Substrate conformational dynamics facilitate structure-specific recognition of gapped DNA by DNA polymerase

DNA-binding proteins utilise different recognition mechanisms to locate their DNA targets; some proteins recognise specific DNA sequences, while others interact with specific DNA structures. While sequence-specific DNA binding has been studied extensively, structure-specific recognition mechanisms remain unclear. Here, we study structure-specific DNA recognition by examining the structure and dynamics of DNA polymerase I Klenow Fragment (Pol) substrates both alone and in DNA–Pol complexes. Using a docking approach based on a network of 73 distances collected using single-molecule FRET, we determined a novel solution structure of the single-nucleotide-gapped DNA–Pol binary complex. The structure resembled existing crystal structures with regards to the downstream primer-template DNA substrate, and revealed a previously unobserved sharp bend (∼120°) in the DNA substrate; this pronounced bend was present in living cells. MD simulations and single-molecule assays also revealed that 4–5 nt of downstream gap-proximal DNA are unwound in the binary complex. Further, experiments and coarse-grained modelling showed the substrate alone frequently adopts bent conformations with 1–2 nt fraying around the gap, suggesting a mechanism wherein Pol recognises a pre-bent, partially-melted conformation of gapped DNA. We propose a general mechanism for substrate recognition by structure-specific enzymes driven by protein sensing of the conformational dynamics of their DNA substrates

Characterization of organic fluorophores for in vivo FRET studies based on electroporated molecules.

In vivo single-molecule fluorescence and Förster resonance energy transfer (FRET) techniques are excellent tools for studying spatial distribution, the nanoscale structure and conformational changes in living cells. We have recently introduced an electroporation-based method to internalize DNA and proteins labeled with organic fluorophores into living bacteria and established the ability for long-lived single-molecule fluorescence and FRET measurements. However, further developments, such as optimization of electroporation conditions, evaluation of organic fluorophore performance in vivo and quantitative single-cell FRET analysis, are needed to make the method more robust and general. Using singly-labeled DNA fragments, we optimized internalization efficiency and cell viability at six electroporation voltages, achieving >60% loading and viability similar to non-treated cells. We characterized the photostability and brightness of three donor fluorophores and four acceptor fluorophores in vivo; Cy3B, Atto647 and Atto647N performed best with photobleaching lifetimes of ∼20 s, 46 s and 92 s, respectively, and brightness values of ∼4000 photons per second under the same illumination conditions. We used three doubly-labeled DNA FRET standards (having in vitro FRET efficiencies of ∼17%, ∼42%, and ∼88%) and an alternating-laser excitation scheme to measure apparent FRET efficiencies at the single-cell level. We showed that we could differentiate DNA FRET standards at the single-cell level. Our approach offers a powerful method for the study of intramolecular changes or complex formation using FRET at the single-cell level in live bacteria

In vivo single-RNA tracking shows that most tRNA diffuses freely in live bacteria

Transfer RNA (tRNA) links messenger RNA nucleotide sequence with amino acid sequence during protein synthesis. Despite the importance of tRNA for translation, its subcellular distribution and diffusion properties in live cells are poorly understood. Here, we provide the first direct report on tRNA diffusion localization in live bacteria. We internalized tRNA labeled with organic fluorophores into live bacteria, applied single-molecule fluorescence imaging with single-particle tracking and localized and tracked single tRNA molecules over seconds. We observed two diffusive species: fast (with a diffusion coefficient of ∼8 μm2/s, consistent with free tRNA) and slow (consistent with tRNA bound to larger complexes). Our data indicate that a large fraction of internalized fluorescent tRNA (>70%) appears to diffuse freely in the bacterial cell. We also obtained the subcellular distribution of fast and slow diffusing tRNA molecules in multiple cells by normalizing for cell morphology. While fast diffusing tRNA is not excluded from the bacterial nucleoid, slow diffusing tRNA is localized to the cell periphery (showing a 30% enrichment versus a uniform distribution), similar to non-uniform localizations previously observed for mRNA and ribosomes

Stable end-sealed DNA as robust nano-rulers for in vivo single-molecule fluorescence

Single-molecule fluorescence and Förster resonance energy transfer (smFRET) are important tools for studying molecular heterogeneity, cellular organization, and protein structure in living cells. However, in vivo smFRET studies are still very challenging, and a standardized approach for robust in vivo smFRET measurements is still missing. Here, we synthesized protected DNAs with chemically linked ends as robust in vivo nano-rulers. We efficiently internalized doubly-labeled end-sealed DNA standards into live bacteria using electroporation and obtained stable and long-lasting smFRET signatures. Single-molecule fluorescence signals could be extended to ∼1 min by studying multi-fluorophore DNA standards. The high stability of protected DNA standards offers a general approach to evaluate single-molecule fluorescence and FRET signals, autofluorescence background, and fluorophore density, and hence, quality check the workflow for studying single-molecule trajectories and conformational dynamics of biomolecules in vivo

Stable end-sealed DNA as robust nano-rulers for in vivo single-molecule fluorescence

Single-molecule fluorescence and Fand#246;rster resonance energy transfer (smFRET) are important tools for studying molecular heterogeneity, cellular organization, and protein structure in living cells. However, in vivo smFRET studies are still very challenging, and a standardized approach for robust in vivo smFRET measurements is still missing. Here, we synthesized protected DNAs with chemically linked ends as robust in vivo nano-rulers. We efficiently internalized doubly-labeled end-sealed DNA standards into live bacteria using electroporation and obtained stable and long-lasting smFRET signatures. Single-molecule fluorescence signals could be extended to and#8764;1 min by studying multi-fluorophore DNA standards. The high stability of protected DNA standards offers a general approach to evaluate single-molecule fluorescence and FRET signals, autofluorescence background, and fluorophore density, and hence, quality check the workflow for studying single-molecule trajectories and conformational dynamics of biomolecules in vivo

In vivo single-RNA tracking shows that most tRNA diffuses freely in live bacteria

Transfer RNA (tRNA) links messenger RNA nucleotide sequence with amino acid sequence during protein synthesis. Despite the importance of tRNA for translation, its subcellular distribution and diffusion properties in live cells are poorly understood. Here, we provide the first direct report on tRNA diffusion localization in live bacteria. We internalized tRNA labeled with organic fluorophores into live bacteria, applied single-molecule fluorescence imaging with single-particle tracking and localized and tracked single tRNA molecules over seconds. We observed two diffusive species: fast (with a diffusion coefficient of ∼8 μm2/s, consistent with free tRNA) and slow (consistent with tRNA bound to larger complexes). Our data indicate that a large fraction of internalized fluorescent tRNA (>70%) appears to diffuse freely in the bacterial cell. We also obtained the subcellular distribution of fast and slow diffusing tRNA molecules in multiple cells by normalizing for cell morphology. While fast diffusing tRNA is not excluded from the bacterial nucleoid, slow diffusing tRNA is localized to the cell periphery (showing a 30% enrichment versus a uniform distribution), similar to non-uniform localizations previously observed for mRNA and ribosomes

Optimized delivery of fluorescently labeled proteins in live bacteria using electroporation.

Studying the structure and dynamics of proteins in live cells is essential to understanding their physiological activities and mechanisms, and to validating in vitro characterization. Improvements in labeling and imaging technologies are starting to allow such in vivo studies; however, a number of technical challenges remain. Recently, we developed an electroporation-based protocol for internalization, which allows biomolecules labeled with organic fluorophores to be introduced at high efficiency into live E. coli (Crawford et al. in Biophys J 105 (11):2439-2450, 2013). Here, we address important challenges related to internalization of proteins, and optimize our method in terms of (1) electroporation buffer conditions; (2) removal of dye contaminants from stock protein samples; and (3) removal of non-internalized molecules from cell suspension after electroporation. We illustrate the usability of the optimized protocol by demonstrating high-efficiency internalization of a 10-kDa protein, the ω subunit of RNA polymerase. Provided that suggested control experiments are carried out, any fluorescently labeled protein of up to 60 kDa could be internalized using our method. Further, we probe the effect of electroporation voltage on internalization efficiency and cell viability and demonstrate that, whilst internalization increases with increased voltage, cell viability is compromised. However, due to the low number of damaged cells in our samples, the major fraction of loaded cells always corresponds to non-damaged cells. By taking care to include only viable cells into analysis, our method allows physiologically relevant studies to be performed, including in vivo measurements of protein diffusion, localization and intramolecular dynamics via single-molecule Förster resonance energy transfer