Direct observation of specific messenger RNA in a single living cell under a fluorescence microscope

We observed the expression of human c-fos mRNA in a living transfected Cos7 cell under a fluorescence microscope by detecting hybrid formed with two fluorescently labeled oligodeoxynucleotides (oligoDNAs) and c-fos mRNA in the cytoplasm. Two fluorescent oligoDNAs were prepared, each labeled with a fluorescence molecule different from the other. When two oligoDNAs hybridized to an adjacent sequence on the target mRNA, the distance between the two fluorophores became very close and fluorescence resonance energy transfer (FRET) occurred, resulting in changes in fluorescence spectra. To find sequences of high accessibility of c-fos RNA to oligoDNAs, several sites that included loop structures on the simulated secondary structure were selected. Each site was divided into two halves, and the pair of fluorescent oligoDNAs complementary to the sequence was synthesized. Each site was examined for the efficiency of hybridization to c-fos RNA by measuring changes in fluorescence spectra when c-fos RNA was added to the pair of oligoDNAs in solution. A 40 mer specific site was found, and the pair of oligoDNAs for the site were microinjected into Cos7 cells that expressed c-fos mRNA. To block oligoDNAs from accumulating in the nucleus, oligoDNA was bound to a macromolecule (streptavidin) to prevent passage of nuclear pores. Hybridization of the pair of oligoDNAs to c-fos mRNA in the cytoplasm was detected in fluorescence images indicating FRET.     

Time-resolved FRET fluorescence spectroscopy of visible fluorescent protein pairs

Förster resonance energy transfer (FRET) is a powerful method for obtaining information about small-scale lengths between biomacromolecules. Visible fluorescent proteins (VFPs) are widely used as spectrally different FRET pairs, where one VFP acts as a donor and another VFP as an acceptor. The VFPs are usually fused to the proteins of interest, and this fusion product is genetically encoded in cells. FRET between VFPs can be determined by analysis of either the fluorescence decay properties of the donor molecule or the rise time of acceptor fluorescence. Time-resolved fluorescence spectroscopy is the technique of choice to perform these measurements. FRET can be measured not only in solution, but also in living cells by the technique of fluorescence lifetime imaging microscopy (FLIM), where fluorescence lifetimes are determined with the spatial resolution of an optical microscope. Here we focus attention on time-resolved fluorescence spectroscopy of purified, selected VFPs (both single VFPs and FRET pairs of VFPs) in cuvette-type experiments. For quantitative interpretation of FRET–FLIM experiments in cellular systems, details of the molecular fluorescence are needed that can be obtained from experiments with isolated VFPs. For analysis of the time-resolved fluorescence experiments of VFPs, we have utilised the maximum entropy method procedure to obtain a distribution of fluorescence lifetimes. Distributed lifetime patterns turn out to have diagnostic value, for instance, in observing populations of VFP pairs that are FRET-inactive.     

Quantitative time domain analysis of lifetime‐based Förster resonant energy transfer measurements with fluorescent proteins: Static random isotropic fluorophore orientation distributions

Förster resonant energy transfer (FRET) measurements are widely used to obtain information about molecular interactions and conformations through the dependence of FRET efficiency on the proximity of donor and acceptor fluorophores. Fluorescence lifetime measurements can provide quantitative analysis of FRET efficiency and interacting population fraction. Many FRET experiments exploit the highly specific labelling of genetically expressed fluorescent proteins, applicable in live cells and organisms. Unfortunately, the typical assumption of fast randomization of fluorophore orientations in the analysis of fluorescence lifetime‐based FRET readouts is not valid for fluorescent proteins due to their slow rotational mobility compared to their upper state lifetime. Here, previous analysis of effectively static isotropic distributions of fluorophore dipoles on FRET measurements is incorporated into new software for fitting donor emission decay profiles. Calculated FRET parameters, including molar population fractions, are compared for the analysis of simulated and experimental FRET data under the assumption of static and dynamic fluorophores and the intermediate regimes between fully dynamic and static fluorophores, and mixtures within FRET pairs, is explored. Finally, a method to correct the artefact resulting from fitting the emission from static FRET pairs with isotropic angular distributions to the (incorrect) typically assumed dynamic FRET decay model is presented.      

Imaging protein-protein interactions using fluorescence resonance energy transfer microscopy

Fluorescence resonance energy transfer (FRET) detects the proximity of fluorescently labeled molecules over distances >100 A. When performed in a fluorescence microscope, FRET can be used to map protein-protein interactions in vivo. We here describe a FRET microscopy method that can be used to determine whether proteins that are colocalized at the level of light microscopy interact with one another. This method can be implemented using digital microscopy systems such as a confocal microscope or a wide-field fluorescence microscope coupled to a charge-coupled device (CCD) camera. It is readily applied to samples prepared with standard immunofluorescence techniques using antibodies labeled with fluorescent dyes that act as a donor and acceptor pair for FRET. Energy transfer efficiencies are quantified based on the release of quenching of donor fluorescence due to FRET, measured by comparing the intensity of donor fluorescence before and after complete photobleaching of the acceptor. As described, this method uses Cy3 and Cy5 as the donor and acceptor fluorophores, but can be adapted for other FRET pairs including cyan fluorescent protein and yellow fluorescent protein.     

Adenovirus type-5 entry and disassembly followed in living cells by FRET, fluorescence anisotropy, and FLIM

We have used fluorescence resonance energy transfer (FRET) to follow the process of capsid disassembly for adenovirus (Ad) serotype 5 (Ad5) in living CHO-CAR cells. Ad5 were weakly labeled on their capsid proteins with FRET donor and acceptor fluorophores. A progressive decrease in FRET efficiency recorded during Ad5 uptake revealed that the time course of Ad5 capsid disassembly has two sequential protein dissociation rates with half-times of 3 and 60 min. Fluorescence anisotropy measurements of the segmental motions of fluorophores on Ad5 indicate that the first rate is linked to the detachment from the capsid of the protruding, flexible fiber proteins. The second rate was shown to report on the combined dissociation of protein IX, penton base, and hexons, which form the rigid icosahedral capsid shell. Fluorescence lifetime imaging microscopy measurements using a pH-sensitive probe provided information on the pH of the microenvironment of Ad5 particles during intracellular trafficking, and confirmed that the fast fiber dissociation step occurred at the onset of endocytosis. The slower dissociation phase was shown to coincide with the escape of Ad5 from endocytic compartments into the cytosol, and its arrival at the nuclear membrane. These results demonstrate a rapid, quantitative live-cell assay for the investigation of virus-cell interactions and capsid disassembly.     

FRET between cardiac Na+ channel subunits measured with a confocal microscope and a streak camera

When and where proteins associate is a central question in many biomolecular studies. F?rster resonance energy transfer (FRET) measurements can be used to address this question when the interacting proteins are labeled with appropriate donor and acceptor fluorophores. We describe an improved method to determine FRET efficiency that uses a mode-locked laser, a confocal microscope and a streak camera. We applied this method to study the association of alpha and beta(1) subunits of the human cardiac sodium channel. The subunits were tagged with the cyan and yellow variants of the green fluorescent protein (GFP) and expressed in human embryonic kidney (HEK293) cells. Pronounced FRET between the channel subunits in the endoplasmic reticulum (ER) suggested that the subunits associate before they reach the plasma membrane. The described method allows simultaneous measurement of donor and acceptor fluorescence decays and provides an intrinsically validated estimate of FRET efficiency.     

A Protein L -Based Immunodiagnostic Approach Utilizing Time-Resolved F?rster Resonance Energy Transfer

Chelated lanthanides such as europium (Eu) have uniquely long fluorescence emission half-lives permitting their use in time-resolved fluorescence (TRF) assays. In Förster resonance energy transfer (FRET) a donor fluorophore transfers its emission energy to an acceptor fluorophore if in sufficiently close proximity. The use of time-resolved (TR) FRET minimizes the autofluorescence of molecules present in biological samples. In this report, we describe a homogenous immunoassay prototype utilizing TR-FRET for detection of antibodies in solution. The assay is based on labeled protein L, a bacterial protein that binds to immunoglobulin (Ig) light chain, and labeled antigen, which upon association with the same Ig molecule produce a TR-FRET active complex. We show that the approach is functional and can be utilized for both mono- and polyvalent antigens. We also compare the assay performance to that of another homogenous TR-FRET immunoassay reported earlier. This novel assay may have wide utility in infectious disease point-of-care diagnostics.     

Fluorescence resonance energy transfer (FRET) and competing processes in donor-acceptor substituted DNA strands: a comparative study of ensemble and single-molecule data

We studied the fluorescence resonance energy transfer (FRET) efficiency of different donor-acceptor labeled model DNA systems in aqueous solution from ensemble measurements and at the single molecule level. The donor dyes: tetramethylrhodamine (TMR); rhodamine 6G (R6G); and a carbocyanine dye (Cy3) were covalently attached to the 5'-end of a 40-mer model oligonucleotide. The acceptor dyes, a carbocyanine dye (Cy5), and a rhodamine derivative (JA133) were attached at modified thymidine bases in the complementary DNA strand with donor-acceptor distances of 5, 15, 25 and 35 DNA-bases, respectively. Anisotropy measurements demonstrate that none of the dyes can be observed as a free rotor; especially in the 5-bp constructs the dyes exhibit relatively high anisotropy values. Nevertheless, the dyes change their conformation with respect to the oligonucleotide on a slower time scale in the millisecond range. This results in a dynamic inhomogeneous distribution of donor/acceptor (D/A) distances and orientations. FRET efficiencies have been calculated from donor and acceptor fluorescence intensity as well as from time-resolved fluorescence measurements of the donor fluorescence decay. Dependent on the D/A pair and distance, additional strong fluorescence quenching of the donor is observed, which simulates lower FRET efficiencies at short distances and higher efficiencies at longer distances. On the other hand, spFRET measurements revealed subpopulations that exhibit the expected FRET efficiency, even at short D/A distances. In addition, the measured acceptor fluorescence intensities and lifetimes also partly show fluorescence quenching effects independent of the excitation wavelength, i.e. either directly excited or via FRET. These effects strongly depend on the D/A distance and the dyes used, respectively. The obtained data demonstrate that besides dimerization at short D/A distances, an electron transfer process between the acceptor Cy5 and rhodamine donors has to be taken into account. To explain deviations from FRET theory even at larger D/A distances, we suggest that the pi-stack of the DNA double helix mediates electron transfer from the donor to the acceptor, even over distances as long as 35 base pairs. Our data show that FRET experiments at the single molecule level are rather suited to resolve fluorescent subpopulations in heterogeneous mixture, information about strongly quenched subpopulations gets lost.     

Combination of novel green fluorescent protein mutant TSapphire and DsRed variant mOrange to set up a versatile in planta FRET-FLIM assay

Förster resonance energy transfer (FRET) measurements based on fluorescence lifetime imaging microscopy (FLIM) are increasingly being used to assess molecular conformations and associations in living systems. Reduction in the excited-state lifetime of the donor fluorophore in the presence of an appropriately positioned acceptor is taken as strong evidence of FRET. Traditionally, cyan fluorescent protein has been widely used as a donor fluorophore in FRET experiments. However, given its photolabile nature, low quantum yield, and multiexponential lifetime, cyan fluorescent protein is far from an ideal donor in FRET imaging. Here, we report the application and use of the TSapphire mutant of green fluorescent protein as an efficient donor to mOrange in FLIM-based FRET imaging in intact plant cells. Using time-correlated single photon counting-FLIM, we show that TSapphire expressed in living plant cells decays with lifetime of 2.93 ± 0.09 ns. Chimerically linked TSapphire and mOrange (with 16-amino acid linker in between) exhibit substantial energy transfer based on the reduction in the lifetime of TSapphire in the presence of the acceptor mOrange. Experiments performed with various genetically and/or biochemically known interacting plant proteins demonstrate the versatility of the FRET-FLIM system presented here in different subcellular compartments tested (cytosol, nucleus, and at plasma membrane). The better spectral overlap with red monomers, higher photostability, and monoexponential lifetime of TSapphire makes it an ideal FRET-FLIM donor to study protein-protein interactions in diverse eukaryotic systems overcoming, in particular, many technical challenges encountered (like autofluorescence of cell walls and fluorescence of pigments associated with photosynthetic apparatus) while studying plant protein dynamics and interactions.Single- and dual-color fluorescence imaging with intrinsically fluorescent proteins is increasingly being used to study the expression, targeting, colocalization, turnover, and associations of diverse proteins involved in different plant signal transduction pathways (for review, see Fricker et al., 2006). Concurrent with the use of fluorescence-based cell biology, Förster resonance energy transfer (FRET) has emerged as a convenient tool to study the dynamics of protein associations in vivo. The technique exploits the biophysical phenomenon of nonradiative energy transfer from a donor fluorophore to an appropriately positioned acceptor at a nanometer scale (1–10 nm; Jares-Erijman and Jovin, 2003). In living cells, FRET occurs when two proteins (or different domains within a single protein) fused to suitable donor and acceptor fluorophores physically interact, thus bringing the donor and the acceptor within the favorable proximity for energy transfer (Immink et al., 2002; Bhat et al., 2006). This results in a decrease in the donor''s fluorescence intensity (or quantum yield [QY]) and excited-state lifetime (Gadella et al., 1999). Furthermore, if the acceptor molecule is a fluorophore, then FRET additionally results in an increase in the acceptor''s emission intensity (sensitized emission; Shah et al., 2001; Bhat et al., 2006).However, the exploitation and use of fluorescent marker proteins to study protein trafficking and associations in plants can be problematic because plant cells contain a number of autofluorescent compounds (e.g. lignin, chlorophyll, phenols, etc.) whose emission spectra interfere with that of the most commonly used green or red fluorescent protein fluorophores and/or their spectral variants. For example, lignin fluorescence in roots, vascular tissues, and cell walls of aerial plant parts interferes with imaging at wavelengths between 490 and 620 nm, whereas the chlorophyll autofluorescence in green aerial plant parts is prevalent between 630 and 770 nm (Chapman et al., 2005). Consequently, conventional imaging of GFP and its closest spectral variants (like cyan fluorescent protein [CFP] and yellow fluorescent protein [YFP]) is most likely to be problematic in roots, whereas red-shifted intrinsic fluorescent proteins (including monomeric red fluorescent protein and recently identified spectral variants like mStrawberry and mCherry) may be hard to discriminate in chloroplast-containing aerial tissues (Chapman et al., 2005). The problems get further compounded in FRET assays because the autofluorescence arising from phenols, lignin, and chlorophyll can limit the choice of fluorophores suitable for in planta FRET assays.CFP and YFP have been widely used as a donor-acceptor pair in in planta FRET measurements (Bhat et al., 2006; Dixit et al., 2006). However, in photophysical terms, this pair is less than ideal for FRET imaging. Both have broad excitation and emission spectra with a small Stokes shift (Chapman et al., 2005). Second, QY of CFP (QY = 0.4) is relatively lower than that of YFP (QY = 0.61), and thus a significantly higher (and rather cell damaging) amount of excitation energy is needed to induce FRET (Dixit et al., 2006). Additionally, CFP displays multiexponential lifetimes with a shorter (1.3 ns) and a longer (2.6 ns) component (Becker et al., 2006). Although the deviation from the single-component decay is reasonably small (Tramier et al., 2002; Becker et al., 2006), the shorter CFP lifetime component can erroneously be interpreted as being the result of lifetime reduction due to energy transfer. At the same time, weak or transient protein associations may get masked and thus remain undetected. Whereas the parental wild-type GFP is extremely photostable and shows a monoexponential decay pattern (excited-state lifetime 3.16 ± 0.03 ns; Striker et al., 1999; Volkmer et al., 2000; Shaner et al., 2005), its close spectral overlap with YFP makes it unsuitable as a donor in GFP-YFP FRET experiments. Likewise, wild-type or enhanced GFP (or YFP) as a donor to red-shifted monomers as acceptors is suboptimal because the 488-nm (or 514-nm) laser line commonly used to excite GFP (or YFP) cross excites most of the red monomers (e.g. mOrange, mStrawberry) because of their broad excitation spectra (Zapata-Hommer and Griesbeck, 2003; Shaner et al., 2004).Recently, TSapphire (Q69M/C70P/V163A/S175G; excitation/emission 399/511 nm), a variant of the Sapphire (T203I) mutant of wild-type GFP with improved folding properties and better pH sensitivity, was described (Zapata-Hommer and Griesbeck, 2003). The T203I mutation in TSapphire (and original Sapphire as well) abolishes the 475-nm excitation peak found in the wild-type GFP (Tsien, 1998). TSapphire is efficiently excited below 410 nm, which makes it ideal for studying plant protein dynamics and interactions because, at this wavelength, there is negligible excitation of the autofluorescing chlorophyll pigments. Furthermore, TSapphire also represents a good donor to red monomer acceptors that are negligibly excited at this wavelength (Shaner et al., 2004). Using a purified Zn²⁺ sensor with TSapphire and mOrange as a donor-acceptor pair, Shaner and colleagues demonstrated the ratiometric intramolecular FRET between the two fluorophores in vitro (Shaner et al., 2004). The sensor yielded a 6-fold ratiometric increase (562/514-nm mOrange/TSapphire emission ratio) upon Zn²⁺ binding.However, currently there are no reports demonstrating the application and use of TSapphire and monomeric red-shifted fluorophores as donor-acceptor FRET pairs to probe intermolecular protein-protein interactions in vivo. In this article, we demonstrate in vivo FRET-fluorescence lifetime imaging microscopy (FLIM) between the donor TSapphire and the acceptor mOrange. We show that TSapphire expressed in living plant cells decays with a monoexponential lifetime of 2.93 ± 0.09 ns, which is in agreement with the published lifetime for its parent wild-type GFP (3.2 ns; Striker et al., 1999; Volkmer et al., 2000). Furthermore, we demonstrate intramolecular FRET-FLIM between chimerically linked TSapphire and mOrange (with a 16-amino acid linker in between). When fused to genetically known interacting proteins and expressed in intact living cells, the donor and the acceptor fluorophores show energy transfer in different subcellular compartments indicative of intermolecular protein-protein interactions. These results validate the versatility of the proposed in vivo FRET-FLIM assay based on the donor TSapphire and the acceptor mOrange, which turns out to work with both soluble and membrane proteins.     

Quantitative fluorescence resonance energy transfer measurements using fluorescence microscopy.

Fluorescence resonance energy transfer (FRET) is a technique used for quantifying the distance between two molecules conjugated to different fluorophores. By combining optical microscopy with FRET it is possible to obtain quantitative temporal and spatial information about the binding and interaction of proteins, lipids, enzymes, DNA, and RNA in vivo. In conjunction with the recent development of a variety of mutant green fluorescent proteins (mtGFPs), FRET microscopy provides the potential to measure the interaction of intracellular molecular species in intact living cells where the donor and acceptor fluorophores are actually part of the molecules themselves. However, steady-state FRET microscopy measurements can suffer from several sources of distortion, which need to be corrected. These include direct excitation of the acceptor at the donor excitation wavelengths and the dependence of FRET on the concentration of acceptor. We present a simple method for the analysis of FRET data obtained with standard filter sets in a fluorescence microscope. This method is corrected for cross talk (any detection of donor fluorescence with the acceptor emission filter and any detection of acceptor fluorescence with the donor emission filter), and for the dependence of FRET on the concentrations of the donor and acceptor. Measurements of the interaction of the proteins Bcl-2 and Beclin (a recently identified Bcl-2 interacting protein located on chromosome 17q21), are shown to document the accuracy of this approach for correction of donor and acceptor concentrations, and cross talk between the different filter units.     

Cell surface detection of membrane protein interaction with homogeneous time-resolved fluorescence resonance energy transfer technology

Direct or indirect interactions between membrane proteins at the cell surface play a central role in numerous cell processes, including possible synergistic effects between different types of receptors. Here we describe a method and tools to analyze membrane protein-protein interaction at the surface of living cells. This technology is based on the use of specific antibodies directed against each partner and labeled either with europium cryptate or with Alexa Fluor 647. This allows the measurement of a fluorescence resonance energy transfer (FRET) signal in a time-resolved manner if both antibodies are in close proximity. This approach is here validated using the heterodimeric gamma-aminobutyrate B receptor as a model. We show that after washing out the unbound antibodies, the time-resolved FRET signal can be measured together with the expression level of both partners via the quantification of the donor and the acceptor fluorophores bound to the cells. Thanks to the high sensitivity of this method and to the low concentration of antibodies required, we show that the signal can also be measured directly after the incubation period without washing out the unbound antibody (homogeneous time-resolved FRET). As such, this method is highly sensitive, reproducible, and compatible with the development of high-throughput screening protocols.     

Protein localization in living cells and tissues using FRET and FLIM

Interacting proteins assemble into molecular machines that control cellular homeostasis in living cells. While the in vitro screening methods have the advantage of providing direct access to the genetic information encoding unknown protein partners, they do not allow direct access to interactions of these protein partners in their natural environment inside the living cell. Using wide-field, confocal, or two-photon (2p) fluorescence resonance energy transfer (FRET) microscopy, this information can be obtained from living cells and tissues with nanometer resolution. One of the important conditions for FRET to occur is the overlap of the emission spectrum of the donor with the absorption spectrum of the acceptor. As a result of spectral overlap, the FRET signal is always contaminated by donor emission into the acceptor channel and by the excitation of acceptor molecules by the donor excitation wavelength. Mathematical algorithms are required to correct the spectral bleed-through signal in wide-field, confocal, and two-photon FRET microscopy. In contrast, spectral bleed-through is not an issue in FRET/FLIM imaging because only the donor fluorophore lifetime is measured; also, fluorescence lifetime imaging microscopy (FLIM) measurements are independent of excitation intensity or fluorophore concentration. The combination of FRET and FLIM provides high spatial (nanometer) and temporal (nanosecond) resolution when compared to intensity-based FRET imaging. In this paper, we describe various FRET microscopy techniques and its application to protein-protein interactions.     

Fluorescence resonance energy transfer-based stoichiometry in living cells

Imaging of fluorescence resonance energy transfer (FRET) between fluorescently labeled molecules can measure the timing and location of intermolecular interactions inside living cells. Present microscopic methods measure FRET in arbitrary units, and cannot discriminate FRET efficiency and the fractions of donor and acceptor in complex. Here we describe a stoichiometric method that uses three microscopic fluorescence images to measure FRET efficiency, the relative concentrations of donor and acceptor, and the fractions of donor and acceptor in complex in living cells. FRET stoichiometry derives from the concept that specific donor-acceptor complexes will give rise to a characteristic FRET efficiency, which, if measured, can allow stoichiometric discrimination of interacting components. A first equation determines FRET efficiency and the fraction of acceptor molecules in complex with donor. A second equation determines the fraction of donor molecules in complex by estimating the donor fluorescence lost due to energy transfer. This eliminates the need for acceptor photobleaching to determine total donor concentrations and allows for repeated measurements from the same cell. A third equation obtains the ratio of total acceptor to total donor molecules. The theory and method were confirmed by microscopic measurements of fluorescence from cyan fluorescent protein (CFP), citrine, and linked CFP-Citrine fusion protein, in solutions and inside cells. Together, the methods derived from these equations allow sensitive, rapid, and repeatable detection of donor-, acceptor-, and donor-acceptor complex stoichiometry at each pixel in an image. By accurately imaging molecular interactions, FRET stoichiometry opens new areas for quantitative study of intracellular molecular networks.     

Development of a novel FRET immunosensor technique

We report on a novel technique to develop an optical immunosensor based on fluorescence resonance energy transfer (FRET). IgG antibodies were labeled with acceptor fluorophores while one of three carrier molecules (protein A, protein G, or F(ab')2 fragment) was labeled with donor fluorophores. The carrier molecule was incubated with the antibody to allow specific binding to the Fc portion. The labeled antibody-protein complex was then exposed to specific and nonspecific antigens, and experiments were designed to determine the 'in solution' response. The paper reports the results of three different donor-acceptor FRET pairs, fluorescein isothiocyanate/tetramethylrhodamine isothiocyanate, Texas Red/Cy5, and Alexa Fluor 546/Alexa Fluor 594. The effects of the fluorophore to protein conjugation ratio (F/P ratio) and acceptor to donor fluorophore ratios between the antibody and protein (A/D ratio) were examined. In the presence of specific antigens, the antibodies underwent a conformational change, resulting in an energy transfer from the donor to the acceptor fluorophore as measured by a change in fluorescence. The non-specific antigens elicited little or no changes. The Alexa Fluor FRET pair demonstrated the largest change in fluorescence, resulting in a 35% change. The F/P and A/D ratio will affect the efficiency of energy transfer, but there exists a suitable range of A/D and F/P ratios for the FRET pairs. The feasibility of the FRET immunosensor technique was established; however, it will be necessary to immobilize the complexes onto optical substrates so that consistent trends can be obtained that would allow calibration plots.     

The Impact of Heterogeneity and Dark Acceptor States on FRET: Implications for Using Fluorescent Protein Donors and Acceptors

Förster resonance energy transfer (FRET) microscopy is widely used to study protein interactions in living cells. Typically, spectral variants of the Green Fluorescent Protein (FPs) are incorporated into proteins expressed in cells, and FRET between donor and acceptor FPs is assayed. As appreciable FRET occurs only when donors and acceptors are within 10 nm of each other, the presence of FRET can be indicative of aggregation that may denote association of interacting species. By monitoring the excited-state (fluorescence) decay of the donor in the presence and absence of acceptors, dual-component decay analysis has been used to reveal the fraction of donors that are FRET positive (i.e., in aggregates)._However, control experiments using constructs containing both a donor and an acceptor FP on the same protein repeatedly indicate that a large fraction of these donors are FRET negative, thus rendering the interpretation of dual-component analysis for aggregates between separately donor-containing and acceptor-containing proteins problematic. Using Monte-Carlo simulations and analytical expressions, two possible sources for such anomalous behavior are explored: 1) conformational heterogeneity of the proteins, such that variations in the distance separating donor and acceptor FPs and/or their relative orientations persist on time-scales long in comparison with the excited-state lifetime, and 2) FP dark states.     

Time-gated in vivo autofluorescence imaging of dental caries.

Laser-induced time-resolved autofluorescence from carious lesions of human teeth was studied by means of ultrashort pulsed laser systems, time-correlated single photon counting and time-gated imaging. Carious regions exhibited a slower fluorescence decay with a main 17 ns fluorescence lifetime than healthy hard dental tissue. The long-lived fluorophore present in carious lesions only emits in the red spectral region. Fluorescence decay time and spectral characteristics are typical of fluorescent metal-free porphyrin monomers. The spatial distribution of the long-lived endogenous porphyrin fluorophore within the tooth material was detected by time-gated nanosecond autofluorescence imaging. In particular, high contrast video images were obtained with an appropriate time delay of 15 ns to 25 ns between excitation and detection due to the suppression of short-lived autofluorescence of healthy tissue. First in vivo applications are reported indicating the potential of time-resolved fluorescence diagnostics for early caries- and dental plaque detection.     

Structural information on nanomolecular systems revealed by FRET

Our newly developed fluorescence resonance energy transfer (FRET) based technique, fluorescence nanotomography (FN), is used to determine the morphology and dynamics of some soft materials and bio-molecules by attaching donor (D) fluorophores and acceptors (A) to the investigated structure and using fluorescence lifetime measurements to reveal the D-A distance distribution function rhoDA(r). We report the effect of the limited sizes of the donor and acceptor, effect of porous polymer, and molecular structure and phase transition in phospholipid bilayers.     

Multiplexed FRET to image multiple signaling events in live cells

We report what to our knowledge is a novel approach for simultaneous imaging of two different Förster resonance energy transfer (FRET) sensors in the same cell with minimal spectral cross talk. Previous methods based on spectral ratiometric imaging of the two FRET sensors have been limited by the availability of suitably bright acceptors for the second FRET pair and the spectral cross talk incurred when measuring in four spectral windows. In contrast to spectral ratiometric imaging, fluorescence lifetime imaging (FLIM) requires measurement of the donor fluorescence only and is independent of emission from the acceptor. By combining FLIM-FRET of the novel red-shifted TagRFP/mPlum FRET pair with spectral ratiometric imaging of an ECFP/Venus pair we were thus able to maximize the spectral separation between our chosen fluorophores while at the same time overcoming the low quantum yield of the far red acceptor mPlum. Using this technique, we could read out a TagRFP/mPlum intermolecular FRET sensor for reporting on small Ras GTP-ase activation in live cells after epidermal growth factor stimulation and an ECFP/Venus Cameleon FRET sensor for monitoring calcium transients within the same cells. The combination of spectral ratiometric imaging of ECFP/Venus and high-speed FLIM-FRET of TagRFP/mPlum can thus increase the spectral bandwidth available and provide robust imaging of multiple FRET sensors within the same cell. Furthermore, since FLIM does not require equal stoichiometries of donor and acceptor, this approach can be used to report on both unimolecular FRET biosensors and protein-protein interactions with the same cell.     

Fluorescence-based glucose sensors

There is an urgent need to develop technology for continuous in vivo glucose monitoring in subjects with diabetes mellitus. Problems with existing devices based on electrochemistry have encouraged alternative approaches to glucose sensing in recent years, and those based on fluorescence intensity and lifetime have special advantages, including sensitivity and the potential for non-invasive measurement when near-infrared light is used. Several receptors have been employed to detect glucose in fluorescence sensors, and these include the lectin concanavalin A (Con A), enzymes such as glucose oxidase, glucose dehydrogenase and hexokinase/glucokinase, bacterial glucose-binding protein, and boronic acid derivatives (which bind the diols of sugars). Techniques include measuring changes in fluorescence resonance energy transfer (FRET) between a fluorescent donor and an acceptor either within a protein which undergoes glucose-induced changes in conformation or because of competitive displacement; measurement of glucose-induced changes in intrinsic fluorescence of enzymes (e.g. due to tryptophan residues in hexokinase) or extrinsic fluorophores (e.g. using environmentally sensitive fluorophores to signal protein conformation). Non-invasive glucose monitoring can be accomplished by measurement of cell autofluorescence due to NAD(P)H, and fluorescent markers of mitochondrial metabolism can signal changes in extracellular glucose concentration. Here we review the principles of operation, context and current status of the various approaches to fluorescence-based glucose sensing.