Skip Navigation

This Article
Right arrow Abstract Freely available
Right arrow Print PDF (227K) Freely available
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Services
Right arrow Email this article to a friend
Right arrow Similar articles in this journal
Right arrow Similar articles in ISI Web of Science
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Add to My Personal Archive
Right arrow Download to citation manager
Right arrow Search for citing articles in:
ISI Web of Science (5)
Right arrow Commercial Re-use Guidelines
for Open Access NAR Content
Google Scholar
Right arrow Articles by Coman, D.
Right arrow Articles by Russu, I. M.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Coman, D.
Right arrow Articles by Russu, I. M.
Social Bookmarking
Add to CiteULike   Add to Connotea   Add to Del.icio.us  
What's this?

Published online 9 February 2004

Nucleic Acids Research, 2004, Vol. 32, No. 3 878-883
© 2004 Oxford University Press

Site-resolved stabilization of a DNA triple helix by magnesium ions

Daniel Coman and Irina M. Russu*

Department of Chemistry and Molecular Biophysics Program, Wesleyan University, Middletown, CT 06459, USA

*To whom correspondence should be addressed. Tel: +1 860 685 2428; Fax: +1 860 685 2211; Email: irussu{at}wesleyan.edu

Received October 29, 2003; Revised and Accepted December 18, 2003


   ABSTRACT
TOP
 ABSTRACT
INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Proton exchange and NMR spectroscopy have been used to define the effects of Mg2+ ions upon the stability of individual base pairs in the intramolecular parallel triple helix formed by the DNA oligonucleotide d(GAAGAGGTTTTTCCTCTTCTTTTTCTTCTCC). The rates of exchange of individual Watson–Crick and Hoogsteen imino protons in the DNA triple helix were measured in the absence and in the presence of Mg2+ ions. The results reveal that Mg2+ lowers the exchange rates of most imino protons in the structure by stabilizing the corresponding base pairs in their native closed conformation. Comparison of the DNA triple helix containing Na+ counterions to the same helix containing Mg2+ counterions shows that these stabilizing effects result, in large part, from Mg2+ ions closely associated with the DNA. Moreover, the effects are site-specific and depend on the number and location of protonated cytosines relative to the observed base. These findings provide new insights into the molecular roles of C+·GC triads in determining the stability of DNA triple-helical structures.


   INTRODUCTION
TOP
 ABSTRACT
 INTRODUCTION
MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Triple-helical structures offer a powerful approach for recognition of specific base sequences in DNA (1,2). These structures are formed by binding of an oligonucleotide strand into the major groove of a DNA duplex. Depending on the orientation of this third strand, two families of DNA triplexes can be distinguished (3). In the pyrimidine–purine–pyrimidine (Y·RY) family, the third strand is rich in thymines and protonated cytosines, and binds parallel to the purine-rich strand of the duplex. Due to the requirement for cytosine protonation, these structures are stable at acidic pH. In purine–purine–pyrimidine (R·RY) triple helices, the third strand is purine-rich and binds in the opposite orientation, anti-parallel to the purine strand of the duplex.

The formation and stability of DNA triple-helical structures are critically influenced by divalent cations, such as magnesium (4). Generally, the cations promote formation and increase stability of the triple-helical structure. For example, in the absence or at low concentrations of other cations, Mg2+ ions raise the melting temperature of Y·RY triplexes, and increase the equilibrium constant for the binding of the third strand to the duplex (5–10). The efficiency of Mg2+ ions in enhancing the stability of Y·RY triplexes is significantly greater than that of monovalent ions (8–10).

The effects of mono- and divalent cations on the stability of DNA triple helices have been explained by theoretical models derived from the counterion condensation theory or from solutions of the cylindrical Poisson–Boltzmann equation (8,11). In DNA triple-helical structures, the presence of the third strand creates a high linear charge density. Like in double helices, counterions accumulate in the vicinity of the DNA, or condense onto it, to neutralize and screen the phosphate charges. The resulting decrease in repulsive electrostatic free energy stabilizes the structure (12). Analysis of cation effects in Y·RY triple helices is complicated by the electrostatic potential created by the protonated cytosines in the third strand. Experimental evidence has demonstrated that the number of protonated cytosines and their location in the structure profoundly affect the stability of Y·RY triplexes and their dependence on cations (9,10,13–15). However, theoretical models have not yet been used to analyze cations effects in Y·RY triple helices containing protonated cytosines.

In the present work, we have addressed the question of the stabilization of DNA triple helices by Mg2+ ions using proton exchange and nuclear magnetic resonance (NMR) spectroscopy. The approach used allows characterization of Mg2+-induced effects on stability at the level of individual base pairs. The DNA oligonucleotide investigated is shown in Figure 1. Our previous structural studies have shown that this DNA assumes a single conformation in solution. The conformation is that of an intramolecular Y·RY triple helix in which the pyrimidine sequence C15+ to C21+ orients parallel to the purine ‘strand’ in the major groove of the duplex part of the structure (16).



View larger version (15K):
[in this window]
[in a new window]
  		Figure 1. (A) Base sequence and folded conformation of the DNA triple helix investigated. Watson–Crick hydrogen bonds are indicated by asterisks, and Hoogsteen hydrogen bonds are indicated by dots. The imino proton resonances for the bases shown in bold are observable in the NMR spectra. The numbering of the bases is the same as that used in our previous characterization of this triple helix (16). (B) Structures of canonical T·AT and C+·GC triads (31).

 

   MATERIALS AND METHODS
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
RESULTS
 DISCUSSION
 REFERENCES
 
DNA samples
The DNA oligonucleotide was synthesized using phosphoramidite chemistry on an automated DNA synthesizer (Applied Biosystems model 381A). The DNA was purified by reverse-phase HPLC on a PRP-1 column (Hamilton) in 50 mM triethylammonium acetate buffer at pH 7 (with a gradient of 5–32% acetonitrile in 39 min). The counterions were replaced with Na+ or Mg2+ ions by repeated centrifugation (6–8 times) through Centricon YM-3 tubes (Amicon Inc.) using 0.5 M NaCl or 0.5 M MgCl2 solutions. The DNA solution was desalted by repeated centrifugation (6–8 times) against water. The NMR samples contained DNA in water at a concentration of 1.6 mM [based on a calculated extinction coefficient of 261 O.D.260/µmol (17)]. The pH of the sample (pH 4.6 ± 0.1) was measured at 5°C, before and after each NMR experiment.

NMR experiments
The NMR experiments were performed on a Varian INOVA 500 spectrometer operating at 11.75 T, at 5°C. This temperature is well below the range of temperatures in which melting of the triple helix occurs (namely, 35°C for the transition from triplex to hairpin duplex, and 48°C for the melting of the duplex, as measured by UV spectroscopy). One-dimensional (1D) NMR spectra were obtained using the Jump-and-Return pulse sequence (18). The imino proton exchange rates were measured by transfer of magnetization from water and in hydrogen/deuterium (H/D) exchange experiments.

In the experiments of transfer of magnetization from water, the exchange was initiated by inverting selectively the water proton resonance using a Gaussian 180° pulse (5.7–6.0 ms). A weak gradient (0.21 gauss/cm) was applied during the exchange delay following water inversion, in order to prevent the effects of radiation damping upon the recovery of water magnetization to equilibrium. At the end of the exchange delay, a second Gaussian pulse (1.7–1.8 ms) was applied to bring the water magnetization back to the oZ axis. The observation was with the Jump-and-Return pulse sequence. Twenty-two values of the exchange delay in the range from 2 to 600 ms were used in each experiment. The exchange rates were calculated from the dependence of the intensity of the proton resonance of interest on the exchange delay as we have previously described (19,20). The lowest exchange rate that can be measured reliably using this transfer of magnetization method is ~0.3 s–1 at 5°C (16).

In H/D exchange experiments, the DNA samples in water were dried down to 30–60 µl by flushing with argon, and the exchange was initiated by adding D2O. The final volume fraction of D2O was between 90 and 95%. In total, 96 transients were accumulated for each spectrum with a total acquisition time of 3.85 min per spectrum. The exchange rate was calculated from the dependence of the intensity of the corresponding resonance on the exchange delay (16). Due to the time elapsed between the initiation of the exchange and the first NMR spectrum (3–6 min), the fastest exchange rate that could be measured accurately in these experiments is 4 x 10–3 s–1.

Imino proton exchange in DNA
The exchange of DNA imino protons with solvent protons occurs via a structural opening reaction that brings the imino proton into an open state. In this state, the hydrogen bond holding the imino proton is broken such that the proton can be transferred to proton acceptors (21,22). The acceptors can be nitrogen atoms of other bases within the same DNA molecule or proton acceptors present in solution (e.g. OH– and water) (22). The exchange rate observed experimentally depends upon the kinetic parameters of the opening reaction as (21):

kex = kop x kex,open/(kcl + kex,open)1

where kop and kcl are the opening and the closing rate, respectively, and kex,open is the rate of exchange from the open state. Two kinetic regimes can be distinguished depending on how the rate of exchange from the open state compares with the rate of closing: (i) when kex,open << kcl (EX2 regime), the observed rate of exchange is proportional to kex,open:

kex = Kop x kex,open2

where Kop = kop/kcl is the equilibrium constant for the opening reaction of the base containing the imino proton. (ii) When kex,open >> kcl (EX1 regime), the exchange occurs in each opening event and

kex = kop3


   RESULTS
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
DISCUSSION
 REFERENCES
 
Figure 2 shows the NMR resonances of imino protons of the DNA triple helix investigated, in the absence and in the presence of 100 mM Mg2+. The resonances originate from imino protons involved in Watson–Crick hydrogen bonds (N3H in thymines and N1H in guanines) and in Hoogsteen hydrogen bonds (N3H in thymines and protonated cytosines, Fig. 1). The resonances from the protonated cytosines in the first and in the last triad (i.e. C21+ and C15+) are not observed because they are broadened by fast exchange with solvent. Comparison of the two spectra in Figure 2, in the absence and in the presence of Mg2+, reveals only small differences in the chemical shifts of imino proton resonances. This indicates that Mg2+ ions do not change significantly the conformation of the triple helix.



View larger version (30K):
[in this window]
[in a new window]
  		Figure 2. NMR resonances of imino protons in the DNA triple helix investigated in 90% H2O/10% D2O at pH 4.6 and at 5°C, in the absence of Mg2+ ions (A) and in the presence of 100 mM Mg2+ ions (B). The assignments of the resonances have been previously obtained by this laboratory (16).

 
We have measured the rates of exchange of the imino protons in the DNA triple helix with solvent protons. The rates span five orders of magnitude, namely, from ~5 x 10–4 to ~50 s–1 at 5°C. The exchange of imino protons in the protonated cytosines C18+ and C20+, and in terminal guanines occurs on a time scale of seconds or faster. The exchange rates of these protons were measured in experiments of transfer of magnetization from water as illustrated in Figure 3A. In contrast, the exchange of imino protons in thymines and in the central guanine G11 is much slower, and was measured in H/D exchange experiments (Fig. 3B).



View larger version (33K):
[in this window]
[in a new window]
  		Figure 3. Selected imino proton spectra of the DNA triple helix in transfer of magnetization experiments (A) and in H/D exchange experiments (B). The exchange delay is given for each spectrum. The imino proton resonances that show changes in intensity in each experiment are indicated.

 
The effect of Mg2+ ions upon the exchange of imino protons was investigated using two samples of the DNA triple helix. In the first sample, the DNA contained Na+ as counterions [henceforth abbreviated DNA(Na+)]. The proton exchange rates for this sample were measured in the absence and in the presence of 100 mM Mg2+. The results are illustrated in Figure 4 with the exchange curves of imino protons in G8 and T3. Clearly, for both protons, the exchange in the presence of 100 mM Mg2+ is significantly slower than that in the absence of the ion (i.e. exchange rates 1.94 versus 13.0 s–1 for G8, and 2.1 x 10–4 versus 5.2 x 10–4 s–1 for T3). The exchange rates for all imino protons in this sample, in the absence and in the presence of 100 mM Mg2+ [k0ex(Na+) and kMgex, respectively], are summarized in Table 1. Higher concentrations of Mg2+ did not induce further changes in the exchange rates. For the second DNA sample [henceforth abbreviated DNA(Mg2+)], the Na+ counterions were replaced with Mg2+. The exchange rates of imino protons were measured for a solution of this triple helix in water, and are given in the fourth column of Table 1 [k0ex(Mg2+)]. For most imino protons, the exchange rates decrease in the presence of 100 mM Mg2+ ions, or when Na+ counterions are replaced with Mg2+. The exceptions to this trend are the imino protons in C+20 and T19. For C+20, the exchange rate remains constant upon adding 100 mM Mg2+ to the DNA solution or upon replacing Na+ with Mg2+ counterions. For T19, the exchange rate increases upon adding 100 mM Mg2+ ions. A larger increase in the exchange rate of this proton is observed upon replacing Na+ with Mg2+ counterions.



View larger version (19K):
[in this window]
[in a new window]
  		Figure 4. Examples of the dependence of the intensity of imino proton resonances on the exchange delay. Upper panel: exchange of imino proton in G8 measured in transfer of magnetization experiments. Lower panel: exchange of imino proton in T3 measured in H/D exchange experiments. Triangles represent results for the DNA(Na+) sample in water, and squares represent results for the same sample in the presence of 100 mM Mg2+ ions.

 

View this table:
[in this window]
[in a new window]
  		Table 1. Effect of Mg2+ ions on the exchange rates of imino protons (s–1) and the free energy changes in base-pair opening reactions (kcal/mol) in the DNA triple helix investigated at pH 4.6 and at 5°C
 

   DISCUSSION
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
REFERENCES
 
Molecular origins of Mg2+ effects on imino proton exchange rates
The exchange of imino protons in DNA triple helices has been previously characterized by this and other laboratories (16,19,20,23). Under experimental conditions similar to those used in the present work, the exchange of most imino protons is in the EX2 regime (equation 2), where the observed exchange rate is proportional to the equilibrium constant for the opening reaction (Kop). In the open state of the base pair, the imino proton is transferred directly to water molecules or to nitrogen atoms in neighboring bases [for example, for Watson–Crick base pairs, imino protons in thymine and guanine are transferred to adenine N1 and cytosine N3, respectively (19)]. For protonated cytosines, the exchange is in EX1 regime (equation 3). This is because the imino proton is transferred, upon opening of the Hoogsteen C+·G base pair, to the N7 atom of the guanine, and the rate of this transfer is very high. Thus, the observed exchange rate provides directly the rate of opening of the Hoogsteen C+·G base pair.

The changes in exchange rates observed in this work could originate from Mg2+-induced changes in the equilibrium constant of the opening reaction (Kop) and/or in the exchange rate from the open state (kex, open). Several observations suggest that the effects of Mg2+ ions upon exchange from the open state are small. In free deoxyribonucleotides, the exchange rates of imino protons are independent of Mg2+ concentration. For example, we have found that, under the experimental conditions used in this work (i.e. water at pH 4.6 and at 5°C), the exchange rates are 185 ± 6 s–1 for the imino proton in guanosine 5'-monophosphate and 15.3 ± 0.1 s–1 for the imino proton in thymidine 5'-monophosphate. These exchange rates are constant for Mg2+ concentrations up to 100 mM. In DNA structures, Mg2+ ions affect the local electrostatic potential at individual bases (24–26). However, these effects are not expected to influence the rate of exchange of imino protons from the open state because, as explained above, the acceptors involved in exchange (i.e. DNA bases and water) are uncharged. The absence of a significant effect of Mg2+ upon proton transfer rates in the open state is also suggested by the observation that the exchange rate of imino proton in C+18 changes in the presence of Mg2+ (Table 1). The exchange of this proton is in EX1 regime (equation 3) and thus, is independent of the rate of exchange from the open state. Therefore, for this base, the effect of Mg2+ should result from an alteration of the rate of opening of the C+18·G11 base pair. These arguments suggest that Mg2+ does not influence significantly proton transfer reactions from the open state. Instead, it is more likely that Mg2+ ions change the imino proton exchange rates by affecting the equilibrium constant Kop and the energetics of the structural opening reactions for individual base pairs.

Effects of Mg2+ ions upon single-site energetics in the DNA triple helix
The effects of Mg2+ upon various sites in the DNA triple helix can be quantitatively compared by assuming that the changes in imino proton exchange rates result solely from changes in the equilibrium constant Kop. This constant is related to the free energy change in the opening reaction as (21):

{Delta}Gop = –RT ln Kop4

Accordingly, when the exchange is in EX2 regime (equation 2), the changes in exchange rates can be recast as variations in the free energy changes {Delta}Gop at individual sites. For example, for the DNA(Na+) sample, when the change in exchange rate is induced by increasing the concentration of Mg2+ from 0 to 100 mM, the change in {Delta}Gop at any site is:

where the superscript ‘0’ refers to exchange and opening reactions in the absence of Mg2+ ions, and the superscript ‘Mg’ refers to the same reactions in the presence of 100 mM Mg2+. Similarly, when the change in exchange rate is induced by replacing Na+ counterions with Mg2+ counterions, the {delta}{Delta}Gop at any site is:

where the counterion closely associated with the DNA (Na+ or Mg2+) is indicated in parentheses. The calculated values of {delta}{Delta}Gop for each base in the DNA triple helix are shown in the last columns of Table 1. For most bases, the free energy change for opening increases in the presence of Mg2+. This suggests that Mg2+ stabilizes the DNA triple-helical structure by increasing the lifetime of most base pairs in their native, paired state.

An insight into the molecular origin of this Mg2+-induced stabilization of base pairs can be obtained by comparing the free energy variations observed upon replacing counterions, {delta}{Delta}Gop(Na+ -> Mg2+), to the total free energy variations, {delta}{Delta}GMgop, seen at 100 mM Mg2+. As shown in Figure 5, the {delta}{Delta}Gop(Na+ -> Mg2+) values are linearly correlated to the {delta}{Delta}GMgop values according to the following equation:



View larger version (19K):
[in this window]
[in a new window]
  		Figure 5. Correlation between the changes in stabilization free energy observed upon replacing counterions, {delta}{Delta}Gop(Na+ -> Mg2+), and the total {delta}{Delta}GMgop changes observed at 100 mM Mg2+. The fitted line is: {delta}{Delta}Gop(Na+ -> Mg2+) = (–0.06 ± 0.02) + (0.80 ± 0.02) {delta}{Delta}GMgop

 
{delta}{Delta}Gop(Na+ -> Mg2+) = (–0.06 ± 0.02) +     (0.80 ± 0.02) {delta}{Delta}GMgop7

This result suggests that the Mg2+ counterions closely associated with the DNA contribute approximately 80% to the total change in stabilization free energy induced by Mg2+ at each site. The remaining 20% of the effect results from bulk Mg2+ ions in solution.

The stabilizing effects of Mg2+ ions depend on the position of the base pair in the base sequence and in the structure. This observation is illustrated in Figure 6. A dominant factor in this dependence is the location of the base relative to the cytosines in the ‘third’ strand. Previous NMR investigations have shown that the pK values of third-strand cytosines in Y·RY triple helices are 5.5 or higher (15). Therefore, at the pH used in the present study (pH 4.6), the cytosines in the ‘third’ strand are mostly in the protonated state. The influence of these protonated cytosines is clearly evident for the other bases in the ‘third’ strand. When protonated cytosines are present on both sides of the base (like for T19), the Mg2+-induced variations in {Delta}Gop are negative and the base pair is destabilized by Mg2+. When a thymine is placed next to a single protonated cytosine, the effect depends on its location. For example, the {delta}{Delta}GMgop value for T17 is half of that for T16. This difference most likely reflects the effect of changing the position of the neighboring protonated cytosine from the 3'- to the 5'-side of the base. Protonated cytosines also influence the Mg2+-induced stabilization of the C+·G Hoogsteen base pairs themselves. For an isolated C+·G pair like C18+·G11, Mg2+ induces a total stabilization of 0.3 kcal/mol. In contrast, for the C20+·G13 pair whose neighbor is also charged, the change in stability is negligible (Table 1).



View larger version (33K):
[in this window]
[in a new window]
  		Figure 6. Site-resolved energetic effects of Mg2+ ions upon the DNA triple helix investigated. Open columns represent {delta}{Delta}GMgop values for Watson–Crick base pairs. Filled columns represent {delta}{Delta}GMgop values for Hoogsteen base pairs. For G11 and G13, the lowest values of {delta}{Delta}GMgop (Table 1) are shown.

 
Protonated cytosines have been previously shown to greatly affect the overall stability of Y·RY triple helices (9,13–15,27–30). Large numbers of protonated cytosines generally stabilize the structure. The highest stabilization is observed for triplexes in which C+·GC triads alternate with T·AT triads (10,28,30). The stabilization diminishes when cytosines are placed next to each other (9,13,15,29,30). The latter effect reflects the fact that the unfavorable electrostatic potential created by adjacent protonated cytosines overcomes the stabilizing electrostatic attraction between the protonated base and the negatively charged phosphodiester backbone. Recent results have demonstrated that the same unfavorable electrostatic potential, created by clustering protonated cytosines next to each other, also affects the Mg2+-induced increase in melting temperature. For example, Fox and co-workers (10) have compared the melting of several 15-triad intermolecular triple helices of different base sequences. The largest Mg2+-induced increase in melting temperature was observed for the triplex containing the C+TT repeat in the third strand (namely, 11.1°C upon addition of 50 mM MgCl2). In contrast, for triplexes containing the C+C+T or C+TC+T repeats in the third strand, the corresponding increases in melting temperature were much smaller (i.e. 3.1 and 5.0°C, respectively). These findings are fully consistent with our conclusion that pairs of protonated cytosines, located either adjacent to each other or on both sides of the base, diminish or even eliminate the stabilization of base pairs by Mg2+ ions.

In summary, in the present work we have demonstrated that the exchange of imino protons is sensitive to the interactions of Mg2+ ions with DNA triple helices. Moreover, as we have shown, imino proton exchange can be used to probe the energetic effects of the ions at specific sites in DNA. The potential of this approach holds promise for future site-resolved investigations of interactions of metal ions with other nucleic acid systems.


   ACKNOWLEDGEMENT
 
This work was supported by a grant from the National Science Foundation (MCB-9723694).


   REFERENCES
TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 

  1. Soyfer,V.N. and Potaman,V.N. (1995) Triple-Helical Nucleic Acids. Springer-Verlag, New York, NY.

  2. Potaman,V.N. (2003) Applications of triple-stranded nucleic acid structures to DNA purification, detection and analysis. Expert Rev. Mol. Diagn., 3, 481–496.[CrossRef][ISI][Medline]

  3. Mirkin,S.M. and Frank-Kamenetskii,M.D. (1994) H-DNA and related structures. Annu. Rev. Biophys. Biomol. Struct., 23, 541–576.[ISI][Medline]

  4. Cheng,Y.-K. and Pettitt,B.M. (1992) Stabilities of double- and triple-strand helical nucleic acids. Prog. Biophys. Mol. Biol., 58, 225–257.[CrossRef][ISI][Medline]

  5. Pilch,D.S., Brousseau,R. and Shafer,R.H. (1990) Thermodynamics of triple helix formation: spectrophotometric studies on the d(A)10·2d(T)10 and d(C3+T4C3+)·d(G3A4G3)·d(C3T4C3) triple helices. Nucleic Acids Res., 18, 5743–5750.[Abstract/Free Full Text]

  6. Durand,M., Peloille,S., Thuong,N.T. and Maurizot,J.C. (1992) Triple-helix formation by an oligonucleotide containing one (dA)12 and two (dT)12 sequences bridged by two hexaethylene glycol chains. Biochemistry, 31, 9197–9204.[CrossRef][Medline]

  7. Rougee,M., Faucon,B., Mergny,J.L., Barcelo,F., Giovannangeli,C., Garestier,T. and Helene,C. (1992) Kinetics and thermodynamics of triple-helix formation: effects of ionic strength and mismatches. Biochemistry, 31, 9269–9278.[CrossRef][Medline]

  8. Singleton,S.F. and Dervan,P.B. (1993) Equilibrium association constants for oligonucleotide-directed triple helix formation at single DNA sites: linkage to cation valence and concentration. Biochemistry, 32, 13171–13179.[CrossRef][Medline]

  9. Sugimoto,N., Wu,P., Hara,H. and Kawamoto,Y. (2001) pH and cation effects on the properties of parallel pyrimidine motif DNA triplexes. Biochemistry, 40, 9396–9405.[CrossRef][Medline]

  10. James,P.L., Brown,T. and Fox,K.R. (2003) Thermodynamic and kinetic stability of intermolecular triple helices containing different proportions of C+·GC and T·AT triplets. Nucleic Acids Res., 31, 5598–5606.[Abstract/Free Full Text]

  11. Bond,J.P., Anderson,C.F. and Record,M.T.J. (1994) Conformational transitions of duplex and triplex nucleic acid helices: thermodynamic analysis of effects of salt concentration on stability using preferential interaction coefficients. Biophys. J., 67, 825–836.[Abstract/Free Full Text]

  12. Record,M.T.,Jr, Zhang,W. and Anderson,C.F. (1998) Analysis of effects of salts and uncharged solutes on protein and nucleic acid equilibria and processes: a practical guide to recognizing and interpreting polyelectrolyte effects, Hofmeister effects and osmotic effects of salts. Adv. Protein Chem., 51, 281–352.[ISI][Medline]

  13. Volker,J. and Klump,H.H. (1994) Electrostatic effects in DNA triple helices. Biochemistry, 33, 13502–13508.[CrossRef][Medline]

  14. Asensio,J.L., Lane,A.N., Dhesi,J., Bergqvist,S. and Brown,T. (1998) The contribution of cytosine protonation to the stability of parallel DNA triple helices. J. Mol. Biol., 275, 811–822.[CrossRef][ISI][Medline]

  15. Leitner,D., Schroder,W. and Weisz,K. (2000) Influence of sequence-dependent cytosine protonation and methylation on DNA triplex stability. Biochemistry, 39, 5886–5892.[CrossRef][Medline]

  16. Coman,D. and Russu,I.M. (2002) Site-resolved energetics in DNA triple helices containing G.TA and T.CG triads. Biochemistry, 41, 4407–4414.[CrossRef][Medline]

  17. Cantor,C.R., Warshaw,M.M. and Shapiro,H. (1970) Oligonucleotide interactions. III. Circular dichroism studies of the conformation of deoxyoligonucleotides. Biopolymers, 9, 1059–1077.[CrossRef][ISI][Medline]

  18. Plateau,P. and Gueron,M. (1982) Exchangeable proton NMR without base-line distortion, using new strong-pulse sequences. J. Am. Chem. Soc., 104, 7310–7311.[CrossRef][ISI]

  19. Powell,S.W., Jiang,L. and Russu,I.M. (2001) Proton exchange and base-pair opening in a DNA triple helix. Biochemistry, 40, 11065–11072.[CrossRef][Medline]

  20. Jiang,L. and Russu,I.M. (2001) Proton exchange and local stability in a DNA triple helix containing a G.TA triad. Nucleic Acids Res., 29, 4231–4237.[Abstract/Free Full Text]

  21. Englander,S.W. and Kallenbach,N.R. (1984) Hydrogen exchange and structural dynamics of proteins and nucleic acids. Q. Rev. Biophys., 16, 521–655.[ISI]

  22. Gueron,M. and Leroy,J.L. (1995) Studies of base pair kinetics by NMR measurement of proton exchange. Methods Enzymol., 261, 383–413.[ISI][Medline]

  23. Cain,R.J. and Glick,G.D. (1998) Use of cross-links to study the conformational dynamics of triplex DNA. Biochemistry, 37, 1456–1464.[CrossRef][Medline]

  24. Benight,A.S., Schurr,J.M., Flynn,P.F., Reid,B.R. and Wemmer,D.E. (1988) Melting of a self-complementary DNA minicircle. Comparison of optical melting theory with exchange broadening of the nuclear magnetic resonance spectrum. J. Mol. Biol., 200, 377–399.[CrossRef][ISI][Medline]

  25. Misra,V.K. and Draper,D.E. (2001) A thermodynamic framework for Mg2+ binding to RNA. Proc. Natl Acad. Sci. USA, 98, 12456–12461.[Abstract/Free Full Text]

  26. Sharp,K.A. and Honig,B. (1995) Salt effects on nucleic acids. Curr. Opin. Struct. Biol., 5, 323–328.[CrossRef][ISI][Medline]

  27. Plum,G.E. and Breslauer,K.J. (1995) Thermodynamics of an intramolecular DNA triple helix: a calorimetric and spectroscopic study of the pH and salt dependence of thermally induced structural transitions. J. Mol. Biol., 248, 679–695.[CrossRef][ISI][Medline]

  28. Roberts,R.W. and Crothers,D.M. (1996) Prediction of stability of DNA triplexes. Proc. Natl Acad. Sci. USA, 93, 4320–4325.[Abstract/Free Full Text]

  29. Wu,P., Kawamoto,Y., Hara,H. and Sugimoto,N. (2002) Effect of divalent cations and cytosine protonation on thermodynamic properties of intermolecular DNA double and triple helices. J. Inorg. Chem., 91, 277–285.

  30. Soto,A.M., Loo,J. and Marky,L.A. (2002) Energetic contribution for the formation of TAT/TAT, TAT/CGC+ and CGC+/CGC+ base triplet stacks. J. Am. Chem. Soc., 124, 14355–14363.[CrossRef][ISI][Medline]

  31. Frank-Kamenetskii,M.D. and Mirkin,S.M. (1995) Triplex DNA structures. Annu. Rev. Biochem., 64, 65–95.[ISI][Medline]


Add to CiteULike CiteULike   Add to Connotea Connotea   Add to Del.icio.us Del.icio.us    What's this?


This article has been cited by other articles:


Home page
 RNAHome page
P. V. Cornish, S. N. Stammler, and D. P. Giedroc
The global structures of a wild-type and poorly functional plant luteoviral mRNA pseudoknot are essentially identical
RNA, November 1, 2006; 12(11): 1959 - 1969.
[Abstract] [Full Text] [PDF]

Home page
 J. Biol. Chem.Home page
D. Coman and I. M. Russu
Base Pair Opening in Three DNA-unwinding Elements
J. Biol. Chem., May 27, 2005; 280(21): 20216 - 20221.
[Abstract] [Full Text] [PDF]

This Article
Right arrow Abstract Freely available
Right arrow Print PDF (227K) Freely available
Right arrow Alert me when this article is cited
Right arrow Alert me if a correction is posted
Services
Right arrow Email this article to a friend
Right arrow Similar articles in this journal
Right arrow Similar articles in ISI Web of Science
Right arrow Similar articles in PubMed
Right arrow Alert me to new issues of the journal
Right arrow Add to My Personal Archive
Right arrow Download to citation manager
Right arrow Search for citing articles in:
ISI Web of Science (5)
Right arrow Commercial Re-use Guidelines
for Open Access NAR Content
Google Scholar
Right arrow Articles by Coman, D.
Right arrow Articles by Russu, I. M.
Right arrow Search for Related Content
PubMed
Right arrow PubMed Citation
Right arrow Articles by Coman, D.
Right arrow Articles by Russu, I. M.
Social Bookmarking
Add to CiteULike   Add to Connotea   Add to Del.icio.us  
What's this?