Single-molecule Fluorescence Imaging Research Articles

Single-Molecule Approaches to Membrane Nanotubes

Membrane nanotubes (MNT) are thin (50∼200 nm in diameter), long-ranged (< hundreds of micrometer) membrane tubes that are formed by a physical connection between actin-driven protrusions from cell surfaces, which expedite intercellular communications between cells. However, the process of formation of MNTs that are heterogeneous even in the same cell type has been poorly understood. To explore the dynamic formation of MNTs, we visualized and manipulated MNTs in real time using single-molecule fluorescence imaging combined with optical tweezers. Real-time pulling and imaging a MNT attached to beads optically trapped revealed the detailed mechanical properties of how two protrusive F-actin bundles are connected. We also followed individual epidermal growth factor receptor (EGFR) on MNTs in various living cells, which allows for studying the mechanics of the transport of ligand-receptor signaling through MNTs. We will present how we achieved the single molecule tracking of receptors moving along a MNT that is placed in 3D space without interrupting the bead trapping.

Single-Molecule Analysis of Colocalized Epigenetic Modifications

Post-translational modifications of histones, which mediate many nuclear processes, is one of the most well characterized epigenetic mechanisms. In recent years, it has become evident that specific combinations of histone modifications represent various chromatin states, and are associated with different regulatory functions. However, standard methods like chromatin immunoprecipitation probe one histone modification at a time; thus, the combinatorial patterns at each histone or nucleosome are largely unknown. Here, we apply single-molecule fluorescent imaging in analyzing the coexisting histone modifications. We first demonstrate the method using reconstituted nucleosomes installing tetra-acetylated-lysines at histone 4. Once the assay is validated, it can be applied in the study of the coexisting active and repressive histone marks in different cell types, especially stem cells during differentiation. Other applications include the colocalization of histone variants, DNA methylation, transcription factors, and chromatin-binding proteins. We expect this method to elucidate the functions of chromatin in different states, with the ultimate goal in providing a complete picture of how epigenome is modulated.

Single-Molecule Fluorescence Imaging of Interfacial DNA Hybridization Kinetics at Selective Capture Surfaces.

Accurate knowledge of the kinetics of complementary oligonucleotide hybridization is integral to the design and understanding of DNA-based biosensors. In this work, single-molecule fluorescence imaging is applied to measuring rates of hybridization between fluorescently labeled target ssDNA and unlabeled probe ssDNA immobilized on glass surfaces. In the absence of probe site labeling, the capture surface must be highly selective to avoid the influence of nonspecific adsorption on the interpretation of single-molecule imaging results. This is accomplished by increasing the probe molecule site densities by a factor of ∼100 compared to optically resolvable sites so that nonspecific interactions compete with a much greater number of capture sites and by immobilizing sulfonate groups to passivate the surface between probe strands. The resulting substrates exhibit very low nonspecific adsorption, and the selectivity for binding a complementary target sequence exceeds that of a scrambled sequence by nearly 3 orders of magnitude. The population of immobilized DNA probe sites is quantified by counting individual DNA duplexes at low target concentrations, and those results are used to calibrate fluorescence intensities on the same sample at much higher target concentrations to measure a full binding isotherm. Dissociation rates are determined from interfacial residence times of individual DNA duplexes. Equilibrium and rate constants of hybridization, K(a) = 38 (±1) μM(-1), k(on) = 1.64 (±0.06) × 10(6) M(-1) s(-1), and k(off) = 4.3 (±0.1) × 10(-2) s(-1), were found not to change with surface density of immobilized probe DNA, indicating that hybridization events at neighboring probe sites are independent. To test the influence of probe-strand immobilization on hybridization, the kinetics of the probe target reaction at the surface were compared with the same reaction in free solution, and the equilibrium constants and dissociation and association rates were found to be nearly equivalent. The selectivity of these capture surfaces should facilitate sensitive investigations of DNA hybridization at the limit of counting molecules. Because the immobilized probe DNA on these surfaces is unlabeled, photobleaching of a probe label is not an issue, allowing capture substrates to be used for long periods of time or even reused in multiple experiments.

Single-Molecule Imaging With One Color Fluorescence.

Single-molecule fluorescence imaging is a powerful tool that enables real-time observation of DNA-protein or RNA-protein interactions with a nanometer precision. Here, we provide a detailed procedure for a previously developed single-molecule fluorescence method, termed "single-molecule protein-induced fluorescence enhancement" (smPIFE). While smFRET (Förster resonance energy transfer) requires both donor and acceptor, protein-induced fluorescence enhancement (PIFE) employs a single dye and measures the increase in fluorescence intensity induced by protein binding near the dye. PIFE displays distance sensitivity within 0-4nm, making it a powerful complementary or alternative tool to FRET method. In this chapter, we will discuss the various ways that PIFE has been utilized to study protein-nucleic acid interactions.

Single-Molecule Imaging to Characterize the Transport Mechanism of the Nuclear Pore Complex.

In the eukaryotic cell, a large macromolecular channel, known as the Nuclear Pore Complex (NPC), mediates all molecular transport between the nucleus and cytoplasm. In recent years, single-molecule fluorescence (SMF) imaging has emerged as a powerful tool to study the molecular mechanism of transport through the NPC. More recently, techniques such as single-molecule localization microscopy (SMLM) have enabled the spatial and temporal distribution of cargos, transport receptors and even structural components of the NPC to be determined with nanometre accuracy. In this protocol, we describe a method to study the position and/or motion of individual molecules transiting through the NPC with high spatial and temporal precision.

DNA-Protein Interactions Studied Directly Using Single Molecule Fluorescence Imaging of Quantum Dot Tagged Proteins Moving on DNA Tightropes.

Many protein interactions with DNA require specific sequences; however, how these sequences are located remains uncertain. DNA normally appears bundled in solution but, to study DNA-protein interactions, the DNA needs to be elongated. Using fluidics single DNA strands can be efficiently and rapidly elongated between beads immobilized on a microscope slide surface. Such "DNA tightropes" offer a valuable method to study protein search mechanisms. Real-time fluorescence imaging of these interactions provides quantitative descriptions of search mechanism at the single molecule level. In our lab, we use this method to study the complex process of nucleotide excision DNA repair to determine mechanisms of damage detection, lesion removal, and DNA excision.

Label-free Imaging of Microtubules with Sub-nm Precision Using Interferometric Scattering Microscopy

Current in vitro optical studies of microtubule dynamics tend to rely on fluorescent labeling of tubulin, with tracking accuracy thereby limited by the quantum yield of fluorophores and by photobleaching. Here, we demonstrate label-free tracking of microtubules with nanometer precision at kilohertz frame rates using interferometric scattering microscopy (iSCAT). With microtubules tethered to a glass substrate using low-density kinesin, we readily detect sequential 8 nm steps in the microtubule center of mass, characteristic of a single kinesin molecule moving a microtubule. iSCAT also permits dynamic changes in filament length to be measured with <5 nm precision. Using the arbitrarily long observation time enabled by label-free iSCAT imaging, we demonstrate continuous monitoring of microtubule disassembly over a 30 min period. The ability of iSCAT to track microtubules with nm precision together with its potential for label-free single protein detection and simultaneous single molecule fluorescence imaging represent a unique platform for novel approaches to studying microtubule dynamics.

Direct Fluorescent Imaging of Translocation and Unwinding by Individual DNA Helicases.

The unique translocation and DNA unwinding properties of DNA helicases can be concealed by the stochastic behavior of enzyme molecules within the necessarily large populations used in ensemble experiments. With recent technological advances, the direct visualization of helicases acting on individual DNA molecules has contributed significantly to the current understanding of their mechanisms of action and biological functions. The combination of single-molecule techniques that enable both manipulation of individual protein or DNA molecules and visualization of their actions has made it possible to literally see novel and unique biochemical characteristics that were previously masked. Here, we describe the execution and use of single-molecule fluorescence imaging techniques, focusing on methods that include optical trapping in conjunction with epifluorescent imaging, and also surface immobilization in conjunction with total internal reflection fluorescence visualization. Combined with microchannel flow cells and microfluidic control, these methods allow individual fluorescently labeled protein and DNA molecules to be imaged and tracked, affording measurement of DNA unwinding and translocation at single-molecule resolution.

Detection of the barium daughter in 136Xe →136Ba+2e− by in situ single-molecule fluorescence imaging

A robust technique for rejection of all γ-ray induced backgrounds in the search for the decay 136Xe→136Ba+2e− is needed to proceed to ton-scale detection systems. Efficient detection of the barium daughter would provide a long-sought pathway toward this goal. Single-molecule fluorescent imaging may offer a new way to detect the barium daughter atom in a naturally ionized state. A doubly charged barium ion can initiate a chelation process with a non-fluorescent precursor molecule, leading to a highly fluorescent complex. Repeated photo-excitation of the complex can reveal both presence and location of a single ionized atom with high precision and selectivity. Detection would be automatic, and is accomplished within the active volume of a xenon gas Time Projection Chamber operating at high pressure.

Single-molecule fluorescence imaging to quantify membrane protein dynamics and oligomerization in living plant cells

Measuring the mobility and interactions of proteins is key to understanding cellular signaling mechanisms; however, quantitative analysis of protein dynamics in living plant cells remains a major challenge. Here we describe an automated, single-molecule protocol based on total internal reflection fluorescence microscopy (TIRFM) imaging that allows protein tracking and subunit counting in living plant cells. This protocol uses TIRFM to image transgenic plant tissues expressing fluorescently tagged proteins that are localized to the plasma membrane. Next, a tracking algorithm quantifies dynamic changes in fluorescent protein motion types, temporary particle displacement and protein photobleaching steps. This protocol allows researchers to study the kinetic characteristics of heterogeneously distributed proteins. The approach has potential applications for studies of protein dynamics and subunit stoichiometry for a wide variety of plasma membrane and intracellular proteins in living plant cells and other biological specimens visualized by TIRFM or other fluorescence imaging techniques. The whole protocol can be completed in 5-6 h.

Distinct Cellular Assembly Stoichiometry of Polycomb Complexes on Chromatin Revealed by Single-molecule Chromatin Immunoprecipitation Imaging

Epigenetic complexes play an essential role in regulating chromatin structure, but information about their assembly stoichiometry on chromatin within cells is poorly understood. The cellular assembly stoichiometry is critical for appreciating the initiation, propagation, and maintenance of epigenetic inheritance during normal development and in cancer. By combining genetic engineering, chromatin biochemistry, and single-molecule fluorescence imaging, we developed a novel and sensitive approach termed single-molecule chromatin immunoprecipitation imaging (Sm-ChIPi) to enable investigation of the cellular assembly stoichiometry of epigenetic complexes on chromatin. Sm-ChIPi was validated by using chromatin complexes with known stoichiometry. The stoichiometry of subunits within a polycomb complex and the assembly stoichiometry of polycomb complexes on chromatin have been extensively studied but reached divergent views. Moreover, the cellular assembly stoichiometry of polycomb complexes on chromatin remains unexplored. Using Sm-ChIPi, we demonstrated that within mouse embryonic stem cells, one polycomb repressive complex (PRC) 1 associates with multiple nucleosomes, whereas two PRC2s can bind to a single nucleosome. Furthermore, we obtained direct physical evidence that the nucleoplasmic PRC1 is monomeric, whereas PRC2 can dimerize in the nucleoplasm. We showed that ES cell differentiation induces selective alteration of the assembly stoichiometry of Cbx2 on chromatin but not other PRC1 components. We additionally showed that the PRC2-mediated trimethylation of H3K27 is not required for the assembly stoichiometry of PRC1 on chromatin. Thus, these findings uncover that PRC1 and PRC2 employ distinct mechanisms to assemble on chromatin, and the novel Sm-ChIPi technique could provide single-molecule insight into other epigenetic complexes.

Referenced Single-Molecule Measurements Differentiate between GPCR Oligomerization States

The extent to which Rhodopsin family G-protein-coupled receptors (GPCRs) form invariant oligomers is contentious. Recent single-molecule fluorescence imaging studies mostly argue against the existence of constitutive receptor dimers and instead suggest that GPCRs only dimerize transiently, if at all. However, whether or not even transient dimers exist is not always clear due to difficulties in unambiguously distinguishing genuine interactions from chance colocalizations, particularly with respect to short-lived events. Previous single-molecule studies have depended critically on calculations of chance colocalization rates and/or comparison with unfixed control proteins whose diffusional behavior may or may not differ from that of the test receptor. Here, we describe a single-molecule imaging assay that 1) utilizes comparisons with well-characterized control proteins, i.e., the monomer CD86 and the homodimer CD28, and 2) relies on cell fixation to limit artifacts arising from differences in the distribution and diffusion of test proteins versus these controls. The improved assay reliably reports the stoichiometry of the Glutamate-family GPCR dimer, γ-amino butyric acid receptor b2, whereas two Rhodopsin-family GPCRs, β2-adrenergic receptor and mCannR2, exhibit colocalization levels comparable to those of CD86 monomers, strengthening the case against invariant GPCR oligomerization.

Base pair distance analysis in single DNA molecule by direct stochastic optical reconstruction microscopy

Abstract Precise fluorescence imaging of single λ-DNA molecules for base pair distance analysis requires a super-resolution technique, as these distances are on the order of diffraction limit. Individual λ-DNA molecules intercalated with the fluorescent dye YOYO-1 were investigated at subdiffraction spatial resolution by direct stochastic optical reconstruction microscopy (dSTORM). Various dye-to-DNA base pair ratios were imaged by photoswitching YOYO-1 between the fluorescent state and the dark state using two laser sources. The acquired images were reconstructed into a super-resolution image by applying Gaussian fitting to the centroid of the point spread function. By measuring the distances between localized fluorophores, the base pair distances in single DNA molecules for dye-to-DNA base pair ratios of 1:50, 1:100, and 1:500 were calculated to be 17.1 ± 0.8 nm, 34.3 ± 2.2 nm, and 170.3 ± 8.1 nm, respectively, which were in agreement with theoretical values. These results demonstrate that intercalating dye in a single DNA molecule can be photoswitched without the use of an activator fluorophore, and that super-localization precision at a spatial resolution of ∼17 nm was experimentally achieved.

Plasmon-Enhanced Fluorescence from Single Proteins in Living Bacteria

The sensitivity and resolution of single-molecule fluorescence imaging in biology are mainly limited by two known weaknesses of fluorescent proteins: label brightness and photostability. In this work, we use patterned gold substrates to achieve plasmon-enhanced emission from intrinsically fluorescent proteins in living pathogenic bacteria cells. By coupling membrane-bound single fluorescent protein fusions to the virulence regulator TcpP in living Vibrio cholerae bacteria to extracellular gold nanotriangle arrays, we use plasmonics to improve our measurements of this important question in pathogenesis: how does V. cholerae produce its deadly toxin? Based on a simple experimental geometry, we observe a 1.3× enhancement in the rate of emission and a 1.4× enhancement in the number of photons detected prior to photobleaching. Furthermore, by enhancing both the rate of emission and the total number of photons detected from single-molecule fluorescent probes in live cells, we show that plasmon-enhanced fluoresc...

Functional Dynamics within the Human Ribosome Regulate the Rate of Active Protein Synthesis

The regulation of protein synthesis contributes to gene expression in both normal physiology and disease, yet kinetic investigations of the human translation mechanism are currently lacking. Using single-molecule fluorescence imaging methods, we have quantified the nature and timing of structural processes in human ribosomes during single-turnover and processive translation reactions. These measurements reveal that functional complexes exhibit dynamic behaviors and thermodynamic stabilities distinct from those observed for bacterial systems. Structurally defined sub-states of pre- and post-translocation complexes were sensitive to specific inhibitors of the eukaryotic ribosome, demonstrating the utility of this platform to probe drug mechanism. The application of three-color single-molecule fluorescence resonance energy transfer (smFRET) methods further revealed a long-distance allosteric coupling between distal tRNA binding sites within ribosomes bearing three tRNAs, which contributed to the rate of processive translation.

Detecting the barium daughter in 136Xe 0-νββ decay using single-molecule fluorescence imaging techniques

Single-molecule fluorescent imaging may provide an avenue to efficiently detect the Ba++ daughter atom in the decay 136Xe → Ba + 2e−, and, unambiguously associate the birth point in space within the electron trajectories of the decay event. Chelation of doubly-charged alkaline earth elements such as calcium and barium by certain precursor molecules converts the resulting complex from a non-fluorescent to a fluorescent state. Repeated photo-excitation of a single fluorescent complex reveals both presence and location with high precision. This technique, widespread now in biochemistry, biophysics and biology, may permit a similar discriminating response in a large high-pressure xenon gas TPC for the Ba++ ion from xenon double-beta decay. The TPC measures the event time and energy of the two nascent electrons, as well as topology and position in 3-D from their trajectories in the gas. Measurement of the 2-D location of the molecular ion after arrival at the cathode plane permits an association of ion with the event. Demonstration of an efficient, highly specific detection of the barium daughter would provide a long-sought pathway to a background-free result in the search for this decay mode, of central importance for determining the nature of the neutrino.

Cryo-electron microscopy and single molecule fluorescent microscopy detect CD4 receptor induced HIV size expansion prior to cell entry

Viruses are often thought to have static structure, and they only remodel after the viruses have entered target cells. Here, we detected a size expansion of virus particles prior to viral entry using cryo-electron microscopy (cryo-EM) and single molecule fluorescence imaging. HIV expanded both under cell-free conditions with soluble receptor CD4 (sCD4) targeting the CD4 binding site on the HIV-1 envelope protein (Env) and when HIV binds to receptor on cellular membrane. We have shown that the HIV Env is needed to facilitate receptor induced virus size expansions, showing that the ‘lynchpin’ for size expansion is highly specific. We demonstrate that the size expansion required maturation of HIV and an internal capsid core with wild type stability, suggesting that different HIV compartments are linked and are involved in remodelling. Our work reveals a previously unknown event in HIV entry, and we propose that this pre-entry priming process enables HIV particles to facilitate the subsequent steps in infection.

RETRACTED ARTICLE: Discovery of a novel inhibitory mechanism of kaempferol on TGF-β ligand-receptor interaction by single-molecule techniques

The corresponding author, Yong Yang from China Medical University, would like to retract the article ‘‘Discovery of a novel inhibitory mechanism of kaempferol on TGF-? ligand-receptor interaction by single-molecule techniques’’ since submission has not been authorized by the research supervisor of the author. Moreover, parts of the introduction have been duplicated from the paper ‘‘A single-molecule study of the inhibition effect of Naringenin on transforming growth factor-b ligand-receptor binding’’, 2011, DOI:10.1039/c1cc10778j. The online version of this article contains the full text of the retracted article as electronic supplementary material. Supporting information Supplementary Fig. 1 Fluorescence intensity by flow cytometry using biotinylated TGF-b1 and avidin-FITC. Supplementary Fig. 2 Single-molecule fluorescence imaging of TbRII-GFP monomers and dimers. Distribution of the fluorescence intensities of single GFP molecules imaged on coverslips. Supplementary Fig. 3 Two representative time courses of TbRII-GFP emission show one-step bleaching for monomers and two-step bleaching for dimers. Supplementary Video 1 Imaging of TbRII-GFP molecules on the cell membrane of live HeLa cells.

Introducing a fluorescence-based standard to quantify protein partitioning into membranes

The affinity of peripheral membrane proteins for a lipid bilayer can be described using the partition coefficient (KP). Although several methods to determine KP are known, all possess limitations. To address some of these issues, we developed both: a versatile method based on single molecule detection and fluorescence imaging for determining KP, and a simple measurement standard employing hexahistidine-tagged enhanced green fluorescent protein (eGFP-His6) and free standing membranes of giant unilamellar vesicles (GUVs) functionalized with NTA(Ni) lipids as binding sites. To ensure intrinsic control, our method features two measurement modes. In the single molecule mode, fluorescence correlation spectroscopy (FCS) is applied to quantify free and membrane associated protein concentrations at equilibrium and calculate KP. In the imaging mode, confocal fluorescence images of GUVs are recorded and analyzed with semi-automated software to extract protein mean concentrations used to derive KP. Both modes were compared by determining the affinity of our standard, resulting in equivalent KP values. As observed in other systems, eGFP-His6 affinity for membranes containing increasing amounts of NTA(Ni) lipids rises in a stronger-than-linear fashion. We compared our dual approach with a FCS-based assay that uses large unilamellar vesicles (LUVs), which however fails to capture the stronger-than-linear trend for our NTA(Ni)-His6 standard. Hence, we determined the KP of the MARCKS effector domain with our FCS approach on GUVs, whose results are consistent with previously published data using LUVs. We finally provide a practical manual on how to measure KP and understand it in terms of molecules per lipid surface.

Single-molecule imaging of a three-component ordered actin disassembly mechanism.

The mechanisms by which cells destabilize and rapidly disassemble filamentous actin networks have remained elusive; however, Coronin, Cofilin and AIP1 have been implicated in this process. Here using multi-wavelength single-molecule fluorescence imaging, we show that mammalian Cor1B, Cof1 and AIP1 work in concert through a temporally ordered pathway to induce highly efficient severing and disassembly of actin filaments. Cor1B binds to filaments first, and dramatically accelerates the subsequent binding of Cof1, leading to heavily decorated, stabilized filaments. Cof1 in turn recruits AIP1, which rapidly triggers severing and remains bound to the newly generated barbed ends. New growth at barbed ends generated by severing was blocked specifically in the presence of all three proteins. This activity enabled us to reconstitute and directly visualize single actin filaments being rapidly polymerized by formins at their barbed ends while simultanteously being stochastically severed and capped along their lengths, and disassembled from their pointed ends.