Abstract
We present here the backbone and side-chain NMR assignments of YFP Venus, a 238-residue protein that emits yellow fluorescence in its native state. Venus is a variant of the green fluorescent protein (GFP), which has improved chromophore maturation and brightness, and the photochemistry and photophysics of which are insensitive to experimental conditions, such as the pH value and buffer content, making it a favourable biomarker.
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Biological context
The green fluorescent protein (GFP) from the jelly fish Aequorea Victoria is one of the most commonly used biomarkers used in biological research leading to the Nobel Prize in Chemistry 2008 (Shaner et al. 2007; Tsien 1998). It features the spontaneous formation of a chromophore that involves an auto-catalytic cyclisation and subsequent oxidation of the backbone of residues 65–67 without the need for enzymes or added cofactors. This makes GFP an ideal fusion tag for a myriad of applications, such as monitoring protein expression, localisation, and mapping interactions in vivo and in vitro by using the fluorescence of GFP as a reporter. GFP consists of 238 residues that fold into an 11-stranded β-barrel which wraps around the central α-helix—where the chromophore is located and buried in the hydrophobic core—to form a β-can structure. Over the last decade, an array of GFP variants has been identified from natural sources (primarily from marine animals) or engineered additionally by mutagenesis. By altering the side-chain composition of the chromophore itself, i.e., residues 65–67, as well as that of the surrounding residues, the reported GFP variants cover a broad spectrum of fluorescence excitation and emission wavelengths ranging from blue to red, which makes it most versatile for various applications. While the wild type GFP requires a few hours for the chromophore to mature and its spectral properties are highly sensitive to experimental conditions, e.g., pH and salt contents, a yellow fluorescent protein (YFP), Venus, has been developed to yield rapid chromophore maturation, higher quantum yield, and insensitivity to environmental changes (Nagai et al. 2002). These desirable properties of Venus have made it an ideal fluorescence probe in for FRET (Shimozono and Miyawaki 2008) and single molecule studies (Yu et al. 2006).
The usefulness of GFP variants as biomarkers relies on a robust folding capacity of these proteins. A structure-based rational design is a key factor in the further improvement of the folding properties as well as the photochemistry and photophysics of GFP variants (Jackson et al. 2006). While more than 100 crystal structures of GFP variants have been deposited in the Protein Data Bank to date, including that of Venus (Rekas et al. 2002), NMR assignment data are, at present, only available at the backbone level for a single GFP variant, GFPuv (Georgescu et al. 2003; Khan et al. 2003). The availability of backbone assignments renders the identification of highly stable structural elements in GFPuv at a residue-specific level under native and denaturing conditions (Huang et al. 2007). Dynamics studies of the structural perturbations in GFPuv resulting from point mutations have also been reported (Seifert et al. 2003). Moreover, a very recent report that employed 1D 1H NMR has identified intriguing indications of folding intermediate of a GFP variant by following the upfield shifted methyl proton resonances, although no side-chain assignments of GFP are currently available (Andrews et al. 2007).
We report here the backbone and side-chain 1H, 15N and 13C assignments of YFP Venus with an emphasis on the I/L/V side-chain methyl groups. These assignments, in particular of the side-chain reporters, should enable us to obtain structural insights at an atomic resolution to delineate the complex folding processes and the common features within the GFP family.
Methods and experiments
The gene encoding YFP Venus was a kind gift from Prof. Atsushi Miyawaki at the Brain Science Institute, RIKEN, Japan, and was sub-cloned into a pET21 vector with a hexahistidine tag at the N-terminus. 1H, 15N (>95%), 13C (>95%) and uniformly 2H (~70%), 15N (>95%), 13C (>95%) labelled protein was expressed in the E. coli strain BL21 (DE3) and purified using a Ni-column (Ni-NTA Superflow; Qiagen) followed by gel filtration chromatography (Superdex 75; GE). Selective 13C labelling, [U-15N, 13C-aa], was achieved by addition of 13C/15N (>98%; Spectral Isotope) labelled amino acids to 0.5 l of 15N-labelled minimal media (1 mM final concentration for each amino acid type) 20 min prior to IPTG induction. The cell cultures were harvested after 1.5 and 3 h of growth at 37°C; prolonged cell growth did not show significant scrambling of the supplemented amino acid types. Selective suppression of 15N labelling, [U-15N, \aa], was achieved by addition of unlabelled amino acids to 15N-labelled minimal media following the same protocol as that for selective 13C labelling. Six amino acid type-specific (un)labellings were made—[U-15N, 13C-I/F/V/L], [U-15N, 13C-V/L], [U-15N, 13C-F, \K], [U-15N, \M\K\I\L], [U-15N, \M\I] and [U-15N, \K\L]—to facilitate residue-specific backbone assignments by comparing the 15N–1H projections of corresponding HNCO and 13C coupled {15N–1H} TROSY spectra to identify the sequential (i − 1) and intraresidue correlations of the selectively (un)labelled amino acid types.
Purified protein was then concentrated to ca. 400 μM and buffer exchanged into Tris-HCl, HEPES, MES or phosphate buffers to yield sample pH pf 6.0, 6.6, 7.6, 8.0, 9.6, in the presence of 0.002% NaN3. For backbone assignments, TROSY versions of the triple resonance experiments (HNCA, HNCACB, intra-HNCACB, HNCO, HN(CA)CO) were recorded using a 2H(70%)/13C/15N labelled sample. Experiments were performed at 37°C on a Bruker Avance 700 MHz spectrometer equipped with a cryogenic triple resonance probe (Bruker BioSpin). The chemical shifts of individual spin systems (HN, N, Cα, Cβ and C′) collected manually and the backbone resonance assignments were achieved iteratively through a combination of computer-aided automated assignment using the programme MARS (Jung and Zweckstetter 2004) and visual inspections. For side-chain resonance assignments, 3D 1H–15N NOESY-HSQC, 3D 1H–13C NOESY-HSQC, 3D HcCH-COSY, 3D HcCH-TOCY and 3D hCCH-COSY spectra were recorded using the [U-15N, 13C-I/V/L] labelled sample, and HBHA(CO)NH were also recorded using the 2H(70%)/13C/15N labelled sample, and the resonances were assigned manually. All NMR data were processed and analysed by TopSpin (Bruker BioSpin), NMRPipe (Delaglio et al. 1995) and Sparky (Goddard and Kneller) software packages.
Extent of assignment and data deposition
An array of experimental conditions including pH values (ranging from 6.0 to 9.6; Fig. 1) and temperatures (ranging from 20 to 47°C; data not shown) have been tested to obtain an optimal condition for the assignment purpose based on the spectral quality and the number of observed crosspeaks in the {15N–1H} TROSY spectra. While some crosspeaks exhibit marked chemical shift changes and intensity changes under different conditions, the overall number of crosspeaks, however, is essentially the same throughout the wide range of tested conditions (Fig. 1). Overall, broader linewidths are observed at lower pH values and low temperatures (data not shown). In particular, the NMR sample of Venus begins to show visible signs of aggregation at pH 6.0, consistent with expectation of the loss of charges when close to the theoretical isoelectric point of 5.85, close to the pKa of the yellow fluorescence of Venus, 5.8, below which point the fluorescence intensity is lost rapidly (Rekas et al. 2002). The backbone assignment of Venus was therefore carried out using primarily data recorded at pH 7.6 and at 37°C; 3D HNCA, 3D HNCO and 3D 1H–15N NOESY-HSQC, recorded at pH 6.6 and at 37°C, were used to identify or confirm additional assignments. The condition used here is the closest to those under which Venus is used as a spectroscopic probe in vivo and therefore most useful for future structural studies associated with the in vivo data.
Following a standard sequential assignment procedure, 90% of all assignable 1HN–15N pairs (201 out of 224) and 86% of all 13C′, 13Cα and 13Cβ (592 out of 690) resonances of Venus have been assigned (Fig. 1). The relatively low level of assignment is in part due to the limited number of backbone amide crosspeaks available for the assignment; essentially all the resolved crosspeaks in the {15N–1H} TROSY spectrum observed across a wide range of pH and temperature values have been assigned. Structural mapping of the unassigned residues revealed a cluster encompassing parts of strands 3, 7, 8, 10 and 11 (Fig. 2a), forming a surface that largely overlaps with the dimer interface with which Venus self-associates in the crystalline state (Rekas et al. 2002) (Fig. 2b). Under NMR conditions, the hydrodynamic radius (Rh) derived through pulse field gradient diffusion measurements is ca. 6-fold larger than that of an immunoglobulin domain (14 kDa), while a factor of two is expected for a monomeric Venus in solution. The unexpectedly large Rh is in fact concentration-dependent, suggesting that Venus undergoes transient interactions in solution to form not only dimers but also higher order oligomers which contribute to the loss of resonances corresponding to the unassigned residues.
Note that triply labelled NMR samples (2H/13C/15N) with partial deuteration (~70%) were prepared to alleviate the relaxation loss due to the moderate size of Venus (27 kDa), leading to a prolonged 15N transverse relation time of 42.3 ± 5.9 ms, which is sufficiently long for most triple resonance experiments (unpublished data). The 70% partial deuteration was necessary in order to retain part of the highly protected amide groups whose hydrogen exchange rates are exceeding low even in the presence of chemical denaturants or strong acids, and the refolding of Venus is not efficient (some have half lives of several months; unpublished data). Perdeuteration that requires back-exchange for the amide protons through cycles of unfolding and refolding procedures is therefore not desirable.
Although similar in sequence compositions (differs in 10 out of 238 residues), significant differences can be found in the 2D {15N–1H} HSQC spectra of Venus and GFPuv (not shown). Comparison of the Cα chemical shifts of Venus with respect to the two sets of previously reported values of GFPuv, which report secondary structure contents, revealed systematic offsets. We therefore re-referenced the deposited assignments, BMRB entries 5144 (Georgescu et al. 2003) and 5666 (Khan et al. 2003), using the online server SHIFTCOR (http://redpoll.pharmacy.ualberta.ca/shiftcor/ (Zhang et al. 2003)), and corrections of 3.08 and −0.30 ppm, respectively, were carried out to yield two similar overall profiles of the secondary Cα chemical shifts of GFPuv that are in general agreement with that of Venus. The differences of secondary Cα chemical shifts between YFP and GFPuv, ΔΔδCα = Δδ YFPCα − Δδ GFPCα , are −0.26 ± 1.55 and 0.13 ± 1.17 ppm for BMRB entries 5144 and 5666, respectively (Fig. 3). The two assignments were obtained under very similar conditions, both in phosphate buffered saline (pH 7.0 for BMRB 5144 and pH 7.2 for BMRB 5666) and at 310 K. Close inspection into the differences between the two, however, revealed marked deviations for BMRB entry 5144 from those of Venus (determined at pH 7.4), particularly in loop regions connecting individual β-strands, suggesting some degrees of pH-dependent conformational rearrangements in GFP. Common in these two GFPuv assignments, in relation with the observed deviations from those of Venus, are the Cα shifts of T38, H169, E172, P192 and L194, all of which are conserved and are located in the loop regions. Overall, the deviations of Cα chemical shifts between GFPuv and Venus suggest that the solution structures of the two GFP variants are highly similar and that marginal conformational differences occur only in the loop regions.
In addition to the backbone assignments, we assigned nine out of 10 alanine side-chain methyl groups through a combination of HBHA(CO)NH and 3D 1H–15N NOESY-HSQC. Additionally, 82% (84 out of 102) of all side-chain methyl groups in Ile, Val and Leu (most of the unassigned resonances are located in the loop regions which exhibit severe spectral overlaps) were assigned using a [U-15N, 13C-I/F/V/L] labelled sample (Fig. 4). Future studies are underway to investigate in detail the structural and dynamical characteristics of these side-chain methyl groups. The assigned chemical shifts have been deposited in the BMRB under accession number 15826.
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Acknowledgments
STDH is a recipient of a Netherlands Ramsay and a Human Frontier Science Program Long-term Fellowship (LT0798/2005). CB is holding a Studienstiftung des Deutschen Volkes scholarship and is supported by the Erasmus/Sokrates program. LDC is a NH&MRC C.J. Martin Fellow. CMD acknowledges funding from the Wellcome and Leverhulme Trusts. We thank Prof. Atsushi Miyawaki for providing the DNA plasmid of Venus, Dr. John Christodoulou for helpful discussion, and the staff of the Biomolecular NMR Facility, Department of Chemistry, University of Cambridge. Financial support by the Access to Research Infrastructures activity in the 6th Framework Program of the EC (Contract # RII3-026145, EU-NMR) for conducting the research at CERM is gratefully acknowledged.
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Hsu, ST.D., Behrens, C., Cabrita, L.D. et al. 1H, 15N and 13C assignments of yellow fluorescent protein (YFP) Venus. Biomol NMR Assign 3, 67–72 (2009). https://doi.org/10.1007/s12104-009-9143-y
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DOI: https://doi.org/10.1007/s12104-009-9143-y