data demonstrating a DNA repair defect in response to folate depletion, and (2) critically compare and contrast the experimental designs utilized in folate/colorectal cancer research and the corresponding impact on tissue folate status and critical colorectal cancer endpoints. Our analysis suggests that there is still an important need for a comprehensive evaluation of the impact of differential dietary prescriptions on blood and tissue folate status.

1. Introduction

Folate deficiency has been linked to a variety of pathologic conditions and cancers. Perhaps most notably, folate is required during pregnancy for normal development of the neural tube closure. Once the connection between reduced dietary folate consumption and neural tube defects (NTDs) was well established, the FDA mandated fortification of grain-based foods with folic acid. This mandate resulted in a >25% decrease in incidence of NTDs in the United States [1]. This fortification resulted in a slight bump in average serum folate levels in the United States from approximately 12 ng/mL to approximately 19 ng/mL [2]. Normal range for serum folate concentration in humans is 2.7–17 ng/mL [3]. Thus, folate fortification has resulted in a positive public health outcome for its intended population, women of childbearing age, through moderate increases in serum folate levels and significant reduction in NTD incidence. However, folate is also strongly connected through epidemiological data to an increased risk to develop colorectal cancer. Unlike prevention of NTDs which targets young, healthy populations, colorectal cancer is primarily a disease of aging. Concern for whether folate fortification may be detrimental in this population group is born from rodent studies demonstrating a potentially negative effect of folate supplementation on disease pathology. The purpose of this paper is to evaluate this concern with a particular focus on the impact of folate depletion and supplementation in rodent models. We have focused on data evaluating colorectal cancer phenotypes.

Folate is ingested from food, primarily from fruits and vegetables in the form of polyglutamated folate, and from folate supplements (primarily folic acid), and is ultimately metabolised into a variety of oxidized and reduced forms with varying levels of methylation, thoroughly reviewed elsewhere [4]. The different folate forms are essential for purine synthesis, methionine remethylation (and therefore S-adenosyl methionine metabolism), and thymidylate synthesis, all of which can play important roles in genomic stability. The work from Fenech’s lab has been instrumental in establishing that chromosomal instability arises when folate is depleted, primarily in the form of micronuclei [5, 6]. Recently, Crasta et al. have demonstrated that micronuclei can induce further genomic instability through errors in chromosome segregation and genomic integration, as well as through chromothripsis, a process linked to carcinogenesis through massive chromosomal breakage and rearrangement [7]. These data provide a potentially direct mechanism for the carcinogenicity of folate depletion.

Micronuclei originate from acentric chromosomes, chromatid fragments, or whole chromosomes that fail to attach properly to the mitotic spindle during anaphase and therefore do not segregate properly during cytokinesis [5]. Experimental data demonstrates that folate depletion causes micronuclei formation [810], and genetic data likewise establishes a role for folate metabolism in micronuclei formation. SNPs in the reduced folate carrier (RFC) gene (G80A), the methionine reductase (MTR) gene (A2756G), and the MTHFR gene (C677T and A1298C) are associated with the formation of micronuclei [1113]. Interestingly, SNPs in several DNA base excision repair genes have also been associated with micronuclei formation: OGG1 (C1245G), TDG (G595A), and XRCC1 (C26304T, G26466A, and G28152A) [14]. We suggest that a reduced ability to fully repair uracil in DNA results in an accumulation of DNA damage that promotes strand breakage and micronuclei formation.

2. Evidence That Folate Depletion Inhibits DNA Repair

Evidence collected from a variety of laboratories over the past decades has demonstrated an accumulation of DNA damage and/or mutations when folate is deficient. The mutagenic response to ENU (ethyl nitrosourea) is greater when folate is deficient [15]; EMS (ethyl methanesulfonate) and folate depletion induce a synergistic accumulation of DNA damage in Chinese hamster ovary (CHO) cells [16], and increased damage in response to MMS (methyl methane sulfonate) and hydrogen peroxide is seen in human colon epithelial cells when folate is depleted [17]; folate depletion makes human lymphocytes more sensitive to hydrogen peroxide [18], and more oxidative damage accumulates in response to amyloid β-peptide in neuronal cells depleted of folate [19]. These examples of accumulating damage point to an inability to repair the types of DNA damage repaired by the DNA base excision repair (BER) pathway. We directly tested the BER capacity of tissues exposed to oxidative DNA damage and found that folate depletion prevented induction of the BER pathway [20]. Further, we have shown that DNA strand breaks that arise in response to folate depletion accumulate to a larger degree when the BER pathway is genetically altered to have 50% reduction in capacity [21], demonstrating a direct role for the BER pathway in the DNA damage phenotypes of folate depletion.

Folate deficiency has been shown to result in an accumulation of uracil in DNA, a BER substrate, likely through altered thymidylate synthesis and a resulting dUMP/TMP imbalance. Uracil is uniquely removed from DNA by the BER pathway in a DNA-polymerase-β-(β-pol-) dependent fashion. In response to uracil accumulation, BER is initiated by a uracil DNA glycosylase (predominantly Udg). The processing of uracil induces transient DNA strand breaks that are ultimately resolved as repair is completed, as described in Figure 1. As such, if folate deficiency inhibits the BER pathway specifically as we have shown, we should then expect the folate deficient phenotype to mimic that of BER deficiency. In addition to accumulating DNA single-strand breaks, mutation frequencies, and DNA damage sensitivity described above, these folate-specific phenotypes also include chromosome breakage, micronucleus formation, defects in chromosomal condensation, and expression of chromosomal fragile sites ([2226]. Many of these same phenotypes are induced by deficient BER such that the phenotypes of folate depletion closely mimic the phenotypes of BER deficiency. In Table 1 we present the phenotypes expressed by BER mutants. These phenotypes include uracil accumulation; mutation induction, increased DNA base damage, increased levels of DNA single and double strand breaks, microsatellite instability, and increased levels of sister chromatid exchange (SCE) and chromosomal aberrations (referenced in Table 1 [20, 21, 2762]). Our observation that folate depletion induced a phenotype very similar to that of BER depletion suggested to us that folate depletion might exert an inhibitory effect on activity of the BER pathway.

Table 1: Genome instability phenotypes in base excision repair mutant models.
Figure 1: Biochemistry of base excision repair in uracil removal. Uracil removal is carried out as depicted, with initiation of removal by a uracil-excising DNA glycosylase (UDG depicted). All the uracil-excising glycosylases are monofunctional and leave behind an abasic lesion with an intact DNA backbone. An endonuclease (Apex 1) incises the DNA backbone 5′ to the abasic lesion, generating a 3′hydroxyl group and a 5′deoxyribose flap. A DNA polymerase (DNA polymerase β) inserts the correct nucleotide, then, in conjunction with a scaffolding protein (XRCCI), excises the deoxyribose flap. This step represents the rate-determining step in uracil-initiated base excision repair. Ligation of the scission in the phosphodiester backbone (ligase III and Xrcc1) completes repair and restores intact DNA structure. The single-strand break induced by Apex1 persists until ligation is complete and presents a potentially cytotoxic lesion if left incompletely repaired.

Accordingly, we have recently shown that the inhibitory effect of folate depletion on BER is achieved in part through inhibiting transactivation of the rate-limiting activity of BER, β-pol. Early work on the β-pol promoter clearly identified the CRE palindrome as being essential for ATF/CREB activation of the promoter [63]. We have identified a region within the β-pol CRE element that is blocked when folate is depleted, and prevents transactivation when folate is deficient [20]. Demonstrating direct inhibition of the BER response to DNA damage is important with respect to connecting the phenotypes of folate depletion and BER deficiency. We suggest that the BER inhibition of folate depletion is dependent on initiation of the BER response without completion of repair, resulting in a repair imbalance. This comes from reports that the clastogenic phenotypes of BER deficiency are wholly dependent on glycosylase-mediated initiation of BER [64].

2.1. Uracil as a Source of Imbalanced Base Excision Repair and Double-Strand Break Formation

Glycosylase-mediated induction of BER begins a series of enzymatic reactions that induces a break in the phosphodiester backbone; a break that persists until repair is completed (Figure 1). We have shown that folate depletion induces uracil DNA glycosylase (UDG) activity in liver without a corresponding induction of the rest of the pathway, generating an imbalance in BER and an accumulation of DNA single-strand breaks [21]. Others have likewise shown accumulation of single strand breaks and double strand breaks in response to folate depletion [65, 66]. Strand breaks set the stage for chromosomal instability including dicentric formation, anaphase bridges, and gross amplifications/deletions [67]. We propose that it is through these uracil-initiated strand breaks and chromosomal aberrations that folate promotes micronuclei formation, a likely carcinogenic precursor. Recently, MacFarlane et al. have demonstrated a key role for uracil misincorporation as a driving force in the colorectal carcinogenesis of folate depletion ([68]). Folate depletion and serine hydroxymethyltransferase heterozygosity (SHMT+/−) resulted in a twofold increase in number of colon tumors in the APCmin model of intestinal tumorigenesis. Moreover colonic DNA uracil content doubled when SHMT−/+ mice were folate depleted, correlating to observed decreases in thymidylate synthesis protein abundance. SHMT uses serine as the one carbon donor to convert tetrahydrofolate (THF) to 5,10 methyleneTHF, the 1C donor for conversion of dUMP to TMP. These results directly connect the increased tumorigenesis observed in colons of SHMT−/+ to changes in thymidylate synthesis and resultant uracil misincorporation into DNA.

3. Folate Depletion and Colorectal Carcinogenesis

Many epidemiological studies support the protective effect of folate in prevention of colorectal cancer. Most recently, a meta-analysis of 13 human studies shows a positive correlation between folate consumption and protection from colorectal cancer [69]. Accordingly, many rodent studies demonstrate that folate depletion increases tumorigenesis and/or the development of precursor lesions (aberrant crypt foci, ACF) in response to colon carcinogens. In the past decade, this protective effect of folate supplementation and detrimental effect of folate depletion have been called into question in response to several studies in which folate supplementation increased the numbers of tumors in tumor models of colorectal carcinogenesis, and correspondingly folate depletion reduced tumor development or aberrant crypt formation. These contradictory findings have been reviewed [70], and the short explanation is that folate supplementation is potentially detrimental during the promotion phase of carcinogenesis, either as a function of carcinogen exposure or genetic manipulation.

3.1. Analysis of Dietary Intervention Strategies and Impact of Folate Status and Intestinal Endpoints

Conclusions about the potential dangers of folate on colorectal cancer development may be based, in some instances, on unequal comparisons. A primary objective of this paper is to complete a careful analysis of dietary intervention studies to evaluate the importance that differences in model systems and/or dietary interventions may have on critical colorectal cancer endpoints. In Table 2, we have tabulated this information to allow facile comparison of dietary interventions across studies. We have included information on the following: animal model, diet source (when provided), length of dietary intervention, whether the study design included use of antibiotics to prevent microbial production of folates in the colon or use of wire-bottom caging to prevent coprophagy, and, the impact of the dietary intervention on folate levels (when provided). Included are studies that present data pertaining specifically to colorectal cancer endpoints, including mutation frequency, ACF, and intestinal tumors [7181]. (These endpoints are presented in detail in Table 4). What we find is that the typical dietary intervention uses a dietary prescription of 2 mg/kg folate for the control group, with experimental groups of 0 mg/kg folate (deficient) and 8 mg/kg (supplemented). Some studies have used 20 mg/kg folate as a hypersupplemented group as well, which does not appear to confer additional advantage or disadvantage. Some studies have used 8 mg/kg folate as the control diet [73] and some have used 5 mg/kg folate as the control diet [82], which makes comparison across studies difficult. As standard chow diets provide on average 8–10 mg/kg folic acid, these study designs facilitate comparisons across studies in which undefined diets have been used. However, it does make interpretation of the data difficult within the context of folate dose on cancer risk. This is illustrated in the summary data we present (Table 3) on percent change in blood folate and colonic folate status in response to dietary intervention. Using 2 mg/kg folate as control, there is a 50–96% decrease in blood folate at 0 mg/kg folate (with the use of antibiotics or prevention of coprophagy), and a 58–140% increase at 8 mg/kg folate. This makes it difficult to interpret the role of folate depletion and/or supplementation when the comparison is between 8 mg/kg and 0 mg/kg folate.

Table 2: Impact of experimental design on blood and tissue folate.
Table 3: Impact of dietary intervention on blood and colon folate status.
Table 4: Impact of experimental design on critical colorectal cancer endpoints.

Duration of dietary intervention appears to affect the impact on folate status. Very few studies have measured colonic folate status in response to dietary depletion, which is the target tissue of interest for this paper. But in two papers in which this was determined there seems to be a significant impact of increasing the length of the study on colonic folate levels. After 8 weeks of feeding, rats exhibit a 35% decrease in colon folate levels [83], but after 20 weeks there is a 72% decline [75]. The data in mice seems odd, in that the colon folate levels are more depleted after 5 weeks of dietary intervention [68] than after 16 weeks [84], but these studies are confounded by alterations in choline and other B vitamins. Further, these mouse studies were carried out in the absence of methods for reducing assimilation of microbial-produced folates in the colon, and there is a possibility that with the extended intervention time (16 weeks) animals adapt to reduced dietary availability of nutrients through increased coprophagy.

There also seems to be a differential sensitivity to folate depletion between mice and rats. From the limited data available, mice appear to become severely depleted (>90% reduced blood folate) after 8 weeks of feeding [21], while rats are only about 50% depleted at 8 weeks [83], 1996, but >90% depleted by 11 weeks or more of dietary folate restriction [85]. This holds true for colonic folate status as well. However, whether this 3-week difference is meaningful is unclear.

The information in Table 3 clearly demonstrates the importance of antibiotic and/or wire-bottom cages for inducing the most severe folate depletion. The average reduction in blood folate when antibiotics and/or wire-bottom cages are used is >80% (with the majority of studies showing >90%), while the absence of these factors induces a more modest 61% reduction. Further evidence for the importance of severe dietary restrictions to induce a meaningful decline in folate status is the finding that 32 weeks of feeding 0.5 mg/kg folate without antibiotics or wire-bottom cages resulted in no change in blood folate status [78]. It would be useful to have data on the impact of folate depletion on colonic folate status with and without contribution from microbially produced folates, but that information is not available without the confounding of choline deficiency [68] or riboflavin, B6, and B12 deficiencies [84]. A systematic evaluation of dietary factors on target tissue folate status would be informative.

3.2. Impact of Dietary Folate Restriction on Colorectal Cancer Endpoints

These considerations aside, there is a definite impact of altering blood and tissue folate status on colorectal cancer endpoints. And these differences seem to be clearly dependent on the stage of cancer development. Table 4 outlines studies in which colorectal cancer endpoints have been analyzed in response to dietary folate manipulations. It is very clear that in rats exposed to DMH (dimethylhydrazine), ENU (ethyl nitroso-urea), or AOM (azoxymethane) that dietary folate depletion is detrimental if the diet is begun prior to carcinogen exposure. Rats exposed to DMH had a 70% increase in colon tumors [83] and a 66% increase in ACF [85] when folate was depleted in the diet. In response to AOM, the increase in aberrant crypt foci was more modest at 12% increase [86], likely a function of a less restrictive dietary intervention (no antibiotics or wire-bottom caging). Because colorectal cancer is believed to be initiated by mutations in key genes, we also analyzed a paper in which the mutagenic response to ENU was evaluated (not a colon carcinogen) and found that ENU increased mutant frequency 8-fold when folate was depleted [15]. However, a very different effect is seen when diet is begun after carcinogen exposure. With respect to ACF and tumor formation, when folate depletion began post-AOM exposure, a slight decrease in ACF and tumor diameter was seen in the folate depleted group (0 mg/kg foalte) and a 47% increase was seen in the folate supplemented group (8 mg/kg folate) [76], suggesting that presence of folate was permissive for ACF and tumor formation. With respect to colon adenocarcinomas, Le Leu et al. [73] found that the total number of adenocarcinomas was 3-fold higher in the 8 mg/kg folate group as compared to the 0 mg/kg group. Clearly in this example folate depletion was protective against AOM-induced colon adenocarcinomas and folate supplementation was detrimental, but it remains unclear how either of these groups would have compared to an adequate folate diet of 2 mg/kg folate.

In mouse studies, data are confounded by genotype differences in models predisposed to develop gastrointestinal tumors, as well as other genetic manipulations devised to investigate the role(s) of certain pathways on colon tumorigenesis. In total we present 4 mouse studies showing a protective effect of folate on colon tumorigenesis, and 2 studies showing both detrimental and protective effects. Each study presents its own limitations preventing direct comparisons and solid conclusions. For example, in the mouse, two studies have been completed that reach two different conclusions. In the MacFarlane et al. study [68], three Shmt genotypes were investigated, wildtype, heterozygous, and null mutants. The authors found an effect of diet on tumor number and size in the Shmt heterozygous mice only, showing a 2-fold increase in both variables when folate was deficient. However, in this study choline was also depleted, making it difficult to know the specific impact of folate on tumorigenesis. In contrast, Song et al. [77] found that at 3 months folate depletion was detrimental (more ACF and more ileal adenomas as compared to 2 mg/kg folate), but that by 6 months folate depletion was significantly protective against the development of ileal adenomas. Oddly, folate supplementation was also protective, with the 2 mg/kg folate group having the highest number of ileal adenomas. The protective effect of folate observed in the MacFarlane et al. was seen only in the Shmt heterozygous animals, which is to say that in the wildtype animals which provides the appropriate comparison to the Song et al. study, no effect of diet was seen on tumorigenesis. Of note, neither of these studies utilized either antibiotics or wire-bottom caging, such that the impact of the dietary intervention on tissue specific folate status was likely moderate.

In two studies using a different APC model, the APC1638N mouse, riboflavin, B6, and B12 deficiencies were investigated along with folate deficiency such that the conclusions are not specific to folate. Additionally, both these studies avoided use of antibiotics and wire-bottom caging, so the impact of dietary intervention on folate status was moderate (see Table 3). Interestingly, in the Liu et al. study, this moderate folate depletion resulted in an approximate 40% decline in colon folate status. The Ciappio study measured small intestinal folate levels and found no difference in response to dietary manipulation; findings that are somewhat counterintuitive. With respect to the critical endpoints, the Liu et al. study found an almost 2-fold increase in tumor incidence (50% compared to 91%) in response to folate (and other B vitamins) depletion. This corresponded to an increased number of tumors/animal and a slight increase in aberrant crypt numbers. Ciappio et al. investigated the impact of maternal diet on cancer in offspring. Mothers were depleted during pregnancy and weaning, then offspring were separated into vitamin B-sufficient-, deficient- and supplemented-groups. Notably, the folate level in the vitamin-B-deficient group was 0.5 mg/kg folate, which effectively resulted in no changes in serum or small intestinal folate. This suggests that changes observed in critical endpoints may not be due to folate status but rather to other B-vitamins. Nonetheless, they observe a strongly protective effect of B-vitamin supplementation on both tumor incidence and multiplicity (~60% reduction). Oddly, B-vitamin supplementation resulted in the lowest target tissue (small intestine) and blood folate levels making it difficult to interpret the data with respect to tissue folate status. However, it is noteworthy that the deficient group exhibited the worst tumor invasiveness of all groups, clearly an important endpoint.

In the only study to investigate tumorigenesis in response to folate depletion in a mouse strain other than C57bl/6, Knock et al. have shown that folate depletion increased the number of duodenal tumors in the BALB/c strain [81]. Unfortunately folate status was not determined, but the use of antibiotics suggests that these animals would have been significantly depleted. This was a relatively small number of animals (2/16 developed the duodenal tumors), but none of the mice in the control group developed tumors, so there is a definite effect in these animals as compared to the C57bl/6. The effect of strain differences in susceptibility to dietary intervention is potentially quite interesting. Studies have demonstrated significant copy number changes between strains, and even between substrains [87, 88], and these changes could potentially account for the observed differences. Along these lines, it’s also important to consider the impact that multiple crossings into different strains (129 for making transgenics, e.g.) may have. Even with what is presumed to be adequate backcrossing, it’s inevitable that some DNA sequence does not get fully backcrossed out. In this reviewer’s opinion, this consideration has broad implications, but implications that also present opportunities for exploitation of copy number change-induced phenotype effects. To my knowledge, the only other study that has shown increased incidence of cancer in response to dietary folate manipulation was Pogribny and James [79], in which methyl donor deficiency resulted in liver tumors. To date, there are no studies showing that dietary folate (or methyl donor, or B-vitamin) deficiency induces colon tumors in rodents in the absence of carcinogen exposure. Even the genetic manipulations do not induce colon tumors, so data for answering this question is lacking.

Two studies present data demonstrating both protective and detrimental effects of folate on critical endpoints. Song et al. [77] described above, found that at 3 months of age in the mouse folate was protective, while at 6 months of age provision of folate was detrimental. These findings suggest that folate may help prevent initiation (3 months) while fueling tumor growth during promotion (6 months), consistent with the rat studies showing that folate drives tumorigenesis in the initiated colon. In the Ventrella-Lucente et al. paper [59], the impact of DNA base excision repair (BER) capacity on the tumorigenesis of folate depletion was investigated using a mouse model of BER deficiency [57]. This model develops lymphoma and adenocarcinoma in the absence of chemical exposure [58], suggesting that they would be more susceptible to the carcinogenic impact of folate deficiency. Using ACF as the critical endpoint, they demonstrated that folate depletion more than doubled the number of ACF in response to DMH exposure, consistent with the findings in rat models described above [83, 85]. However, in the BER mutant animals (DNA polymerase β heterozygotes), the reverse effect was seen on ACF formation. Here folate depletion significantly reduced the total number of ACF in response to DMH. DNA repair deficiencies are modifiers of penetrance [89], but typically in the opposite direction observed in the Ventrella-Lucente paper. However, another study looking at the mouse likewise found that a DNA repair mutant (Ku70) ameliorated the impact of the APC mutation on tumorigenesis [90]. This study did not investigate a role for folate, but demonstrates the counterintuitive impact that loss of DNA repair capacity can have on tumorigenesis.

4. Conclusions

It becomes clear that while each study presents important information regarding the impact of folate on genomic stability in the colon, that there is some problem with a lack of consistency across study designs that prevent us from arriving at definitive conclusions. As the body of literature on folate continues to grow, these gaps in knowledge will be filled. We suggest that there is still an important need for a comprehensive study investigating the impact of differential folate prescriptions on blood and tissue folate status. We have shown here that the duration of feeding, dosage of folate, and use or avoidance of antibiotics and/or wire-bottom caging all impact the severity of folate depletion. Another point to consider is the difference in total blood folate levels between rodents and humans. The normal range for serum folate in humans is 2.7–17 ng/mL, manyfold lower than the average values observed in mice and rats. The range for mouse values reported in Table 2 is 39–170 ng/mL, for an average of 82.5 ng/mL, or about 8-fold higher than human values. The absolute values for rats reported in Table 2 range from 34 to 684 ng/mL. Excluding the two very high values (657 and 684 ng/mL), the average rat blood folate level is 60 ng/mL—6-fold greater than human. In essence, the dietary regimens that we consider to be folate depleted in rodent studies seem only to bring rodent levels to within normal limits for human values, and then only when the most severe diets are utilized. This is an observation that should be duly considered when theoretically extrapolating mouse data to human diseases. However, with respect to expressed phenotypes within one model system we can confidently state these to be a function of folate status, regardless of how these values compare to folate levels in independent model systems. One last point to be made is that fortification of grain products is not analogous to the folate supplementation regimes used in these animal studies. Fortification of grain products with folic acid is intended to prevent deficiency of folate, and this public health action has effectively increased average folate levels from 12 ng/mL to approximately 19 ng/mL [2]. This increase is still far less than the 60 ng/mL (rat) and 80 ng/mL (mouse) levels attained on the maintenance (2 mg/kg) diets, such that fears of detrimental effects of folate fortification are unwarranted. That is, folate fortification is not folate supplementation and concerns that fortification of grains with folic acid is dangerous are unsupported by data in the literature.


This work was supported by a grant from the Ellison Medical Foundation [DCC].


  1. J. M. Lawrence, D. B. Petitti, M. Watkins, and M. A. Umekubo, “Trends in serum folate after food fortification,” The Lancet, vol. 354, no. 9182, pp. 915–916, 1999. View at Publisher · View at Google Scholar · View at Scopus
  2. S. H. Zeisel, “Importance of methyl donors during reproduction,” American Journal of Clinical Nutrition, vol. 89, no. 2, pp. 673S–677S, 2009. View at Publisher · View at Google Scholar · View at Scopus
  3. Folic acid-Test, MedlinePlus Medical Encyclopedia.
  4. M. Lucock, “Folic acid: nutritional biochemistry, molecular biology, and role in disease processes,” Molecular Genetics and Metabolism, vol. 71, no. 1-2, pp. 121–138, 2000. View at Publisher · View at Google Scholar · View at Scopus
  5. M. Fenech, “Folate, DNA damage and the aging brain,” Mechanisms of Ageing and Development, vol. 131, no. 4, pp. 236–241, 2010. View at Publisher · View at Google Scholar · View at Scopus
  6. M. Fenech, “Folate (vitamin B9) and vitamin B12 and their function in the maintenance of nuclear and mitochondrial genome integrity,” Mutation Research, vol. 733, no. 1-2, pp. 21–33, 2012. View at Publisher · View at Google Scholar
  7. K. Crasta, N. J. Ganem, R. Dagher et al., “DNA breaks and chromosome pulverization from errors in mitosis,” Nature, vol. 482, no. 7383, pp. 53–58, 2012. View at Google Scholar
  8. P. Thomas, J. Wu, V. Dhillon, and M. Fenech, “Effect of dietary intervention on human micronucleus frequency in lymphocytes and buccal cells,” Mutagenesis, vol. 26, no. 1, pp. 69–76, 2011. View at Publisher · View at Google Scholar · View at Scopus
  9. S. Beetstra, P. Thomas, C. Salisbury, J. Turner, and M. Fenech, “Folic acid deficiency increases chromosomal instability, chromosome 21 aneuploidy and sensitivity to radiation-induced micronuclei,” Mutation Research, vol. 578, no. 1-2, pp. 317–326, 2005. View at Publisher · View at Google Scholar · View at Scopus
  10. T. Teo and M. Fenech, “The interactive effect of alcohol and folic acid on genome stability in human WIL2-NS cells measured using the cytokinesis-block micronucleus cytome assay,” Mutation Research, vol. 657, no. 1, pp. 32–38, 2008. View at Publisher · View at Google Scholar · View at Scopus
  11. V. Dhillon, P. Thomas, and M. Fenech, “Effect of common polymorphisms in folate uptake and metabolism genes on frequency of micronucleated lymphocytes in a South Australian cohort,” Mutation Research, vol. 665, no. 1-2, pp. 1–6, 2009. View at Publisher · View at Google Scholar · View at Scopus
  12. H. Ishikawa, Y. Tian, F. Piao et al., “Genotoxic damage in female residents exposed to environmental air pollution in Shenyang city, China,” Cancer Letters, vol. 240, no. 1, pp. 29–35, 2006. View at Publisher · View at Google Scholar · View at Scopus
  13. N. Botto, M. G. Andreassi, S. Manfredi et al., “Genetic polymorphisms in folate and homocysteine metabolism as risk factors for DNA damage,” European Journal of Human Genetics, vol. 11, no. 9, pp. 671–678, 2003. View at Publisher · View at Google Scholar · View at Scopus
  14. V. S. Dhillon, P. Thomas, G. Iarmarcovai, M. Kirsch-Volders, S. Bonassi, and M. Fenech, “Genetic polymorphisms of genes involved in DNA repair and metabolism influence micronucleus frequencies in human peripheral blood lymphocytes,” Mutagenesis, vol. 26, no. 1, pp. 33–42, 2011. View at Publisher · View at Google Scholar · View at Scopus
  15. R. F. Branda, M. Hacker, A. Lafayette et al., “Nutritional folate deficiency augments the in vivo mutagenic and lymphocytotoxic activities of alkylating agents,” Environmental and Molecular Mutagenesis, vol. 32, no. 1, pp. 33–38, 1998. View at Google Scholar
  16. R. F. Branda, A. R. Lafayette, J. P. O'Neill, and J. A. Nicklas, “The effect of folate deficiency on the hprt mutational spectrum in Chinese hamster ovary cells treated with monofunctional alkylating agents,” Mutation Research, vol. 427, no. 2, pp. 79–87, 1999. View at Publisher · View at Google Scholar · View at Scopus
  17. S. J. Duthie, S. Narayanan, S. Blum, L. Pirie, and G. M. Brand, “Folate deficiency in vitro induces uracil misincorporation and DNA hypomethylation and inhibits DNA excision repair in immortalized normal human colon epithelial cells,” Nutrition and Cancer, vol. 37, no. 2, pp. 245–251, 2000. View at Google Scholar · View at Scopus
  18. S. J. Duthie and A. Hawdon, “DNA instability (strand breakage, uracil misincorporation, and defective repair) is increased by folic acid depletion in human lymphocytes in vitro,” The FASEB Journal, vol. 12, no. 14, pp. 1491–1497, 1998. View at Google Scholar · View at Scopus
  19. I. I. Kruman, T. S. Kumaravel, A. Lohani et al., “Folic acid deficiency and homocysteine impair DNA repair in hippocampal neurons and sensitize them to amyloid toxicity in experimental models of Alzheimer's disease,” Journal of Neuroscience, vol. 22, no. 5, pp. 1752–1762, 2002. View at Google Scholar · View at Scopus
  20. A. Unnikrishnan, T. M. Prychitko, H. V. Patel et al., “Folate deficiency regulates expression of DNA polymerase β in response to oxidative stress,” Free Radical Biology and Medicine, vol. 50, no. 2, pp. 270–280, 2011. View at Publisher · View at Google Scholar · View at Scopus
  21. D. C. Cabelof, J. J. Raffoul, J. Nakamura, D. Kapoor, H. Abdalla, and A. R. Heydari, “Imbalanced base excision repair in response to folate deficiency is accelerated by polymerase β haploinsufficiency,” The Journal of Biological Chemistry, vol. 279, no. 35, pp. 36504–36513, 2004. View at Publisher · View at Google Scholar · View at Scopus
  22. R. C. Menzies, P. E. Crossen, P. H. Fitzgerald, and F. W. Gunz, “Cytogenetic and cytochemical studies on marrow cells in B 12 and folate deficiency,” Blood, vol. 28, no. 4, pp. 581–594, 1966. View at Google Scholar · View at Scopus
  23. P. B. Jacky, B. Beek, and G. R. Sutherland, “Fragile sites in chromosomes: possible model for the study of spontaneous chromosome breakage,” Science, vol. 220, no. 4592, pp. 69–70, 1983. View at Google Scholar · View at Scopus
  24. J. J. Yunis and A. L. Soreng, “Constitutive fragile sites and cancer,” Science, vol. 226, no. 4679, pp. 1199–1204, 1984. View at Google Scholar · View at Scopus
  25. G. R. Sutherland, “Heritable fragile sites on human chromosomes. I. Factors affecting expression in lymphocyte culture,” American Journal of Human Genetics, vol. 31, no. 2, pp. 125–135, 1979. View at Google Scholar · View at Scopus
  26. C. Fonatsch, “A simple method to demonstrate the fragile X chromosome in fibroblasts,” Human Genetics, vol. 59, no. 2, article 186, 1981. View at Google Scholar · View at Scopus
  27. H. Nilsen, G. Stamp, S. Andersen et al., “Gene-targeted mice lacking the Ung uracil-DNA glycosylase develop B-cell lymphomas,” Oncogene, vol. 22, no. 35, pp. 5381–5386, 2003. View at Publisher · View at Google Scholar · View at Scopus
  28. M. Endres, D. Biniszkiewicz, R. W. Sobol et al., “Increased postischemic brain injury in mice deficient in uracil-DNA glycosylase,” Journal of Clinical Investigation, vol. 113, no. 12, pp. 1711–1721, 2004. View at Publisher · View at Google Scholar · View at Scopus
  29. G. Kronenberg, C. Harms, R. W. Sobol et al., “Folate deficiency induces neurodegeneration and brain dysfunction in mice lacking uracil DNA glycosylase,” Journal of Neuroscience, vol. 28, no. 28, pp. 7219–7230, 2008. View at Publisher · View at Google Scholar · View at Scopus
  30. C. Rada, J. M. Di Noia, and M. S. Neuberger, “Mismatch recognition and uracil excision provide complementary paths to both Ig switching and the A/T-focused phase of somatic mutation,” Molecular Cell, vol. 16, no. 2, pp. 163–171, 2004. View at Publisher · View at Google Scholar · View at Scopus
  31. Q. An, P. Robins, T. Lindahl, and D. E. Barnes, “C→T mutagenesis and γ-radiation sensitivity due to deficiency in the Smug1 and Ung DNA glycosylases,” The EMBO Journal, vol. 24, no. 12, pp. 2205–2213, 2005. View at Publisher · View at Google Scholar · View at Scopus
  32. A. Klungland, I. Rosewell, S. Hollenbach et al., “Accumulation of premutagenic DNA lesions in mice defective in removal of oxidative base damage,” Proceedings of the National Academy of Sciences of the United States of America, vol. 96, no. 23, pp. 13300–13305, 1999. View at Publisher · View at Google Scholar · View at Scopus
  33. O. Minowa, T. Arai, M. Hirano et al., “Mmh/Ogg1 gene inactivation results in accumulation of 8-hydroxyguanine in mice,” Proceedings of the National Academy of Sciences of the United States of America, vol. 97, no. 8, pp. 4156–4161, 2000. View at Publisher · View at Google Scholar · View at Scopus
  34. M. Kunisada, K. Sakumi, Y. Tominaga et al., “8-Oxoguanine formation induced by chronic UVB exposure makes Ogg1 knockout mice susceptible to skin carcinogenesis,” Cancer Research, vol. 65, no. 14, pp. 6006–6010, 2005. View at Publisher · View at Google Scholar · View at Scopus
  35. N. Yang, H. Galick, and S. S. Wallace, “Attempted base excision repair of ionizing radiation damage in human lymphoblastoid cells produces lethal and mutagenic double strand breaks,” DNA Repair, vol. 3, no. 10, pp. 1323–1334, 2004. View at Publisher · View at Google Scholar · View at Scopus
  36. Y. Xie, H. Yang, C. Cunanan et al., “Deficiencies in mouse Myh and Ogg1 result in tumor predisposition and G to T mutations in codon 12 of the K-ras oncogene in lung tumors,” Cancer Research, vol. 64, no. 9, pp. 3096–3102, 2004. View at Publisher · View at Google Scholar · View at Scopus
  37. S. Hirano, Y. Tominaga, A. Ichinoe et al., “Mutator phenotype of MUTYH-null mouse embryonic stem cells,” The Journal of Biological Chemistry, vol. 278, no. 40, pp. 38121–38124, 2003. View at Publisher · View at Google Scholar · View at Scopus
  38. B. P. Engelward, G. Weeda, M. D. Wyatt et al., “Base excision repair deficient mice lacking the Aag alkyladenine DNA glycosylase,” Proceedings of the National Academy of Sciences of the United States of America, vol. 94, no. 24, pp. 13087–13092, 1997. View at Publisher · View at Google Scholar · View at Scopus
  39. R. F. Branda, J. P. O'Neill, E. M. Brooks, C. Powden, S. J. Naud, and J. A. Nicklas, “The effect of dietary folic acid deficiency on the cytotoxic and mutagenic responses to methyl methanesulfonate in wild-type and in 3-methyladenine DNA glycosylase-deficient Aag null mice,” Mutation Research, vol. 615, no. 1-2, pp. 12–17, 2007. View at Publisher · View at Google Scholar · View at Scopus
  40. L. B. Meira, C. A. Moroski-Erkul, S. L. Green et al., “Aag-initiated base excision repair drives alkylation-induced retinal degeneration in mice,” Proceedings of the National Academy of Sciences of the United States of America, vol. 106, no. 3, pp. 888–893, 2009. View at Publisher · View at Google Scholar · View at Scopus
  41. M. T. A. Ocampo, W. Chaung, D. R. Marenstein et al., “Targeted deletion of mNth1 reveals a novel DNA repair enzyme activity,” Molecular and Cellular Biology, vol. 22, no. 17, pp. 6111–6121, 2002. View at Publisher · View at Google Scholar · View at Scopus
  42. M. Takao, S. I. Kanno, T. Shiromoto et al., “Novel nuclear and mitochondrial glycosylases revealed by disruption of the mouse Nth1 gene encoding an endonuclease III homolog for repair of thymine glycols,” The EMBO Journal, vol. 21, no. 13, pp. 3486–3493, 2002. View at Publisher · View at Google Scholar · View at Scopus
  43. N. Yang, M. A. Chaudhry, and S. S. Wallace, “Base excision repair by hNTH1 and hOGG1: a two edged sword in the processing of DNA damage in γ-irradiated human cells,” DNA Repair, vol. 5, no. 1, pp. 43–51, 2006. View at Publisher · View at Google Scholar · View at Scopus
  44. B. Karahalil, N. C. de Souza-Pinto, J. L. Parsons, R. H. Elder, and V. A. Bohr, “Compromised incision of oxidized pyrimidines in liver mitochondria of mice deficient in NTH1 and OGG1 glycosylases,” The Journal of Biological Chemistry, vol. 278, no. 36, pp. 33701–33707, 2003. View at Publisher · View at Google Scholar · View at Scopus
  45. D. Cortázar, C. Kunz, J. Selfridge et al., “Embryonic lethal phenotype reveals a function of TDG in maintaining epigenetic stability,” Nature, vol. 470, no. 7334, pp. 419–423, 2011. View at Publisher · View at Google Scholar · View at Scopus
  46. C. B. Millar, J. Guy, O. J. Sansom et al., “Enhanced CpG mutability and tumorigenesis in MBD4-deficient mice,” Science, vol. 297, no. 5580, pp. 403–405, 2002. View at Publisher · View at Google Scholar · View at Scopus
  47. O. J. Sansom, J. Zabkiewicz, S. M. Bishop, J. Guy, A. Bird, and A. R. Clarke, “MBD4 deficiency reduces the apoptotic response to DNA-damaging agents in the murine small intestine,” Oncogene, vol. 22, no. 46, pp. 7130–7136, 2003. View at Publisher · View at Google Scholar · View at Scopus
  48. M. Kucherlapati, K. Yang, M. Kuraguchi et al., “Haploinsufficiency of Flap endonuclease (Fen1) leads to rapid tumor progression,” Proceedings of the National Academy of Sciences of the United States of America, vol. 99, no. 15, pp. 9924–9929, 2002. View at Publisher · View at Google Scholar · View at Scopus
  49. E. Larsen, C. Gran, B. E. Sæther, E. Seeberg, and A. Klungland, “Proliferation failure and gamma radiation sensitivity of Fen1 null mutant mice at the blastocyst stage,” Molecular and Cellular Biology, vol. 23, no. 15, pp. 5346–5353, 2003. View at Publisher · View at Google Scholar · View at Scopus
  50. L. B. Meira, S. Devaraj, G. E. Kisby et al., “Heterozygosity for the mouse Apex gene results in phenotypes associated with oxidative stress,” Cancer Research, vol. 61, no. 14, pp. 5552–5557, 2001. View at Google Scholar · View at Scopus
  51. J. Huamani, C. A. McMahan, D. C. Herbert et al., “Spontaneous mutagenesis is enhanced in Apex heterozygous mice,” Molecular and Cellular Biology, vol. 24, no. 18, pp. 8145–8153, 2004. View at Publisher · View at Google Scholar · View at Scopus
  52. D. L. Cheo, L. B. Meira, D. K. Burns, A. M. Reis, T. Issac, and E. C. Friedberg, “Ultraviolet B radiation-induced skin cancer in mice defective in the Xpc, Trp53, and Apex (HAP1) genes: genotype-specific effects on cancer predisposition and pathology of tumors,” Cancer Research, vol. 60, no. 6, pp. 1580–1584, 2000. View at Google Scholar · View at Scopus
  53. R. S. Tebbs, M. L. Flannery, J. J. Meneses et al., “Requirement for the Xrcc1 DNA base excision repair gene during early mouse development,” Developmental Biology, vol. 208, no. 2, pp. 513–529, 1999. View at Publisher · View at Google Scholar · View at Scopus
  54. D. R. McNeill, P. C. Lin, M. G. Miller et al., “XRCC1 haploinsufficiency in mice has little effect on aging, but adversely modifies exposure-dependent susceptibility,” Nucleic Acids Research, vol. 39, no. 18, pp. 7992–8004, 2011. View at Publisher · View at Google Scholar
  55. H. Saribasak, R. W. Maul, Z. Cao et al., “XRCC1 suppresses somatic hypermutation and promotes alternative nonhomologous end joining in Igh genes,” The Journal of Experimental Medicine, vol. 208, no. 11, pp. 2209–2216, 2011. View at Publisher · View at Google Scholar
  56. R. S. Tebbs, L. H. Thompson, and J. E. Cleaver, “Rescue of Xrcc1 knockout mouse embryo lethality by transgene-complementation,” DNA Repair, vol. 2, no. 12, pp. 1405–1417, 2003. View at Publisher · View at Google Scholar · View at Scopus
  57. D. C. Cabelof, Z. Guo, J. J. Raffoul et al., “Base excision repair deficiency caused by polymerase β haploinsufficiency: accelerated DNA damage and increased mutational response to carcinogens,” Cancer Research, vol. 63, no. 18, pp. 5799–5807, 2003. View at Google Scholar · View at Scopus
  58. D. C. Cabelof, Y. Ikeno, A. Nyska et al., “Haploinsufficiency in DNA polymerase β increases cancer risk with age and alters mortality rate,” Cancer Research, vol. 66, no. 15, pp. 7460–7465, 2006. View at Publisher · View at Google Scholar · View at Scopus
  59. L. F. Ventrella-Lucente, A. Unnikrishnan, A. B. Pilling et al., “Folate deficiency provides protection against colon carcinogenesis in DNA polymerase β haploinsufficient mice,” The Journal of Biological Chemistry, vol. 285, no. 25, pp. 19246–19258, 2010. View at Publisher · View at Google Scholar · View at Scopus
  60. D. Allen, D. C. Herbert, C. A. McMahan et al., “Mutagenesis is elevated in male germ cells obtained from DNA polymerase-beta heterozygous mice,” Biology of Reproduction, vol. 79, no. 5, pp. 824–831, 2008. View at Publisher · View at Google Scholar · View at Scopus
  61. D. J. Bentley, J. Selfridge, J. K. Millar et al., “DNA ligase I is required for fetal liver erythropoiesis but is not essential for mammalian cell viability,” Nature Genetics, vol. 13, no. 4, pp. 489–491, 1996. View at Publisher · View at Google Scholar · View at Scopus
  62. N. Puebla-Osorio, D. B. Lacey, F. W. Alt, and C. Zhu, “Early embryonic lethality due to targeted inactivation of DNA ligase III,” Molecular and Cellular Biology, vol. 26, no. 10, pp. 3935–3941, 2006. View at Publisher · View at Google Scholar · View at Scopus
  63. S. G. Widen, P. Kedar, and S. H. Wilson, “Human β-polymerase gene. Structure of the 5′-flanking region and active promoter,” The Journal of Biological Chemistry, vol. 263, no. 32, pp. 16992–16998, 1988. View at Google Scholar · View at Scopus
  64. R. W. Sobolt, M. Kartalou, K. H. Almeida et al., “Base excision repair intermediates induce p53-independent cytotoxic and genotoxic responses,” The Journal of Biological Chemistry, vol. 278, no. 41, pp. 39951–39959, 2003. View at Publisher · View at Google Scholar · View at Scopus
  65. I. P. Pogribny, A. G. Basnakian, B. J. Miller, N. G. Lopatina, L. A. Poirier, and S. J. James, “Breaks in genomic DNA and within the p53 gene are associated with hypomethylation in livers of folate/methyl-deficient rats,” Cancer Research, vol. 55, no. 9, pp. 1894–1901, 1995. View at Google Scholar · View at Scopus
  66. C. Courtemanche, A. C. Huang, I. Elson-Schwab, N. Kerry, B. Y. Ng, and B. N. Ames, “Folate deficiency and ionizing radiation cause DNA breaks in primary human lymphocytes: a comparison,” The FASEB Journal, vol. 18, no. 1, pp. 209–211, 2004. View at Google Scholar · View at Scopus
  67. H. K. Lindberg, X. Wang, H. Järventaus, G. C. M. Falck, H. Norppa, and M. Fenech, “Origin of nuclear buds and micronuclei in normal and folate-deprived human lymphocytes,” Mutation Research, vol. 617, no. 1-2, pp. 33–45, 2007. View at Publisher · View at Google Scholar · View at Scopus
  68. A. J. MacFarlane, C. A. Perry, M. F. McEntee, D. M. Lin, and P. J. Stover, “Shmt1 heterozygosity impairs folate-dependent thymidylate synthesis capacity and modifies risk of Apcmin-mediated intestinal cancer risk,” Cancer Research, vol. 71, no. 6, pp. 2098–2107, 2011. View at Publisher · View at Google Scholar · View at Scopus
  69. D. H. Kim, S. A. Smith-Warner, D. Spiegelman et al., “Pooled analyses of 13 prospective cohort studies on folate intake and colon cancer,” Cancer Causes and Control, vol. 21, no. 11, pp. 1919–1930, 2010. View at Publisher · View at Google Scholar · View at Scopus
  70. J. B. Mason, “Folate, cancer risk, and the Greek god, Proteus: a tale of two chameleons,” Nutrition Reviews, vol. 67, no. 4, pp. 206–212, 2009. View at Publisher · View at Google Scholar · View at Scopus
  71. G. Varela-Moreiras and J. Selhub, “Long-term folate deficiency alters folate content and distribution differentially in rat tissues,” Journal of Nutrition, vol. 122, no. 4, pp. 986–991, 1992. View at Google Scholar · View at Scopus
  72. R. K. Le Leu, G. P. Young, and G. H. McIntosh, “Folate deficiency diminishes the occurrence of aberrant crypt foci in the rat colon but does not alter global DNA methylation status,” Journal of Gastroenterology and Hepatology, vol. 15, no. 10, pp. 1158–1164, 2000. View at Publisher · View at Google Scholar · View at Scopus
  73. R. K. Le Leu, G. P. Young, and G. H. McIntosh, “Folate deficiency reduces the development of colorectal cancer in rats,” Carcinogenesis, vol. 21, no. 12, pp. 2261–2265, 2000. View at Google Scholar · View at Scopus
  74. H. Ghandour, B. F. Lin, S. W. Choi, J. B. Mason, and J. Selhub, “Folate status and age affect the accumulation of L-isoaspartyl residues in rat liver proteins,” Journal of Nutrition, vol. 132, no. 6, pp. 1357–1360, 2002. View at Google Scholar · View at Scopus
  75. S. W. Choi, S. Friso, G. G. Dolnikowski et al., “Biochemical and molecular aberrations in the rat colon due to folate depletion are age-specific,” Journal of Nutrition, vol. 133, no. 4, pp. 1206–1212, 2003. View at Google Scholar · View at Scopus
  76. G. M. Lindzon, A. Medline, K. J. Sohn, F. Depeint, R. Croxford, and Y. I. Kim, “Effect of folic acid supplementation on the progression of colorectal aberrant crypt foci,” Carcinogenesis, vol. 30, no. 9, pp. 1536–1543, 2009. View at Publisher · View at Google Scholar · View at Scopus
  77. J. Song, A. Medline, J. B. Mason, S. Gallinger, and Y. I. Kim, “Effects of dietary folate on intestinal tumorigenesis in the ApcMin mouse,” Cancer Research, vol. 60, no. 19, pp. 5434–5440, 2000. View at Google Scholar · View at Scopus
  78. E. D. Ciappio, Z. Liu, R. S. Brooks et al., “Maternal B vitamin supplementation from preconception through weaning suppresses intestinal tumorigenesis in Apc1638N mouse offspring,” Gut, vol. 60, no. 12, pp. 1695–1702, 2011. View at Publisher · View at Google Scholar
  79. I. P. Pogribny, B. J. Miller, and S. J. James, “Alterations in hepatic p53 gene methylation patterns during tumor progression with folate/methyl deficiency in the rat,” Cancer Letters, vol. 115, no. 1, pp. 31–38, 1997. View at Publisher · View at Google Scholar · View at Scopus
  80. J. Trasler, L. Deng, S. Melnyk et al., “Impact of Dnmt1 deficiency, with and without low folate diets, on tumor numbers and DNA methylation in min mice,” Carcinogenesis, vol. 24, no. 1, pp. 39–45, 2003. View at Publisher · View at Google Scholar · View at Scopus
  81. E. Knock, L. Deng, Q. Wu, D. Leclerc, X. L. Wang, and R. Rozen, “Low dietary folate initiates intestinal tumors in mice, with altered expression of G2-M checkpoint regulators polo-like kinase 1 and cell Division cycle 25c,” Cancer Research, vol. 66, no. 21, pp. 10349–10356, 2006. View at Publisher · View at Google Scholar · View at Scopus
  82. S. J. Duthie, G. Grant, L. P. Pirie, A. J. Watson, and G. P. Margison, “Folate deficiency alters hepatic and colon MGMT and OGG-1 DNA repair protein expression in rats but has no effect on genome-wide DNA methylation,” Cancer Prevention Research, vol. 3, no. 1, pp. 92–100, 2010. View at Publisher · View at Google Scholar · View at Scopus
  83. Y. I. Kim, R. N. Salomon, F. Graeme-Cook et al., “Dietary folate protects against the development of macroscopic colonic neoplasia in a dose responsive manner in rats,” Gut, vol. 39, no. 5, pp. 732–740, 1996. View at Google Scholar · View at Scopus
  84. Z. Liu, E. D. Ciappio, J. W. Crott et al., “Combined inadequacies of multiple B vitamins amplify colonic Wnt signaling and promote intestinal tumorigenesis in BAT-LacZxApc1638N mice,” The FASEB Journal, vol. 25, no. 9, pp. 3136–3145, 2011. View at Publisher · View at Google Scholar
  85. C. D. Davis and E. O. Uthus, “Dietary folate and selenium affect dimethylhydrazine-induced aberrant crypt formation, global DNA methylation and one-carbon metabolism in rats,” Journal of Nutrition, vol. 133, no. 9, pp. 2907–2914, 2003. View at Google Scholar · View at Scopus
  86. K. S. Al-Numair, M. I. Waly, A. Ali et al., “Dietary folate protects against azoxymethane-induced aberrant crypt foci development and oxidative stress in rat colon,” Experimental Biology and Medicine, vol. 236, no. 9, pp. 1005–1011, 2011. View at Publisher · View at Google Scholar
  87. T. A. Graubert, P. Cahan, D. Edwin et al., “A high-resolution map of segmental DNA copy number variation in the mouse genome,” PLoS Genetics, vol. 3, no. 1, article e3, 2007. View at Publisher · View at Google Scholar · View at Scopus
  88. P. Cahan, Y. Li, M. Izumi, and T. A. Graubert, “The impact of copy number variation on local gene expression in mouse hematopoietic stem and progenitor cells,” Nature Genetics, vol. 41, no. 4, pp. 430–437, 2009. View at Publisher · View at Google Scholar · View at Scopus
  89. D. C. Cabelof, “Haploinsufficiency in mouse models of DNA repair deficiency: modifiers of penetrance,” Cellular and Molecular Life Sciences, vol. 69, no. 5, pp. 727–740, 2012. View at Publisher · View at Google Scholar
  90. V. B. Holcomb, F. Rodier, Y. Choi et al., “Ku80 deletion suppresses spontaneous tumors and induces a p53-mediated DNA damage response,” Cancer Research, vol. 68, no. 22, pp. 9497–9502, 2008. View at Publisher · View at Google Scholar · View at Scopus