Hue-shifted monomeric variants of Clavulariacyan fluorescent protein: identification of the molecular determinants of color and applications in fluorescence imaging
© Ai et al; licensee BioMed Central Ltd. 2008
Received: 15 February 2008
Accepted: 06 March 2008
Published: 06 March 2008
In the 15 years that have passed since the cloning of Aequorea victoria green fluorescent protein (avGFP), the expanding set of fluorescent protein (FP) variants has become entrenched as an indispensable toolkit for cell biology research. One of the latest additions to the toolkit is monomeric teal FP (mTFP1), a bright and photostable FP derived from Clavularia cyan FP. To gain insight into the molecular basis for the blue-shifted fluorescence emission we undertook a mutagenesis-based study of residues in the immediate environment of the chromophore. We also employed site-directed and random mutagenesis in combination with library screening to create new hues of mTFP1-derived variants with wavelength-shifted excitation and emission spectra.
Our results demonstrate that the protein-chromophore interactions responsible for blue-shifting the absorbance and emission maxima of mTFP1 operate independently of the chromophore structure. This conclusion is supported by the observation that the Tyr67Trp and Tyr67His mutants of mTFP1 retain a blue-shifted fluorescence emission relative to their avGFP counterparts (that is, Tyr66Trp and Tyr66His). Based on previous work with close homologs, His197 and His163 are likely to be the residues with the greatest contribution towards blue-shifting the fluorescence emission. Indeed we have identified the substitutions His163Met and Thr73Ala that abolish or disrupt the interactions of these residues with the chromophore. The mTFP1-Thr73Ala/His163Met double mutant has an emission peak that is 23 nm red-shifted from that of mTFP1 itself. Directed evolution of this double mutant resulted in the development of mWasabi, a new green fluorescing protein that offers certain advantages over enhanced avGFP (EGFP). To assess the usefulness of mTFP1 and mWasabi in live cell imaging applications, we constructed and imaged more than 20 different fusion proteins.
Based on the results of our mutagenesis study, we conclude that the two histidine residues in close proximity to the chromophore are approximately equal determinants of the blue-shifted fluorescence emission of mTFP1. With respect to live cell imaging applications, the mTFP1-derived mWasabi should be particularly useful in two-color imaging in conjunction with a Sapphire-type variant or as a fluorescence resonance energy transfer acceptor with a blue FP donor. In all fusions attempted, both mTFP1 and mWasabi give patterns of fluorescent localization indistinguishable from that of well-established avGFP variants.
In 1992 the scientific community was gifted with a research tool that profoundly and irreversibly changed the way researchers approach the study of protein function in live cells . The tool was, of course, the gene encoding the Aequorea victoria green fluorescent protein (avGFP) . Soon after the first demonstrations of functional expression of the gene encoding avGFP in organisms other than jellyfish [3, 4], published reports of the use of fluorescent proteins (FPs) for microscopy applications 'took off' . Since that time, the impact of FPs on the life sciences has continued to increase with each passing year and this growth shows no signs of slowing . One important driving force behind the ever-increasing popularity of FPs is the fact that researchers continue to create FPs with wavelength-shifted absorbance and/or emission wavelengths and/or improved or novel properties (for example, increased brightness, improved photostability or photoactivation) [6, 7]. Improved FPs facilitate life science research by minimizing technical hurdles that otherwise complicate their use in imaging applications. For example, FPs with improved photostability enable time-lapse imaging over greater durations. FPs with novel properties can inspire the development of entirely new applications that would otherwise be impractical or even impossible. This has certainly been the case with photoactivatable FPs that have enabled cellular imaging at resolutions beyond the diffraction limit .
In this work we report on our efforts to engineer a series of new colors of mTFP1-derived FPs through the use of site-directed mutagenesis and random mutagenesis with library screening. This work has provided important insight into the amino acid determinants of color in mTFP1. In addition we have undertaken a thorough assessment of mTFP1 fusion proteins to determine whether such constructs exhibit their expected pattern of subcellular localization. Together these new results further establish mTFP1, and its suitably optimized hue-shifted variants, as useful new additions to the toolkit of FPs for cell biology research.
Results and discussion
Blue-shifted variants of mTFP1
A series of computational studies have provided support for the idea that there is a partial transfer of charge from the phenolate moiety to the imidazolinone moiety (Figure 1A) in the excited state of the avGFP anion [21, 22]. Since the phenolate is more electron rich in the ground state than in the excited state, factors that contribute to charge stabilization will tend to increase the energy barrier for charge transfer and shift the excitation and emission peaks to higher-energy wavelengths (that is, towards the blue). The crystal structures of mTFP1  and amFP486  (a tetrameric cyan-fluorescing FP from Anemonia majano) revealed that these homologous blue-shifted FPs both have structurally analogous histidine imidazoles, His197 of mTFP1 and His199 of amFP486, stacked against the phenolate ring of the chromophore (Figure 2A and 2B). Owing to the involvement of the imidazole in a quadrupole salt bridge network (with Glu148, Glu215 and Arg70 in mTFP1; Glu150, Glu217 and Arg72 in amFP486) it is likely to have significant cationic character. A simple electrostatic interpretation of the imidazole-chromophore interaction might therefore suggest that this cationic character is helping to stabilize anionic character on the phenolate ring. Other mutagenesis-based studies have provided support for the idea that the side chain of the residue aligning with residue His163 of mTFP1 (Figure 2A), or a buried water molecule that occupies the cavity when the side chain is small (as is the case of Ala165 in amFP486 as shown in Figure 2B), also has an important role in stabilizing anionic character on the phenolate ring . Henderson and Remington have proposed that the electrostatic interaction with His199 is of greater significance than the interaction with the water molecule in the residue 165 side-chain cavity for causing the blue-shifted emission of the amFP486 chromophore . The relative importance of His197 and His163 with respect to the blue-shift of the mTFP1 chromophore has not been investigated.
We reasoned that if this electrostatic-based mechanism for 'fine tuning' of the emission wavelength is indeed operative in mTFP1, variants with alternative chromophore structures, should also be blue-shifted relative to their avGFP analogs. Two qualifications are that formation of the excited state still involves charge transfer to the imidazolinone ring and that significant repacking of the side chains lining the chromophore-containing cavity does not occur with the new chromophore structure. To investigate whether this mechanism for blue-shifting the fluorescence could be translated to alternative chromophore structures, we created the Tyr67Trp and Tyr67His mutants of mTFP1. The chromophore structures of mTFP1-Y67W and mTFP1-Y67H are chemically identical to that of avGFP-derived ECFP and EBFP, respectively (Figures 1B and 1C). Accordingly, we expected that the absorbance and fluorescence emission maxima of mTFP1-Y67W and ECFP (and mTFP1-Y67H and enhanced blue FP (EBFP)) would be similar but not necessarily identical. If differences between the spectra of the two proteins were observed, they must be attributable to the effect of the protein environment on the chromophore.
Measuring the absorbance and emission spectra of purified mTFP1-Y67W revealed that this protein is fluorescent, exhibits the typical double-humped peaks associated with a tryptophan-derived chromophore and is blue-shifted relative to ECFP (Figure 3B). Considering the mean wavelength at half maximum intensity, the excitation and emission peaks are shifted by 13 and 13.5 nm, respectively. This result contrasts with a previous report in which it was demonstrated that the analogous substitution in amFP486 results in a protein that is not blue-shifted relative to avGFP-derived CFP . The purified mTFP1-Y67H variant exhibited no significant fluorescence, but did have a strong absorbance peak that was blue-shifted by 10.5 nm (mean wavelength at half maximum intensity relative to avGFP-derived EBFP (Figure 3C).
These results demonstrate that the protein-chromophore interactions responsible for blue shifting the absorbance and emission maxima (that is raising the energy of the excited state) of mTFP1 are not entirely dependent on the presence of a tyrosine-derived chromophore. In the crystal structure of mTFP1, the imidazole of His163 is observed to be making a hydrogen bond with the phenolate oxygen of the chromophore (Figure 2A). An analogous interaction is not possible in the mTFP1-Y67H or mTFP1-Y67W variants. In contrast, the close stacking of the His197 imidazole against the chromophore phenolate is an interaction that could be preserved in the mTFP1-Y67W or mTFP1-Y67H variants. We conclude that the hydrogen bond with His163 is not significant with respect to the blue-shift of mTFP1 and it is either the close stacking of the His197 imidazole and/or a hydrogen bond-independent electrostatic effect of His163 that is responsible for the blue-shift. Based on the interaction of His163 with the carboxylate of Asp144 (Figure 2A), it is plausible that the imidazole could have significant cationic character.
Red shifted variants of mTFP1
Properties of hue-shifted mTFP1 variants
Excitation maximum (nm)
Emission maximum (nm)
Brightnessa (mM-1 cm-1)
So is His163 solely responsible for the blue-shift of mTFP1 or does His197 also play a role? That is, does the emission maximum of 503 nm for mTFP1-H163M represent an appropriate 'reference' state for this particular chromophore structure when located in this particular chromophore cavity and in the complete absence of any blue-shifting effects? Previous work suggests that the answer to the latter question is probably no, and the emission maximum of the reference state is more likely to be approximately 515 nm. One piece of evidence supporting this suggestion is that the emission maximum of amFP486-H199T is 515 nm . This variant has essentially an identical chromophore cavity to mTFP1, with the obvious exception of the His199Thr replacement. The second piece of evidence in support of this suggestion is that the avGFP-T203H mutant has a fluorescence emission at 517 nm when excited at 475 nm (see ). Residue Thr203 of avGFP  is structurally aligned with His197 of mTFP1 (compare Figures 2A and 2C), and thus avGFP-T203H likely has an imidazole-chromophore stacking interaction similar to that of mTFP1 . However, unlike the positively charged imidazole of His197 in mTFP1, the imidazole of His203 in avGFP-T203H is expected to be in the neutral-charge state.
In a later section we describe the discovery of the Thr73Ala substitution that red-shifted the fluorescence of mTFP1-K139E/H163M from 503 to 515 nm. However, it is appropriate to discuss the implications of this fortunate finding in the current context. In the crystal structure of mTFP1, the hydroxyl group of Thr73 is hydrogen-bonded to the guanidium group of Arg70: a key participant of the quadrupole salt-bridge network responsible for maintaining the imidazole of His197 in the positively charged state (Figure 2A). We propose that the loss of the Thr73-Arg70 hydrogen bond in the Thr73Ala mutant perturbs the salt-bridge network such that the cationic character of His197 imidazole is greatly diminished or abolished. Accordingly, the Thr73Ala mutant effectively separates the electrostatic role of His197 from its additional roles in maintaining the chromophore environment and reveals that the electrostatic effect of this residue accounts for a blue-shift of at least 12 nm.
Our mutagenesis-based study supports the conclusion that His163 and His197 act in concert to blue-shift the fluorescence emission of the mTFP1 chromophore through an electrostatic mechanism. The contribution of both residues is effectively identical with 11 and 12 nm of blue-shift attributed to His163 and His197, respectively. This result is essentially consistent with previous studies of amFP486 which have suggested complementary roles for His199 and the water molecule adjacent to Ala165 in achieving the blue-shift [20, 23]. The crystallographic and mutational study by Henderson and Remington supports the conclusion that the water molecule adjacent to Ala165 has a less significant contribution than His199 . In mTFP1 the (plausibly) cationic imidazole group of His163 could contribute a significant amount of electrostatic stabilization to electron density on the phenolate ring. A similar interaction is not possible in amFP486 since a lone water molecule sits in the location occupied by the His163 imidazole of mTFP1. A caveat is that the electron density modeled as a water in the amFP486 structure could actually be a sodium ion or other cation (S J Remington, personal communication), in which case an electrostatic contribution would not be unreasonable.
Directed evolution of the red shifted variant of mTFP1
Intrigued by the high apparent fluorescent brightness of mTFP1-H163M (hereafter designated G1), we subjected this template to directed evolution in an effort create a new GFP variant that could potentially be useful for live cell imaging. Error-prone polymerase chain reaction (PCR) was used to create libraries of genetic variants, the gene libraries were expressed in Escherichia coli, and colonies were screened for bright green fluorescence. The brightest green fluorescent colony identified in the first round of screening was found to express a G1 variant with the additional mutation Lys139Met (designated G2). This variant was used as the template for a second round of library construction and screening. The brightest variant identified in the second round was found to be mTFP1-T73A/K139M/H163M (designated G3). It is interesting to note that the Thr73Ala mutation present in G3 is structurally aligned with the Ser72Ala mutation that has been reported to improve the brightness of avGFP variants . No further improvements were identified during a third round of screening of randomly mutated variants based on the G3 template. In vitro characterization (Table 1) of the purified green fluorescing variants revealed that relative fluorescent brightness to be 1, 1.5 and 1.9 for G1, G2 and G3, respectively. While both G1 and G2 had fluorescence maxima at 503 nm, G3 was further red-shifted to 515 nm. The implications of this result have been discussed above.
Further investigation of the G2 and G3 variants revealed that the dimmer G2 was 11.8-fold more photostable than the brighter G3 variant. In our experience mutations that improve fluorescent brightness are much more readily identified than mutants that improve photostability. For this reason we forsook the brighter G3 variant and continued optimization based on the G2 template. Saturation mutagenesis at three positions chosen based on their proximity to the chromophore (Ala66, Val161 and Ile199) resulted in the identification of a further improved variant containing the Ala66Ser substitution. A subsequent round of random mutagenesis resulted in the identification of the Ser216Ile substitution. Additional rounds of random mutagenesis yielded no further improvements. The end product of this process is a brightly fluorescent GFP (emission maximum = 509 nm) that is equivalent to mTFP1-A66S/K139E/H163M/S216I and has been designated mWasabi. The fluorescence emission maximum of mWasabi is intermediate between that of G1 and G3, suggesting that there has been a perturbation of the salt-bridge network. It has been previously reported that avGFP with a Ser at residue 65 is 5 nm red-shifted from avGFP with an Ala at residue 65 (see ). As observed in the avGFP-S65T structure (Figure 2C), the hydroxyl group of the Ser at residue 66 of mWasabi could potentially form a new hydrogen bond with Glu215 and partially disrupt its ability to contribute to the critical salt-bridge network.
In vitro characterization of mWasabi (Table 1) revealed that it is 1.6-fold brighter than EGFP, making it one of the brightest and most photostable FPs currently available . Another notable feature of mWasabi is its very narrow excitation and emission peaks (Figure 3D) that are reminiscent of the spectrum of Renilla GFP  and monomeric Azami-Green . Narrower peaks allow for more efficient excitation and gathering of emission when used in combination with bandpass filters, and reduce the degree of bleed-through in multicolor imaging.
Two-color imaging with mWasabi and Sapphire
Imaging of mTFP1 and mWasabi fusion proteins
Both mTFP1 and its green-emitting progeny, mWasabi, are the products of an extensive process of protein engineering and directed evolution. During the development of these proteins, substantial effort was expended to find variants with the desired color, high fluorescent brightness, high folding and maturation efficiency and high photostability. Our in vitro characterization of these proteins confirms that we were indeed successful in engineering proteins with the desired properties. However, the ultimate goal of this research is not to simply develop new FPs, but rather to develop FPs that will be useful tools for fluorescence imaging in living cells. To be generally useful for live cell imaging, a FP should retain its favorable properties either when fused to a variety of proteins or when targeted to a variety of subcellular compartments. In addition, the FP should not perturb the normal localization or biological function of the protein to which it is genetically fused. Such a perturbation can be caused by oligomerization of the FP: a problem that should not be relevant to monomeric FPs such as mTFP1 and mWasabi.
In this manuscript we have described a series of mutagenesis experiments that have provided fundamental insight into the amino acids that dictate the color of the mTFP1 chromophore. Our data supports the conclusion that His163 and His197 act in an independent and additive fashion to increase the energy of the electronic transitions responsible for absorbance and fluorescence. Although determining the precise details of the mechanism are beyond the scope of this paper, our results are consistent with a previous proposal that electrostatic stabilization of charge density on the phenolate ring is a general means of achieving blue-shifted emission in FPs .
Our investigations into the amino acid determinants of the color of mTFP1 led us to a series of hue-shifted variants, one of which was subjected to further engineering and directed evolution to eventually produce mWasabi. While mWasabi is an exceptionally bright and reasonably photostable GFP, we readily acknowledge that for most experiments EGFP or Emerald should remain the GFP of choice. However, there are a number of specific applications, such as two-color imaging in conjunction with a Sapphire-type variant or as a FRET acceptor with a BFP donor, where the negligible excitation of mWasabi at 400 nm provides a substantial benefit. Both mTFP1 and mWasabi are well behaved in protein chimeras, offering a bright and photostable fluorescent signal with no significant perturbation of the localization or function of the protein of interest. This combination of desirable features firmly establishes mTFP1 and mWasabi as useful members of the FP toolkit.
Synthetic DNA oligonucleotides for cloning and library construction were purchased from Integrated DNA Technologies (Coralville, IA). PCR products and products of restriction digests were purified by gel electrophoresis and extraction using either the GenCatch™ gel extraction kit (Epoch Biolabs, TX) or the QIAquick™ gel extraction kit (QIAGEN, Valencia, CA). Plasmid DNA was purified from overnight cultures by using either the GeneJET™ Plasmid Miniprep Kit (Fermentas, ON) or the QIAprep Spin Miniprep kit (QIAGEN, Valencia, CA). Restriction endonucleases were purchased from either Invitrogen or New England Biolabs. Dye terminator cycle sequencing using the DYEnamic ET kit (Amersham Biosciences) was used to confirm the complete cDNA sequences for all FP variants and fusion constructs. Sequencing reactions were analyzed at the University of Alberta Molecular Biology Service Unit and the Florida State University Bioanalytical and Molecular Cloning DNA Sequencing Laboratory. All filters for fluorescence screening and imaging were purchased from Chroma Technology (Rockingham, VT), Omega Filters (Brattleboro, VT) and Semrock (Rochester, NY). The nucleotide sequence of mWasabi has been deposited in the GenBank® nucleotide sequence database under accession number EU024648.
Mutagenesis and library construction
Mutagenesis was performed by overlap PCR or error-prone PCR as described previously . The PCR products were digested with Xho1 and EcoR1 and ligated into pBAD/His B vector digested with the same two enzymes (Invitrogen). The crude ligation mixture was used to transform electrocompetent E. coli strain DH10B (Invitrogen) which were then plated on Luria-Bertani (LB)/agar plates supplemented with ampicillin (0.1 mg/ml) and l-arabinose (0.02%). Plates were incubated for 14 h at 37°C prior to picking individual colonies (in the case of site-directed mutagenesis for creation of blue shifted variants) or fluorescence-based library screening for red shifted variants.
The screening system has been described previously  and is only described here in brief. The light from a 175 W xenon-arc lamp (Sutter) was passed through a bandpass filter selecting for 460–490 nm light. The light passed into a bifurcated fiber optic bundle (Newport) positioned to illuminate a Petri dish harboring bacterial colonies. The fluorescence emission of the colonies was screened by eye using tinted plastic goggles that block light with a wavelength of less than 500 nm. Colonies with more intense fluorescence were picked for further investigation. Colonies of interest were cultured overnight in 4 ml LB medium containing ampicillin (0.1 mg/ml) and l-arabinose (0.2%). The following day 0.1 ml of each culture was dispensed into individual wells of a clear bottom 96-well plate (Nunc) and the full emission spectra of each variant measured with a Safire2 plate reader equipped with monochromators (Tecan). Variants with the most intense and red-shifted fluorescence emission were used as templates in the subsequent round of library construction.
Protein purification and characterization
For production of protein, E. coli strain LMG194 was transformed with the pBAD/His B expression vector containing the FP gene of interest. A single colony was used to inoculate a 4 ml culture that was allowed to grow overnight (37°C, 225 rpm) before being diluted into 1 l of LB medium supplemented with ampicillin and l-arabinose. The culture was grown for 12 h before cells were harvested by centrifugation and lysed by French Press. Proteins were purified by Ni-NTA chromatography (Amersham). Absorption spectra were recorded on a DU-800 UV-visible spectrophotometer (Beckman) and fluorescence excitation and emission spectra were recorded on a Safire2 plate reader. Reference standards for determining the quantum yields of BFP or GFP variants were quinine sulfate in 0.1 M H2SO4 or EGFP, respectively. Extinction coefficients were calculated using the protein concentration as determined by the bicinchoninic acid (BCA) method (Pierce) and the chromophore absorbance as determined by UV-visible spectroscopy. For fluorescence pKa measurements, the protein of interest was first dialyzed into dilute buffer (5 mM Tris HCl, pH 7.5) before being diluted into a series of 200 mM phosphate and imidazole buffers at various pH values. Fluorescence intensity was measured using a Safire2 plate reader.
For photostability measurements of green-fluorescing variants, microdroplets of either the purified protein (100 μM) or E. coli culture (previously transformed with the expression plasmid and induced) was mixed with mineral oil and vortexed. Approximately 5 μl of this suspension was sandwiched between a glass slide and a glass cover slip. Individual drops were identified by fluorescence microscopy and subjected to photobleaching as previously described . For all experiments, EGFP was subjected to bleaching under identical conditions and used as a reference standard.
Mammalian expression vectors
To create the Sapphire-actin and mWasabi-NLS vectors, the genes encoding Sapphire (also known as H9-40) [2, 13, 33] and mWasabi were PCR amplified with a 5' primer encoding an NheI site and a 3' primer encoding an XhoI site. The purified and digested PCR products were ligated into pEGFP-actin or pEYFP-Nucleus (Clontech), respectively, which had been previously digested with the same restriction enzymes to excise the FP coding sequence. An analogous nuclear localization construct was made for EGFP. All of the other mTFP1 and mWasabi vectors were constructed using C1 and N1 (Clontech-style) cloning vectors. The FPs were amplified with a 5' primer encoding an AgeI site and a 3' primer encoding either a BspEI (C1) or Not1 (N1) site. The purified and digested PCR products were ligated into similarly digested EGFP-C1 and EGFP-N1 cloning vector backbones. To generate fusion vectors, the appropriate cloning vector and an EGFP fusion vector were digested, either sequentially or doubly, with the appropriate enzymes and ligated together after gel purification. Thus, to prepare mTFP1 and mWasabi N-terminal fusions, the following digests were performed: human non-muscle α-actinin, EcoRI and NotI (vector source, Tom Keller, FSU); human cytochrome C oxidase subunit VIII, BamHI and NotI (mitochondria, Clontech); human zyxin, BamHI and NotI (Clare Waterman-Storer, NIH); rat α-1 connexin-43 and rat β-2 connexin-26, EcoRI and BamHI (Matthias Falk, Lehigh University); human H2B, BamHI and NotI (George Patterson, NIH); N-terminal 81 amino acids of human β-1,4-galactosyltransferase, BamHI and NotI (Golgi, Clontech); human microtubule-associated protein EB3, BamHI and NotI (Lynne Cassimeris, Lehigh University); human vimentin, BamHI and NotI (Robert Goldman, Northwestern University); human keratin 18, EcoRI and NotI (Open Biosystems, Huntsville, AL); chicken paxillin, EcoRI and NotI (Alan Horwitz, University of Virginia); rat lysosomal membrane glycoprotein 1, AgeI and NheI (George Patterson, NIH); endoplasmic reticulum (calreticulin signal sequence and KDEL retention sequence), AgeI and EcoRI (Clontech). To prepare mTFP1 and mWasabi C-terminal fusions, the following digests were performed: human β-actin, NheI and BglII (Clontech); human α-tubulin, NheI and BglII (Clontech); human light chain clathrin, NheI and BglII (George Patterson, NIH); human lamin B1, NheI and BglII (George Patterson, NIH); human fibrillarin, AgeI and BglII (Evrogen); human vinculin, NheI and EcoRI (Open Biosystems, Huntsville, AL); peroximal targeting signal 1 (PTS1 – peroxisomes), AgeI and BspEI (Clontech); chicken protein tyrosine kinase 2, AgeI and BglII (Clare Waterman-Storer, NIH); human annexin (A4), AgeI and BspEI (Alen Piljic, EMBL, Heidelberg); human RhoB GTPase with an N-terminal c-Myc epitope tag (endosomes), AgeI and BspEI (Clontech); and the 20-amino acid farnesylation signal from c-Ha-Ras, AgeI and BspEI (membrane, Clontech). DNA for mammalian transfection was prepared by either the Plasmid Midi or Maxi kit (QIAGEN).
Live cell imaging
HeLa epithelial (CCL-2, ATCC) and gray fox lung fibroblast (CCL-168, ATCC) cells were either cultured and transfected as described previously , or grown in a 50:50 mixture of DMEM and Ham's F12 with 12.5% Cosmic calf serum (Hyclone) and transfected with Effectene (QIAGEN). For dual-color imaging, the two expression plasmids were pre-mixed in a 1:1 ratio before transfection. Widefield live cell imaging was performed with a Zeiss Axiovert 200 M microscope equipped with appropriate filter sets (Chroma), a Nikon TE-2000 inverted microscope equipped with Omega filters, or an Olympus IX71 equipped with Semrock filters. Laser scanning confocal microscopy was conducted on a Nikon C1Si and an Olympus FV1000, both equipped with argon-ion 457 and 488 nm lasers and proprietary filter sets. Spinning disk confocal microscopy was performed on an Olympus DSU-IX81 equipped with a Lumen 200 illuminator (Prior, Boston, MA), Semrock filters, and 10-position filter wheels driven by a Lambda 10-3 controller (Sutter, Novato, CA).
Sapphire fluorescence was measured using a 375–415 nm bandpass excitation filter, a 475 nm longpass beamsplitter, and 500–550 nm bandpass emission filters. mTFP1 was imaged with a CFP filter set (96188, Nikon) or a custom set composed of a 430–460 nm bandpass excitation filter, a 475 nm longpass beamsplitter, and a 480–520 nm bandpass emission filter. EGFP and mWasabi were imaged using either a standard EGFP filter set (41017, Chroma), a QuantaMaxTM Green set (Omega), or a BrightLine GFP set (3035B, Semrock).
Aequorea victoria GFP
fluorescence resonance energy transfer
monomeric teal FP
nuclear localization signal
polymerase chain reaction
This research was made possible with financial support from the University of Alberta, CFI, NSERC and Alberta Ingenuity. PW was supported by an NSERC USRA. The authors are grateful to Aillette Sierra Mulet, Kristin Hazelwood, Anna Ozarowska, John D Griffin and Christopher Murphy for technical assistance, S James Remington and J Nathan Henderson for helpful discussion and the University of Alberta MBSU for analysis of DNA sequencing reactions. REC holds a Canada Research Chair in Bioanalytical Chemistry. New fluorescent proteins that originate from the Campbell lab and are described in this manuscript are covered by a US patent application owned by the University of Alberta.
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