Mapping and Use of a Sequence that Targets DNA Ligase I to Sites of DNA Replication In Vivo

Polyclonal antibodies against DNA ligase I were raised in rabbits using a peptide antigen spanning amino acids 1–23 from the mouse enzyme with the addition of N-chloracetyl-glycine at the NH₂ terminus for coupling to the carrier protein KLH (30). The anti-peptide antibody was purified from serum by affinity chromatography as described by Sawin et al. (47) using the peptide antigen coupled to Affi-Gel 10 (Bio Rad, Hercules, CA).

In addition, the following primary antibodies were used: mouse monoclonal anti-PCNA antibody (clone PC 10; Dako, Carpinteria, CA; Zymed, San Francisco, CA), 12CA5 hybridoma supernatant recognizing the Flutag epitope, β-galactosidase (β-gal)-specific mouse monoclonal antibody (Promega, Madison, WI), rabbit polyclonal anti-MTase antiserum (24), and mouse monoclonal anti-5-bromo-2′-deoxyuridine (BrdU) antibody FITC conjugated (Boehringer Mannheim, Mannheim, Germany).

Expression plasmids were derived from pJ3Ω (35) or pEVRF0 (33). The latter was used to add a heterologous NLS (see below). Oligonucleotides encoding a nine-amino acid epitope (YPYDVPDYA; 61) from the hemagglutinin of influenza virus (Flutag) were inserted at the Bsp EI restriction site (codon 307), at the Eag I restriction site (codon 773) or between both sites in the cDNA of human DNA ligase I (ATCC 65856; 2). The β-gal epitope was derived from the β-gal gene of Escherichia coli (amino acids 361-1,069) and was added at the COOH-terminus of all but two deletion constructs. A short nuclear localization signal (NLS) derived from SV40 large T antigen (PKKKRKV) was added at the NH₂ terminus of some deletion constructs to compensate for the loss of their own NLS using a translational fusion vector, as previously described (24). The green fluorescent protein (GFP) fusions were derived from the pRSGFP-C1 and the pEGFPC1 vectors (Clontech, Palo Alto, CA), by inserting a fragment containing the full length or the first 250 amino acids of the human DNA ligase cDNA at the COOH terminus of the open reading frame of both GFP mutants. It is noteworthy that the GFP expressed in these constructs, with an additional 26 amino acids derived from the multiple cloning site added to its COOH terminus, is by itself nuclear and cytoplasmic. Plasmid DNA was purified using columns (Qiagen, Hilden, Germany) according to the instructions of the manufacturer.

Human HeLa cells, monkey Cos 7 cells, and mouse MEL and C3H10T1/2 cells were grown in a humidified incubator at 37°C and 5% CO₂ in DME supplemented with 10% fetal calf serum. Mouse (C2C12) and rat (L6E9) myoblast cells were grown as above except that the media was supplemented with 20% fetal calf serum.

Cos 7 cells were transfected by the DEAE-dextran pretreatment method as described by Leonhardt et al. (24). 2 d later, cells were scraped, extracted, and analyzed as described below. Exponentially growing mouse fibroblasts were transfected by the calcium phosphate-DNA coprecipitation method (15) with glycerol shock treatment (41) ∼8–12 h later. 36–48 h after DNA addition, cells were fixed and stained.

For visualization of GFP-ligase in living cells, transfected fibroblasts plated onto glass-bottom petri dishes were changed to Hepes-buffered medium (10 mM Hepes, pH 7.0, 140 mM NaCl, 5 mM KCl, 1 mM MgCl₂, 2 mM CaCl₂, 10 mM Glucose) and screened with a fluorescence microscope using an FITC filter.

Transfected Cos cells were scraped and extracted as described by Leonhardt et al. (24) in 0.2 M NaCl, 0.32 M sucrose, 0.3% Triton X-100, 20 mM Tris-HCl (pH 7.4), 3 mM MgCl₂, 0.5 mM dithiothreitol, and 0.2 mM phenylmethylsulfonylfluoride. Cell extracts used to characterize the anti-DNA ligase I antibody by immunoblots were made by extraction of cells for 30 min on ice with RIPA buffer (50 mM Tris-HCl, pH 8.0, 150 mM NaCl, 1% NP-40, 0.5% deoxycholate, 0.1% SDS) containing the following protease inhibitors: 1 mM EDTA, 1 mM Pefabloc, 10 μM leupeptin, 10 μM pepstatin, and 10 μM aprotinin. After 5 min centrifugation in the cold, the soluble fraction was analyzed by immunoblot. The protein extracts were dissolved in Laemmli sample buffer, separated by SDS-PAGE under reducing conditions, and transferred to PVDF membranes. After incubation with epitope tag-specific antibodies or anti-DNA ligase I antibodies, followed by HRP-conjugated secondary antibodies, the blots were developed using the ECL detection procedure (Amersham, Buckinghamshire, UK).

Transfected cells were washed in PBS and fixed for 10 min in 3.7% formaldehyde in PBS or for 5 min in cold methanol. All following incubations were performed at room temperature. Formaldehyde-fixed cells were permeabilized for 10 min in 0.25% Triton X-100. Fixed cells were blocked in 5% goat serum or 0.2% gelatin and incubated for 60 min with the respective primary antibodies as described before (7, 24). After extensive washes in 0.1% NP-40, cells were incubated for another 60 min in FITC-conjugated goat anti–mouse or anti–rabbit IgG and biotinylated goat anti–rabbit or anti–mouse IgG antibodies, followed by washing and 30 min incubation in streptavidin-Texas red, as described before (7). DNA was counterstained with Hoechst 33258 and cells were mounted in mowiol with 2.5% DABCO (6). Pulse labeling with BrdU and detection of incorporated BrdU were done as described before (7, 24).

Stained specimens or live cultures were examined and photographed in microscopes (Axiophot and Axiovert; Zeiss, Inc., Thornwood, NY) equipped with phase-contrast and epifluorescence optics, using 40, 63, and 100× oil immersion Plan-Neofluor and Planapochromat objectives. Single Hoechst, FITC, and Texas red filters were used as well as FITC-Texas red dual filters. Pictures were taken with Kodak Ektar and Royal Gold films. Micrographs were scanned, assembled, and annotated with Adobe Photoshop and Canvas software in a Power MacIntosh computer and printed with a Phaser 440 dye sublimation printer (Tektronix). Overlays were mostly generated by photographic double exposure with the two respective filters or directly with a dual filter. In two cases (Fig. 2 C, the upper left early S phase nucleus, and F), overlays were generated digitally using Adobe Photoshop layers.

To identify additional components of nuclear replication foci and to probe the dynamics of nuclear architecture, we analyzed the subcellular localization of DNA ligase I, which is involved in joining Okazaki fragments during lagging-strand DNA synthesis (for review see 29).

Polyclonal antibodies were raised against mammalian DNA ligase I. We used a peptide spanning the first 23 amino acid residues of mouse DNA ligase I, which differs from the human protein in two positions. The antisera were then affinity purified and tested for specificity and species reactivity by immunoblot. As shown in Fig. 1,A, both elution methods (0.2 M glycine-HCl, pH 2.0, and 6 M guanidine hydrochloride) yielded antibody fractions that specifically reacted with mouse DNA ligase I. The predicted size of mammalian DNA ligase I is 101–102 kD, but endogenous as well as recombinant proteins migrate anomalously slowly in SDS-PAGE, which may be due to its high proline content, to the presence of phosphoserine residues, and to the high hydrophilicity of the NH₂-terminal domain (43, 57). The result obtained with our antibodies is in agreement with the previously observed migration of mammalian DNA ligase I. This signal is competed away by pre-incubating the antibodies with the peptide used as antigen but not with a nonspecific peptide, as shown in Fig. 1,B, further confirming its specificity. Finally, we tested for cross-reactivity with homologues from other mammalian species. Fig. 1 C shows that the affinity-purified antibodies specifically recognize proteins of the expected size in extracts from mouse, rat, monkey, and human cells. This result was expected because of the relatively high degree of conservation between human and mouse DNA ligase I cDNAs. Under the conditions used (50 μg of extract) some additional signals can be seen in the monkey cell extracts, even though at much lower intensity.

We then used the affinity-purified antibodies to analyze the subcellular localization of DNA ligase I throughout the cell cycle. Asynchronously growing mouse fibroblasts and myoblasts were labeled with the thymidine analogue BrdU for 5 to 10 min and immediately fixed, to detect subnuclear sites of DNA replication. BrdU incorporation was visualized by staining with BrdU-specific mouse monoclonal antibodies, and samples were also stained for DNA ligase I with the affinity-purified rabbit antibodies. The cells that did not incorporate BrdU, and are therefore in G₁ or G₂ phase, exhibit a dispersed nucleoplasmic distribution of DNA ligase I with exclusion from nucleoli (data not shown). As depicted in Fig. 2, A–C, the nuclei with a punctate subnuclear BrdU pattern show colocalizing DNA ligase-labeled foci, as can be better seen in the overlay of the two images in C. This figure is a composite of nuclei, illustrating different patterns of subnuclear foci observed in both mouse fibroblasts and myoblasts. We further investigated the distribution of DNA ligase in interphase cells by costaining with anti-PCNA antibodies. One subnuclear pattern is presented in Fig. 2, D–F, and clearly shows the colocalization of both PCNA and DNA ligase I at sites of DNA replication. Nuclei with disperse PCNA nucleoplasmic signal, showed the same homogenous distribution of DNA ligase I (data not shown). The DNA ligase I distribution was identical using formaldehyde and methanol fixation.

In mitotic cells, at the metaphase stage shown by the alignment of the chromosomes in the metaphase plate in Fig. 2,J, DNA ligase I is excluded from the condensed chromosomes and distributes in the cytoplasm (Fig. 2,G). Later, during chromatid separation and movement to the spindle poles at anaphase in Fig. 2,K, DNA ligase I continues to be excluded from the condensed chromosomes (Fig. 2,H). At the end of telophase and cytokinesis, when the nuclear envelope reforms around the decondensing chromosomes (Fig. 2,L), DNA ligase I is immediately imported into the nucleus, as shown in Fig. 2 I.

In summary, DNA ligase I is excluded from condensed chromosomes during mitosis and immediately reenters the nucleus upon formation of the nuclear envelope. In interphase cells, it presents a homogenous nucleoplasmic pattern except during S phase, when it redistributes to subnuclear sites of DNA replication.

Since there are no dividing membranes in the nucleus, which could explain the concentration of proteins at these foci, we decided to further investigate the basis for this cell cycle-dependent redistribution. In the case of DNA MTase, a distinct targeting sequence had been identified that is necessary and sufficient for association with replication foci (24). The cDNA of human DNA ligase I has an open reading frame of 919 amino acids (2), and the protein resembles DNA MTase in that it also has a protease-sensitive NH₂-terminal domain, in this case of 249 amino acids.

To test whether we could reproduce the endogenous DNA ligase patterns with recombinant proteins, the enzyme was tagged by adding an epitope from the hemagglutinin of influenza virus (Flutag; Fig. 3,A) and visualized in transfected cells by immunofluorescence microscopy. Double staining with antibodies against DNA MTase, which labels replication foci (24), showed co-localization of DNA ligase I at these sites (Fig. 3,B, a–c). Tagged DNA ligase I, like the endogenous protein, redistributed during the cell cycle and showed the same patterns as DNA MTase and PCNA (Fig. 3 B, and data not shown).

To investigate whether or not DNA ligase I uses a mechanism similar to DNA MTase for association with replication foci, a series of deletion mutants was generated in search for a potential targeting sequence (Fig. 3,A). All fusion proteins were tested for stability in vivo as described before (24). In brief, Cos cells were transfected with the respective expression constructs; protein extracts were made and tested by Western blot analysis (data not shown). All constructs gave stable fusion proteins, which argues against possible artefacts due to instability problems. The apparent molecular weight of the fusion proteins differed in most cases from values deduced from the amino acid sequence. This discrepancy is consistent with the observation that DNA ligase I itself migrates anomalously slow (see Fig. 1). Two different epitope tags, Flutag and a β-gal–derived epitope, were inserted at different positions in the DNA ligase I cDNA, to rule out potential tagging artefacts. Two mutations deleting amino acids 308–772 and 264–919, immediately indicated that the entire catalytic domain was dispensable for association with replication foci. The latter were visualized as in Fig. 3 B, a–c, or by costaining with PCNA-specific antibodies (data not shown).

To fine map the region required for targeting, we constructed a series of COOH-terminal, NH₂-terminal, and internal deletions scanning the entire NH₂-terminal regulatory domain. The structure of these fusion proteins and their respective phenotype is shown in Fig. 3,A. Fig. 3,B, d–f, illustrates one example of a targeting proficient deletion mutant. On the other hand, several deletions within the regulatory domain abolished targeting, meaning the respective fusion proteins did not redistribute to replication foci in S phase nuclei and showed, instead, a dispersed nucleoplasmic distribution (Fig. 3,B, g–h). The fine mapping identified a bipartite-targeting sequence, which encompasses amino acids 1–28 and 111–179. This bipartite targeting sequence is necessary and sufficient to target heterologous proteins (like β-gal from Escherichia coli) to replication foci, since deletion of either part eliminates targeting (Fig. 3,A). Furthermore, this is the only targeting sequence within DNA ligase I, since deletion of just the first 28 amino acids in the context of the full length protein, abrogates targeting (Fig. 3 A). In other words, the catalytic domain (amino acids 250–919) by itself does not localize at replication foci, emphasizing the modular arrangement of targeting sequence and catalytic domain. While this work was in progress, a study geared towards the mapping of the NLS of DNA ligase I was published (34). In that report, one deletion construct lacking the first 115 amino acids was analyzed for subnuclear localization and found to be absent from replication foci, which is consistent with our mapping results.

The regulatory domain also contains the NLS. We found that the first 206 amino acids of DNA ligase I are sufficient for nuclear localization, while fusion proteins containing only the first 112 amino acids were clearly cytoplasmic (data not shown). This finding indicates that nuclear localization of DNA ligase I requires sequences spanning amino acids 112–206, which contains stretches of basic amino acids (e.g., amino acids 120–131 and/or 149–152) that fit the description of a potential NLS (12, 50). A recent report described the mapping of the DNA ligase I NLS to amino acids 119–131 (34), however, deletion of this region (removing amino acids 112–178 in the last ligase–β-gal fusion depicted in Fig. 3 A) does reduce but not abolish nuclear localization, i.e., the overproduced recombinant protein can be found in the nucleus and cytoplasm (data not shown). On the other hand, deletion of the first 28 amino acids also affected nuclear localization. These discrepancies with the previous study (34) can in part be explained because their experiments were based on fusions to a reporter protein that by itself can enter the nucleus.

Our results show that the classical NLSs (amino acids 120–131 and/or 149–152) are not absolutely required and also not sufficient for nuclear localization and that other regions (amino acids 1–28 and 178–206) contribute to the nuclear localization of DNA ligase I, which may be a combination of nuclear uptake and retention, as described for other proteins (48).

The identification of the targeting sequence in the human DNA ligase I raised the question whether or not this sequence was conserved in other proteins present at replication foci and in DNA ligases from other species. The comparison with the DNA MTase targeting sequence (24) shows no detectable similarity. On the contrary, both sequences are rather different; the DNA ligase targeting sequence is extremely hydrophilic, while the DNA MTase is rather hydrophobic (Fig. 4 A). This difference makes sense in view of their different biological function and may simply reflect their targeting to different parts of the replication factories. That is, these various targeting sequences most likely constitute protein–protein interaction surfaces in vivo, which are as diverse as their binding partners.

A comparison with other ATP-dependent DNA ligases shows that the catalytic domain is highly conserved throughout evolution; however, no sequences with homology to the human targeting sequence were detected in lower eukaryotic or prokaryotic homologues (e.g., the comparison with DNA ligase I from Schizosaccharomyces pombe, Fig. 4,B). On the other hand, the targeting sequence is conserved between human and mouse (72% identity; 46), and the human targeting sequence also functions in mouse cells (Figs. 3,B and 5 A). There is also considerable conservation (data not shown) with the Xenopus laevis DNA ligase I (25). The fact that the targeting sequence is missing or is very different in lower eukaryotic and prokaryotic DNA ligases and is also not required for complementation may indicate that it only recently developed in evolution.

So far, the existence of subnuclear replication foci has only been shown by immunofluorescence. We therefore decided to directly probe these structures in living cells and fused the full length as well as the NH₂ terminus alone containing the targeting sequence to the COOH-terminal end of the GFP, as schematically drawn in Fig. 5. The chimeric proteins were expressed in mouse cells and observed live under the microscope using an FITC filter. In addition to a nuclear dispersed distribution (first nucleus on the left hand side of Fig. 5, A and B), several discrete patterns of dots of different sizes and shapes were observed with the chimeric GFP-ligase proteins outlined in Fig. 5. Representative examples of the latter patterns are shown in the four nuclei at the right hand side of each panel. These patterns in live cells match the early, mid, and late S phase patterns reported in fixed and stained cells (14, 37, 40, 58). Based on that classification, the second nucleus from the left exhibits a fine punctate pattern of foci throughout the nucleoplasm characteristic of early S phase. The nucleus in the middle shows a concentration of foci at the nucleolar periphery corresponding to a later S phase stage. The two nuclei at the right hand side have larger foci with often irregular shape or loop-like structures, which are typical of late S phase. All these patterns were also observed by staining fixed cells with anti-DNA ligase I antibodies (Fig. 2) as well as with the other tagged constructs (Fig. 3, and data not shown). These same GFP-ligase–expressing cells were fixed and stained with anti-PCNA and anti-MTase antibody (Cardoso, M.C., R. Reusch, and H. Leonhardt, unpublished results), confirming the colocalization results presented in Figs. 2 and 3. The observation that the NH₂-terminal domain of DNA ligase I (which contains the targeting sequence mapped in Fig. 3) fused at the COOH terminus of GFP (schematically shown in Fig. 5 B) shows the same patterns as the full length DNA ligase I chimera with GFP indicate that the targeting sequence works as a ‘module' and can function in the context of unrelated proteins and irrespective of its location in the fusion construct. Furthermore, they allow direct visualization of subnuclear replication foci in living mammalian cells. The very characteristic redistribution of the GFP-ligase fusion proteins during the cell cycle makes these constructs a unique S phase marker for studies in living cells.

In this study, we describe the subcellular localization of DNA ligase I and analyze the basis for its cell cycle-dependent redistribution. We show that DNA ligase I is excluded from condensed chromosomes in mitotic cells and is rapidly imported into the nucleus upon formation of the nuclear envelope (Fig. 2). In interphase cells, DNA ligase I is homogenously distributed throughout the nucleoplasm except in S phase cells, when it is localized at subnuclear replication foci (Fig. 2). We mapped a bipartite targeting sequence, which is necessary and sufficient for this S phase-dependent redistribution (Fig. 3 A).

It should be mentioned that these results clearly differ from a previous report (34). That report claimed the identification of a targeting sequence solely based on a single deletion mutant not detected at replication foci, which, as a negative result, is by definition, inconclusive. Deletions often alter the overall folding and stability of proteins and can unspecifically affect functions that are far apart in the primary protein structure. For these reasons, a subcellular targeting sequence is usually defined as a protein sequence that (a) is necessary and (b) sufficient for subcellular localization; (c) works position independently; (d) is separated from the catalytic domain, and (e) can target heterologous proteins to the respective subcellular domain. In this study we mapped the targeting sequence of DNA ligase I and demonstrated that this sequence by itself is sufficient to recruit different heterologous proteins to replication foci in S phase cells. The targeting sequence functions as a module independently of its location in the fusion protein (see Figs. 3 and 5) and deletion of this sequence in the context of the entire DNA ligase I protein leaves the catalytic properties untouched (20) but abrogates its S phase-dependent association with replication foci. We show that the DNA ligase I targeting sequence is conserved between the human and mouse enzymes, and the human sequence also targets fusion proteins to replication foci in mouse cells (Fig. 3 B).

In lower eukaryotic homologues (e.g., yeast or Drosophila DNA ligases I) the NH₂-terminal domain is also dispensable for enzyme activity in vitro (1, 45, 55). However, these domains are clearly shorter and exhibit no similarity among each other or to the higher eukaryotic counterparts (Fig. 4,B, and data not shown). Furthermore, a truncated human DNA ligase I protein, with the entire NH₂-terminal domain deleted, is able to rescue yeast DNA ligase I mutant strains (2) but cannot rescue homozygous null DNA ligase I mutant mouse cells (42). The latter indicates that the NH₂-terminal domain of human DNA ligase I has essential functions in mammalian cells that are not required in lower eukaryotes. The identification and mapping of the targeting sequence (Fig. 3) now assigns a function to this domain in vivo and provides a possible explanation for those presumably conflicting in vitro and in vivo results.

Interestingly, the NH₂-terminal regulatory domain is also not conserved in the recently cloned mammalian DNA ligases III and IV, despite a high degree of homology throughout the catalytic domains (8, 60). These two enzymes are able to substitute for DNA ligase I in in vitro DNA repair assays (22, 49) but not in replication assays (31, 59). Altogether, these results suggest a function of the NH₂-terminal domain of DNA ligase I in DNA replication rather than repair, which fits well with our mapping of the targeting to replication foci in this domain. A comparison with the previously identified targeting sequence of the DNA MTase showed no discernible similarities (Fig. 4,A), which suggests that these sequences interface with different components of the replication factory as illustrated in Fig. 6. In this context it is interesting that biochemical fractionation experiments have shown that DNA ligase I is present in megadalton, multiprotein complexes with multiple catalytic activities associated with DNA replication (27, 28, 32, 39, 62). The identification of the targeting sequence now renders possible a directed search for interacting factors and the elucidation of the molecular architecture of these replication factories.

Similar targeting principles seem to apply also to other functional domains of the mammalian nucleus (for review see 23). Thus, targeting sequences were identified in the Drosophila splicing regulators su(w^a) and tra, which are concentrated at distinct nuclear foci called “speckled compartment” (26). Further, the nucleolar localization of the retroviral proteins HTLV-1 Rex (51), HIV-1 Tat (11, 13), and HIV-1 Rev (9, 21) was shown to be mediated by nucleolar targeting sequences. Moreover, nucleolar targeting of HIV-1 Rev was shown to be required for in vivo function (9, 21). Finally, the NH₂-terminal 102 amino acids of p80-coilin, a protein that localizes to nuclear coiled bodies, are necessary and sufficient for targeting to this organelle (63). All of these different sequences have one thing in common: they are necessary and sufficient for targeting to subnuclear domains; however, they do not share similar protein motifs. On the contrary, they are as diverse as their function and the domain to which they target.

The vast majority of studies on nuclear organization have been done on fixed and stained cells, with the caveat of possible artefacts (for review see 10). Several efforts have been undertaken to use physiological buffers and unfixed cells to study subnuclear replication sites. Nevertheless, these studies were performed using permeabilized cells that underwent still extensive manipulation before these subnuclear compartments were visualized (16). Until now, localization of proteins at replication sites had not yet been demonstrated in live cells. The localization of DNA ligase I at replication foci (Fig. 2), the identification of a bipartite targeting sequence in its NH₂-terminal regulatory domain, which mediates cell cycle-specific association (Fig. 3), and the availability of the GFP allowed us to address this issue directly. Chimeric proteins comprising GFP and DNA ligase I (full length or NH₂-terminal domain) allow the visualization of these subnuclear structures in living cells and show patterns indistinguishable from fixed and stained cells (Fig. 5). These findings enable direct visualization of S phase in living cells, which should be very useful for cell cycle studies.

In summary, we describe the subcellular distribution of DNA ligase I during the cell cycle and map the sequence responsible for its association with replication foci in S phase cells. We showed that the targeting sequence works as an independent module and can direct unrelated proteins (like β-gal from Escherichia coli and GFP from Aequorea victoria) to sites of DNA replication irrespective of its position in the fusion protein. The targeting sequence works across species (human and mouse) as well as in different cell types.

Altogether, these results suggest that targeting might be a general principle of nuclear organization and might be a means to cope with the growing complexity in higher eukaryotes as evolution progressed. The targeting sequence, by bringing the catalytic domain to the right place at the right time, allows catalysis to occur at higher order kinetics, which meets the needs of a competitive and demanding environment such as the mammalian nucleus. We propose that the efficient coordination of complex processes such as DNA replication, from controlled initiation to ligation of Okazaki fragments and DNA methylation, might be accomplished in the mammalian nucleus by integration into assembly line-like protein factories (Fig. 6), which increase the effective enzyme concentration, specificity, and processivity. This dynamic nuclear architecture thus constitutes a higher order mechanism of regulating enzyme activity in vivo.

We are grateful to F.C. Luft and H. Haller for encouragement, support, and critical reading of the manuscript. We are indebted to M. Cochran, C. Clark, and L. Steinberg for their very special support of this work, and we would also like to acknowledge D. Hänlein for untiring help and advice with our computers. We thank G. Vargas for constructing a GFP–DNA ligase fusion.

This work was supported in part by a grant from the Deutsche Forschungsgemeinschaft (Le 721/2-1) and from the Max Delbrück Center for Molecular Medicine.

β-gal

β-galactosidase

GFP

green fluorescent protein

MTase

methyltransferase

NLS

nuclear localization sequence

PCNA

proliferating cell nuclear antigen