Quantitative detection of small molecule/DNA complexes employing a force-based and label-free DNA-microarray.

Force-based ligand detection is a promising method to characterize molecular complexes label-free at physiological conditions. Because conventional implementations of this technique, e.g., based on atomic force microscopy or optical traps, are low-throughput and require extremely sensitive and sophisticated equipment, this approach has to date found only limited application. We present a low-cost, chip-based assay, which combines high-throughput force-based detection of dsDNA.ligand interactions with the ease of fluorescence detection. Within the comparative unbinding force assay, many duplicates of a target DNA duplex are probed against a defined reference DNA duplex each. The fractions of broken target and reference DNA duplexes are determined via fluorescence. With this assay, we investigated the DNA binding behavior of artificial pyrrole-imidazole polyamides. These small compounds can be programmed to target specific dsDNA sequences and distinguish between D- and L-DNA. We found that titration with polyamides specific for a binding motif, which is present in the target DNA duplex and not in the reference DNA duplex, reliably resulted in a shift toward larger fractions of broken reference bonds. From the concentration dependence nanomolar to picomolar dissociation constants of dsDNA.ligand complexes were determined, agreeing well with prior quantitative DNAase footprinting experiments. This finding corroborates that the forced unbinding of dsDNA in presence of a ligand is a nonequilibrium process that produces a snapshot of the equilibrium distribution between dsDNA and dsDNA.ligand complexes.

Molecular force balance measurements reveal that double-stranded DNA unbinds under force in rate-dependent pathways.

Strand separation of double-stranded DNA is a crucial step for essential cellular processes such as recombination and transcription. By means of a molecular force balance, we have analyzed the impact of different pulling directions and different force-loading rates on the unbinding process of short double-stranded DNA. At loading rates above 9 x 10(5) pN/s, we found a marked difference in rupture probability for pulling the duplex in 3'-3' direction compared to a 5'-5' direction, indicating different unbinding pathways. We propose a mechanism by which unbinding at low loading rates is dominated by nondirectional thermal fluctuations, whereas mechanical properties of the DNA become more important at high loading rates and reveal the asymmetry of the phosphoribose backbone. Our model explains the difference of 3'-3' and 5'-5' unbinding as a kinetic process, where the loading rate exceeds the relaxation time of DNA melting bubbles.

Predicting the rupture probabilities of molecular bonds in series.

An assembly of two receptor ligand bonds in series will typically break at the weaker complex upon application of an external force. The rupture site depends highly on the binding potentials of both bonds and on the loading rate of the applied force. A model is presented that allows simulations of force-induced rupture of bonds in series at a given force and loading rate based on the natural dissociation rates kR0,S0 and the potential width DeltaxR,S of the reference and sample bonds. The model is especially useful for the analysis of differential force assay experiments. This is illustrated by experiments on molecular force balances consisting of two 30-bp oligonucleotide duplexes where kR0,S0 and DeltaxR,S have been determined for different single nucleotide mismatches. Furthermore, prediction of the rupture site of two bonds in series is demonstrated for DNA duplexes in combination with streptavidin/biotin and anti-digoxigenin/digoxigenin, respectively.