substrate specificity of human endonuclease iii (hnth1): effect of
TRANSCRIPT
Substrate Specificity of Human Endonuclease III (hNth1): Effect of Human AP
Endonuclease 1 (APE1) on hNth1 Activity
Dina R. Marenstein‡, Michael K. Chan‡, Alvin Altamirano*, Ashis K. Basu*, Robert J.
Boorstein‡, Richard P. Cunningham§ and George W. Teebor‡¶.
‡ Department of Pathology and Kaplan Comprehensive Cancer Center, New York University
School of Medicine, New York, NY 10016. *Department of Chemistry, University of
Connecticut, Storrs, CT 06269. § Department of Biological Sciences, The University at Albany,
SUNY, Albany, NY 12222.
Running Title: Substrate-specific modulation of hNth1 activity by APE1
¶ To whom correspondence should be addressed:
Dept. of Pathology, New York University Medical Center. 550 First Ave., New York, N.Y.
10016. Tel.: 212-263-5473; Fax: 212-263-8211; Email: [email protected].
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Copyright 2003 by The American Society for Biochemistry and Molecular Biology, Inc.
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SUMMARY
Base excision repair of oxidized pyrimidines in human DNA is initiated by the DNA N-
glycosylase/AP lyase, hNth1, the homolog of E. coli endonuclease III (Nth). In contrast to Nth,
the DNA N-glycosylase activity of hNth1 was 7 fold greater than its AP lyase activity when the
DNA substrate contained a thymine glycol (Tg) opposite adenine (Tg:A) (1). When Tg was
opposite guanine (Tg:G), the 2 activities were of the same specific activity as the AP lyase
activity of hNth1 against Tg:A (2). We now demonstrate that hNth1 was inhibited by the product
of its DNA N-glycosylase activity directed against Tg:G, the AP:G site. In contrast, hNth1 was
not as inhibited by the AP:A site arising from release of Tg from Tg:A. Addition of human AP
endonuclease (APE1) increased dissociation of hNth1 from the DNA N-glycosylase generated
AP:A site, resulting in abrogation of AP lyase activity and an increase in turnover of the DNA
N-glycosylase activity of hNth1. Addition of APE1 did not abrogate hNth1 AP lyase activity
against Tg:G. The stimulatory protein YB-1, (1), added to APE1, resulted in an additive increase
in both activities of hNth1 regardless of base pairing. Tg:A is formed by oxidative attack on
thymine opposite adenine. Tg:G is formed by oxidative attack on 5-methylcytosine opposite
guanine (3). It is possible that the in vitro substrate selectivity of mammalian Nth1 and the
concomitant selective stimulation of activity by APE1 are indicative of selective repair of
oxidative damage in different regions of the genome.
INTRODUCTION
Like its E. coli homolog, endonuclease III (Nth), hNth1 is a bifunctional DNA N-
glycosylase/AP lyase which removes ring-saturated pyrimidines, be they hydrated, reduced or
oxidized, from the DNA backbone as the initial step of base excision repair (BER) of such
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modified residues 1. The oxidation product of thymine, 5,6-dihydroxy-5,6-dihydrothymine
(thymine glycol [Tg]) is a widely studied model substrate for hNth1, which catalyzes its release
from DNA via its DNA N-glycosylase activity. This enzymatic activity is mediated via
formation of a transient Schiff base (imino) DNA-enzyme intermediate, an example of covalent
catalysis and a characteristic of all known bifunctional DNA N-glycosylases/AP lyases (4,5).
The Schiff base moiety has been hypothesized to be required for the enzymatic catalysis of the
β-elimination reaction, which effects DNA strand cleavage 3’ to the abasic (apurinic/apyrimidinic,
AP) site formed as product of the release of the base from the 2’-deoxyribose moiety to which it
was linked. The hydrolysis of the Schiff base intermediate can occur in the absence of, or
following, enzyme-catalyzed β-elimination (the AP lyase activity), resulting in DNA strand
cleavage. The enzymatic catalysis of β-elimination by DNA N-glycosylases/AP lyases has been
shown to be initiated via abstraction of the deoxyribose pro-S-2’-hydrogen by a basic amino
acid in the enzyme active site. Several factors, including pH, can affect the efficiency of the AP
Lyase step by affecting substrate binding and proton abstraction (5).
Based on the results of studies with Nth, the 2 activities of hNth1, DNA N-glycosylase
and β-elimination catalysis, require the formation of the Schiff base intermediate and were
thought to occur concomitantly. However, data from our laboratory and from other laboratories
indicated that DNA N-glycosylase and β-elimination catalysis by mammalian members of the
endonuclease III enzyme superfamily was not concurrent under the assay conditions employed
(1, 6-8). We were the first to report that the DNA N-glycosylase activity and the AP lyase
activity of hNth1 were not concurrent i.e. that the rate of AP lyase mediated strand cleavage was
much slower than the rate of DNA N-glycosylase mediated base release. These results were
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similar to the non-concurrence of base release and strand cleavage reported for mammalian 8-
oxoguanine DNA N-glycosylase homologue, Ogg1 (8). In this report, we present data
demonstrating that the dissociation of the 2 activities of hNth1 is dependent on the nature of the
orphan base opposite the Tg residue in DNA.
In our studies of the properties of hNth1, we have focused our attention on protein
modulators of hNth1 activities. This approach resulted from our original observation that the
enzymatic properties of mammalian endonuclease III homologs were strikingly different from
bacterial endonuclease III. Our laboratory was the first to identify mammalian endonuclease III
homologs and describe their distinct kinetic properties (9, 10). These observations spurred us to
isolate novel proteins which might modulate the enzyme activities of mammalian Nth1. A yeast
2 hybrid search resulted in identification of the pluripotent transcription factor Y-box binding
protein 1 (YB-1, also known as DNA binding protein B) as a stimulator of hNth1 activity (1).
We now report further aspects of the proteomics of hNth1-initiated BER, based on the
effects of human AP endonuclease APE1/HAP-1/ref-1 (APE1) on hNth1 activity. APE1, a
human homologue of E. coli exonuclease III (Xth), catalyses the hydrolysis of the
phosphodiester bond 5’ to AP sites, generating a free 3’ hydroxyl end for the initiation of DNA
polymerase repair synthesis.
APE1 has recently been demonstrated to play a significant role in the coordination of
BER. APE1 has been shown to modulate the activities of several major DNA N-glycosylases,
although physical interaction between APE1 and most of these DNA N-glycosylases has not
been demonstrated (6, 7, 11, 12). The functional interaction between APE1 and DNA N-
glycosylases is consistent with the model of the coordinated activities of BER enzymes at sites of
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DNA damage (13-16). Two groups independently demonstrated the stimulation of hOgg1 by
APE1 (6, 7). Both groups demonstrated that APE1 replaced hOgg1 bound to the AP site
following base release and prior to hOgg1-catalysed β↑elimination. This resulted in bypass of
the AP lyase step and an increase in hOgg1 turnover. In this paper we report similar findings
with hNth1 and APE1. However, stimulation by APE1 proved to be dependent on the nature of
the orphan base opposite the Tg residue in DNA.
EXPERIMENTAL PROCEDURES
Proteins- Expression and purification of recombinant hNth1 was induced as described
previously (10). hNth1 concentration was quantified using an extinction coefficient of 1 O.D. at
A410 = 69.4 µM for the C-terminal cubane 4[Fe-S] cluster (17). YB-1 was expressed with a 6x
His tag in Trichoplusia ni cells and purified as described (1). DNA polymerase β was a gift from
S.H. Wilson (NIEHS) and APE1 was a gift from D. M. Wilson III (University of California).
FPG enzyme was purchased from New England Biolabs and UDG enzyme was purchased from
Invitrogen.
2’-Deoxyribose oligonucleotides- The 30-mer 2’-deoxyribose oligonucleotide substrate
containing a Tg residue at position 13 d(GATCCTCTAGCGTgCGACCTGCAGGCATGCA)
was prepared as described (1). The 30-mer 2’-deoxyribose oligonucleotide substrate containing
a uracil (U) residue at position 13 of the identical sequence, as well as the complementary 2’-
deoxyribose oligonucleotides were synthesized by the N.Y.U. School of Medicine Department of
Cell Biology. 2’-Deoxyribose oligonucleotides were deblocked, deprotected and purified by
20% denaturing PAGE. The 2’-deoxyribose oligonucleotides were gel purified and labeled at
the 5’-end using [γ-32P]ATP (NEN) and T4 Polynucleotide Kinase (Invitrogen) or at the 3’-
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end using [α-32P]ddATP (Amersham Biosciences) and Terminal Transferase (New England
Biolabs). All labeled nucleotides were purified by G-25 spin column filtration (Amersham
Biosciences) and annealed to the complementary strand which contained an adenine or guanine
base opposite the Tg or U residue.
Enzyme Assays- Unless otherwise indicated, assays were performed at 37°C in buffer
containing 50 mM HEPES pH 7.6, 100 mM KCl, 0.1 mg/mL BSA, 5mM MgCl2 and 1 mM
DTT. Enzyme, protein and substrate were diluted to working conditions in assay buffer and
equilibrated at 37°C. MgCl2 independent assays were performed with the above reaction buffer
recipe minus the addition of MgCl2, in the presence of 5 mM EDTA, which permits binding of
APE1 to DNA but inhibits its endonuclease activity (18). Reactions contained 40 nM [32P] 5’-
end labeled 2’-deoxyribose oligonucleotide substrate duplex, 5 nM hNth1 with or without 20
nM APE1. Two sets of 10 µL aliquots were taken at the indicated time periods and snap frozen
in ethanol and dry ice, after which one set was treated with 5 µL of 0.5 M putrescine pH 8.0 to
measure base release. The treated assay mixtures were then heated at 95°C for 5 min, followed
by the addition of 15 µL of loading dye (95% deionized formamide, 10 mM EDTA, 0.05%
Bromophenol Blue, and 0.05% Xylene Cyanol). To measure strand cleavage, samples were
treated with an equal volume of loading dye. All samples were then heated at 55°C for 5 min and
products were separated by 20% PAGE in 7M urea and 1 x TBE. Low substrate concentration
assays were performed with 20 nM hNth1 and 20 nM [32P] 5’-end labeled 2’-deoxyribose
oligonucleotide substrate duplex. At indicated times, aliquots were taken and treated as above.
Multiple turnover assays at Vmax were performed individually in 10 µL volumes containing
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reaction buffer, the indicated concentration of [32P] 5’-end labeled 2’-deoxyribose
oligonucleotide substrate duplex, and 20 nM hNth1 with or without 100 nM YB-1 and/or 100
nM APE1. The reactions were split into two 5 µL aliquots, snap-frozen in ethanol and dry ice
and treated as described above.
To discriminate between endonucleolytic and AP lyase products, reactions were
performed using [α-32P]ddAMP 3’-end labeled 2’-deoxyribose oligonucleotide substrate
duplex. Reactions contained the indicated substrate and enzyme concentrations and were
incubated at 37°C for 30 min. NaBH4 was added to 100 mM and the reactions were incubated at
37°C for 20 min for reduction of the 2’-deoxyribose 5’-phosphate moiety (19). The products
were purified by G-25 spin column filtration prior to separation and analysis.
Single turnover assays contained 10 nM [α-32P]ddAMP 3’-end labeled 2’-deoxyribose
oligonucleotide duplex and 100 nM hNth1 with or without 100 nM APE1 in a volume of 220 µL.
Enzyme reaction mixtures were incubated together for 2 min prior to initiation of the assay upon
addition of substrate. To measure base release, 5 µL aliquots were removed at indicated time
periods, snap frozen and treated with 5 µL of 0.5 M putrescine pH 8.0. The treated assay
mixtures were then heated at 95°C for 5 min, followed by the addition of 10 µL of loading dye.
To measure strand cleavage and determine incision products, 5 µL aliquots were removed at
indicated time periods, snap frozen and treated with an equal volume of 0.5 M NaBH4 at 37°C
for 20 min for the reduction of the dRP moiety. Samples were then filtered through a G-25 spin
column and treated with an equal volume of loading dye. Samples were then heated at 55°C for 5
min and products were separated by 20% PAGE in 7M urea and 1 x TBE. All products were
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analyzed quantitatively via phosphorimaging using a Molecular Imager FX System with
Quantity One Software (Bio-Rad).
Crosslinking of Enzyme to 2’-Deoxyribose Oligonucleotide Substrate (Enzyme Trapping)– For
NaBH4 reduction, assays contained 400 nM of the indicated [32P] 5’-end labeled 2’-
deoxyribose oligonucleotide duplex and 20 nM hNth1 with or without 100 nM APE1 and/or 100
nM YB-1 in a volume of 10 µL. After a 15 min incubation, reaction mixtures were treated with
5 µL of 0.5 M NaBH4 and incubated at 37°C for 5 min. After addition of an equal volume of
Laemmli SDS-loading buffer, samples were boiled in preparation for separation and analysis.
All samples were separated by 12% SDS PAGE and analyzed quantitatively via
phosphorimaging as above.
RESULTS
Differential Processing of Tg Opposite Adenine and Tg Opposite Guanine by hNth1- We
previously demonstrated, using a Tg:A-containing substrate, that the initial rate of DNA N-
glycosylase-mediated release of Tg by hNth1 was much greater than the rate of AP lyase-
mediated DNA strand cleavage (1). Since all previous assays with Tg had been done with
adenine as the opposite base, and since this may not be the only context in which Tg occurs in
vivo, we decided to look at hNth1 activity against substrates containing Tg paired opposite
guanine (2). Figure 1 is confirmation of our previous data. The assay was carried out in a shorter
reaction period than we previously used revealing that the difference between the rate of base
release and strand cleavage of a Tg:A substrate was even greater than we had reported, differing
by an order of magnitude. In sharp contrast, the AP lyase activity of hNth1 was the same as its
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DNA N-glycosylase activity against a Tg:G substrate. The DNA N-glycosylase activity of the
enzyme against Tg:A appeared to reach Vmax at substrate concentrations greater than 400 nM.
However, as we previously reported, hNth1 does not follow Michaelis-Menten pseudo-zero
order kinetics (1). Instead, the apparent kcat (which includes the rates of product release)
increased with increasing hNth1 concentration, suggesting positive cooperativity in hNth1
substrate processing. This observation and interpretation has been corroborated and expanded
upon by Liu and Roy (20). Because of this phenomenon, kcat and Km values for the duplex 2’-
deoxyribose oligonucleotide substrates vary with enzyme concentration. As we previously
suggested, the V vs. S data of Figure 1 reflect the fact that the enzyme was dissociating from the
DNA N-glycosylase generated AP:A site and initiating base release on new Tg:A substrates
without catalyzing β-elimination (1). However, when the substrate was Tg:G there was no
evidence of enzyme dissociation from AP:G (2).
APE1 Increases hNth1 Processing of Tg:A-containing 2’-Deoxyribose oligonucleotide
Substrates– We looked at the effect of APE1 on the activities of hNth1. There is evidence that
APE1 interacts with DNA N-glycosylases in BER as part of a “single-nucleotide BER relay”
involved in the coordination of processing of BER pathway intermediates (13, 21, 22).
Figure 2 shows that addition of APE1 increased hNth1 activity against a Tg:A substrate.
The stimulation of hNth1 activity was independent of the enzymatic activity of APE1. The assay
mixture lacked MgCl2 and contained sufficient EDTA to abrogate APE1-mediated
endonucleolytic cleavage but not the binding of APE1 to DNA (18). Identical experiments with
Tg:G substrates showed no increase in hNth1 substrate processing in the presence of APE1 (data
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not shown). We found that the optimum ratio for stimulation of hNth1 by APE1 varied with both
hNth1 and substrate concentration, ranging from 1:1 to 1:10. We suggest that this variability was
due, at least in part, to the positive cooperativity exhibited by hNth1 (1, 20).
APE1 Abrogates hNth1 AP Lyase Activity on Tg:A Containing Substrates But Not Tg:G
Containing Substrates- Having determined that the effect of APE1 on hNth1 activity differed
with substrate, we characterized the incision products generated by APE1 and hNth1 with the 2
substrates. The incision products generated by hNth1 in the presence of APE1 in vitro differed
with each substrate. Figure 3 is the gel analysis of the incision products of [32P] 3’-end labeled
Tg:A and Tg:G-containing 2’-deoxyribose oligonucleotide duplex substrates generated by
hNth1 in the presence or absence of APE1. In contrast to the experiments shown in Figure 2,
MgCl2 was added to the reaction to activate the endonucleolytic activity of APE1. The 2’-
deoxyribose 5’-phosphate (dRP) residue generated by APE1-catalyzed endonucleolytic
cleavage of an AP site is extremely labile and not retained during electrophoresis. Reduction by
NaBH4 prior to electrophoresis stabilizes the sugar moiety and permits size discrimination
between 5-endonucleolytic and 3-β-elimination AP lyase products (19). The AP lyase product
(p-17-p*ddA) can be seen in lanes containing hNth1 alone, with either Tg:A or Tg:G substrate
(lanes 2 and 4 respectively). Addition of APE1 to hNth1 using Tg:A produced a higher
molecular weight incision product, which is the endonucleolytic product (p-rAP-p-17-p*ddA)
generated by APE1 (lane 3). In the case of the Tg:G substrate, no change in the size of the
incision product was detected upon APE1 addition, indicating that the AP lyase activity of hNth1
was unaffected by APE1 with this substrate (lane 5). In this figure, there are 2 marker lanes for
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the β-elimination product, one with Tg:G containing substrate and one with U:A containing
substrate (lanes 6 and 8, respectively). The formamidopyrimidine-DNA N-glycosylase (FPG)
enzyme is a DNA N-glycosylase with β/δ elimination activity. Since the substrate is 3’-labeled,
the only product observed with FPG enzyme is the β-elimination product (lane 6). A second
marker lane for the β-elimination product is the AP-site containing substrate generated by
incubation of U:A-containing substrate with UDG and hNth1 to generate the AP lyase product
(p-17-p*ddA) (lane 8). The U:A-containing substrate incubated with UDG and APE1 serves as
the marker for the endonucleolytic product (p-rAP-p-17-p*ddA) (lane 7).
Incision Products Generated by hNth1 in the Presence or Absence of APE1, YB-1 and β -pol
Differ In Vitro- Since our previous work had identified YB-1 as a modifier of hNth1 activity,
we next investigated whether the addition of YB-1 together with APE1 had any effect on the
nature of the incision products of hNth1 with [32P]ddAMP 3’-end labeled Tg:A-containing 2’-
deoxyribose oligonucleotide duplex substrate (Figure 4). The addition of YB-1 in the presence
or absence of APE1 increased product formation (lanes 2 and 4). However, it did not change the
nature of the incision product, which in the presence of APE1 was the endonucleolytic product
(p-rAP-p-17-p*ddA) (lanes 3 and 4).
Since hNth1 did not demonstrate AP lyase activity against Tg:A sites in the presence of
APE1, we investigated whether the removal of the dRP residue could be effected by DNA
polymerase β (β-pol). Figure 4 demonstrates the reappearance of the β-elimination product
upon the addition of β-pol to hNth1 and APE1 with a Tg:A substrate (lane 7). This observation
is consistent with the known dRPase activity of β-pol (22). The marker lane for the β↑
elimination product (p-17-p*ddA) contains FPG enzyme (lane 9).
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Similar experiments with an N-terminal deletion mutant of hNth1, lacking amino acids
1-57, produced the same results in the presence of APE1 and YB-1 (data not shown),
suggesting that the effects of YB-1 and APE1 are not mediated by the N-terminus of hNth1.
APE1 Does Not Increase DNA N-Glycosylase Activity of hNth1 Under Conditions of Single
Turnover- To elucidate the mechanism by which APE1 affects hNth1 activity, we asked if APE1
changed the catalytic properties of hNth1 or whether it affected product inhibition. To address
this, we conducted the reaction under single turnover conditions where [E]>>[S], using
[32P]ddAMP 3’-end labeled substrates to determine the nature of the incision product. Since all
substrate molecules are bound by enzyme under single turnover conditions, the rates which
determine product formation are dependent only on the rate of base release (Schiff base
formation) and β-elimination (24). If APE1 did not affect either of these catalytic properties,
then there should be no stimulation under conditions of single turnover.
Figure 5 illustrates that no stimulatory effect of DNA N-glycosylase activity was
observed under conditions where neither enzyme turnover nor substrate binding contributed
significantly to the rate of the reaction. A complete abrogation of the AP lyase-mediated AP site
cleavage was seen with the Tg:A substrate (Figure 5A). This is consistent with the results of
Figure 3 (lane 3) and Figure 4 (lane 3).
Interestingly, in the case of the Tg:G substrate, addition of APE1 increased the rate of
hNth1 AP lyase activity (Figure 5B). We previously mentioned that addition of APE1 did not
result in increased product formation by hNth1 under turnover conditions using Tg:G. Thus, the
results of Figure 5B suggest that hNth1 remained tightly bound to the nicked AP:G DNA which
is the product of AP lyase activity.
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With both Tg:A and Tg:G substrates, the binding to the substrate and base release was
rapid, while β-elimination-catalyzed cleavage of the resulting AP site was clearly the rate
limiting reaction. Under single turnover conditions, the lag of the AP lyase step behind the DNA
N-glycosylase step was only slightly longer for Tg:A than Tg:G, indicating that the difference in
processing of the 2 substrates was due to enzyme turnover determined by the relative
dissociation rates of hNth1 from its products (Figure 5). Further evidence for this is shown in
Figure 6, in which both hNth1 and Tg:A and Tg:G substrates were present at low, equimolar
concentrations. Under these conditions, the dissociation of the DNA N-glycosylase and AP lyase
activities of hNth1 were apparent against the Tg:A substrate, but there was no dissociation
between the 2 activities against the Tg:G substrate.
APE1 Stimulates hNth1 Activity Under Conditions of Vmax- In order to determine whether
APE1 increased the maximal rate of turnover for the enzyme, we tested stimulation by APE1
under conditions of Vmax for both DNA N-glycosylase and AP lyase activities using 20 nM
hNth1 and 400 nM Tg:A substrate identical to the conditions of Figure 1. However, in the
experiments of Figure 7 MgCl2 was added to activate APE1 endonucleolytic activity. In
reactions containing hNth1 alone or hNth1 with YB-1, DNA cleavage was due solely to hNth1-
catalyzed β-elimination. For all 4 sets of experiments in this figure, DNA N-glycosylase activity
was quantified by measuring the cleavage of hNth1-generated AP sites by treatment with
organic base (putrescine) which effects cleavage via β-elimination (25). In reactions containing
APE1, all cleavage was the result of APE1 activity. Addition of APE1 resulted in a 2 fold
increase in the number of hNth1-generated AP sites as compared to hNth1 alone. Addition of
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YB-1 also caused a 2 to 3 fold increase in DNA N-glycosylase activity as we previously
described (1). Like YB-1, APE1 increased the kcat of hNth1 (as a DNA N-glycosylase) under
conditions of substrate excess. The last experiment of this group indicates that the effects of
APE1 and YB-1 were additive, resulting in a close to 4 fold increase in product. This combined
stimulation could actually be much greater, since, under our experimental conditions, most of the
substrate had been processed within 15 min.
Corroborating our results of experiments performed under low Tg:G substrate
concentrations, the addition of APE1 to hNth1 using substrate under conditions of Vmax (400
nM Tg:G) did not result in increased product formation (data not shown). Interestingly, hNth1
activity against Tg:G was stimulated by addition of YB-1, but there was no additive effect with
APE1 (data not shown).
APE1 Addition Decreases the Half Life of Covalent ES Complexes Formed by hNth1 with Its
Substrate- In order to investigate the effect of APE1 on the reaction intermediates of hNth1 with
its substrate, we used the reducing agent NaBH4, to trap the covalent ES intermediate (Figure 8).
NaBH4 is a strong reducing agent, capable of reducing the Schiff base as well as existing AP
sites (26). Therefore, the trapping of the covalent reaction intermediate with NaBH4 (Figure 8)
revealed the number of covalent complexes present in the reaction mixture at a given time point,
in this case, 15 min. For Tg:A substrate under steady state conditions, the addition of APE1
resulted in a decrease in the steady-state number of complexes initiated by hNth1 15 min after
the start of the reaction when the rate of product formation was still linear with time. There was
no significant change in the number of steady-state complexes with the Tg:G substrate upon
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APE1 addition. The addition of YB-1 resulted in a greater number of complexes with both
substrates, corroborating our previous data (1 and data not shown). The marked reduction in the
number of ES complexes (Tg:A) in the presence of both YB-1 and APE1 is a reflection of the
increased stimulation of hNth1 turnover, resulting in almost total substrate processing within 15
min. This data suggests that APE1 decreased the half-life of the enzyme-substrate covalent
intermediate, thereby stimulating dissociation of hNth1 from the AP:A site without catalyzing β↑
elimination, consistent with results of other laboratories studying the effect of APE1 on hOgg1 (6,
7).
DISCUSSION
The generation of Tg in DNA occurs through oxidative attack on the pyrimidine bases.
Tg opposite adenine can be formed by direct hydroxyl radical attack under aerobic conditions on
thymine in situ opposite its correctly paired base. As a blocker of both DNA and RNA
polymerases, Tg opposite adenine is a cytotoxic lesion (27). When Tg is bypassed by a DNA
polymerase, adenine is usually incorporated opposite Tg (27). Since the 2’-deoxynucleotide
triphosphate of Tg has been shown to be a poor substrate for polymerase incorporation,
formation of Tg:G is unlikely to be the result of insertional mispairing (28).Thus, the formation
of Tg:G is due primarily to direct oxidative attack on 5-methylcytosine resulting in deamination
and oxidation as we previously demonstrated (3). This modification is likely to occur in CpG
islands, which are rich in 5-methylcytosine and play a role in the regulation of gene expression.
In contrast to Tg:A, Tg:G is potentially mutagenic because, if unrepaired and bypassed by a
DNA polymerase, the insertion of adenine opposite the Tg would lead to a CGàTA transition
mutation as well as a disruption in methylation patterns (3).
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We here further investigated the mechanism of the difference of activities of hNth1
against Tg when it is paired with a different orphan base. While hNth1 exhibited marked
dissociation between its DNA N-glycosylase and AP lyase activities when the substrate was
Tg:A, the enzyme demonstrated concomitant DNA N-glycosylase and AP lyase activities when
the substrate was Tg:G. While the rates for base release by the enzyme were much greater for
Tg:A than for Tg:G, the rates for AP lyase activity initiated by hNth1 against Tg:A and Tg:G
were nearly identical. Our data indicate that this discrepancy was due to the presence or absence
of hNth1 turnover rather than inherent differences in reaction rates.
Furthermore, we report that APE1 stimulated hNth1 activity against Tg:A by abrogation
of the AP lyase step, presumably by effecting the dissociation of hNth1 from the AP site, thereby
increasing the turnover of the DNA N-glycosylase activity of hNth1 (Figure 9A). Thus, in the
presence of APE1, hNth1 essentially becomes a monofunctional DNA N-glycosylase against
Tg:A but not against Tg:G. Similar results have been reported hOgg1 (6, 7). While we did not
observe stimulation of hNth1 product formation by APE1 with Tg:G under turnover conditions,
we did observe APE1 stimulation of hNth1-catalyzed β-elimination with Tg:G under single
turnover conditions (Figure 5B). Taken together, this data suggests that hNth1 remains bound to
the nicked AP site product. This indicates that APE1 did not mitigate the inhibition of hNth1 by
the nicked DNA product of β-elimination of the AP:G site (Figure 9B). While we had
previously suggested Schiff base hydrolysis (k4) and product release (k5) not to be rate limiting,
our current data suggests the opposite (1). The observation that YB-1 did stimulate Tg:G
substrate processing by hNth1 suggests that YB-1 may effect product release as well as the
steady-state equilibrium between the Schiff base ES intermediate and the non-covalent ES
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intermediate.
What is a possible mechanistic reason for differential activity of hNth1 acting on Tg:A
vs. Tg:G? A detailed in vitro analysis of hNth1 substrate processing by Eide et al. revealed that
the β-elimination activity of hNth1 was strongly dependent upon the nature of the orphan base
pairing with an AP site, being a 100 fold greater with AP:G as compared to AP:A (29). Thus, the
difference in hNth1 processing of Tg:A vs. Tg:G may be a reflection of the affinity of hNth1 for
AP:G vs. AP:A. From our turnover data (Figures 1 and 6), we conclude that the AP lyase activity
of hNth1 against the AP-site containing substrate is dependent on the binding affinity of hNth1
for the AP site. Thus, the dissociation of hNth1 from the AP:A substrate following the enzymatic
release of Tg suggests a low binding affinity of hNth1 for the AP:A site. This is shown in the
kinetic mechanism outlined in Figure 9A, where k6 represents the hydrolysis of the Schiff base
without catalysis of β-elimination and k7 represents the dissociation of the enzyme from the AP
site. Our data suggests that APE1 drives the steady state equilibrium from the covalent (Schiff
base, E=S2) to the non-covalent (ES2) intermediate between hNth1 and its AP:A substrate,
resulting in the dissociation (E+S2) of hNth1 from the AP:A site. The higher affinity of hNth1
for AP:G is depicted by virtually unobservable values for k6 and k7 , in which case all Schiff
base formation results in catalysis of β-elimination and formation of AP lyase product (E=P2)
(Figure 9B). Since APE1 stimulates hNth1 AP lyase activity with Tg:G without stimulating
turnover, we suggest that hNth1 remains tightly bound to its AP lyase product (E=P2).
The different activities that we observed with hNth1 in vitro may be indicative of the
involvement of different substrate-dependent interacting and modifying proteins in vivo. Certain
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lesions, by virtue of their mutagenic or toxic characteristics, may be preferentially channeled
down a particular BER pathway i.e. long-patch or short patch BER. It has been suggested that
the intrinsic properties of the DNA N-glycosylase involved in the initial recognition and
removal of the damaged base may be responsible for BER pathway selection (30). In this case,
the intrinsic properties may include the pairing base discrimination exhibited by hNth1.
The in vivo significance of AP lyase activity is poorly understood. The removal of the
damaged base by the DNA N-glycosylase generates an AP site, which is a labile, and therefore
dangerous, intermediate for the cell. AP sites are the universal intermediates for all BER, and it is
postulated that most of these sites are processed by APE1 (31). Our studies with hNth1 are
consistent with studies performed with mammalian Ogg1, which suggested that AP site
processing is the rate-limiting step in BER initiated by bifunctional DNA N-glycosylase/AP
lyases (8). As we previously proposed, severe oxidative stress or UV irradiation would result in
the formation of a large number of damaged bases throughout cellular DNA (1). In theory, the
spontaneous removal of the damage via concomitant DNA N-glycosylase/AP lyase activity by
bifunctional DNA N-glycosylase/AP lyases would result in the simultaneous formation of a
large number of DNA strand breaks, a cytotoxic intermediate. In support of this hypothesis,
recent data on H2O2 sensitivity in E. coli identified the intermediates of Tg repair, rather than
the persistence of Tg, as significant contributors to cell death (32). The delayed AP lyase activity
and product inhibition inherent in hNth1 activity may allow for the regulation of AP site
processing. The substrate specific product inhibition exhibited by hNth1 may also represent the
channeling of AP site processing into specific BER pathways in different regions of the genome.
The rate of removal of Tg from cellular DNA has been shown to be very slow, as compared to
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the removal of uracil or the repair of AP sites in DNA and has been reported to consist mostly of
short patch BER involving β-pol (23, 33, 34). Our data suggests that it is the AP lyase activity of
β-pol that is responsible for the removal of the dRP residue left by hNth1-catalyzed base
release followed by APE1-catalyzed hydrolysis of the 5-phosphate bond. The fact that β-pol is
the primary polymerase involved in the major Tg removal pathway supports this model (34, 35).
The pivotal role played by APE1 physically connects the activities of the initial BER factors to
the DNA repair synthesis enzymes, such as β-pol, Flap endonuclease 1 (FEN-1), and DNA
ligase (13, 21, 31). Data from our laboratory and others have shown that interactions between
BER enzymes and other proteins can stimulate damage recognition or excision, suggesting the
probability of multiprotein complex formation in the initial events of BER (1, 6, 7, 36-39).
APE1 is not limited to its role in BER, but is a composite of the different activities of the
enzyme as a reduction-oxidation (redox) factor (40). Notably, APE1 has been shown to control
the activity of p53 through redox alteration and p53, in turn, has been shown to play a role in
BER (40-44). Like YB-1, APE1 has been shown to be a pluripotent factor, and may be a key
effector of the relationships between mammalian BER, oxidative signaling, transcription
regulation, and cell-cycle control (40,45).
We previously demonstrated that YB-1 affected hNth1 activity via the steady state
equilibrium between the covalent (E=S2) and non-covalent (ES2) enzyme-DNA intermediate
(1). We proposed that this equilibrium may be a checkpoint for modulation of hNth1 activity (1).
In this report, we show that APE1 modulated hNth1 activity at the same equilibrium point albeit
to a different effect. Thus, although YB-1 and APE1 seem to modulate hNth1 activity in
opposite ways, they have a synergistic effect in vitro. The overall effect on hNth1 activity by
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these 2 factors is to increase hNth1 turnover and substrate processing. Whether this has
significance in vivo remains to be determined.
In conclusion, we have performed further analyses into the mechanism of hNth1 activity
and identified substrate-specific enzymatic properties. We have also demonstrated a functional
interaction between hNth1 and the major mammalian AP endonuclease, APE1. This interaction
is dependent on the nature of the orphan base opposite Tg.
We recently reported, as has another laboratory (46), that Nth1 -/- mice are viable and
exhibit no abnormal phenotype. Extracts of tissues of Nth1-/- mice expressed an enzyme
activity that cleaved Tg:G substrate more rapidly than Tg:A substrates. This pattern seems to be
in direct contrast to the substrate selectivity of hNth1. Whether the substrate selectivity of Nth1
is a reflection of actual differences in Nth1 mediated in vivo processing of Tg:A vs. Tg:G, and
whether the selective stimulatory effects of APE1 affect processing, awaits further elucidation.
REFERENCES
1. Marenstein, D.R., Ocampo, M.T.A., Chan, M.K., Altamirano, A., Basu, A.K., Boorstein, R.J.,
Cunningham, R.P., and Teebor, G.W. (2001) J. Biol. Chem. 276, 21242-21249.
2. Ocampo, M.T.A., Chaung, W., Marenstein, D.R., Chan, M.K., Altamirano, A., Basu, A.K.,
Boorstein, R.J.,Cunningham, R.P., and Teebor, G.W. (2002) Mol. Cell. Biol. 22, 6111-6121.
3. Zuo, S., Boorstein, R.J., and Teebor, G.W. (1995) Nucleic Acids Res. 23, 3239-3243.
4. O’Handley, S., Scholes, C.P., and Cunningham, R.P. (1995) Biochemistry 34, 2528-2536.
5. McCullough, A.K., Dodson, M.L., and Lloyd, R.S. (1999) Annu. Rev. Biochem. 68,255-285.
6. Hill, J.W., Hazra T,K., Izumi ,T., and Mitra, S. (2001) Nucleic Acids Res. 29, 430-438.
7. Vidal,A.E., Dickson, I.D., Boiteux, S., and Radicella, J.P. (2001) Nucleic Acids Res. 29,
20
by guest on April 12, 2018
http://ww
w.jbc.org/
Dow
nloaded from
1285-1292.
8. Zharkov, D.O., Rosenquist, T.A., Gerchman, S.E., and Grollman AP. (2000) J. Biol. Chem.
275, 28607-28617.
9. Hilbert T.P., Boorstein, R.J., Kung, H.C., Bolton, P.H., Xing, D., Cunningham, R.P., and
Teebor, G.W. (1996) Biochemistry 35, 2505-2511.
10. Hilbert T.P., Chaung, W., Boorstein, R.J., Cunningham, R.P., and Teebor, G.W. (1997) J.
Biol. Chem. 272, 6733-6740.
11. Yang, H., Clendenin, W.M., Wong, D., Demple, B., Slupska, M.M., Chiang, J.H., and Miller,
J.H. (2001) Nucleic Acids Res. 29, 743-752.
12. Parker, A., Gu, Y., Mahoney, W., Lee, S.H., Singh, K.K., and Lu, A.L. (2001) J. Biol. Chem.
276, 5547-5555.
13. Wilson, S.H., and Kunkel, T.A. (2000) Nat Struct Biol. 7, 176-178.
14. Kavli, B., Sundheim, O., Akbari, M., Otterlei, M., Nilsen, H., Skorpen, F., Aas, P.A., Hagen,
L., Krokan, H.E., and Slupphaug, G., (2002) J Biol Chem. 277, 39926-39936.
15. Hardeland, U., Steinacher, R., Jiricny, J., and Schar, P. (2002 ) EMBO J. 21,1456-1464.
16. Privezentzev, C.V., Saparbaev, M., and Laval, J. (2001 ) Mutat. Res. 480-481, 277-284.
17. Cunningham, R.P., Asahara, H., Bank, J.F., Scholes, C.P., Salerno, J.C., Surerus, K., Munck,
E., McCracken, J., Peisach, J., and Emptage, M.H. (1989) Biochemistry 28, 4450-4455.
18. Mckenzie, J.A. and Strauss, P.R. (2001) Biochemistry 40, 13254-13261.
19. Ischenko, A.A. and Saparbaev, M.K. (2002) Nature 415, 183-187.
20. Liu, X. and Roy, R.(2002) J. Mol.Biol. 321, 265-276.
21
by guest on April 12, 2018
http://ww
w.jbc.org/
Dow
nloaded from
21. Mol, D.C., Izumi, T., Mitra, S., and Tainer, J.A., (2000) Nature 403, 451-456.
22. Ranalli, T.A., Tom, S., and Bambara, R.A.(2002) J. Biol. Chem. 277, 41715-41724.
23. Srivastava, D.K., Berg, B.J., Prasad, R., Molina, J.T., Beard, W.A., Tomkinson, A.E., and
Wilson, S.H. (1998) J. Biol. Chem. 273, 21203-21209.
24. Porello, S.L., Leyes, A.E., and David, S.S. (1998) Biochemistry 37, 14756-14764.
25. Mazumder, A., Gerlt, J.A., Absalon, M.J., Stubbe, J., Cunningham, R.P., Withka, J., and
Bolton, P.H.( 1991) Biochemistry 30,1119-1126.
26. Piersen, C.E., Prince, M.A., Augustine, M.L., Dodson, M.L., and Lloyd, R.S. (1995) J. Biol.
Chem. 270, 23475-23484.
27. Wallace, S.S. (2002) Free. Radic. Biol. Med. 33, 1-14.
28. Purmal, A.A., Bond, J.P., Lyons, B.A., Kow, Y.W., and Wallace, S.S. (1998) Biochemistry
37, 330-338.
29. Eide, L., Luna, L., Gustad E.C., Henderson, P.T., Essigman J.T., Demple B., and Seeberg, E.
(2001) Biochemistry 40, 6653-6659.
30. Fortini, P., Parlanti, E., Sidorkina, O.M., Laval, J., and Dogliotti, E. (1999) J. Biol. Chem.
274, 15230-15236.
31. Tom, S., Ranalli, T.A., Podust, V.N., and Bambara, R.A.(2001) J. Biol. Chem. 276, 48781-
48789.
22
by guest on April 12, 2018
http://ww
w.jbc.org/
Dow
nloaded from
32. Alanazi, M., Leadon, S.A., and Mellon, I. (2002) Nucleic Acids Res. 30, 4583-4591.
33. Dianov, G.L., Thybo, T., Dianova, I.I., Lipinski, L.J., and Bohr, V. (2000) J. Biol. Chem.
275, 11809-11813.
34. Podlutsky, A.J., Dianova, I., Wilson, S.H., Bohr, V.A., and Dianov, G.L. (2001)
Biochemistry 40, 809-813.
35. Sobol, R.W., Prasad, R., Evenski, A., Baker, A., Yang, X.P., Horton, J.K., and Wilson, S.H.
(2000) Nature 405, 807-10.
36. Klungland, A., Hoss, M., Gunz, D., Constantinou A., Clarkson, S.G., Doetsch, P.W., Bolton,
P., Wood R.D., and Lindahl, T. (1999) Mol. Cell. 3, 33-42.
37. Bessho T. (1999) Nucleic Acids Res. 27, 979-983.
38. Aspinwall, R., Rothwell, D.G., Roldan-Arjona, T., Anselmino, C., Ward, C.J., Cheadle, J.P.,
Sampson, J.R., Lindahl, T., Harris, P.C., and Hickson, I.D. (1997) Proc. Natl. Acad. Sci. USA
94, 109-114.
39. Ikeda, S., Biswas, T., Roy, R., Izumi, T., Boldogh, I., Kurosky, A., Sarker, A.H., Seki, S.,
and Mitra, S. (1998) J. Biol. Chem. 273, 21585-21593.
40. Kelley, M.R. and Parsons, S.H. (2001) Antioxid. Redox. Signal. 3, 671-683.
41. Seo, Y.R., Fishel, M.L., Amundson, S., Kelley, M.R., and Smith, M.L. (2002 ) Oncogene
21, 731-737.
42. Zhou, J., Ahn, J., Wilson, S.H., and Prives, C. (2001) EMBO J. 20, 914-923.
43. Offer, H., Milyavsky, M., Erez, N., Matas, D., Zurer, I., Harris, C.C., and Rotter, V. (2001)
23
by guest on April 12, 2018
http://ww
w.jbc.org/
Dow
nloaded from
Oncogene 20, 581-589.
44. Seo, Y.R., Kelley, M.R., and Smith M.L. (2002) Proc. Natl. Acad. Sci. USA 99, 14548-
14553.
45. Evans , A.R., Limp-Foster, M., Kelley, M.R.(2000) Mutat. Res. 461,83-108.
46. Takao, M., Kanno, S., Shiromoto T, Hasegawa, R., Ide, H., Ikeda, S., Sarker, A.H., Seki, S.,
Xing, J.Z., Le, X.C., Weinfeld, M., Kobayashi, K., Miyazaki, J., Muijtjens, M., Hoeijmakers,
J.H., van der Horst, G., Yasui, A., and Sarker, A.H. (2002) EMBO J. 21, 3486-3493.
AKNOWLEDGMENTS
D Supported by the Department of Pathology, New York University School of Medicine and by
an award from the New York University School of Medicine Research Bridging Support Fund
(G.W.T.), NIEHS grant ES 09127 (A.K.B.) and by GM 46312 (R.P.C.). We thank Dr. David M.
Wilson III for supplying APE1and Dr. Samuel H. Wilson for supplying DNA Polymerase β.
FOOTNOTES
Abbreviations:
1hNth1, human endonuclease III homologue 1; AP, apurinic/apyrimidinic; Ogg1, 8-
oxoguanine-DNA N-glycosylase; YB-1, Y-Box binding protein 1; BER, base excision repair;
SDS, sodium dodecyl sulfate; PAGE, polyacrylamide gel electrophoresis; Tg, thymine glycol;
rAP, reduced apurinic/apyrimidinic; dRP, 2’-deoxyribose phosphate; APE1,
apurinic/apyrimidinic endonuclease 1; TBE, Tris-Borate EDTA; FPG, formamidopyrimidine-
DNA N-glycosylase; UDG, Uracil DNA N-glycosylase; β-pol, DNA polymerase β.
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FIGURE LEGENDS
Figure 1. hNth1 activity against Tg:A vs. Tg:G-containing 2-deoxyribose oligonucleotide
duplex substrates. 20 nM hNth1 was incubated with specified concentrations of [32P] 5’-end
labeled 2-deoxyribose oligonucleotide duplex substrate containing either an A (circles) or G
(squares) opposite the Tg moiety. Open symbols denote DNA N-glycosylase activity determined
by putrescine treatment of reaction products. Solid symbols denote AP lyase activity. Mean
values were calculated from 2 independent experiments and did not vary by more than 10%.
Figure 2. Effect of APE1 on hNth1 activity against a Tg:A-containing 2’-deoxyribose
oligonucleotide duplex substrate. 40 nM Tg:A-containing [32P] 5’-end labeled 2’-deoxyribose
oligonucleotide duplex substrate was incubated with 5 nM hNth1 with (squares) or without
(circles) 20 nM APE1. APE1 endonucleolytic activity is abrogated in the absence of MgCl2 and
the presence of 5 mM EDTA. Open symbols denote DNA N-glycosylase activity determined by
putrescine treatment of reaction products. Solid symbols denote AP lyase activity.
Figure 3. Effect of APE1 on the incision products generated by hNth1 in vitro against Tg:A and
Tg:G–containing 2’-deoxyribose oligonucleotide duplex substrates. Reactions contained 10 nM
Tg:A or Tg:G-containing [32P]ddAMP 3’-end labeled 2’-deoxyribose oligonucleotide duplex
substrate, 20 nM hNth1 and 10 nM APE1, as indicated. Lane 6 contained 1 unit of FPG enzyme.
Another marker lane for the β-elimination product is also shown with a U-containing radio-
labeled substrate incubated with UDG and hNth1 (p-17-p*ddA, where * denotes the labeled
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phosphate). The U-containing substrate was incubated with UDG and APE1 to generate a
marker for the endonucleolytic product (p-rAP-p-17-p*ddA). Reactions were incubated at
37°C for 30 min prior to addition of NaBH4. followed by analysis as described in experimental
procedures.
Figure 4. Effects of APE1, YB-1 and β -pol on the incision products generated by hNth1 in
vitro against Tg:Acontaining 2-deoxyribose oligonucleotide substrates. Reactions contained 20
mM dNTPs, 16.6 nM Tg:A-containing [32P]ddAMP 3’-end labeled duplex 2’-deoxyribose
oligonucleotide substrate, 16.6 nM hNth1, 8.3 nM APE1, 8.3 nM β-pol and 83 nM YB-1, as
indicated. Lane 9 contained 1 unit of FPG enzyme as a marker lane for the β-elimination product
(p-17-p*ddA, where * denotes the labeled phosphate). Reactions were incubated at 37°C for 30
min prior to addition of NaBH4. followed by analysis as described in experimental procedures.
Figure 5. Representative plot of the effect of APE1 on single-turnover kinetics of hNth1 with
Tg:A (Panel A) and Tg:G–containing (Panel B) 2’-deoxyribose oligonucleotide duplex
substrates. Reactions contained 10 nM Tg:A (A) or Tg:G-containing (B) [32P]ddAMP 3’-end
labeled 2’-deoxyribose oligonucleotide substrate duplex, 100 nM hNth1 with (squares) or
without (circles) 100 nM APE1. Open symbols denote DNA N-glycosylase activity determined
by putrescine treatment of reaction products. Solid symbols denote AP lyase activity. Reactions
were incubated at 37°C for the indicated time period after which aliquots were stopped by snap
freezing. One set was treated with putrescine and the other with NaBH4.Analysis was as
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described in experimental procedures.
Figure 6. Representative plot of product formation by hNth1 against Tg:A and Tg:G-containing
2’-deoxyribose oligonucleotide duplex substrates as a function of time under multiple-turnover
conditions. Reactions contained 20 nM Tg:A (circles) or Tg:G-containing (squares) [32P] 5’-
end labeled 2’-deoxyribose oligonucleotide duplex substrate as indicated, with 20 nM hNth1.
Open symbols denote DNA N-glycosylase activity determined by putrescine treatment of
reaction products. Solid symbols denote AP lyase activity.
Figure 7. Effect of APE1 on hNth1 activity against a Tg:A-containing 2’-deoxyribose
oligonucleotide duplex under conditions of Vmax. Reactions consisted of 20 nM hNth1
incubated with 400 nM Tg:A [32P] 5’-end labeled 2’-deoxyribose oligonucleotide duplex
substrate with 100nM YB-1 and/or 100 nM APE1, as indicated, for a reaction time of 15 min.
Black bars denote DNA cleavage, either by hNth1-catalyzed AP lyase activity (in the absence of
APE1) or APE1 endonucleolytic activity (in the presence of APE1). Grey bars represent reaction
products treated with putrescine. In the absence of APE1, these denote hNth1 DNA N-
glycosylase activity. In the presence of APE1, all AP sites generated by hNth1 DNA N-
glycosylase activity were endonucleolytically cleaved by APE1. Mean values and standard
deviations were calculated from 3 independent experiments.
Figure 8. Representative plot of the effect of APE1 and YB-1 on steady state levels of hNth1
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Schiff base intermediate with Tg-containing 2’-deoxyribose oligonucleotide duplex. Trapping
of the covalent ES intermediate using NaBH4. Reactions contained 400 nM Tg:A (solid) or Tg:G
(striped)-containing [32P] 5’-end labeled 2’-deoxyribose oligonucleotide duplex substrate with
20 nM hNth1, 100 nM YB-1 and/or 100 nM APE1, as indicated. Reactions were incubated at
37°C for 15 min after which NaBH4 was added to a concentration of 100 mM and the reactions
were incubated for another 2 min at 37°C prior to the addition of Laemmli SDS sample buffer.
Figure 9. Kinetic scheme for the effect of APE1 on hNth1 Activity against Tg:A (A) and Tg:G-
containing (B) 2’-deoxyribose oligonucleotide duplex substrate.
S1 ; the substrate with modified base (i.e. Tg) intact.
S2 ; the substrate containing an AP site after base release.
P1 ; the 3’ end of the β-eliminated 2’-deoxyribose oligonucleotide.
P2 ; the 5’ end of the β-eliminated 2’-deoxyribose oligonucleotide.
= ; the Schiff base between E and S.
k2 ; the rate of base release
k3 ; the rate of β-elimination
k4 ; the rate of Schiff base hydrolysis
k-6 and k6 ; the steady state of Schiff base resolution
k-7 and k7 ; the binding and release of the non-covalently bound AP site moiety.
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(A) The inhibition of k3 by APE1 drives the reaction towards k6/k7, the dissociation of hNth1
from the AP:A substrate, which results in increased turnover, a faster reaction rate and a shorter
half-life for the covalent ES intermediate. This leaves an AP site ready for processing by APE1
and repair synthesis. (B) The effect of APE1 on k3 results in an increased rate of AP lyase
activity. However, there is no evidence that the hNth1 is driven to dissociate from the β-
elimination product and turnover is not significantly affected.
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Boorstein, Richard P. Cunningham and George W. TeeborDina R. Marenstein, Michael K. Chan, Alvin Altamirano, Ashis K. Basu, Robert J.
endonuclease 1 (APE1) on hNth1 activitySubstrate specificity of human endonuclease III (hNth1): Effect of human AP
published online January 8, 2003J. Biol. Chem.
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