Changes in Organization of Crithidia fasciculata Kinetoplast DNA Replication Proteins during the Cell Cycle

C. fasciculata were cultured in brain heart infusion (Difco Laboratories, Inc., Detroit, MI) containing 10 μg/ml hemin, and were grown at 28°C in a shaking water bath. Synchronization by hydroxyurea arrest was performed as described (Pasion et al., 1994). In brief, a cell culture in late log phase (∼10⁸ cells/ml) was diluted to 10⁷ cells/ml and incubated for 6 h in medium with 200 μg/ml hydroxyurea. Synchronized cells were collected by centrifugation (4,000 rpm, 10 min, room temperature) (HS4 rotor; Sorvall, Newtown, CT), resuspended in fresh medium without hydroxyurea, and then allowed to grow at 28°C for an additional 6 h.

Several parameters of synchronized cultures were analyzed at 30-min intervals. Cell density was determined by counting in a hemacytometer. The fraction of dividing cells was determined by phase and fluorescence microscopy on fixed cells stained with 4,6-diamidino-2-phenylindole (DAPI) (see below for fixation conditions). Cells with two nuclei that had not completed cytokinesis were counted as dividing. The rate of DNA synthesis was determined by measuring [³H]thymidine incorporation during a 10 min pulse. [³H]Thymidine (1 mCi/ml, 81 Ci/mmol, 10 μl; NEN Life Science Products, Boston, MA) was added to 65 μl of culture and incubated for 10 min at 28°C. The cells were then treated with proteinase K in SDS and the DNA was extracted with phenol/chloroform/iso-amyl-alcohol. The labeled DNA was bound to Whatman DE81 paper (Clifton, NJ), washed in 0.5 M sodium phosphate, pH 7.0, and then counted in a scintillation counter.

The anti-DNA primase was a mouse polyclonal serum (Li and Englund, 1997). The anti-topo II was mouse mAb 3A4 (a gift of D.S. Ray, University of California, Los Angeles, CA) (Melendy et al., 1988). The anti-pol β was rabbit serum JH167, raised against recombinant protein, the preparation of which will be described elsewhere. Anti-pol β serum was affinity purified on recombinant antigen bound to Immobilon P membrane (Harlow and Lane, 1988).

Aliquots (10 ml) from a synchronized C. fasciculata culture were taken at 30-min intervals. Cells were harvested by centrifugation (Sorvall HS-4 rotor, 7 min, 2,500 g), washed in PBS (137 mM NaCl, 2.7 mM KCl, 4.3 mM Na₂HPO₄, 1.4 mM KH₂PO₄) and lysed at 10⁹ cells/ml in 1% NP-40, 200 mM Tris-HCl, pH 7.5, 25 mM NaCl, 20 mM EDTA, 4 mM PMSF, 4 μg/ml leupeptin, 1 μg/ml pepstatin A, 50 μg/ml antipain. Crude lysates were cleared by centrifugation for 15 min in a microfuge at 4°C, and supernatants were frozen in dry ice/ethanol and stored at −70°C. SDS-PAGE (10% gel) and transfer to Immobilon P membranes (Amersham Life Science, Arlington Heights, IL) were performed as described (Torri and Englund, 1995). Membranes were blocked for 60 min in 5% BSA in TBST (20 mM Tris-HCl, pH 7.5, 0.5 M NaCl, 0.1% Triton X-100), and were probed with a 1:1,000 dilution of anti-pol β antibody. After three 15-min washes in TBST, membranes were probed for 1 h with a 1:1,000 dilution of ¹²⁵I-protein A (30 mCi/mg, 100 μCi/ml; Amersham Life Science) in TBST and washed as above. Membranes were exposed to a Fuji PhosphorImager plate for 15 h, and the results were quantitated using MacBas software (V2.31).

All procedures were conducted at room temperature unless otherwise indicated. Cells were centrifuged for 1 min in a microfuge, washed, and then resuspended in 1 vol of PBS. Aliquots (25 μl, ∼5 × 10⁵ cells) were spotted on poly-l-lysine–coated slides and the cells were allowed to adhere for 10 min. For immunofluorescence against DNA primase and pol β, cells were fixed in 2% paraformaldehyde for 5 min, washed twice in PBS with 0.1 M glycine, pH 8.6, for 3 min, washed once in PBS for 3 min, and then immersed in methanol at −20°C overnight. Two different fixation methods were used to detect topo II. Cells were fixed either as described above, or fixed by methanol overnight at −20°C. These fixation methods yield comparable results. After fixation, slides were rehydrated with three 5-min washes in PBS before a 30-min incubation in blocking buffer (10% goat serum, 0.9× PBS). Primary antibodies were diluted in blocking buffer (topo II antibody, 1:20; pol β antibody, 1:50; primase antibody, 1:250), and slides were incubated at room temperature for 1 h. Slides were washed three times for 5 min in PBS, and then were incubated 45 min with a 1:250 dilution of secondary antibody (see figure legends). Slides were given three 5-min washes in PBS with 0.1 μg/ml DAPI included in the first two washes. Finally, slides were mounted in Mowiol (Boehringer Mannheim Corp., Indianapolis, IN) with 2.5% 1,4-diazobicyclo-[2.2.2]-octane (DABCO) as an antifade agent.

Fluorescein-5(6)-carboxamidocaproyl-[5-(3-aminoallyl)]-2′-deoxy-uridine-5′-triphosphate (dUTP-F) labeling has been used previously in our laboratory to analyze isolated kDNA networks (Guilbride and Englund, 1998) and is based on a method previously used for identifying cells undergoing apoptosis (Gavrieli et al., 1992). For in situ labeling of minicircle gaps, cells were adhered to slides, fixed in PFA as described above, and incubated for 10 min at room temperature in equilibration buffer (200 mM potassium cacodylate, 25 mM Tris-HCl, pH 6.6, 0.2 mM DTT, 2.25 mM CoCl₂, and 0.25 mg/ml BSA). Slides were then incubated with 25 μl reaction buffer containing 180 mM potassium cacodylate, 22.5 mM Tris-HCl, pH 6.6, 0.18 mM DTT, 2.0 mM CoCl₂, 0.23 mg/ml BSA, 0.1 mM EDTA, 10 μM dATP, 10 units of terminal deoxynucleotidyltransferase (TdT; Boehringer Mannheim Corp.), and 5 μM dUTP-F (Boehringer Mannheim Corp.). After 60 min at room temperature, the reaction was stopped with a 10 min wash in 2× SSC (0.3 M NaCl, 30 mM Na₂ citrate). Slides were then washed three times for 5 min in PBS before proceeding with immunofluorescence.

We found, as previously reported, that in asynchronously-growing cells pol β and topo II have similar patterns of localization to two antipodal sites flanking the kDNA disk (Melendy et al., 1988; Ferguson et al., 1992). To further characterize the antipodal localizations of topo II and pol β, we used double-label immunofluorescence to probe both enzymes. We observed that pol β and topo II colocalized to the same sites at the network edge, as shown in Fig. 1. In addition, we observed that in some cells with topo II concentrated in these antipodal sites, a small amount of the enzyme is also detected either between these sites, in the region of the kDNA network (Fig. 2 d), or in a region adjacent to the flagellar face of the network (data not shown).

Our next objective was to localize the pol β at different stages of the cell cycle using cells synchronized with hydroxyurea. We followed the growth of synchronized cultures through two cell division cycles, measuring the rate of incorporation of [³H]thymidine into total cellular DNA, the percentage of dividing cells, and the density of cells in the culture (Fig. 2,a). After release from hydroxyurea arrest, the rate of [³H]thymidine incorporation (Fig. 2,a, open squares) peaks at 30 and 180 min, each peak indicating an S phase. This incorporation is due to synthesis of both nuclear DNA (75% of total) and kDNA (25% of total) (Englund, 1979) that replicate in approximate synchrony (Cosgrove and Skeen, 1970). Sudden increases in the percentage of cells with two nuclei (Fig. 2 a, closed circles) at 120 and 270 min mark passage of the culture through mitosis and indicate the timing of the subsequent cell division. Cytokinesis occurs fairly quickly, and thus the populations of dividing cells also contain some mitotic cells and daughter cells already in G1. This characterization of the C. fasciculata cell cycle agrees with data previously reported (Pasion et al., 1994) and is reproducible between experiments.

Using a synchronized culture, we found that detection of pol β in the antipodal sites is cell cycle dependent. The number of cells with this antipodal localization pattern peaks at 30–60 and 240–270 min, during interphase (Fig. 2,b, closed triangles; c, upper panels). The percentage of cells with this localization pattern decreases during the peak of cell division, however, when only 7% show this localization (Fig. 2,b). Unexpectedly, when not localized in the antipodal sites, the pol β is not detectable by immunofluorescence (Fig. 2 c, lower panels).

Our inability to detect pol β immunofluorescence in the population of dividing cells raised the possibility that the enzyme abundance may change during the cell cycle. To address this issue, we performed Western blots on whole cell lysates taken at 30 min intervals during synchronized growth of a C. fasciculata culture. We found that the enzyme is present at similar levels in all time points (Fig. 3 a). Thus while the pol β protein is continuously present, it is detectable by immunofluorescence only at certain cell cycle stages. Possible explanations of the inability to immunolocalize this enzyme will be addressed in Discussion.

To determine whether this cyclic localization pattern was a feature of all enzymes detected in the antipodal sites, we also examined topo II localization at different cell cycle stages, using the same culture as was used for pol β. In this experiment synchronized cells were scored for the presence or absence of topo II in both antipodal sites. During interphase most cells have topo II in both antipodal sites (Figs. 2,b, open squares; d, upper panels), but the percentage of cells with topo II concentrated in these sites decreases during cell division (120 and 300–330 min). Thus the periodicity of topo II localization to both antipodal sites is similar to that of the pol β. Unlike pol β, however, topo II is detectable by immunofluorescence in virtually all cells at all stages of the cell cycle. When topo II is not detected in the antipodal sites, it is present either in a diffuse pattern near the kDNA (Fig. 2 d, lower panels) or in other localization patterns that will be discussed below.

These experiments indicate that both topo II and pol β are periodically detected in the two antipodal sites flanking the network edge. There are significant differences, however, in the timing of these changes in enzyme localization (Fig. 2,b, pol β, closed triangles; topo II, open squares). For example, at the 120-min time point 30% of cells have topo II localized in both antipodal sites, while <10% have pol β in this location. In addition, after cell division the accumulation of topo II in the two antipodal sites precedes that of pol β (Fig. 2 b, see 180-min time point). To further evaluate these differences between topo II and pol β it was necessary to determine the timing of the changes in localization with greater precision. We therefore developed a new method to determine the kDNA replication status in individual, fixed cells from an asynchronous culture. This method, coupled with immunolocalization of the two enzymes, allowed a correlation of enzyme localization with the stage of kDNA replication in individual cells.

We determined the kDNA replication stage by fluorescence microscopy of individual cells in which fluorescein-labeled dUTP (dUTP-F) had been incorporated in situ into the endogenous gaps in newly replicated minicircles by terminal deoxynucleotidyl transferase (TdT). This analysis was facilitated by the well-characterized distribution of covalently-closed and gapped minicircles in pre-replication, replicating, and post-replication kDNA in both isolated networks (Englund, 1978; Pérez-Morga and Englund, 1993; Guilbride and Englund, 1998) and for networks in vivo (Ferguson et al., 1992).

Fig. 4 shows images of the kinetoplast region of dUTP-F–labeled cells from an asynchronous culture. In vivo, the kDNA network is condensed into a disk positioned perpendicularly to the flagellum, and therefore fluorescent images usually provide a view of the edge of the disk, as in Fig. 4, c and i. In fixed cells the kDNA disk is occasionally re-oriented, or “tipped,” providing a view of the face of the disk. The frequency of tipped networks can be increased by a mild protease treatment (examples in Fig. 4, e, g, and h) (Ferguson et al., 1992). Since images of a tipped disk are more informative about the degree of replication in a partially replicated network, we chose most examples in Fig. 4 with the disk tipped.

Pre-replication networks do not label with dUTP-F because the minicircles are all covalently closed (Fig. 4, a–c). In contrast, networks undergoing replication have a peripheral ring of dUTP-F label and a central zone of unlabeled minicircles (Fig. 4, e–g). kDNA at an early stage of replication has a narrow peripheral ring (Fig. 4,e) that increases in thickness during the replication process (Fig. 4, e–g). Replicating networks (Fig. 4, d–i) are always flanked by two antipodally positioned, bright dUTP-F spots. These bright spots colocalize with pol β and topo II (see below), and their intense labeling by dUTP-F is probably due to the presence of highly gapped, free minicircle replication intermediates (Johnson, 1998). Fig. 4,d shows a network flanked by antipodal spots of dUTP-F, but without the peripheral ring of fluorescence. This image likely represents the earliest stage of kDNA replication before a significant number of gapped minicircles have been attached to the network periphery. Consistent with this possibility, the dUTP-F fluorescence in Fig. 4,d was weak and required a longer (58 s) exposure time than other images in Fig. 4, e–l (1.5–4 s). Some replicating networks, while flanked by bright dUTP-F spots, appear to lack an unlabeled central zone (Fig. 4,h). In these cases, in the final stages of kDNA replication, the central unlabeled zone is probably too small to have been observed with fluorescence microscopy. Since the network in Fig. 4,i is positioned vertically it is impossible to determine whether it is early or late in the replication process, but it is characterized as replicating because of the antipodally positioned bright dUTP-F spots. Postreplication kDNA networks label uniformly with dUTP-F because all of the minicircles are gapped, and these networks are not flanked by bright dUTP-F spots (Fig. 4, j–l). Some postreplication networks appear irregularly shaped, often like a “V,” and do not lie in a single plane of focus (Fig. 4,l). Networks with this irregular structure may be beginning the network scission process. Repair of the remaining minicircle gaps occurs before network scission (Pérez-Morga and Englund, 1993b) and results in reduction and ultimately elimination of dUTP-F fluorescence (Fig. 4,m is probably a partially repaired network). Finally, after network scission, the cells contain two kDNA networks that do not incorporate dUTP-F as all the minicircles are covalently closed (Fig. 4 n).

We used immunofluorescence to determine the location of pol β in cells that had been first labeled with dUTP-F to determine the stage of kDNA replication (see Table I and Fig. 5). In cells which had not initiated kDNA replication, we detected no pol β immunofluorescence (Fig. 5, a–b). In contrast, 100% of the cells undergoing kDNA replication had pol β localized in the two antipodal sites (Fig. 5, c–e) that co-localize with the two bright spots of dUTP-F fluorescence. After replication is complete, different patterns of pol β localization were observed. In 54% of these cells, pol β was found in the two antipodal sites (Fig. 5,f). At this stage of kDNA replication, some weak pol β signal is also detected in the kDNA region (Fig. 5,f). The rest of the post-replication networks either contain no detectable pol β immunofluorescence (33%, Fig. 5,h) or the enzyme is in other locations (13% of post-replication cells, see Fig. 5,g). Finally, in dividing cells which have two daughter kDNA networks (following gap repair and network scission), none showed detectable pol β immunofluorescence (Fig. 5 i).

At certain stages of kDNA replication the pattern of topo II localization in cells labeled with dUTP-F differed significantly from that of pol β (Table I; Fig. 6). Before the onset of kDNA replication all cells had topo II detectable in the kinetoplast region; in 22% topo II was found to be diffuse throughout the kDNA region (Fig. 6,a). In nearly half (43%) of pre-replication cells topo II was localized to both antipodal sites (Fig. 6,d), but surprisingly, 35% had topo II concentrated at only a single site at the network edge (Fig. 6, b and c).

As with pol β, all cells undergoing kDNA replication had topo II concentrated in both antipodal sites, which colocalized with the bright spots of dUTP-F fluorescence (Fig. 6, e–g). Additionally, some weaker topo II signal was detected in the region of the kDNA network. After network replication, topo II remains localized to both antipodal sites in 73% of cells (Fig. 6, h–j), but it has a more diffuse localization in the kDNA region in the other 27% (Fig. 6,k). Once the processes of network repair and scission are complete, 60% of cells still have topo II localized in two discrete sites, although now each daughter network is associated with only a single site of topo II localization (Fig. 6, l and m). The remaining 40% of these cells have topo II diffusely localized in the kDNA region (Fig. 6 n).

Given the cell cycle variation in localization pattern of pol β and topo II, we were interested to determine whether the localization of enzymes not detected in the antipodal sites also varied during the cell cycle. To this end, we performed immunolocalization of the DNA primase in conjunction with hydroxyurea synchronization. In asynchronous cells, primase is localized to regions adjacent to the faces of the kDNA disk (Li and Englund, 1997). Using synchronized cultures we found that the primase is detectable in virtually all cells (Fig. 7,a), and is similarly localized to the two network faces at all stages of the cell cycle (see Fig. 7 b for examples of cells in S phase; and c for examples of dividing cells).

The specific location of replication enzymes in unique sites surrounding the kDNA network is one of the most striking features of the kDNA replication system. In this paper we demonstrate the colocalization of pol β and topo II, and use two independent methods to analyze the changes in location of three replication enzymes during the cell cycle. Surprisingly, we found that these enzymes acted differently. The DNA primase, localized adjacent to the faces of the kDNA disk, was invariant during the cell cycle. In contrast, pol β and topo II colocalize to the antipodal sites during the period of kDNA replication, but behaved differently at other cell cycle stages.

Although pol β is located in the antipodal sites throughout kDNA replication (Figs. 2 and 5; Table I), this localization pattern is not static. Despite constant levels of protein (indicated by Western blots, see Fig. 3), the enzyme ceases to be detectable by immunofluorescence shortly after network replication is complete. Pol β remains undetectable by immunofluorescence throughout G1, and then reappears in the antipodal sites abruptly at the onset of kDNA replication. This coincidence of renewed detectability of pol β and the initiation of kDNA replication is striking, and suggests these events are coordinately regulated. Furthermore, the appearance of pol β in the two antipodal sites precisely at the onset of kDNA replication suggests that this enzyme has an essential role in that process. Given its lack of fidelity and low processivity (Torri et al., 1994), however, it is unlikely to be the major replicative enzyme, and we have recently detected and partially purified a second mitochondrial DNA polymerase which may play that role (Klingbeil, M., and P.T. Englund, unpublished observations). Since pol β enzymes efficiently fill gapped templates (Torri et al., 1994; Singhal et al., 1995), the C. fasciculata pol β is well positioned in the antipodal sites to function in the partial repair of the highly gapped minicircle progeny, a process known to occur just before reattachment to the network (Kitchin et al., 1985). Later in the Discussion section we will comment on the lack of detectability of pol β by immunofluorescence during part of the cell cycle.

Topo II, like pol β, is always detected in the two antipodal sites during kDNA replication (Figs. 2 and 6, and Table I). Unlike pol β, however, topo II is detected by immunofluorescence at all cell cycle stages, and is antipodally localized in some pre-replication and postreplication cells. In addition, at these times before and after kDNA replication, topo II is frequently localized to a single site at the network edge in some cells. Presumably, after kDNA replication, a post-replication network associated with two antipodally-positioned sites divides into two daughter networks, each associated with a single site. Consistent with this hypothesis, we never observed a post-scission network flanked by two antipodal sites. Thus, during cell division, each daughter cell must inherit a single site and a daughter kDNA network, yielding a G1 cell with a single site associated with the pre-replication network. The second antipodal site must then form during G1.

What is the nature of the two antipodal sites to which pol β and topo II colocalize? It is unlikely that the sites are comprised of stoichiometric complexes of these enzymes, since crude estimates of their relative abundance (based on recovery of activity during purification) indicate that pol β is ∼50-fold more abundant than topo II.

Our detection of topo II in discrete site(s) at all cell cycle stages suggests that these sites are permanent structures in the mitochondrial architecture. The sites are consistently found in the same focal plane and antipodal position relative to the kDNA (Ferguson et al., 1992), indicating their fixed position within the mitochondrial matrix. Such organized sites for enzyme localization may ensure not only that newly replicated minicircles are attached at opposing edges of the network (Simpson and Simpson, 1976; Pérez-Morga and Englund, 1993a), but could also establish the spatial configuration of other processes in the maintenance of the kDNA network. For example, one could speculate a role for the sites in establishing the line of cleavage in the center of the network before network scission. That the primase is also localized in fixed positions throughout the cell cycle indicates that this enzyme may also associate with structural elements that are permanent components of the mitochondrial matrix. Clearly, to further understand the intramitochondrial organization of these proteins it will be necessary to identify other components of both the antipodal sites and the areas colocalizing with primase.

As fixed components within the mitochondrion, these localization sites may also associate with structures within the mitochondrial membrane, or even outside the mitochondrion. Experiments on Saccharomyces cerevisiae demonstrated that the mtDNA is anchored to the mitochondrial membrane, and such anchoring explains the non-random mtDNA inheritance patterns (Nunnari et al., 1997). In bacteria, accumulating evidence suggests multiprotein complexes bridging the cell membrane and the bacterial genome function in chromosome maintenance and inheritance (Firshein and Kim, 1997; Mohl and Gober, 1997). In T. brucei, the kDNA network is physically attached (through the mitochondrial membrane) to the basal bodies (Robinson and Gull, 1991). Furthermore, kDNA segregation is dependent upon the microtubule-mediated basal body separation (Robinson and Gull, 1991). A basal body–kDNA network association is also found in C. fasciculata (Robinson, D.R., and P.T. Englund, unpublished observations). Unfortunately, antibodies specific to either basal bodies or the network attachment site in C. fasciculata are currently unavailable. However, experiments correlating the relative positions of the topo II–localization sites with sites of basal body–kDNA attachment could elucidate the possible functions of these localization sites in kDNA maintenance or segregation.

We do not know why pol β is undetected by immunofluorescence at some cell cycle stages, since the steady state protein level does not change (Fig. 2). One possibility is that pol β is dynamically localized to the antipodal sites during the cell cycle. The enzyme could assemble at the antipodal sites during kDNA replication, subsequently disassemble, and disperse throughout the mitochondrial matrix. When not sequestered in the antipodal sites the enzyme may be too dilute for immunofluorescence detection. Our attempts to detect dispersed pol β signal with long exposures resulted only in amplification of background signal throughout the cell, and the result was not distinguishable from control experiments in which we used only secondary antibody. Another explanation is that during G1 and cytokinesis pol β epitopes may be obscured, or masked, by protein–protein interactions that make the protein unrecognizable to antibodies in situ. The “masked” pol β could be located either in the antipodal sites, or dispersed throughout the mitochondrion.

Candidates for proteins that may interact with pol β include DNA repair enzymes. Mammalian nuclear pol β has been well characterized for its role in base excision repair (Nealon et al., 1996; Sobol et al., 1996), and it is known to form complexes with other base excision repair enzymes such as AP endonuclease (Bennett et al., 1997) and DNA ligase (Prasad et al., 1996). The abundance of reactive oxygen species, which are known to damage DNA, in mitochondria may necessitate such a repair pathway in this organelle (Richter, 1995). In support of this possibility we have recently detected and partially purified an abundant AP endonuclease (a key enzyme in the base excision repair pathway) from C. fasciculata mitochondria (Saxowsky, T., and P.T. Englund, unpublished observations). Thus in C. fasciculata mitochondria, pol β may function in kDNA replication by filling in minicircle gaps, and then subsequently interact with base excision repair enzymes and fulfill a second role in DNA repair.

This work has implications for the control of kDNA replication. Unlike mammalian mitochondrial DNA (see Introduction), kDNA replication has been known for many years to proceed during a discrete phase of the cell cycle, with timing close to that of the nuclear S phase (Cosgrove and Skeen, 1970; Simpson and Braly, 1970; Woodward and Gull, 1990). Little is known about either the molecular factors that trigger the initiation of kDNA replication or the synchronization of this event with nuclear DNA replication. Ray and co-workers have shown a cell cycle dependence in the periodic accumulation of mRNA levels of genes for certain proteins involved in kDNA and nuclear replication (Pasion et al., 1994; Brown and Ray, 1997; Hines and Ray, 1997). Their finding obviously relates to kDNA replication control and the synchrony of replication of nuclear and kDNA. We suggest that the intramitochondrial reorganization of certain replication enzymes may also play a role in control of kDNA replication. It will be of great interest to identify the factors that trigger these enzymes to assemble at discrete sites around the kDNA, and to further understand the nature and function of these antipodal sites.

We thank D. Ray for the gift of the anti–topo II antibody, C. Li for anti-primase antibody, A. Torri for preparation of the pol β expression construct, and V. Klein for early morning assistance. We thank T. Shapiro, B. Sollner-Webb, and members of our lab for critical reading of the manuscript, and D. Robinson, L. Rocco Carpenter, and T. Shapiro for many helpful discussions.

This work was supported by a grant (GM27608) from the National Institutes of Health. C.E. Johnson was supported in part by National Institutes of Health training grant 2T32 GM07445.

kDNA

kinetoplast DNA

pol β

DNA polymerase β

topo II

topoisomerase II

DAPI

4,6-diamidino-2-phenylindole

TdT

terminal deoxynucleotidyltransferase

dUTP-F

fluorescein-5(6)-carboxamidocaproyl-[5-(3-aminoallyl)-2′-deoxy-uridine-5′-triphosphate

RP-A

replication protein A