Transgenerational epigenetic inheritance results from incomplete erasure of parental epigenetic marks during epigenetic reprogramming at fertilization. The significance of this phenomenon, and the mechanism by which it occurs, remains obscure. Here, we show that genetic mutations in Drosophila may cause epigenetic alterations that, when inherited, influence tumor susceptibility of the offspring. We found that many of the mutations that affected tumorigenesis induced by a hyperactive JAK kinase, HopTum-l, also modified the tumor phenotype epigenetically, such that the modification persisted even in the offspring that did not inherit the modifier mutation. We analyzed mutations of the transcription repressor Krüppel (Kr), which is one of the hopTum-l enhancers known to affect ftz transcription. We demonstrate that the Kr mutation causes increased DNA methylation in the ftz promoter region, and that the aberrant ftz transcription and promoter methylation are both transgenerationally heritable if HopTum-l is present in the oocyte. These results suggest that genetic mutations may alter epigenetic markings in the form of DNA methylation, which are normally erased early in the next generation, and that JAK overactivation disrupts epigenetic reprogramming and allows inheritance of epimutations that influence tumorigenesis in future generations.
It is well known that many genetic mutations in oncogenes or tumor suppressors can cause or greatly increase a person's susceptibility to cancer. It is generally assumed that persons should feel relieved if they have not inherited the particular “cancer-causing” mutation carried by their parents. However, we found that, under certain circumstances, fruit flies carrying tumor suppressor gene mutations can pass the increased tumor risk to all offspring, even those that have not inherited the particular mutation. A likely scenario is that many genetic mutations can lead to epigenetic alterations, that is, changes in the chemical modifications of DNA or the proteins that bind to DNA in the chromosomes, and these changes can have global effects on cell function. Normally, these epigenetic alterations are wiped out and reset in the early embryo, but under certain circumstances such alterations can be inherited. Interestingly, we found evidence that a particular oncoprotein, an overactivated form of a cell-signaling molecule called JAK kinase, can counteract the epigenetic resetting program that normally operates in the early embryo. Thus, the failure of epigenetic reprogramming allows the inheritance of parental epigenetic alterations that affect susceptibility to tumors.
Citation: Xing Y, Shi S, Le L, Lee CA, Silver-Morse L, et al. (2007) Evidence for Transgenerational Transmission of Epigenetic Tumor Susceptibility in Drosophila. PLoS Genet 3(9): e151. doi:10.1371/journal.pgen.0030151
Editor: Harmit S. Malik, Fred Hutchinson Cancer Research Center, United States of America
Received: April 3, 2007; Accepted: July 19, 2007; Published: September 7, 2007
Copyright: © 2007 Xing et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This study was supported in part by National Institutes of Health grants (R01GM077046 and R01GM65774) and an American Cancer Society Research Scholar Grant (RSG-06-196-01-TBE) to WXL. WXL was supported by a Leukemia and Lymphoma Society Career Development Program Scholar Grant (1087–08).
Competing interests: The authors have declared that no competing interests exist.
Abbreviations: 5-aza-dC, 5-aza-2′-deoxycytidine; C, cytosine; G, guanine; HDAC, histone deacetylase; T, thymidine; TI, tumor index; TSA, tricostatin A
Epigenetic regulation of gene expression refers to repression or activation of gene expression via covalent modifications of DNA or histones, such as methylation or acetylation, without changing the DNA sequence of the gene [1–3]. Epigenetic modifications are usually stably heritable through subsequent cell divisions, resulting in permanent changes in gene expression profiles, such as those associated with terminal differentiation. However, at critical stages in normal development or disease situations, cells undergo genome-wide epigenetic reprogramming, erasing preexisting epigenetic marks and establishing a new set of marks. For instance, major epigenetic reprogramming occurs at fertilization prior to zygotic development, at dedifferentiation that leads to cancer development, and during somatic cell nuclear transfer, a procedure used for cloning or obtaining embryonic stem cells [4–7].
However, epigenetic marks are not always completely erased from one generation to the next. For instance, genomic imprinting, where clusters of genes or whole chromosomes are preferentially inactivated depending on their parental origin [8,9], can be considered an exception to epigenetic reprogramming, because in this case parental epigenetic markings are retained in the zygote. Loss of imprinting has been shown to increase the likelihood that cancer will develop [10–12]. Furthermore, human diseases, such as Prader-Willi and Angelman syndromes  and hereditary nonpolyposis colorectal cancer , are associated with germline inheritance of epimutations. Though transgenerational epigenetic inheritance has been documented for a variety of eukaryotic organisms ranging from plants to humans , the precise mechanisms that regulate epigenetic marking and erasure, as well as those that protect certain epigenetic marks from being reset, are not clear.
We have previously undertaken a genetic approach in order to identify genes that are important for hopTum-l-induced tumorigenesis in Drosophila, and in the process, have found that JAK signaling globally counteracts heterochromatin formation . Further analyses of the identified mutations indicated that a number of those mutations that genetically modify hopTum-l tumorigenicity also do so epigenetically. In fact, hopTum-l itself plays an essential role in the maintenance of parental origin epigenetic alterations that subsequently affect tumorigenesis in a transgenerational manner. These results indicate a novel function for the hopTum-l oncogene: it interferes with the epigenetic reprogramming process.
Paternal-Effect Modification of Tum-l Tumorigenicity
We previously conducted a genetic screen for modifiers of the hopTum-l hematopoietic tumorigenic phenotype and identified 37 modifier mutations [M(Tum-l)] that dominantly enhanced or suppressed hopTum-l tumorigenesis in hopTum-l/+; M(Tum-l)/+ transheterozygotes . Hematopoietic tumors in hopTum-l-containing flies were quantified by tumor index (TI) (see Materials and Methods and also ). Interestingly, many of the M(Tum-l) mutations (24/37) exhibited paternal-effect modification of hopTum-l tumorigenicity, such that when hopTum-l/+ females were mated to males heterozygous for the modifier mutation (M[Tum-l]/+), tumorigenesis associated with hopTum-l was modified (enhanced or suppressed) in the F1 generation regardless of the inheritance of M(Tum-l) (Table 1). The transgenerational effects were confirmed with rebalanced stocks, indicating that they are unlikely to be due to different genetic backgrounds. Since little or no paternal cytoplasmic proteins are carried in the sperm, the observed paternal effects on the zygote suggest an epigenetic mechanism. Possibly, the M(Tum-l) mutations caused epigenetic alterations in the paternal chromosomes and these epigenetic changes were maintained through male meiosis and transmitted to the F1 generation, thereby influencing hopTum-l tumorigenicity.
Genetic and Epigenetic Modification of hopTum-l Tumorigenicitydoi:10.1371/journal.pgen.0030151.t001
Transgenerational Tumor Modification Depends on Maternal hopTum-l Mutation
To understand the nature of the transgenerational epigenetic modification of hopTum-l tumorigenicity by the M(Tum-l) mutations, we conducted a detailed analysis of Kr, which is one of the first zygotically transcribed “gap” genes whose activity is required for the correct segmentation of the embryo . First, we tested two loss-of-function alleles of Kr (Kr1 and Kr2) and found that they both enhanced hopTum-l genetically and epigenetically (Figure 1A; unpublished data), confirming Kr as an E(Tum-l) with epigenetic effects.
Figure 1. Epigenetic Enhancement of hopTum-l Tumorigenicity by Kr1 or TSA Treatment Requires Maternal hopTum-l
(A) Representative F1 progeny adult flies of indicated genotypes with blood tumors (black masses; arrows) in the abdomen are shown. The parents of these flies were hopTum-l/+ females and wild type males (left), or hopTum-l/+ females and Kr1/CyO males (center and right).
(B–D) The tumor indices of progeny flies (genotypes are indicated in bottom right) are shown as mean and standard deviation of at least three independent crosses. “Control cross F1” were from hopTum-l/+ crossed to wild type. Parental genotypes are indicated on the top. FM7 and CyO are marked balancer chromosomes for the X and second chromosomes carrying a wild-type copy of the hop and Kr genes, respectively. Note that when hopTum-l was inherited from the mother (B, D), but not from the father (C), Kr1 epigenetically enhanced hopTum-l tumorigenicity.
(E) Total protein extracts from adult flies raised on food containing 4.5 μM TSA were subjected to SDS-PAGE and blotted with anti-acetyl-H3. The membrane was stripped and reblotted with anti-H3 (full-length gel image is shown in Figure S1). Quantification of three independent blots is shown to the right.
(F) Tumor indices of F1 progeny from wild-type flies treated or untreated (control) with TSA and hopTum-l/+ females or males as shown. The F1 were raised in the absence of TSA. Tumors were counted in F1 that inherited hopTum-l. Note the parent-of-origin differential effects on the tumorigenesis of F1 flies. Three independent crosses with >200 progeny from each cross were counted. *, p < 0.01; **, p < 0.001, Student's t-test.doi:10.1371/journal.pgen.0030151.g001
To rule out any genetic background effects, we extensively outcrossed a Kr1 allele, and isogenized and rebalanced it over a CyO balancer chromosome that in previous testing showed no enhancement of hopTum-l (see Materials and Methods). The new iso-Kr1/CyO stock again enhanced hopTum-l tumorigenicity both genetically and epigenetically, such that when hopTum-l/+ females were crossed to iso-Kr1/CyO males both hopTum-l/+; Kr1/+ and hopTum-l/+; +/CyO progeny exhibited significantly higher TI (Figure 1B, columns 2 and 3). Interestingly, when F1 males of +/Y; +/CyO, which did not inherit Kr1, were backcrossed to hopTum-l/+ females, we found that the enhancement persisted in the F2 generation in the absence of Kr1, but diminished in the F3 (Figure 1B, columns 4 and 5). Since half and a quarter of the P0 paternal DNA contents (originally exposed Kr1) are inherited in the F2 and F3 generation, respectively, the diluting effect of the enhancement in the absence of the original mutation (Kr1) is consistent with the idea that the modification is epigenetic in nature and is distributed genome wide at multiple loci. To rule out the possibility that Kr1 induced genome-wide genetic mutations, we conducted the reciprocal cross, mating iso-Kr1/CyO females with rare escaper hopTum-l/Y males. We found that Kr1 enhanced hopTum-l only genetically but not epigenetically, such that the TI increased in hopTum-l/+; Kr1/+ but not in hopTum-l/+; +/CyO female progeny flies (Figure 1C). The result of the reciprocal cross confirms that the modification is epigenetic in nature, as genetic mutations (changes in DNA sequence) would not be reversible under normal circumstances. However, such a result could also suggest a parent-specific effect of Kr on the hopTum-l mutation.
To test whether the epigenetic effects of Kr1 are specific for the male genome, we mated hopTum-l/+; Kr1/CyO recombinant females to wild-type males. In this cross, the tumor phenotype associated with hopTum-l was enhanced in both hopTum-l/+; Kr1/+ and hopTum-l/+; CyO/+ progeny flies (Figure 1D), indicating that the presence of Kr1 in the female parent can also have epigenetic effects on hopTum-l tumorigenicity in the F1 generation. Thus, it appeared that Kr1 was capable of epigenetically altering both male and female genomes, and these alterations could be transmitted through both male and female meioses to the F1. However, the inheritance and/or ability of these parental origin alterations to modify hopTum-l tumorigenicity epigenetically in the F1 progeny appeared to depend on the presence of hopTum-l as a maternal mutation.
Transgenerational Epigenetic Effects of Histone Deacetylase Inhibitors on Tum-l Tumorigenicity
To further test the ability of maternal hopTum-l to maintain parental origin epigenetic changes, we examined the effects of histone deacetylase (HDAC) inhibitors on hopTum-l tumorigenicity. Since Rpd3, encoding an HDAC, was identified as one of the genes which, when mutated, exhibited both genetic and epigenetic enhancement of hopTum-l tumorigenicity (Table 1), we reasoned that the epigenetic effect of an Rpd3 mutation on hopTum-l tumorigenicity might be mimicked by HDAC inhibitors such as tricostatin A (TSA) and sodium butyrate. Indeed, TSA treatment caused increased levels of acetylated histone H3 (Figure 1E), and increased the tumor index of hopTum-l/+ flies from 0.38 to 0.96 ± 0.06 (p < 0.01). Consistent with a transgenerational epigenetic effect, when wild-type flies that had been treated with TSA were mated with untreated hopTum-l/+ females and the progeny were raised in the absence of the drug, the TI of hopTum-l/+ F1 progeny was also significantly increased (Figure 1F). As with Kr1, no epigenetic effect was found in the reciprocal cross (Figure 1F), suggesting that the presence of hopTum-l in the early embryo is important for TSA treatment to have a transgenerational epigenetic effect on hopTum-l tumorigenicity. A similar transgenerational epigenetic effect on hopTum-l tumorigenicity was also found with another HDAC inhibitor, sodium butyrate (unpublished data).
Maternal hopTum-l Mutation Maintains Krüppel Mutant Phenotypes in Its Absence
To investigate the maternal hopTum-l-dependent transgenerational inheritance of epigenetic changes at the level of gene expression, we examined the effects of hopTum-l on Kr-dependent expression of the pair-rule gene fushi-tarazu (ftz), which encodes a homeodomain protein required for embryonic patterning . It has been shown that Kr heterozygous embryos exhibit defects in ftz expression . In wild-type embryos, ftz is expressed in seven stripes at the onset of gastrulation (Figure 2A). In Kr1/+ embryos, however, ftz stripe 3 is narrow or weak (Figure 2B; also see ). The same ftz stripe 3 phenotype was found in Kr2/+ embryos (unpublished data). We wondered whether the defects in ftz expression might involve epigenetic alterations, and whether these defects could be passed to the next generation in the presence of maternal hopTum-l mutation. Indeed, we found that the ftz promoter region is differentially methylated in Kr heterozygotes (see below).
Figure 2. Maternal hopTum-l Maintains Kr1 Mutant Phenotypes in Absence of Kr1
ftz expression pattern in stage 4 embryos from a ftz-lacZ transgene carried on the CyO balancer chromosome was analyzed by anti-β-gal staining. Embryos were produced by crosses indicated to the left. Note the wild-type ftz expression pattern in (A) and (C). Also note that the ftz stripe 3 (arrow) is faint or missing Kr1 heterozygotes (B) or in progeny from hopTum-l/+ females and Kr1/ftz-lacZ males (D), which did not inherit Kr1.doi:10.1371/journal.pgen.0030151.g002
We reasoned that if hopTum-l promotes transmission of parental origin epigenetic alterations to the next generation, then the ftz stripe 3 defect caused by Kr1 could be retained in embryos from hopTum-l/+ mothers and Kr1/+ fathers that did not inherit Kr1. To test this, we examined ftz expression from a ftz-lacZ transgene carried on the CyO balancer chromosome, which contains the Kr+ allele and segregates from Kr1 in the F1 when Kr1/CyO ftz-lacZ flies are used as a parent. In embryos from male and female Kr1/CyO ftz-lacZ flies, 70% (n = 61/87) of the β-gal+ embryos exhibited the typical Kr1 heterozygous defects, characterized by weakened or narrowed stripe 3 expression (Figure 2B), suggesting that all embryos that are genotypically Kr1/CyO ftz-lacZ exhibit the stripe 3 defect. When Kr1/CyO ftz-lacZ flies were crossed to wild-type flies, in the F1 embryos, ftz-lacZ was expressed in seven stripes identical to those in the wild-type background, such that these stripes were more or less evenly spaced and similar in intensity (Figure 2A; n = 54). When hopTum-l females were mated to +/CyO ftz-lacZ males, we found wild-type ftz-lacZ pattern and no stripe 3 defects similar to those in Kr1 heterozygotes in the F1 embryos (Figure 2C; n = 78). Notably, although the JAK/STAT pathway is involved in regulating even-skipped stripe 3 expression [20,21], ftz expression seemed not affected in hopTum-l mutants. This is consistent with a lack of STAT-binding sites in the ftz promoter region (unpublished data). However, when Kr1/CyO ftz-lacZ males were mated to hopTum-l females, 94% of the F1 β-gal+ embryos retained the stripe 3 defect characteristic of Kr1 heterozygotes (Figure 2D; n = 48/51). Since in this mating scheme ftz-lacZ segregated from Kr1, embryos that expressed the ftz-lacZ trangene would not inherit Kr1 and were genotypically +/+ for the Kr locus. Thus, the presence of hopTum-l caused retention of the Kr1-specific defective ftz expression pattern in embryos that did not inherit the Kr1 mutation. These results demonstrate that hopTum-l can cause transgenerational inheritance of epigenetic changes at a transcriptional level.
Transgenerational Inheritance of Kr-Induced ftz Promoter Methylation
To identify the epigenetic alterations caused by Kr mutations, we examined the DNA methylation status of the 620-bp minimal ftz enhancer in the ftz-lacZ transgene, as the expression of this ftz-lacZ is epigenetically modified by Kr1. DNA methylation is the predominant epigenetic modification, and methylation of CpG islands is responsible for gene silencing and genomic imprinting in mammals [5–7]. There is evidence for the presence of DNA methylation in Drosophila [22,23]. Drosophila has a Dnmt2-like DNA methyltransferase that mediates methylation of cytosine residues in vivo , although the biochemical activity of Drosophila Dnmt2 as a DNA methyltransferase is still to be shown. Methylated cytosines in both CG and CT dinucleotides have been found in many transposons and repetitive sequences in Drosophila genomic DNA , and increased promoter DNA methylation is associated with gene silencing .
We first assessed the methylation status of the ftz minimal enhancer (Figure 3A) by digesting total genomic DNA with a methylation-sensitive restriction enzyme BstUI, which cuts unmethylated but not methylated CGCG sequences, followed by quantification of the undigested DNA by PCR. By comparing the time courses of BstUI digestion of genomic DNA samples isolated from Kr+/− versus wild-type control flies, we concluded that the former is more resistant to BstUI digestion (Figure 3B and 3C, top panels). Digestion of the same DNA samples with a methylation-insensitive restriction enzyme HaeIII produced no differences between the two samples (Figure 3B and 3C, bottom panels). These results suggest that the minimal enhancer of ftz-lacZ in Kr+/− flies is more methylated than in wild-type flies.
Figure 3. Increased Methylation of ftz Regulatory Region in Kr+/− Animals and Its Inheritance
(A) Schematic representation of the ftz-lacZ reporter, showing the minimal ftz 5′ regulatory region previously shown to be sufficient to drive expression of a ftz-lacZ reporter transgene in ftz patterns . Arrows above and below the horizontal line represent PCR primers used to amplify a 778-bp fragment, encompassing the 620-bp minimal ftz enhancer (see Figure S2 for sequence). Bent arrow indicates the start of the lacZ sequence. Vertical bars above and below the line represent positions of recognition sequences for restriction enzymes BstUI (CGCG) and HaeIII (GGCC), respectively.
(B–E) Time courses of restriction digests of genomic DNA with enzymes sensitive (BstUI) or insensitive (HaeIII) to methylated DNA are shown as agarose gel pictures and quantifications. Genomic DNA was isolated from Kr1/CyO ftz-lacZ and +/CyO ftz-lacZ (wild-type control) adult flies (B, C), or from the F1 progeny flies of Kr1/CyO ftz-lacZ males crossed to hopTum-l/+ females or wild-type females (D, E), and digested with the indicated enzymes for the indicated times (minutes). Digested DNA was amplified with PCR primers shown in (A) and run on an agarose gel. Note that the genomic DNA from Kr+/− flies or from the F1 progeny of hopTum-l/+ females and Kr1/CyO ftz-lacZ males is more resistant to BstUI digestion than the controls.
(F, G) Digested genomic DNA purified from embryos was immunoprecipitated by antibodies to methylated cytosine and amplified by PCR primers shown in (A). Embryos derived from wild-type or Kr+/− parents (F), or from Kr1/ftz-lacZ males crossed to wild-type (top) or Tum-l/+ (bottom) females (G) were used for DNA isolation. Note the presence of higher levels of 5-meC in the ftz-lacZ promoter in Kr+/− embryos or in those from Tum-l/+ females crossed to Kr1/ftz-lacZ males.doi:10.1371/journal.pgen.0030151.g003
We next investigated whether the Kr-dependent differential methylation of the ftz minimal enhancer can be passed to the next generation. We crossed Kr1/CyO ftz-lacZ flies to hopTum-l/+ and wild type females, respectively, and isolated genomic DNA from the F1 flies that inherited the ftz-lacZ transgene. We analyzed the methylation status of the 620-bp minimal ftz enhancer using methylation-sensitive and -insensitive restriction digests as described above. Indeed, we found the ftz enhancer in F1 flies of hopTum-l/+ females and Kr1/CyO ftz-lacZ males was more resistant to a methylation-sensitive restriction enzyme than the ftz enhancer in F1 flies of +/+ females and Kr1/CyO ftz-lacZ males (Figure 3D and 3E), consistent with the idea that hopTum-l promotes transgenerational inheritance of epigenetic changes.
We employed a second method to confirm that the promoter of the ftz-lacZ transgene has increased DNA methylation in Kr mutants and that this methylation status is transgenerationally inheritable in the presence of hopTum-l maternal mutation. We isolated total genomic DNA from embryos of different parental genotypes, digested with restriction enzymes, and incubated with antibodies against methylated cytosine. Quantification of immunoprecipitated DNA indicates that that the ftz-lacZ fragment was more methylated in embryos of Kr1/CyO ftz-lacZ flies (Figure 3F) and the higher levels of methylation was maintained in embryos from Kr1/CyO ftz-lacZ fathers and hopTum-l mothers (Figure 3G).
Finally, to further demonstrate the differential methylation of the ftz minimal enhancer in different genetic backgrounds or pedigrees, we treated the genomic DNA samples with sodium bisulfite, which converts cytosines (C) to thymidines (T), and then cloned and sequenced independent clones for each sample. Sequencing results indicated the presence of two CG (or CT)-rich “islands” in the ftz minimal enhancer that are preferentially methylated in Kr+/− samples or in embryos of Kr1/CyO ftz-lacZ father and hopTum-l mothers (Figure 4). Thus, Kr mutations indeed induce epigenetic alterations, as exemplified by increased DNA methylation in the ftz minimal enhancer, and such alterations are normally erased, but are transmitted to the next generation if an overactivated JAK kinase is present in the early embryo.
Figure 4. Methylation of CG/T “Islands” in the ftz Minimal Enhancer
Genomic DNA isolated from animals of different genotypes was treated with sodium bisulfite and independent clones of the ftz-lacZ were sequenced. Sequencing results of two CG- or CT-rich boxes in the ftz minimal enhancer from animals of indicated genotypes are shown in red boxes, with the original sequences on top. Numbers above the sequences indicate positions from the forward PCR primer (see Figure S2 for primer sequence). Numbers to the left indicate sample numbers of independent clones. Unmethylated C's, which are converted to T's following bisulfite treatment, are indicated by open circles. Methylated C's, which remain as C's following bisulfite treatment, are represented as filled circles. (A) Genomic DNA was isolated from Kr1/CyO ftz-lacZ and +/CyO ftz-lacZ (wild-type control) adult flies (clones 1–15) and embryos (clones 16–20), and (B) from embryos of Kr1/CyO ftz-lacZ males crossed to hopTum-l/+ females or wild-type females. Note that there are more unconverted C's in lower panels, indicating higher levels of methylation in these samples. Low background levels (<1%) of unconverted C's were found in other regions for both samples. (C) Sample chromatograms with clone number indicated.doi:10.1371/journal.pgen.0030151.g004
5-Aza-dC Treatment Promotes Tumorigenesis but Inhibits the Epigenetic Effects of Kr on hopTum-l Tumorigenicity
Since the epigenetic effects of Kr mutations involve DNA methylation, we investigated the effects of inhibiting DNA methylation on the ability of Kr mutations in promoting hopTum-l tumorigenesis. We raised flies in food containing the DNA methyltransferase inhibitor 5-aza-2′-deoxycytidine (5-aza-dC) and determined the effects of drug treatment on hopTum-l–dependent blood tumor formation. When raised at 100 μM 5-aza-dC (a nonlethal dose), hopTum-l/+ flies exhibited dramatically increased tumors compared with untreated hopTum-l/+ flies, with TI increased from 0.41 ± 0.05 (untreated; n = 116) to 1.27 ± 0.15 (treated; n = 68; p < 0.001). Such results are in line with TSA treatment (see above). Similar to the effects of TSA treatment, when wild-type male flies raised in 5-aza-dC were crossed to hopTum-l/+ females and allowed to produce eggs in the absence of the drug, the F1 flies exhibited increased TIs (Figure 5), but no TI increase was detected in the reciprocal cross (unpublished data), suggesting a maternal hopTum-l-dependent transgenerational inheritance. Interestingly, we found that treatment with 5-aza-dC, although by itself promotes hopTum-l tumorigenesis, abolished the ability of Kr mutations to epigenetically enhance tumors, such that when Kr1/CyO male flies raised on 5-aza-dC food were crossed to hopTum-l/+ females, the epigenetic effects (associated with CyO), but not the genetic effects of Kr, were abolished (Figure 5). Thus, the DNA methylation methyltransferase inhibitor 5-aza-dC both promotes hopTum-l tumorigenesis and inhibits Kr epigenetic effects. These results suggest that hopTum-l-induced blood tumors can be both enhanced by a general loss of genomic DNA methylation and suppressed by preventing Kr mutation–induced methylation in specific promoters.
Figure 5. Effects of the Methyltransferase Inhibitor 5-Aza-dC on Tumorigenesis
Wild-type or Kr1/CyO flies were raised in food supplemented with (+) or without (−) 5-aza-dC. Male flies of indicated genotypes were then crossed to hopTum-l/+ females and the F1 was raised in regular food in the absence of 5-aza-dC. F1 flies of the indicated genotypes were scored for the presence of melanotic tumors. TIs are shown as average ± standard deviation. * indicates significant difference by Chi-squared test.doi:10.1371/journal.pgen.0030151.g005
We have investigated the effects of genetic and epigenetic mutations on the tumorigenicity of the Drosophila hematopoietic oncogene hopTum-l, and found that hopTum-l and its modifier mutations mutually influence each other, both genetically and epigenetically. In particular, we have shown that a Kr mutation that enhances hopTum-l tumorigenicity induces ftz promoter methylation, which is associated with repression of ftz stripe 3, and that Tum-l promotes transgenerational inheritance of ftz stripe 3 silencing in the F1 generation in the absence of the Kr mutation.
Taken together, these results suggest that the oncogenic JAK kinase encoded by hopTum-l is able to antagonize a cellular program that erases epigenetic markings of parental origin, allowing such epigenetic alterations to be maintained in the F1 even in the absence of the original genetic mutation. The epigenetic alterations in turn influence the risk of hopTum-l-induced tumorigenesis in the F1 generation.
Epigenetic Effects of hopTum-l Modifier Mutations
Many of the M(Tum-l) genes that exhibited paternal-effect modifications encode products with known chromatin remodeling functions. These include HP1, Rpd3, and several Suppressor of variegation (Su[var]) mutations. It is conceivable that flies heterozygous for these mutations have altered chromatin states that could directly influence the epigenetic state of the zygote, leading to paternal effects as shown recently in mice . However, the M(Tum-l) genes that exhibited epigenetic effects on Tum-l tumorigenicity also include those whose functions in chromatin modification are not obvious. These include transcription factors such as Kr and signaling molecules such as the Notch ligand Serrate (Ser). This observation suggests that genetic mutations in genes other than those encoding chromatin remodeling proteins may also cause epigenetic alterations.
Although Kr is expressed only in 20% of the early embryo, lacking Kr causes profound patterning defects, resulting in deletion or defects in over 70% of embryonic segments . As a first zygotically expressed “gap” gene, Kr is in the top tier of the regulatory hierarchy that controls pattern formation of the whole organism . Thus, Kr mutations can affect expression of genes that are not directly regulated by Kr. A Kr neomorphic allele (Krif) has been shown to affect eye development by an epigenetic mechanism . Our results indicate that the Kr mutation, which likely acts early on, results in the establishment of an epigenetic signature in the genome in the form of methylation of particular promoters, such as the ftz promoter. Repression of certain “tumor suppressor genes” may explain the enhancement of the hopTum-l tumorigenic phenotype by Kr mutations. As an epigenetic modification, DNA methylation is believed to be mitotically stable. In support of this notion, we detected similar methylation patterns in the ftz-lacZ promoter in embryos and adult flies of Kr heterozygotes (Figure 4). Although we have not directly examined germ cells, the transgenerational phenomenon suggests that the Kr-dependent epigenetic signature extends to germ cells, which give rise to sperm and eggs. We envision the possibility that the epigenetic signature of germ cells is established early together with somatic cells, and can be affected by mutations in Kr, which might have a global reach in the early embryo. Alternatively, there is constant communication between germ cells and somatic cells during animal development, such that their epigenetic states will stay in “sync.” The precise mechanisms by which germ cells acquire the epigenetic states of somatic cells remain to be investigated.
Requirement of Maternal hopTum-l for Inheritance of Epigenetic Mutations
When hopTum-l is inherited from the mother, its product, a hyperactive JAK kinase, is present in the embryo from the very beginning as a maternal contribution. In contrast, when inherited from the father, the hopTum-l gene product is not present in the early embryo but is expressed as a zygotic gene. Zygotic genes are not transcribed until the midblastula transition or later. The parent-of-origin effect of hopTum-l on the ability of Kr1 to modify its tumorigenicity suggests the following scenario. The M(Tum-l) mutations are capable of altering the state of the chromatin, resulting in epigenetic changes in the genome. These “epigenetic marks” can be maintained through mitosis and meiosis and transmitted to the F1 progeny, where they are normally erased in the zygote during early embryogenesis. However, the hopTum-l mutation, if present in the early embryo as a maternal-effect mutation, is able to preserve certain epigenetic alterations of parental origin. In other words, hopTum-l may play a role in counteracting a mechanism that erases epigenetic marks of parental origin during early embryogenesis.
Materials and Methods
Fly stocks and genetics.
All crosses were carried out at 25 °C on standard cornmeal/agar medium. All fly stocks, including hopTum-l, Kr alleles, CyO [ftz-lacZ], and the Bloomington Deficiency Kit Stocks, are from the Bloomington Drosophila Stock Center (http://flystocks.bio.indiana.edu/). Accession numbers for mutations used in this study are list in Table S1.
Hematopoietic tumors induced by hopTum-l were scored in adult flies, which manifest as melanotic masses most frequently found in the abdomen (see Figure 1A), but were also found in other parts of the body. Tumors of all sizes and locations were scored. Typically more than 200 progeny flies were scored for each cross. More than two independent crosses were scored and the results averaged. Tumorigenicity was quantified by TI, which is defined as the sum of tumor size times occurrence, and divided by the total number of flies of a particular genotype (TI = ∑[tumor size × n]/N, where n is the number of occurrences for a particular tumor size and N is the total number of flies counted for a particular genotype). Tumor size 1 is defined as a tumor with a diameter equal to the width of an average abdominal segment (see Figure 1A). TI 1.0 is equivalent to all flies of a category each having a 1.0 size tumor.
To eliminate genetic background effects, hopTum-l and Kr1 heterozygotes were outcrossed to a y1 w1 stock for ten generations. hopTum-l was monitored by the presence of melanotic tumors in the females in each generation. To recover Kr1 from the outcrossed progeny, ten y w virgin females were selected after five generations of outcrossing and individually crossed to a y1 w1; Sco/CyO ftz-lacZ stock (in y1 w1 background). Three males from the F1 of each cross were individually backcrossed to y1 w1; Sco/CyO ftz-lacZ flies (to maintain a stock) and the same male was testcrossed to Kr2/CyO flies. The presence of Kr1 was inferred by noncomplementation in the testcross, and a y1 w1; Kr1/CyO ftz-lacZ male was used to repeat the same outcrossing procedure one more round to establish an outcrossed y1 w1; Kr1/CyO ftz-lacZ stock.
Antibodies, drug treatment, and embryonic phenotypes.
Anti-H3Ac and anti-H3 (both from Upstate, http://www.upstate.com/) were used as 1:1,000 dilutions in Western blots, sheep anti-5-meCytidine (Abcam, http://www.abcam.com/) was used for precipitating methylated DNA. For treatment with HDAC or methyltransferase inhibitors, flies were cultured in food containing TSA (4.5 μM; Sigma, http://www.sigmaaldrich.com/), sodium butyrate (10 mM, Sigma), or 5-aza-dC (100 μM; MP Biomedicals, http://www.mpbio.com) at 25 °C. To detect β-gal expression from the ftz-lacZ transgene, mouse anti-β-gal (1:1,000; Promega, http://www.promega.com/) and a biotinylated secondary antibody and the ABC Elite Kit (Vector Laboratories, http://www.vectorlabs.com/) were used for whole-mount immunostaining of embryos. Signals were detected with DAB solution according to the manufacturer's recommendations. Stained embryos were dehydrated with ethanol, mounted with Euparal, and photographed with an Axiophot microscope using DIC optics.
Analyses of genomic DNA methylation.
Gemonic DNA was isolated using the DNeasy Tissue kit (Qiagen) according to the manufacturer's instructions with minor modifications. Thirty 1–2-d-old adult flies or 100 μl of 0–12-h embryos of desired genotypes were homogenized in 180 μl of PBS and 20 μl of proteinase K (1 mg/ml) per manufacturer's protocol. The samples were treated with DNase-free RNase A (Sigma) for 2 h at 37 °C prior to column purification. For restriction digests, 3 μg of genomic DNA was incubated with 10 units of BstUI (New England Biolabs, http://www.neb.com/) or 10 units of HaeIII (New England Biolabs) in 60 μl of total volume at 37 °C. At different time points, an aliquot of the digests was removed and heated at 80 °C to inactivate the restriction enzyme. One microliter of each sample was used for PCR amplification with primers specific to ftz-lacZ (forward: 5′-CCCAGGGATCGGACGTAATGTTAT-3′; reverse: 5′-GGATGTGCTGCAAGGCGATTAAGT-3′). Bisulfite treatment was carried out with the EpiTect Bisulfite Kit (Qiagen, http://www1.qiagen.com/) according to the manufacturer's instructions. Genomic DNA (2 μg) was treated in Bisulfite Mix. Treated genomic DNA was amplified with the following strand-specific primers (forward: 5′-TTTAGGGATTGGATGTAATGTTAT-3′; reverse: 5′-AAATATACTACAAAACAATTAAAT-3′). The PCR fragments were cloned into pGEM-T vectors (Promega) and independent plasmid DNA isolates were sequenced. Sequencing was carried out by Gene Gateway (http://www.genegateway.com/). For immunoprecipitation, genomic DNA was first digested to completion with EcoRI and BamHI (New England Biolabs). Digested genomic DNA (2 μg) in 200 μl was used for immunoprecipitation with 5 μl of anti-5-meC (Abcam) or control antibody at 4 °C overnight, together with protein-G beads that had been preabsorbed with sonicated single-stranded salmon sperm DNA. The antibody complex was centrifuged and washed and eluted. The presence of ftz-lacZ promoter sequence was quantified by PCR with the above primers.
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Figure S2. The ftz Minimal Enhancer
Partial sequence of the ftz-lacZ transgene is shown. PCR primers used in amplification of the genomic fragment are indicated in green and purple. Numbers correspond to nucleotide position of the PCR fragment. Two CG or CT-rich sequences are boxed in red.
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Table S1. Accession Numbers for Mutations Used in This Study
(21 KB XLS)
WXL conceived and designed the experiments and wrote the paper. YX, SS, LL, CAL, and LSM performed the experiments. YX, SS, LL, and LSM analyzed the data.
- 1. Grewal SI, Moazed D (2003) Heterochromatin and epigenetic control of gene expression. Science 301: 798–802.
- 2. Jaenisch R, Bird A (2003) Epigenetic regulation of gene expression: How the genome integrates intrinsic and environmental signals. Nat Genet 33(Suppl): 245–254.
- 3. Li E (2002) Chromatin modification and epigenetic reprogramming in mammalian development. Nat Rev Genet 3: 662–673.
- 4. Morgan HD, Santos F, Green K, Dean W, Reik W (2005) Epigenetic reprogramming in mammals. Hum Mol Genet 14(Spec No 1): R47–R58.
- 5. Reik W, Dean W, Walter J (2001) Epigenetic reprogramming in mammalian development. Science 293: 1089–1093.
- 6. Rideout WM 3rd, Eggan K, Jaenisch R (2001) Nuclear cloning and epigenetic reprogramming of the genome. Science 293: 1093–1098.
- 7. Surani MA (2001) Reprogramming of genome function through epigenetic inheritance. Nature 414: 122–128.
- 8. Verona RI, Mann MR, Bartolomei MS (2003) Genomic imprinting: Intricacies of epigenetic regulation in clusters. Annu Rev Cell Dev Biol 19: 237–259.
- 9. Wilkins JF, Haig D (2003) What good is genomic imprinting: The function of parent-specific gene expression. Nat Rev Genet 4: 359–368.
- 10. Falls JG, Pulford DJ, Wylie AA, Jirtle RL (1999) Genomic imprinting: Implications for human disease. Am J Pathol 154: 635–647.
- 11. Walter J, Paulsen M (2003) Imprinting and disease. Semin Cell Dev Biol 14: 101–110.
- 12. Sakatani T, Kaneda A, Iacobuzio-Donahue CA, Carter MG, de Boom Witzel S, et al. (2005) Loss of imprinting of Igf2 alters intestinal maturation and tumorigenesis in mice. Science 307: 1976–1978.
- 13. Buiting K, Gross S, Lich C, Gillessen-Kaesbach G, el-Maarri O, et al. (2003) Epimutations in Prader-Willi and Angelman syndromes: A molecular study of 136 patients with an imprinting defect. Am J Hum Genet 72: 571–577.
- 14. Chan TL, Yuen ST, Kong CK, Chan YW, Chan AS, et al. (2006) Heritable germline epimutation of MSH2 in a family with hereditary nonpolyposis colorectal cancer. Nat Genet 38: 1178–1183.
- 15. Chong S, Whitelaw E (2004) Epigenetic germline inheritance. Curr Opin Genet Dev 14: 692–696.
- 16. Shi S, Calhoun HC, Xia F, Li J, Le L, et al. (2006) JAK signaling globally counteracts heterochromatic gene silencing. Nat Genet 38: 1071–1076.
- 17. Wieschaus E, Nusslein-Volhard C, Kluding H (1984) Kruppel, a gene whose activity is required early in the zygotic genome for normal embryonic segmentation. Dev Biol 104: 172–186.
- 18. Weiner AJ, Scott MP, Kaufman TC (1984) A molecular analysis of fushi tarazu, a gene in Drosophila melanogaster that encodes a product affecting embryonic segment number and cell fate. Cell 37: 843–851.
- 19. Carroll SB, Scott MP (1986) Zygotically active genes that affect the spatial expression of the fushi tarazu segmentation gene during early Drosophila embryogenesis. Cell 45: 113–126.
- 20. Hou XS, Melnick MB, Perrimon N (1996) Marelle acts downstream of the Drosophila HOP/JAK kinase and encodes a protein similar to the mammalian STATs [published erratum appears in Cell 1996 Apr 19;85(2):following 290]. Cell 84: 411–419.
- 21. Yan R, Small S, Desplan C, Dearolf CR, Darnell JE Jr. (1996) Identification of a Stat gene that functions in Drosophila development. Cell 84: 421–430.
- 22. Gowher H, Leismann O, Jeltsch A (2000) DNA of Drosophila melanogaster contains 5-methylcytosine. Embo J 19: 6918–6923.
- 23. Lyko F, Ramsahoye BH, Jaenisch R (2000) DNA methylation in Drosophila melanogaster. Nature 408: 538–540.
- 24. Kunert N, Marhold J, Stanke J, Stach D, Lyko F (2003) A Dnmt2-like protein mediates DNA methylation in Drosophila. Development 130: 5083–5090.
- 25. Salzberg A, Fisher O, Siman-Tov R, Ankri S (2004) Identification of methylated sequences in genomic DNA of adult Drosophila melanogaster. Biochem Biophys Res Commun 322: 465–469.
- 26. Ferres-Marco D, Gutierrez-Garcia I, Vallejo DM, Bolivar J, Gutierrez-Avino FJ, et al. (2006) Epigenetic silencers and Notch collaborate to promote malignant tumours by Rb silencing. Nature 439: 430–436.
- 27. Chong S, Vickaryous N, Ashe A, Zamudio N, Youngson N, et al. (2007) Modifiers of epigenetic reprogramming show paternal effects in the mouse. Nat Genet 39: 614–622.
- 28. Nusslein-Volhard C, Wieschaus E (1980) Mutations affecting segment number and polarity in Drosophila. Nature 287: 795–801.
- 29. Sollars V, Lu X, Xiao L, Wang X, Garfinkel MD, et al. (2003) Evidence for an epigenetic mechanism by which Hsp90 acts as a capacitor for morphological evolution. Nat Genet 33: 70–74.
- 30. Hiromi Y, Kuroiwa A, Gehring WJ (1985) Control elements of the Drosophila segmentation gene fushi tarazu. Cell 43: 603–613.