Abstract
DNA methylation is a key epigenetic modification in mammalian genomes and is dynamically regulated in development and diseases. While enzymes catalyzing DNA methylation have been well characterized, those involved in demethylation have remained elusive until recently. Mounting evidence now suggests that the TET proteins, a family of AlkB-like Fe(II)/α-ketoglutarate-dependent dioxygenases, initiate active DNA demethylation by oxidizing 5-methylcytosine (5mC) to generate 5-hydroxymethylcytosine (5hmC), 5-formylcytosine (5fC), and 5-carboxylcytosine (5caC). In this chapter, we discuss the molecular basis of DNA demethylation in mammalian genomes, focusing on TET proteins and TET-mediated oxidative DNA demethylation. Other potential DNA demethylation pathways are also summarized.
Access provided by CONRICYT-eBooks. Download chapter PDF
Similar content being viewed by others
Keywords
- DNA methylation
- DNA demethylation
- TET proteins
- Dioxygenase
- 5-methylcytosine
- 5-hydroxymethylcytosine
- 5-formylcytosine
- 5-carboxylcytosine
- TDG
1 Introduction
The chromatin of a multicellular organism stores a vast quantity of information that defines the complex gene expression patterns in diverse cell types, and is indispensable for growth and development. This information is stored both genetically in DNA sequences and epigenetically through DNA and histone modifications [1,2,3,4]. However, nearly all cells in an organism (except gametes and some immune cells) contain the same genomic sequences as the zygotic genome and therefore, it is the epigenetic information residing in chromatin that determines a cell’s identity and its corresponding gene expression profiles [5]. Generally, epigenetic information is faithfully propagated to each progeny cell upon division to maintain cell identity, but epigenetic states can also undergo dynamic changes during lineage specification or upon certain environmental stimuli [6]. Aberrant alterations of epigenetic information, such as DNA and histone modifications, are frequently associated with the onset of various human diseases, including cancers [7].
DNA methylation, in particular, is the most common covalent modification of DNA. The best-studied form of DNA methylation is 5-methylcytosine (5mC), which is generated by S-adenosyl-L-methionine (SAM)-dependent DNA methyltransferases (DNMTs), and does not interfere with Watson-Crick base pairing [8, 9]. In mammals, this enzymatically introduced DNA methylation exists predominantly in the CpG dinucleotide context (a cytosine followed by a guanine) and carries epigenetic information typically required for long-term gene silencing. Notably, over 70% of CpGs in somatic mammalian cells are methylated, therefore 5mC has long been the focus of compelling biochemical and genomics studies. In addition to 5mC, other forms of DNA methylation also exist. However, it is important to note that not all DNA methylation is the carrier of epigenetic information. For example, methylation can be introduced by endogenous or exogenous methylation agents-mediated DNA damage [9]. These methylated bases, such as N1-methyladenosine (m1A) and N3-methylcytosine (m3C), are considered cytotoxic or mutagenic as they tend to block or alter Watson-Crick base pairing. In the following sections, we will focus on the demethylation of 5mC, and will use the term DNA methylation to refer to 5mC only.
2 DNA Methylation Machinery
In mammals, three enzymatically active DNMTs, namely DNMT1, DNMT3A and DNMT3B, catalyze the transfer of a methyl group from SAM to the carbon-5 position of cytosine residues in DNA, generating 5mC [8]. DNMT1 preferentially methylates hemimethylated DNA [10], and in the presence of its cofactor UHRF1 (also known as NP95) [11, 12], DNMT1 is mainly responsible for copying DNA methylation patterns to the daughter strands during DNA replication (maintenance methylation). In contrast, DNMT3A and DNMT3B are the main enzymes to establish initial DNA methylation patterns during early embryonic development (de novo methylation), and do not show any preference for hemimethylated DNA [13]. Nevertheless, both maintenance and de novo methylation activities are required for normal development as depletion of DNMT1 or DNMT3B in mice results in embryonic lethality, and Dnmt3a-knockout mice die 4–8 weeks after birth [13, 14].
Structurally, the methyl group of 5mC is located in the major groove of DNA double helix, and is involved in either attracting or repelling many DNA binding proteins [15]. For example, three of the methyl-CpG binding domain (MBD) containing proteins, MeCP2, MBD1, MBD2, and a transcriptional regulator KAISO, have been shown to preferentially bind to methylated DNA and recruit repressor complexes to methylated promoters, leading to subsequent chromatin condensation and gene silencing [16]. On the contrary, DNA methylation can also prevent binding of some transcription factors (TFs), such as YY1 and CTCF [17, 18], to their specific recognition sites. DNA methylation has been demonstrated to play critical roles in various of cellular processes such as genomic imprinting, X-chromosome inactivation, retrotransposon silencing as well as maintenance of cell identity, supporting its general transcription repression function and heritable nature [15].
3 Passive and Active DNA Demethylation
While most histone modifications are readily reversible [19], DNA methylation has been generally viewed as a relatively stable epigenetic mark. Indeed, there is a dedicated maintenance enzyme, DNMT1, to faithfully copy DNA methylation patterns to daughter strands during DNA replication; in addition, the methyl group on 5mC is connected to the base through a C-C bond which exhibits high chemical stability under physiological conditions; furthermore, no DNA demethylase could be identified by 2009 when a large number of histone demethylases had been discovered. Nevertheless, studies in the past decade have indicated that DNA methylation is not as static as once thought. Loss of DNA methylation, or DNA demethylation, has been reported in various biological contexts and can be achieved through either passive or active mechanisms.
As illustrated in Fig. 1, passive DNA demethylation, or replication-dependent dilution of 5mC, refers to loss of 5mC instead of semi conservatively replicating methylation patterns during DNA replication. In the absence of functional maintenance methylation machinery, i.e., DNMT1 and UHRF1, successive cycles of DNA replication can result in gradual dilution of 5mC to achieve global DNA demethylation. Passive DNA demethylation has been demonstrated to play a major role in maternal-genome demethylation of zygotes [20,21,22], and in the whole-genome demethylation of primordial germ cells (PGCs) [23,24,25].
By contrast, active DNA demethylation refers to direct removal of the methyl group from 5mC, or an enzymatic process that removes or modifies 5mC with regeneration of unmodified cytosine. Processes that are initiated with active modification (AM) of 5mC can be further divided into two forms by whether the modified 5mC is converted to unmodified cytosine through passive dilution (PD) or active restoration (AR). Similar to passive DNA demethylation, the AM-PD pathway may be well suited for large-scale DNA demethylation events observed in PGCs and zygotes, which we will discuss in Sect. 4.4. However, the AM-AR pathway and direct removal of the methyl group or the 5mC base may take place rapidly, and are implicated in locus-specific demethylation which requires rapid response towards environmental stimuli. For example, rapid active DNA demethylation was observed at the interleukin-2 (IL-2) promoter-enhancer region in activated T lymphocytes within 20 minutes upon stimulation [26], at the promoter of brain-derived neurotrophic factor (BDNF) in KCl-stimulated postmitotic neurons without DNA replication [27], at several other specific genomic loci in response to nuclear hormone and growth factors [28,29,30]. Thus, these studies suggest that active DNA demethylation could function in the dynamic regulation of genes that require rapid responses to specific environmental stimuli.
4 TET-Mediated Oxidative DNA Demethylation
4.1 TET Family Dioxygenases
While passive DNA demethylation has long been understood and accepted, the mechanism of active DNA demethylation was not understood until recently, following the discovery that TET (ten-eleven translocation) proteins can convert 5mC to its oxidized forms, namely 5-hydroxymethylcytosine (5hmC), 5-formylcytosine (5fC), and 5-carboxylcytosine (5caC). Interestingly, the names of TET genes trace back to the involvement of the human TET1 gene in the ten-eleven translocation [t(10;11)(q22;q23)] in rare cases of acute myeloid leukemia (AML), which fuses the TET1 gene on chromosome 10 with the mixed-lineage leukemia gene (MLL; also known as KMT2A) on chromosome 11 [31, 32]. Along with TET1, two additional genes in this protein family, TET2 and TET3 are also identified based on their sequence homology. Sequence comparison and structural studies have shown that TET proteins are a distinct family of the Fe(II)/α-ketoglutarate (αKG)-dependent dioxygenase superfamily [33, 34], members of which also include JmjC domain containing histone demethylases and AlkB family DNA/RNA repair proteins.
Similar to most Fe(II)/αKG-dependent dioxygenase superfamily members, TET proteins share a conserved DSBH fold (or jelly-roll fold) in their catalytic domains, consisting of eight antiparallel β-strands (I–VIII) and an iron-binding motif (Fig. 2). Unique characteristics are also present in the catalytic domain of TET proteins, such as a cysteine-rich domain adjacent to the N terminus of the DSBH fold, and a large non-conserved low-complexity region between conserved β-strands IV and V [33, 35, 36]. Although the low-complexity region’s function is not clear, the cysteine-rich domain has been shown to stabilize substrate DNA by wrapping around the DSBH core, and is essential for the enzymatic activity [37]. Outside of the catalytic domain, a CXXC (Cysteine-X-X-cysteine) domain is present at the N terminus of both TET1 and TET3. Indeed, TET1 is also known as CXXC6 (CXXC zinc finger 6) and LCX (leukemia-associated CXXC protein). Both in vitro DNA binding assay and structural analyses have revealed that TET proteins’ CXXC domain strongly binds to unmethylated DNA [38]. However, the catalytic domains of TET proteins alone can also bind to DNA and oxidize 5mC without the help of a CXXC domain [39]. Therefore, the catalytic domains of TET proteins may possess a non-sequence-specific DNA-binding capacity whereas the CXXC domain may increase the sequence selectivity to facilitate and regulate binding of TET proteins to their genomic targets [38, 40, 41]. Surprisingly, TET2 does not possess a CXXC domain, which was suggested to be lost during evolution, and is now encoded by a separate, neighboring gene IDAX (also known as CXXC4)[41]. It is worth noting that TET3 has three isoforms, among which only the full-length form contains the CXXC domain [42]. The full-length TET3 was reported to bind to 5caC at CCG sequences through its CXXC domain, and promote DNA demethylation by acting as a regulator of 5caC removal by base excision repair [42].
4.2 TET-Mediated Iterative Oxidation of 5mC
The finding that TET proteins can convert 5mC of DNA to 5hmC by oxidation was a great advance in understanding the mechanisms of DNA demethylation [34]. This finding was initially inspired by the biosynthesis of glucosylated 5-hydroxymethyluracil (base J) in the genome of Trypanosoma brucei, a parasite causing African sleeping sickness. Base J synthesis involves oxidation of thymine to 5-hydroxymethyluracil (5hmU) by J-binding proteins 1 and 2 (JBP1 and JBP2), two enzymes of the Fe(II)/αKG-dependent dioxygenase superfamily [43]. Because of the structural similarity between 5mC and thymine, mammalian homologs of JBP proteins were thought to possess 5mC oxidation activity, and TET family proteins were identified as the mammalian homologs of JBP proteins [33, 34]. Interestingly, the presence of TET genes in animals seems to coincide with the presence of 5mC in the genome [33, 36]. It was then convincingly demonstrated by in vitro biochemical experiments that TET proteins can oxidize 5mC to 5hmC [34]. Moreover, 5hmC is relatively abundant in mouse embryonic stem cells (ESCs) where both TET1 and TET2 are highly expressed, and its presence is TET dependent [34, 39], providing in vivo evidence that 5hmC is generated by TET-mediated oxidation of 5mC.
Fe(II)/αKG-dependent dioxygenase-mediated oxidation reactions typically consist of two stages: dioxygen activation and substrate oxidation (Fig. 3). The dioxygen activation stage is a four-electron process, where Fe(II) and αKG may each contribute two electrons to activate a dioxygen molecule first into bridged peroxo and then into the Fe(IV)-oxo intermediate. In the following substrate oxidation stage, the inert C-H bond of the substrate can be oxidized by the highly active Fe(IV)-oxo species, and finally Fe(IV) is reduced back into Fe(II) to complete the catalytic cycle [44]. During the whole process, four electrons, two from αKG and another two from the substrate C-H bond, are consumed to fully reduce a dioxygen molecule. The two oxygen atoms of the dioxygen molecule are incorporated into the succinate (the oxidized and decarboxylated product of αKG) and the oxidized product (Fig. 3).
Interestingly, some Fe(II)/αKG-dependent dioxygenase are capable to iteratively oxidize the substrate methyl group to carboxyl group. For instance, the thymine-7-hydroxylase, a Fe(II)/αKG-dependent dioxygenase in the thymidine salvage pathway, is known to catalyze a three-step oxidation of thymine to generate 5-carboxyluracil (isoorotate), where the methyl group of thymine is sequentially oxidized to hydroxymethyl group, formyl group, and finally to the carboxyl group, which is subsequently removed by an isoorotate decarboxylase (IDase) to generate uracil [45]. Enlightened by this example, it was proposed that TET proteins might oxidize 5mC not only to 5hmC, but also to 5fC and 5caC [46]. This hypothesis was soon experimentally proved both in vitro and in vivo [47, 48], and was further supported by a structural study that TET2’s active cavity could recognize CpG dinucleotide regardless of its methylation/oxidation status [37].
4.3 TDG-Mediated Excision of 5fC/5caC
Because 5mC can be converted to 5hmC, 5fC and 5caC, these modified bases are naturally considered to be involved in DNA demethylation. However, unlike the N-methyl group in m1A, m3C and methylated histones, which is unstable on the C-N bond and go through spontaneous hydrolytic deformylation upon enzymatic oxidation (i.e., direct removal of the oxidized methyl group) [19], the methyl group of 5mC is connected through a highly stable C-C bond to the rest of the base, and therefore the oxidized 5-substituents remain stable under physiological conditions [9]. Interestingly, although the 5-substituents seem not to be directly removed from 5mC oxidation derivatives, emerging evidence suggests that once converted to 5fC and 5caC, the modified cytosine base can be entirely removed from DNA by thymine-DNA glycosylase (TDG) [48, 49]. DNA demethylation is then completed by replacing the resulting abasic site with unmodified cytosine through the base excision repair (BER) pathway, similar to the active DNA demethylation mechanism in plants [50]. This TET-TDG-BER-mediated DNA demethylation process may take place rapidly, and seems a perfect candidate for locus-specific demethylation which requires rapid response towards environmental stimuli.
TDG belongs to the uracil-DNA glycosylase (UDG) superfamily. It has been well established that TDG can excise pyrimidine moiety from G/U and G/T mispairs in dsDNA by a base-flipping mechanism [51]. Interestingly, TDG also excises properly base-paired cytosine bases with 5-position substituents that destabilize the base-sugar bond (N-glycosidic bond), such as 5-fluorocytosine, indicating that the stability of the N-glycosidic bond contributes to TDG’s substrate specificity [52]. More recent studies further demonstrated that TDG can recognize and remove 5fC and 5caC, but not 5mC, 5hmC, and unmodified cytosine, from DNA duplex when paired with guanine [48, 49]. Indeed, computational analyses suggest that 5fC and 5caC form a more labile N-glycosidic bond compared to unmodified cytosine, 5mC, 5hmC, and even 5-fluorocytosine [53]. Consistently, TDG has a slightly higher binding affinity towards G/5fC and G/5caC pairs than to G/U and G/T mismatches [49]. When co-overexpressed in HEK293 cells [48, 54], TDG efficiently depletes TET-generated 5fC and 5caC; and in contrast, TDG knockdown in mouse ESCs results in a 5–10-fold increase of endogenous 5fC and 5caC [55, 56], providing in vivo evidence that TDG is responsible for 5fC/5caC removal.
Intriguingly, among the four enzymes with UDG activity in mammals (i.e., TDG, UNG, MBD4, and SMUG1), only TDG is required during mouse embryonic development [57,58,59,60], where global DNA methylation reprogramming takes place, implicating that the DNA glycosylase activity of TDG is essential for DNA demethylation. Compared with the other UDGs, the active site of TDG is indeed uniquely configured to accommodate 5fC/5caC and facilitate its cleavage, as revealed by the crystal structure of human TDG in complex with 5caC-containing dsDNA [61]. Consistently, both Tdg-null-mutant and Tdg-catalytic-mutant mice exhibit abnormal DNA methylation and die around embryonic day (E)12.5 [57, 58], confirming a crucial role of the TET-TDG-BER axis in DNA demethylation during embryonic development.
4.4 Replication-Dependent Dilution of 5mC Oxidation Derivatives
TET mediated 5mC oxidation not only initiates the TET-TDG-BER demethylation pathway, but also generates DNA demethylation intermediates (i.e., 5hmC, 5fC, and 5caC) that can be passively diluted in a replication-dependent manner. Mechanistically, hemi-modified CpGs carrying 5hmC, 5fC or 5caC (XG:GC, where X = 5hmC/5fC/5caC) have been demonstrated to be significantly less efficient in being methylated by DNMT1 compared with hemimethylated CpGs (i.e., 5mCG:GC) [62,63,64], therefore, TET-mediated 5mC oxidation can block the maintenance methylation machinery, facilitating replication-dependent DNA demethylation. Because this DNA demethylation process starts with active modification of 5mC, it has been suggested to be regarded as active DNA demethylation (Fig. 1)[65]. The replication-dependent active DNA demethylation has been observed in the paternal genome (to a less extent in the maternal genome) of zygotes and in developing PGCs [21, 22, 66, 67]. However, it is worth noting that global DNA demethylation in zygotes could be largely achieved without 5mC oxidation due to the inhibition of DNMT1 at this stage. Therefore, 5mC oxidation probably only facilitates, but is not indispensable for, replication-dependent whole genome DNA demethylation. The extent to which 5mC oxidation is required for demethylation may depend on the genomic context of the DNA sequence.
4.5 Other Potential TET-Initiated Active DNA Demethylation Pathways
In addition to the two major TET-mediated DNA demethylation pathways discussed above (i.e., the TET-TDG-BER axis and the replication-dependent dilution of 5mC oxidation derivatives) which have been extensively supported by recent biochemical and genetic studies [65], evidence for the existence of other TET-initiated DNA demethylation pathways, in which 5mC oxidation derivatives act as demethylation intermediates, have also been reported.
Firstly, the 5-carboxyl group on 5caC might be removed by a putative decarboxylase to complete DNA demethylation. This mechanism was proposed under the inspiration of the thymidine salvage pathway that we discussed above [46], where the thymine-7-hydroxylase oxidizes the methyl group of thymine to a carboxyl group that is subsequently removed by an isoorotate decarboxylase to convert thymine to uracil [45]. Although the idea of decarboxylation is more energy-efficient compared with the TET-TDG-BER pathway, only one study reported weak 5caC decarboxylase activity in mouse ESC extracts [68]. In addition, the pronounced increase of endogenous 5caC upon TDG depletion has already indicated that TDG is the major enzyme for 5caC removal [55, 56]. Therefore, whether a 5caC decarboxylase exists remains to be explored.
Secondly, the 5-position substituents may be directly removed by DNMTs. It has been reported that both bacteria and mammalian DNMTs could remove the 5-hydroxymethyl group of 5hmC and the 5-carboxyl group of 5caC in vitro to generate unmodified cytosine in the absence of SAM, the methyl donor in a DNMT-mediated DNA methylation reaction [69,70,71]. However, given that SAM is present in all cell types as a general methyl donor of many other essential biochemical reactions, whether DNMT-mediated 5-position substituent removal of 5hmC/5caC can take place in vivo remains questionable.
Thirdly, 5hmC deamination followed by BER has also been implicated in active DNA demethylation. AID (activation-induced deaminase)/APOBEC (apolipoprotein B mRNA editing enzyme, catalytic polypeptide) family of cytidine deaminases typically target unmodified cytosine in single-strand DNA or RNA to generate mutations, which are required for the generation of antibody diversity in B cells, RNA editing, and retroviral defense [72]. Interestingly, one study showed that AID/APOBEC deaminases might deaminate 5hmC to produce 5hmU in HEK293 cells and in the mouse brain [73], indicating a TET-AID/APOBEC-BER axis for active DNA demethylation. But this potential pathway has been questioned due to the following reasons: 1) AID only acts robustly on single-strand DNA but not on double-strand DNA [74]; 2) AID/APOBEC deaminases exhibit no detectable in vitro deamination activity on 5hmC [54, 75]. Therefore, further evidence is required to support this potential active DNA demethylation mechanism.
5 Potential TET-Independent Active DNA Demethylation Mechanisms
While TET proteins have been widely accepted as major players for active DNA demethylation, many other proteins were also historically proposed to play direct roles in demethylating DNA [46, 76]. Here we list some of the putative mechanisms that are independent of TET proteins, however, due to lack of direct evidence or conflicting observations, these demethylation mechanisms must be reexamined to confirm their biological relevance.
Firstly, despite the difficult nature of breaking a C-C bond, enzymatic removal of the 5-methyl group from 5mC is the simplest way to achieve DNA demethylation. The first protein reported to possess this activity is the methylated DNA binding protein MBD2. It was shown that MBD2-mediated 5-methyl group excision could take place in vitro without any cofactors [77]. However, this observation could not be reproduced by other laboratories and MBD-null mice were viable with normal DNA methylation patterns [78], raising the certain whether MBD2 could serve as a functional DNA demethylase in vivo. In addition to MBD2, elongator complex protein3 (ELP3) was also proposed to achieve DNA demethylation by breaking the C-C bond through a radical SAM mechanism [46]. While ELP3 bears a Fe-S radical SAM domain, and was reported to play a role in the paternal genome demethylation in mouse zygotes [79], direct biochemical evidence demonstrating its enzymatic activity is still lacking. Interestingly, an in vitro study has showed that, in the absence of SAM, the mammalian DNMTs (i.e., DNMT3A, DNMT3B, and DNMT1) themselves could also remove the 5-methyl group from 5mC [80], but the physiological relevance of this observation remains unclear due to the widespread presence of SAM in all cell types as discussed above.
Secondly, the entire 5mC base can be erased by a DNA glycosylase to form an abasic site, followed by BER DNA repair pathway to complete active DNA demethylation. In plants, compelling biochemical and genetic evidence has validated this mechanism with the discovery of a family of specialized DNA glycosylases responsible for 5mC excision, namely Demeter (Dme) family proteins [81]. While no obvious mammalian orthologues of Dme family proteins have been identified, two mammalian DNA glycosylases, TDG and MBD4, were reported to have incision activity against 5mC [82, 83]. However, 5mC incision activity of the two enzymes is about 30 times lower compared with that against G/T mismatches. In addition, Mbd4-null mice were viable and exhibit normal DNA methylation patterns [59]. Although Tdg-deficient mice exhibit abnormal DNA methylation and die around E12.5 [57, 58], the phenotype is more likely to be attributed to the loss of 5fC/5caC incision activity of TDG required in the TET/TDG-mediated DNA demethylation as discussed in Sect. 4.3. Thus, whether BER of 5mC by a DNA glycosylase can contribute to DNA demethylation in mammals has yet to be determined.
Thirdly, active DNA demethylation may also be achieved through deamination of 5mC to generate thymine, followed by BER to replace this mismatched thymine to unmodified cytosine. As discussed earlier, AID/APOBEC family proteins show no detectable in vitro deamination activity on 5hmC, however, these deaminases do deaminate 5mC in the context of single-strand DNA in vitro, despite at a 10-fold slower rate compared with that towards their canonical substrate cytosine [54, 75, 84]. Indeed, several lines of evidence has suggested that AID/APOBEC family deaminases play a role in active DNA demethylation, including studies in zebrafish embryos [85], in mouse PGCs [86], in promoting pluripotency in somatic nuclei after fusion with ESCs [87], and in reprogramming of somatic cells to induced pluripotent stem cells (iPSCs) [88]. Nevertheless, due to conflicting observations and the fact that these deaminases only act robustly on single-strand DNA, further mechanistic studies are required to clarify the function of AID/APOBEC proteins in active DNA demethylation. Interestingly, DNMTs, in addition to AID/APOBEC proteins, have also been shown to deaminate 5mC in the absence of SAM in vitro [29]. But again, the physiological relevance of DNMTs’ in vitro deamination activity is uncertain as depletion of SAM is unlikely in living cells.
Fourthly, nucleotide excision repair (NER), which typically repairs bulky DNA lesions generated by exposure to chemicals and radiation, has also been implicated in active DNA demethylation. Multiple lines of evidence have shown that GADD45 (growth arrest and DNA-damage-inducible 45) family proteins could stimulate active DNA demethylation via NER in frog, zebrafish, and mammals [85, 89,90,91]. However, evidence to the contrary also exists [92, 93]. More importantly, the exact underlying mechanism is still unclear. Therefore, the role of GADD45 family proteins and NER in DNA demethylation remains to be elucidated.
6 Regulation of TET-Mediated DNA Demethylation
Precise control of DNA methylation is critical to the maintenance of genome stability as well as cell-type- and developmental-stage-specific gene expression. Therefore, proper regulation of both DNA methylation and demethylation is required in many biological processes, such as development and the onset of diseases. Compared with the regulation of DNA methylation, which has been extensively studied [8, 15], the regulation of DNA demethylation has just begun to be understood. Because TET-mediated 5mC oxidation has become the most accepted mechanism of active DNA demethylation [9, 94], we only discuss factors involved in the regulation of TET-mediated DNA demethylation in the following sections.
6.1 Regulation of TET Expression
Regulation of enzyme abundance is a common way to control its activity in cells. In mouse E10.5 PGCs, transient conversion of 5mC to 5hmC can be readily detected together with a dramatic TET1 upregulation [67, 95, 96], indicating that regulation of TET expression is an important way to regulate DNA demethylation. Indeed, the three TET genes exhibit different expression patterns in a cell-type- and developmental-stage-specific manner: TET1 shows a high-level of expression specifically in mouse E10.5–12.5 PGCs, the inner cell mass (ICM) of blastocysts, as well as ESCs [39, 95]; TET2 is highly expressed in ESCs, and is broadly expressed in various mouse adult tissues [39]; TET3 is the only TET family member that is highly expressed in mouse oocytes and zygotes [97, 98], although it also shows a broad expression pattern in mouse adult tissues.
The regulation of TET expression has been reported at different levels. At the transcriptional level, cell-type-specific transcription factors (TFs) may play a major role. For example, a large cluster of binding sites for core pluripotency TFs are present in the upstream promoter of mouse Tet1 gene [99], in line with the rapid reduction of TET1 expression upon ESC differentiation [47, 100]. At the posttranscriptional level, it has been shown that an oncogenic microRNA miR-22 could negatively regulate TET family proteins in breast cancer development and in hematopoietic stem cell transformation [101, 102]. In addition, one study reported that the CXXC domain-containing protein IDAX could directly interact with the catalytic domain of TET2 to downregulate TET2 protein through caspase-mediated degradation [41]. Moreover, all three TET proteins are direct substrates of calpains, a family of calcium-dependent proteases. Specifically, calpain1 mediates TET1 and TET2 turnover in mouse ESCs, and calpain2 regulates TET3 level during differentiation [103]. Such multiple layers of regulation on TET expression provides a robust control of TET activity in cells.
6.2 Regulation of TET Activity by Metabolites and Nutrients
Given the importance of precise regulation of DNA methylation in various biological processes, it is not surprising that TET activity can be regulated in multiple ways, including the metabolic states and the milieu of cells (e.g., nutritional and developmental signals, stress, and chemical exposure). For example, both adenosine-5′-triphosphate (ATP) and hydroquinone were reported to stimulate TET-mediated 5mC oxidation [48, 104]. More importantly, the five-carbon dicarboxylic acid αKG, which is part of the tricarboxylic acid (TCA) cycle, is an essential co-factor for TET-mediated 5mC oxidation (as discussed in Sect. 4.2,). Therefore, metabolic states of cells, which affect intracellular αKG levels, may influence TET activity. Indeed, it has been reported that global 5hmC levels were rapidly increased together with αKG levels in mouse livers within 30 min after glucose, glutamine or glutamate injection [105].
In contrast, another five-carbon dicarboxylic acid, 2-hydroxyglutarate (2HG), which is chemically analogous to αKG, has been shown to inhibit TET activity by competing with αKG [106, 107]. Cellular accumulation of 2HG is often caused by tumor-associated mutations in the NADP+-dependent isocitrate dehydrogenase genes (IDH1/IDH2), which encode enzymes that normally produce αKG in the cell. These tumor-associated IDH1/IDH2 mutations (R132 of IDH1 and R140/R172 of IDH2) impair αKG production, and obtain an enzymatic activity to convert αKG to 2HG [108, 109], which inhibits TET activity. Consistently, co-expression of mutant IDH enzymes and TET proteins inhibits TET-mediated 5mC to 5hmC conversion [106, 107]. It was hypothesized that the substitution of the keto group on αKG to a hydroxyl group on 2HG might interfere with Fe(II) binding and stabilize the reaction intermediate. In line with this hypothesis, another two metabolites, fumarate and succinate, which also share structural similarity with αKG, both function as competitive inhibitors of Fe(II)/αKG-dependent dioxygenases, including TET proteins. Similar to 2HG, these metabolites are accumulated in a subset of human cancers with inactivation mutations of fumarate hydratase (FH) and succinate dehydrogenase (SDH), respectively [110]. Thus, multiple intracellular metabolites may regulate TET-mediated oxidative DNA demethylation, at least under certain pathological conditions.
Ascorbate (also known as vitamin C), an essential nutrient for humans and certain other animal species, has also been demonstrated to positively regulate TET activity [111,112,113]. In wild-type, but not Tet1/Tet2 deficient mouse ESCs, ascorbate significantly increases the levels of all 5mC oxidation products, particularly 5fC and 5caC by more than an order of magnitude, leading to a global loss of 5mC (~40%) [111, 113]. Ascorbate uniquely interacts with the catalytic domain of TET enzymes, enhancing their catalytic activities likely by promoting their folding and/or recycling of Fe(II) [111]. Intriguingly, ascorbate-induced demethylation has stronger effect on the DNA sequences that gain methylation in cultured ES cells compared to blastocysts, which are typically methylated only after implantation in vivo [113]. These studies suggest that ascorbate is a positive modulator of TET activity and may play a critical role in regulating DNA methylation during development. Further studies are needed to elucidate the sequence specificity of ascorbate-mediated stimulation of TET activity.
6.3 Regulation by TET-Interacting Proteins and DNA-Binding Proteins
In addition to the overall TET activity in cells, the specific targeting of TET proteins, and the regulation of their processivity (i.e., why TET-mediated 5mC oxidation tends to stall at 5hmC, and only proceed to 5fC and 5caC at specific loci) provide another important layer of demethylation control. Emerging evidence indicates that the genomic targeting, activity, and processivity of TET enzymes can be modulated by their interacting proteins and some DNA-binding proteins. The O-linked N-acetylglucosamine (O-GlcNAc) transferase OGT, has been reported to directly interact with, and also GlcNAcylate TET proteins [114,115,116,117,118]. Although OGT binding and GlcNAcylation appear not to regulate the enzymatic activity of TET proteins [115], OGT regulates the subcellular location of TET3 by promoting its nuclear export in high-glucose conditions [118]. Moreover, depletion of OGT in mouse ESCs decreases the association of TET1 with chromatin and alters 5hmC enrichment at certain loci [116, 117], suggesting that OGT plays a specific role in targeting and stabilizing TET proteins to the chromatin. In addition to OGT, the CXXC domain protein IDAX was shown to interact with TET2 and was suggested to recruit TET2 to promoters and CpG islands [41]. Recently, a sequence specific transcription factor WT1 (Wilms tumor protein 1) has also been shown to physically interacts with and recruits TET2 to its target genes to activate their expression [119]. Furthermore, PGC7 (also known as STELLA or DPPA3), a maternal factor essential for early development, was demonstrated in one-cell zygotes to protect maternal genome and the imprinting control regions (ICRs) in paternal genome by inhibiting TET activity through direct interaction [97, 120, 121]. These findings suggest an important role of TET interacting partners in targeting and restricting TET activity in the cell.
In addition to TET interacting proteins, some DNA binding proteins can also regulate DNA demethylation. For example, one study showed that knockdown of methyl-CpG binding domain protein 3 (MBD3), which also binds to 5hmC, caused a strong reduction in global 5hmC level in mouse ESCs [122]. In another study, UHRF2 was identified as a 5hmC-specific binding protein in neuronal progenitor cells, and was shown to be capable of stimulating the processivity of TET1 when co-overexpressed with the catalytic domain of TET1 in HEK293T cells [123]. These observations demonstrate that proteins bound to the substrate DNA of TET enzymes may regulate the enzymes’ activity and processivity, therefore implying a role of DNA binding proteins in controlling DNA demethylation.
7 Concluding Remarks
Ever since the discovery of 5mC oxidation by TET family proteins, there has been tremendous progress in understanding the molecular basis of DNA demethylation. Accumulating biochemical and genetic studies have demonstrated that TET family proteins play a critical role in active DNA demethylation during dynamic regulation of DNA methylation patterns in development and diseases. While the TET-TDG-BER pathway and replication-dependent dilution of 5hmC/5fC/5caC have been generally accepted as the major forces of active DNA demethylation, other potential active DNA demethylation mechanisms have also been reported. It is worth noting that most of those observations were made before knowing the existence of 5hmC/5fC/5caC, and by immunostaining of 5mC or bisulfite sequencing that do not distinguish 5mC from 5hmC or unmodified cytosine from 5fC and 5caC [9]. Therefore, with many new technologies recently developed to map various new modifications in the genome, historically reported active DNA demethylation pathways should be revisited to further advance this exciting field by revealing a more comprehensive understanding on how DNA methylation is dynamically regulated.
References
Bird A (2002) DNA methylation patterns and epigenetic memory. Genes Dev 16(1):6–21
Jenuwein T, Allis CD (2001) Translating the histone code. Science 293(5532):1074–1080
Holliday R, Pugh JE (1975) DNA modification mechanisms and gene activity during development. Science 187(4173):226–232
Riggs AD (1975) X inactivation, differentiation, and DNA methylation. Cytogenet Cell Genet 14(1):9–25
Henikoff S, Greally JM (2016) Epigenetics, cellular memory and gene regulation. Curr Biol 26(14):R644–R648
Bonasio R, Tu S, Reinberg D (2010) Molecular signals of epigenetic states. Science 330(6004):612–616
Easwaran H, Tsai HC, Baylin SB (2014) Cancer epigenetics: tumor heterogeneity, plasticity of stem-like states, and drug resistance. Mol Cell 54(5):716–727
Goll MG, Bestor TH (2005) Eukaryotic cytosine methyltransferases. Annu Rev Biochem 74:481–514
Shen L, Song CX, He C, Zhang Y (2014) Mechanism and function of oxidative reversal of DNA and RNA methylation. Annu Rev Biochem 83:585–614
Hermann A, Goyal R, Jeltsch A (2004) The Dnmt1 DNA-(cytosine-C5)-methyltransferase methylates DNA processively with high preference for hemimethylated target sites. J Biol Chem 279(46):48350–48359
Sharif J, Muto M, Takebayashi S, Suetake I, Iwamatsu A, Endo TA, Shinga J, Mizutani-Koseki Y, Toyoda T, Okamura K, Tajima S, Mitsuya K, Okano M, Koseki H (2007) The SRA protein Np95 mediates epigenetic inheritance by recruiting Dnmt1 to methylated DNA. Nature 450(7171):908–912
Bostick M, Kim JK, Esteve PO, Clark A, Pradhan S, Jacobsen SE (2007) UHRF1 plays a role in maintaining DNA methylation in mammalian cells. Science 317(5845):1760–1764
Okano M, Bell DW, Haber DA, Li E (1999) DNA methyltransferases Dnmt3a and Dnmt3b are essential for de novo methylation and mammalian development. Cell 99(3):247–257
Li E, Bestor TH, Jaenisch R (1992) Targeted mutation of the DNA methyltransferase gene results in embryonic lethality. Cell 69(6):915–926
Li E, Zhang Y (2014) DNA methylation in mammals. Cold Spring Harb Perspect Biol 6(5):a019133
Liu Y, Zhang X, Blumenthal RM, Cheng X (2013) A common mode of recognition for methylated CpG. Trends Biochem Sci 38(4):177–183
Bell AC, Felsenfeld G (2000) Methylation of a CTCF-dependent boundary controls imprinted expression of the Igf2 gene. Nature 405(6785):482–485
Kim J, Kollhoff A, Bergmann A, Stubbs L (2003) Methylation-sensitive binding of transcription factor YY1 to an insulator sequence within the paternally expressed imprinted gene, Peg3. Hum Mol Genet 12(3):233–245
Mosammaparast N, Shi Y (2010) Reversal of histone methylation: biochemical and molecular mechanisms of histone demethylases. Annu Rev Biochem 79:155–179
Rougier N, Bourc'his D, Gomes DM, Niveleau A, Plachot M, Paldi A, Viegas-Pequignot E (1998) Chromosome methylation patterns during mammalian preimplantation development. Genes Dev 12(14):2108–2113
Shen L, Inoue A, He J, Liu Y, Lu F, Zhang Y (2014) Tet3 and DNA replication mediate demethylation of both the maternal and paternal genomes in mouse zygotes. Cell Stem Cell 15(4):459–470
Guo F, Li X, Liang D, Li T, Zhu P, Guo H, Wu X, Wen L, Gu TP, Hu B, Walsh CP, Li J, Tang F, Xu GL (2014) Active and passive demethylation of male and female pronuclear DNA in the mammalian zygote. Cell Stem Cell 15(4):447–458
Seisenberger S, Andrews S, Krueger F, Arand J, Walter J, Santos F, Popp C, Thienpont B, Dean W, Reik W (2012) The dynamics of genome-wide DNA methylation reprogramming in mouse primordial germ cells. Mol Cell 48(6):849–862
Kagiwada S, Kurimoto K, Hirota T, Yamaji M, Saitou M (2013) Replication-coupled passive DNA demethylation for the erasure of genome imprints in mice. EMBO J 32(3):340–353
Vincent JJ, Huang Y, Chen PY, Feng S, Calvopina JH, Nee K, Lee SA, Le T, Yoon AJ, Faull K, Fan G, Rao A, Jacobsen SE, Pellegrini M, Clark AT (2013) Stage-specific roles for tet1 and tet2 in DNA demethylation in primordial germ cells. Cell Stem Cell 12(4):470–478
Bruniquel D, Schwartz RH (2003) Selective, stable demethylation of the interleukin-2 gene enhances transcription by an active process. Nat Immunol 4(3):235–240
Martinowich K, Hattori D, Wu H, Fouse S, He F, Hu Y, Fan G, Sun YE (2003) DNA methylation-related chromatin remodeling in activity-dependent BDNF gene regulation. Science 302(5646):890–893
Kangaspeska S, Stride B, Metivier R, Polycarpou-Schwarz M, Ibberson D, Carmouche RP, Benes V, Gannon F, Reid G (2008) Transient cyclical methylation of promoter DNA. Nature 452(7183):112–115
Metivier R, Gallais R, Tiffoche C, Le Peron C, Jurkowska RZ, Carmouche RP, Ibberson D, Barath P, Demay F, Reid G, Benes V, Jeltsch A, Gannon F, Salbert G (2008) Cyclical DNA methylation of a transcriptionally active promoter. Nature 452(7183):45–50
Thillainadesan G, Chitilian JM, Isovic M, Ablack JN, Mymryk JS, Tini M, Torchia J (2012) TGF-beta-dependent active demethylation and expression of the p15ink4b tumor suppressor are impaired by the ZNF217/CoREST complex. Mol Cell 46(5):636–649
Ono R, Taki T, Taketani T, Taniwaki M, Kobayashi H, Hayashi Y (2002) LCX, leukemia-associated protein with a CXXC domain, is fused to MLL in acute myeloid leukemia with trilineage dysplasia having t(10;11)(q22;q23). Cancer Res 62(14):4075–4080
Lorsbach RB, Moore J, Mathew S, Raimondi SC, Mukatira ST, Downing JR (2003) TET1, a member of a novel protein family, is fused to MLL in acute myeloid leukemia containing the t(10;11)(q22;q23). Leuk Off J Leuk Soc Am Leuk Res Fund UK 17(3):637–641
Iyer LM, Tahiliani M, Rao A, Aravind L (2009) Prediction of novel families of enzymes involved in oxidative and other complex modifications of bases in nucleic acids. Cell Cycle 8(11):1698–1710
Tahiliani M, Koh KP, Shen Y, Pastor WA, Bandukwala H, Brudno Y, Agarwal S, Iyer LM, Liu DR, Aravind L, Rao A (2009) Conversion of 5-methylcytosine to 5-hydroxymethylcytosine in mammalian DNA by MLL partner TET1. Science 324(5929):930–935
McDonough MA, Loenarz C, Chowdhury R, Clifton IJ, Schofield CJ (2010) Structural studies on human 2-oxoglutarate dependent oxygenases. Curr Opin Struct Biol 20(6):659–672
Iyer LM, Abhiman S, Aravind L (2011) Natural history of eukaryotic DNA methylation systems. Prog Mol Biol Transl Sci 101:25–104
Hu L, Li Z, Cheng J, Rao Q, Gong W, Liu M, Shi YG, Zhu J, Wang P, Xu Y (2013) Crystal structure of TET2-DNA complex: insight into TET-mediated 5mC oxidation. Cell 155(7):1545–1555
Xu Y, Xu C, Kato A, Tempel W, Abreu JG, Bian C, Hu Y, Hu D, Zhao B, Cerovina T, Diao J, Wu F, He HH, Cui Q, Clark E, Ma C, Barbara A, Veenstra GJ, Xu G, Kaiser UB, Liu XS, Sugrue SP, He X, Min J, Kato Y, Shi YG (2012) Tet3 CXXC domain and dioxygenase activity cooperatively regulate key genes for Xenopus eye and neural development. Cell 151(6):1200–1213
Ito S, D'Alessio AC, Taranova OV, Hong K, Sowers LC, Zhang Y (2010) Role of Tet proteins in 5mC to 5hmC conversion, ES-cell self-renewal and inner cell mass specification. Nature 466(7310):1129–1133
Liu N, Wang M, Deng W, Schmidt CS, Qin W, Leonhardt H, Spada F (2013) Intrinsic and extrinsic connections of Tet3 Dioxygenase with CXXC zinc finger modules. PLoS One 8(5):e62755
Ko M, An J, Bandukwala H, Chavez L (2013) Modulation of TET2 expression and 5-methylcytosine oxidation by the CXXC domain protein IDAX. Nature 497:122–126
Jin SG, Zhang ZM, Dunwell TL, Harter MR, Wu X, Johnson J, Li Z, Liu J, Szabo PE, Lu Q, Xu GL, Song J, Pfeifer GP (2016) Tet3 reads 5-Carboxylcytosine through its CXXC domain and is a potential Guardian against Neurodegeneration. Cell Rep 14(3):493–505
Borst P, Sabatini R (2008) Base J: discovery, biosynthesis, and possible functions. Annu Rev Microbiol 62:235–251
Krebs C, Galonic Fujimori D, Walsh CT, Bollinger JM Jr (2007) Non-heme Fe(IV)-oxo intermediates. Acc Chem Res 40(7):484–492
Smiley JA, Kundracik M, Landfried DA, Barnes VR Sr, Axhemi AA (2005) Genes of the thymidine salvage pathway: thymine-7-hydroxylase from a Rhodotorula glutinis cDNA library and iso-orotate decarboxylase from Neurospora crassa. Biochim Biophys Acta 1723(1–3):256–264
Wu SC, Zhang Y (2010) Active DNA demethylation: many roads lead to Rome. Nat Rev Mol Cell Biol 11(9):607–620
Ito S, Shen L, Dai Q, Wu SC, Collins LB, Swenberg JA, He C, Zhang Y (2011) Tet proteins can convert 5-methylcytosine to 5-formylcytosine and 5-carboxylcytosine. Science 333(6047):1300–1303
He YF, Li BZ, Li Z, Liu P, Wang Y, Tang Q, Ding J, Jia Y, Chen Z, Li L, Sun Y, Li X, Dai Q, Song CX, Zhang K, He C, Xu GL (2011) Tet-mediated formation of 5-carboxylcytosine and its excision by TDG in mammalian DNA. Science 333(6047):1303–1307
Maiti A, Drohat AC (2011) Thymine DNA glycosylase can rapidly excise 5-formylcytosine and 5-carboxylcytosine: potential implications for active demethylation of CpG sites. J Biol Chem 286(41):35334–35338
Zhang H, Zhu JK (2012) Active DNA demethylation in plants and animals. Cold Spring Harb Symp Quant Biol 77:161–173
Stivers JT, Jiang YL (2003) A mechanistic perspective on the chemistry of DNA repair glycosylases. Chem Rev 103(7):2729–2759
Bennett MT, Rodgers MT, Hebert AS, Ruslander LE, Eisele L, Drohat AC (2006) Specificity of human thymine DNA glycosylase depends on N-glycosidic bond stability. J Am Chem Soc 128(38):12510–12519
Williams RT, Wang Y (2012) A density functional theory study on the kinetics and thermodynamics of N-glycosidic bond cleavage in 5-substituted 2′-deoxycytidines. Biochemistry 51(32):6458–6462
Nabel CS, Jia H, Ye Y, Shen L, Goldschmidt HL, Stivers JT, Zhang Y, Kohli RM (2012) AID/APOBEC deaminases disfavor modified cytosines implicated in DNA demethylation. Nat Chem Biol 8(9):751–758
Shen L, Wu H, Diep D, Yamaguchi S, D'Alessio AC, Fung HL, Zhang K, Zhang Y (2013) Genome-wide analysis reveals TET- and TDG-dependent 5-methylcytosine oxidation dynamics. Cell 153(3):692–706
Song C-X, Szulwach KE, Dai Q, Fu Y, Mao S-Q, Lin L, Street C, Li Y, Poidevin M, Wu H, Gao J, Liu P, Li L, Xu G-L, Jin P, He C (2013) Genome-wide profiling of 5-Formylcytosine reveals its roles in epigenetic priming. Cell 153:678–691
Cortellino S, Xu J, Sannai M, Moore R, Caretti E, Cigliano A, Le Coz M, Devarajan K, Wessels A, Soprano D, Abramowitz LK, Bartolomei MS, Rambow F, Bassi MR, Bruno T, Fanciulli M, Renner C, Klein-Szanto AJ, Matsumoto Y, Kobi D, Davidson I, Alberti C, Larue L, Bellacosa A (2011) Thymine DNA glycosylase is essential for active DNA demethylation by linked deamination-base excision repair. Cell 146(1):67–79
Cortazar D, Kunz C, Selfridge J, Lettieri T, Saito Y, MacDougall E, Wirz A, Schuermann D, Jacobs AL, Siegrist F, Steinacher R, Jiricny J, Bird A, Schar P (2011) Embryonic lethal phenotype reveals a function of TDG in maintaining epigenetic stability. Nature 470(7334):419–423
Millar CB, Guy J, Sansom OJ, Selfridge J, MacDougall E, Hendrich B, Keightley PD, Bishop SM, Clarke AR, Bird A (2002) Enhanced CpG mutability and tumorigenesis in MBD4-deficient mice. Science 297(5580):403–405
Kemmerich K, Dingler FA, Rada C, Neuberger MS (2012) Germline ablation of SMUG1 DNA glycosylase causes loss of 5-hydroxymethyluracil- and UNG-backup uracil-excision activities and increases cancer predisposition of Ung−/−Msh2−/− mice. Nucleic Acids Res 40(13):6016–6025
Zhang L, Lu X, Lu J, Liang H, Dai Q, Xu GL, Luo C, Jiang H, He C (2012) Thymine DNA glycosylase specifically recognizes 5-carboxylcytosine-modified DNA. Nat Chem Biol 8(4):328–330
Hashimoto H, Liu Y, Upadhyay AK, Chang Y, Howerton SB, Vertino PM, Zhang X, Cheng X (2012) Recognition and potential mechanisms for replication and erasure of cytosine hydroxymethylation. Nucleic Acids Res 40(11):4841–4849
Valinluck V, Sowers LC (2007) Endogenous cytosine damage products alter the site selectivity of human DNA maintenance methyltransferase DNMT1. Cancer Res 67(3):946–950
Ji D, Lin K, Song J, Wang Y (2014) Effects of Tet-induced oxidation products of 5-methylcytosine on Dnmt1- and DNMT3a-mediated cytosine methylation. Mol BioSyst 10(7):1749–1752
Kohli RM, Zhang Y (2013) TET enzymes, TDG and the dynamics of DNA demethylation. Nature 502(7472):472–479
Inoue A, Zhang Y (2011) Replication-dependent loss of 5-hydroxymethylcytosine in mouse preimplantation embryos. Science 334(6053):194
Hackett JA, Sengupta R, Zylicz JJ, Murakami K, Lee C, Down TA, Surani MA (2013) Germline DNA demethylation dynamics and imprint erasure through 5-hydroxymethylcytosine. Science 339(6118):448–452
Schiesser S, Hackner B, Pfaffeneder T, Muller M, Hagemeier C, Truss M, Carell T (2012) Mechanism and stem-cell activity of 5-carboxycytosine decarboxylation determined by isotope tracing. Angew Chem Int Ed 51(26):6516–6520
Chen CC, Wang KY, Shen CK (2012) The mammalian de novo DNA methyltransferases DNMT3A and DNMT3B are also DNA 5-hydroxymethylcytosine dehydroxymethylases. J Biol Chem 287(40):33116–33121
Liutkeviciute Z, Lukinavicius G, Masevicius V, Daujotyte D, Klimasauskas S (2009) Cytosine-5-methyltransferases add aldehydes to DNA. Nat Chem Biol 5(6):400–402
Liutkeviciute Z, Kriukiene E, Licyte J, Rudyte M, Urbanaviciute G, Klimasauskas S (2014) Direct decarboxylation of 5-carboxylcytosine by DNA C5-methyltransferases. J Am Chem Soc 136(16):5884–5887
Conticello SG (2008) The AID/APOBEC family of nucleic acid mutators. Genome Biol 9(6):229
Guo JU, Su Y, Zhong C, Ming GL, Song H (2011) Hydroxylation of 5-methylcytosine by TET1 promotes active DNA demethylation in the adult brain. Cell 145(3):423–434
Bransteitter R, Pham P, Scharff MD, Goodman MF (2003) Activation-induced cytidine deaminase deaminates deoxycytidine on single-stranded DNA but requires the action of RNase. Proc Natl Acad Sci U S A 100(7):4102–4107
Rangam G, Schmitz KM, Cobb AJ, Petersen-Mahrt SK (2012) AID enzymatic activity is inversely proportional to the size of cytosine C5 orbital cloud. PLoS One 7(8):e43279
Ooi SK, Bestor TH (2008) The colorful history of active DNA demethylation. Cell 133(7):1145–1148
Bhattacharya SK, Ramchandani S, Cervoni N, Szyf M (1999) A mammalian protein with specific demethylase activity for mCpG DNA. Nature 397(6720):579–583
Santos F, Hendrich B, Reik W, Dean W (2002) Dynamic reprogramming of DNA methylation in the early mouse embryo. Dev Biol 241(1):172–182
Okada Y, Yamagata K, Hong K, Wakayama T, Zhang Y (2010) A role for the elongator complex in zygotic paternal genome demethylation. Nature 463(7280):554–558
Chen CC, Wang KY, Shen CK (2013) DNA 5-methylcytosine demethylation activities of the mammalian DNA methyltransferases. J Biol Chem 288(13):9084–9091
Zhu JK (2009) Active DNA demethylation mediated by DNA glycosylases. Annu Rev Genet 43:143–166
Zhu B, Zheng Y, Hess D, Angliker H, Schwarz S, Siegmann M, Thiry S, Jost JP (2000) 5-methylcytosine-DNA glycosylase activity is present in a cloned G/T mismatch DNA glycosylase associated with the chicken embryo DNA demethylation complex. Proc Natl Acad Sci U S A 97(10):5135–5139
Zhu B, Zheng Y, Angliker H, Schwarz S, Thiry S, Siegmann M, Jost JP (2000) 5-methylcytosine DNA glycosylase activity is also present in the human MBD4 (G/T mismatch glycosylase) and in a related avian sequence. Nucleic Acids Res 28(21):4157–4165
Morgan HD, Dean W, Coker HA, Reik W, Petersen-Mahrt SK (2004) Activation-induced cytidine deaminase deaminates 5-methylcytosine in DNA and is expressed in pluripotent tissues: implications for epigenetic reprogramming. J Biol Chem 279(50):52353–52360
Rai K, Huggins IJ, James SR, Karpf AR, Jones DA, Cairns BR (2008) DNA demethylation in zebrafish involves the coupling of a deaminase, a glycosylase, and gadd45. Cell 135(7):1201–1212
Popp C, Dean W, Feng S, Cokus SJ, Andrews S, Pellegrini M, Jacobsen SE, Reik W (2010) Genome-wide erasure of DNA methylation in mouse primordial germ cells is affected by AID deficiency. Nature 463(7284):1101–1105
Bhutani N, Brady JJ, Damian M, Sacco A, Corbel SY, Blau HM (2010) Reprogramming towards pluripotency requires AID-dependent DNA demethylation. Nature 463(7284):1042–1047
Kumar R, DiMenna L, Schrode N, Liu TC, Franck P, Munoz-Descalzo S, Hadjantonakis AK, Zarrin AA, Chaudhuri J, Elemento O, Evans T (2013) AID stabilizes stem-cell phenotype by removing epigenetic memory of pluripotency genes. Nature 500(7460):89–92
Barreto G, Schafer A, Marhold J, Stach D, Swaminathan SK, Handa V, Doderlein G, Maltry N, Wu W, Lyko F, Niehrs C (2007) Gadd45a promotes epigenetic gene activation by repair-mediated DNA demethylation. Nature 445(7128):671–675
Ma DK, Jang MH, Guo JU, Kitabatake Y, Chang ML, Pow-Anpongkul N, Flavell RA, Lu B, Ming GL, Song H (2009) Neuronal activity-induced Gadd45b promotes epigenetic DNA demethylation and adult neurogenesis. Science 323(5917):1074–1077
Schmitz KM, Schmitt N, Hoffmann-Rohrer U, Schafer A, Grummt I, Mayer C (2009) TAF12 recruits Gadd45a and the nucleotide excision repair complex to the promoter of rRNA genes leading to active DNA demethylation. Mol Cell 33(3):344–353
Engel N, Tront JS, Erinle T, Nguyen N, Latham KE, Sapienza C, Hoffman B, Liebermann DA (2009) Conserved DNA methylation in Gadd45a(−/−) mice. Epigenetics 4(2):98–99
Jin SG, Guo C, Pfeifer GP (2008) GADD45A does not promote DNA demethylation. PLoS Genet 4(3):e1000013
Wu H, Zhang Y (2014) Reversing DNA methylation: mechanisms, genomics, and biological functions. Cell 156(1–2):45–68
Yamaguchi S, Hong K, Liu R, Shen L, Inoue A, Diep D, Zhang K, Zhang Y (2012) Tet1 controls meiosis by regulating meiotic gene expression. Nature 492(7429):443–447
Yamaguchi S, Hong K, Liu R, Inoue A, Shen L, Zhang K, Zhang Y (2013) Dynamics of 5-methylcytosine and 5-hydroxymethylcytosine during germ cell reprogramming. Cell Res 23(3):329–339
Wossidlo M, Nakamura T, Lepikhov K, Marques CJ, Zakhartchenko V, Boiani M, Arand J, Nakano T, Reik W, Walter J (2011) 5-hydroxymethylcytosine in the mammalian zygote is linked with epigenetic reprogramming. Nat Commun 2:241
Iqbal K, Jin SG, Pfeifer GP, Szabo PE (2011) Reprogramming of the paternal genome upon fertilization involves genome-wide oxidation of 5-methylcytosine. Proc Natl Acad Sci U S A 108(9):3642–3647
Ficz G, Branco MR, Seisenberger S, Santos F, Krueger F, Hore TA, Marques CJ, Andrews S, Reik W (2011) Dynamic regulation of 5-hydroxymethylcytosine in mouse ES cells and during differentiation. Nature 473(7347):398–402
Koh KP, Yabuuchi A, Rao S, Huang Y, Cunniff K, Nardone J, Laiho A, Tahiliani M, Sommer CA, Mostoslavsky G, Lahesmaa R, Orkin SH, Rodig SJ, Daley GQ, Rao A (2011) Tet1 and Tet2 regulate 5-hydroxymethylcytosine production and cell lineage specification in mouse embryonic stem cells. Cell Stem Cell 8(2):200–213
Song SJ, Poliseno L, Song MS, Ala U, Webster K, Ng C, Beringer G, Brikbak NJ, Yuan X, Cantley LC, Richardson AL, Pandolfi PP (2013) MicroRNA-antagonism regulates breast cancer Stemness and metastasis via TET-family-dependent chromatin remodeling. Cell 154(2):311–324
Song Su J, Ito K, Ala U, Kats L, Webster K, Sun Su M, Jongen-Lavrencic M, Manova-Todorova K, Teruya-Feldstein J, Avigan David E, Delwel R, Pandolfi Pier P (2013) The oncogenic microRNA miR-22 targets the TET2 tumor suppressor to promote hematopoietic stem cell self-renewal and transformation. Cell Stem Cell 13:87–101
Wang Y, Zhang Y (2014) Regulation of TET protein stability by Calpains. Cell Rep 6(2):278–284
Coulter JB, O'Driscoll CM, Bressler JP (2013) Hydroquinone increases 5-hydroxymethylcytosine formation through ten eleven translocation 1 (Tet1) 5-methylcytosine dioxygenase. J Biol Chem 288(40):28792–28800
Yang H, Lin H, Xu H, Zhang L, Cheng L, Wen B, Shou J, Guan K, Xiong Y, Ye D (2014) TET-catalyzed 5-methylcytosine hydroxylation is dynamically regulated by metabolites. Cell Res 24(8):1017–1020
Figueroa ME, Abdel-Wahab O, Lu C, Ward PS, Patel J, Shih A, Li Y, Bhagwat N, Vasanthakumar A, Fernandez HF, Tallman MS, Sun Z, Wolniak K, Peeters JK, Liu W, Choe SE, Fantin VR, Paietta E, Lowenberg B, Licht JD, Godley LA, Delwel R, Valk PJ, Thompson CB, Levine RL, Melnick A (2010) Leukemic IDH1 and IDH2 mutations result in a hypermethylation phenotype, disrupt TET2 function, and impair hematopoietic differentiation. Cancer Cell 18(6):553–567
Xu W, Yang H, Liu Y, Yang Y, Wang P, Kim SH, Ito S, Yang C, Xiao MT, Liu LX, Jiang WQ, Liu J, Zhang JY, Wang B, Frye S, Zhang Y, Xu YH, Lei QY, Guan KL, Zhao SM, Xiong Y (2011) Oncometabolite 2-hydroxyglutarate is a competitive inhibitor of alpha-ketoglutarate-dependent dioxygenases. Cancer Cell 19(1):17–30
Ward PS, Patel J, Wise DR, Abdel-Wahab O, Bennett BD, Coller HA, Cross JR, Fantin VR, Hedvat CV, Perl AE, Rabinowitz JD, Carroll M, Su SM, Sharp KA, Levine RL, Thompson CB (2010) The common feature of leukemia-associated IDH1 and IDH2 mutations is a neomorphic enzyme activity converting alpha-ketoglutarate to 2-hydroxyglutarate. Cancer Cell 17(3):225–234
Dang L, White DW, Gross S, Bennett BD, Bittinger MA, Driggers EM, Fantin VR, Jang HG, Jin S, Keenan MC, Marks KM, Prins RM, Ward PS, Yen KE, Liau LM, Rabinowitz JD, Cantley LC, Thompson CB, Vander Heiden MG, Su SM (2009) Cancer-associated IDH1 mutations produce 2-hydroxyglutarate. Nature 462(7274):739–744
Xiao M, Yang H, Xu W, Ma S, Lin H, Zhu H, Liu L, Liu Y, Yang C, Xu Y, Zhao S, Ye D, Xiong Y, Guan KL (2012) Inhibition of alpha-KG-dependent histone and DNA demethylases by fumarate and succinate that are accumulated in mutations of FH and SDH tumor suppressors. Genes Dev 26(12):1326–1338
Yin R, Mao S-Q, Zhao B, Chong Z, Yang Y, Zhao C, Zhang D, Huang H, Gao J, Li Z, Jiao Y, Li C, Liu S, Wu D, Gu W, Yang Y-G, Xu G-L, Wang H (2013) Ascorbic acid enhances Tet-mediated 5-methylcytosine oxidation and promotes DNA demethylation in mammals. J Am Chem Soc 135(28):10396–10403
Minor EA, Court BL, Young JI, Wang G (2013) Ascorbate induces ten-eleven translocation (Tet) methylcytosine dioxygenase-mediated generation of 5-hydroxymethylcytosine. J Biol Chem 288(19):13669–13674
Blaschke K, Ebata KT, Karimi MM, Zepeda-Martínez JA, Goyal P, Mahapatra S, Tam A, Laird DJ, Hirst M, Rao A, Lorincz MC, Ramalho-Santos M (2013) Vitamin C induces Tet-dependent DNA demethylation and a blastocyst-like state in ES cells. Nature 500(7461):222–226
Deplus R, Delatte B, Schwinn MK, Defrance M, Méndez J, Murphy N, Ma D, Volkmar M, Putmans P, Calonne E, Shih AH, Levine RL, Bernard O, Mercher T, Solary E, Urh M, Daniels DL, Fuks F (2013) TET2 and TET3 regulate GlcNAcylation and H3K4 methylation through OGT and SET1/COMPASS. EMBO J 32:645–655
Chen Q, Chen Y, Bian C, Fujiki R, Yu X (2013) TET2 promotes histone O-GlcNAcylation during gene transcription. Nature 493:561–564
Vella P, Scelfo A, Jammula S, Chiacchiera F, Williams K, Cuomo A, Roberto A, Christensen J, Bonaldi T, Helin K, Pasini D (2013) Tet proteins connect the O-linked N-acetylglucosamine transferase Ogt to chromatin in embryonic stem cells. Mol Cell 49:645–656
Shi FT, Kim H, Lu W, He Q, Liu D, Goodell MA, Wan M, Songyang Z (2013) Ten-eleven translocation 1 (tet1) is regulated by o-linked N-acetylglucosamine transferase (ogt) for target gene repression in mouse embryonic stem cells. J Biol Chem 288(29):20776–20784
Zhang Q, Liu X, Gao W, Li P, Hou J, Li J, Wong J (2014) Differential regulation of the ten-eleven translocation (TET) family of dioxygenases by O-linked beta-N-acetylglucosamine transferase (OGT). J Biol Chem 289(9):5986–5996
Wang Y, Xiao M, Chen X, Chen L, Xu Y, Lv L, Wang P, Yang H, Ma S, Lin H, Jiao B, Ren R, Ye D, Guan KL, Xiong Y (2015) WT1 recruits TET2 to regulate its target gene expression and suppress leukemia cell proliferation. Mol Cell 57(4):662–673
Nakamura T, Liu YJ, Nakashima H, Umehara H, Inoue K, Matoba S, Tachibana M, Ogura A, Shinkai Y, Nakano T (2012) PGC7 binds histone H3K9me2 to protect against conversion of 5mC to 5hmC in early embryos. Nature 486(7403):415–419
Bian C, Yu X (2014) PGC7 suppresses TET3 for protecting DNA methylation. Nucleic Acids Res 42(5):2893–2905
Yildirim O, Li R, Hung JH, Chen PB, Dong X, Ee LS, Weng Z, Rando OJ, Fazzio TG (2011) Mbd3/NURD complex regulates expression of 5-hydroxymethylcytosine marked genes in embryonic stem cells. Cell 147(7):1498–1510
Spruijt CG, Gnerlich F, Smits AH, Pfaffeneder T, Jansen PWTC, Bauer C, Münzel M, Wagner M, Müller M, Khan F, Eberl HC, Mensinga A, Brinkman AB, Lephikov K, Müller U, Walter J, Boelens R, van Ingen H, Leonhardt H, Carell T, Vermeulen M (2013) Dynamic readers for 5-(hydroxy)methylcytosine and its oxidized derivatives. Cell 152:1146–1159
Author information
Authors and Affiliations
Corresponding author
Editor information
Editors and Affiliations
Rights and permissions
Copyright information
© 2017 Springer International Publishing AG
About this chapter
Cite this chapter
Shi, M., Shen, L. (2017). The Molecular Basis of DNA Demethylation. In: Kaneda, A., Tsukada, Yi. (eds) DNA and Histone Methylation as Cancer Targets. Cancer Drug Discovery and Development. Humana Press, Cham. https://doi.org/10.1007/978-3-319-59786-7_3
Download citation
DOI: https://doi.org/10.1007/978-3-319-59786-7_3
Published:
Publisher Name: Humana Press, Cham
Print ISBN: 978-3-319-59784-3
Online ISBN: 978-3-319-59786-7
eBook Packages: MedicineMedicine (R0)