Abstract
The importance of modified peptides and proteins for applications in drug discovery, and for illuminating biological processes at the molecular level, is fueling a demand for efficient methods that facilitate the precise modification of these biomolecules. Herein, we describe the development of a photocatalytic method for the rapid and efficient dimerization and site-specific functionalization of peptide and protein diselenides. This methodology, dubbed the photocatalytic diselenide contraction, involves irradiation at 450 nm in the presence of an iridium photocatalyst and a phosphine and results in rapid and clean conversion of diselenides to reductively stable selenoethers. A mechanism for this photocatalytic transformation is proposed, which is supported by photoluminescence spectroscopy and density functional theory calculations. The utility of the photocatalytic diselenide contraction transformation is highlighted through the dimerization of selenopeptides, and by the generation of two families of protein conjugates via the site-selective modification of calmodulin containing the 21st amino acid selenocysteine, and the C-terminal modification of a ubiquitin diselenide.
Introduction
Proteins bearing post-translational modifications (PTMs) or designer modifications, such as fluorescent tags, affinity handles and polyethylene glycol (PEG) moieties at pre-determined positions, have emerged as powerful tools to investigate key biological processes and for applications in drug discovery (e.g., for the development of biologics)1,2,3,4,5,6,7. Overexpression in bacterial hosts such as Escherichia coli is the cornerstone of recombinant protein production, however, these systems generally lack the enzymatic machinery capable of introducing complex eukaryotic PTMs. While modified proteins can be produced in E. coli by unnatural amino acid incorporation using genetic code expansion and reprogramming, e.g., amber codon (UAG) suppression technologies8,9,10, the diversity of amino acids that can be installed is largely limited to analogues of tyrosine (Tyr) and lysine (Lys) bearing small modifications to the side chains. In addition, large scale protein production with these methods can be challenging11. Insect or mammalian cell expression systems can instead be used to generate proteins containing native PTMs, however, these modifications are generally present as complex inseparable heterogeneous mixtures12, thus preventing meaningful study of the functional influence of a single PTM structure at a specific site on a protein. An alternative approach to generate homogeneously modified proteins is through synthetic or semi-synthetic means by leveraging peptide ligation chemistry13,14,15,16,17,18,19,20. While synthesis offers unparalleled and exquisite control over the chemical identity of the protein and the locations of modifications (both natural and unnatural), access to larger protein targets, especially via total chemical synthesis, remains a very challenging and labor-intensive task20.
The late-stage functionalization of recombinant proteins has also emerged as a powerful approach to access site-specifically modified proteins2,3,21,22. The most widely employed methods for protein conjugation (and dimerization) rely on the reaction of the nucleophilic side chains of cysteine (Cys) and Lys residues with electrophilic maleimides6 and N-hydroxysuccinimidyl esters3, respectively. Despite the widespread use of these methods for the generation of bioconjugates, including a number of clinically approved biologics, the lack of regioselectivity of these chemistries means that, outside a handful of examples employing non-generalizable pH or surface exposure control23,24, isoxazolinium reagents25 or the use of engineered selectivity-inducing sequence motifs (e.g., π-clamp)26, they cannot usually be employed for the generation of homogeneous and site-specifically modified proteins27. To overcome the drawbacks of the above reaction manifolds, new synthetic methods have been developed for the late-stage functionalization of a specific amino acid side chain within proteins, albeit with varying degrees of chemoselectivity3,22. For example, cysteine (Cys) has been functionalized using a broad array of chemistries, including but not limited to the reaction with thiosulfonates28,29,30, hypervalent iodine reagents31,32,33, alkynyl phosphonoamidates34, strained cyclic systems35, desulfurative radical addition chemistry36, and transition-metal catalyzed arylation chemistry37,38,39,40. Indirect functionalization of Cys has also been performed through elimination of the sulfhydryl side chain to form dehydroalanine, with subsequent elaboration by radical or Michael addition41,42,43. Late-stage functionalization chemistries have also been developed for other proteinogenic amino acid side chains, including, but not limited to methionine (Met) using sulfur-imidation by oxaziridines44, hypervalent iodine reagents45 or photoredox catalysis46, serine (Ser) with phosphorous(V) reagents47 and Tyr using photocatalytic methods48,49,50,51. While each of these methods possesses exquisite chemoselectivity, all suffer from a lack of regioselectivity that arises from targeting amino acids that can occur at multiple positions within a protein sequence. It should be noted that methods have been developed for the regioselective functionalization of the N- or C-terminus of proteins under a variety of different reaction manifolds52,53,54,55,56,57,58.
Collectively, the methods outlined above provide the research community with a plethora of tools for protein modification, however, chemistry that facilitates the truly regioselective modification of proteins at any site of a protein (in addition to the termini) would be a transformative advance for the field. A number of powerful bioorthogonal chemistries59 (e.g., the Huisgen-type azide-alkyne cycloaddition4,60,61, inverse demand Diels Alder chemistry62,63 and the Staudinger reaction64,65) fit this desirable profile by providing absolute control over the site of modification. This is a result of the unique bioorthogonal functional handles employed in these reactions (e.g., azides, alkynes/cyclooctynes, tetrazines, phosphines, etc.) that exhibit minimal or no cross-reactivity with the functionalities found within the 21 proteinogenic amino acids. While some of these reactions can suffer from sluggish kinetics, and in most cases leave a large non-natural scar between the peptide backbone and the target modification, these methods have revolutionized the site-specific labeling of proteins, including within live cells3,59.
Selenocysteine (Sec; U) is commonly referred to as the 21st proteinogenic amino acid and is known to be incorporated into at least 25 discrete selenoproteins in humans66. The unique reactivity of the selenol side chain of Sec, namely its low pKa and high oxidation potential and nucleophilicity relative to Cys, has led to significant interest in leveraging the amino acid for a number of applications in protein science67,68. While Sec has been used for bioconjugation applications, the methods developed to date have centered primarily on alkylation or arylation chemistries which often possess modest chemoselectivity over other nucleophilic side chains (e.g., Cys, Lys), poor kinetics/conversions, and/or use non-biocompatible reaction conditions38,69,70,71,72,73. Nonetheless, given that Sec is a native, yet exceptionally rare amino acid in the proteome, it remains a highly attractive candidate for serving as a linchpin for new protein modification methods with exquisite chemo- and regioselectivity, akin to the powerful biorthogonal chemistries at non-native functionalities highlighted above.
Herein, we describe the development of a photocatalytic method for the rapid and high yielding dimerization and site-specific functionalization of peptides and proteins that capitalizes on unique reactivity at Sec. Specifically, we demonstrate that in the presence of an iridium photocatalyst, a phosphine and blue LED irradiation (λ = 450 nm), peptide and protein diselenides can be cleanly converted to reductively stable selenoethers with the formal extrusion of a single selenium atom. We propose a mechanism for this interesting photocatalytic transformation which is supported by time-resolved photoluminescence (PL) spectroscopy, cyclic voltammetry, as well as comprehensive computational studies. The power of this reaction—called the photocatalytic diselenide contraction (PDC) reaction—is highlighted through the dimerization of several synthetic selenopeptides, and by the site-selective functionalization of recombinantly expressed proteins bearing a diselenide motif.
Results and discussion
Serendipitous discovery of the photocatalytic diselenide contraction (PDC) reaction
In our efforts to develop methods for chemical protein synthesis, we attempted to perform photocatalytic deselenization of Sec on model peptide [H2N-USPGYS-NH2]2 (1) to alanine (Ala) in H2N-ASPGYS-NH2 (2) using Eosin Y as the photocatalyst, the phosphine tris-carboxyethylphosphine (TCEP) and 450 nm blue LED light. Unexpectedly, under these conditions we observed the formation of dimeric selenoether-bridged peptide 3 as a minor side product (Supplementary Figs. 1–3). Intriguingly, generation of selenoether dimer 3 corresponds to the formal extrusion of a single selenium atom from diselenide 1. While there have been early examples that have shown phosphine-mediated disulfide and benzylic diselenide contraction in refluxing benzene or extended UV irradiation74,75, to our knowledge this represents an unprecedented photocatalytic reaction at Sec. Given the potential value of dimerizing selenopeptides to reductively stable selenoether-linked dimeric peptides, together with the lack of precedent for this reaction under mild photocatalytic conditions, we sought to optimize conditions for the preferential formation of selenoether dimer 3 over the deselenization product 2. Gratifyingly, following optimization studies on model peptide 1, we found that treatment with 4 equivalents of the phosphine 1,3,5-triaza-7-phosphaadamantane (PTA) (4), and 1 mol% of the iridium photocatalyst [Ir(dF(CF3)ppy)2(dtbpy)]PF6 (5) with LED irradiation at 450 nm for 1 min, led to exclusive formation of the dimeric selenoether 3, which could be isolated in 76% yield following reverse-phase HPLC purification (Fig. 1A, Supplementary Figs. 4–13, Supplementary Tables 1–4). Importantly, in the absence of phosphine, photocatalyst, or without 450 nm irradiation, no formation of 3 was observed (Supplementary Figs. 14–16). After verifying the identity of selenoether 3 by HRMS (Supplementary Figs. 17–20), we also confirmed the retention of stereochemical integrity at the Cα-center of the Sec residue following PDC by 1H and 77Se NMR spectroscopy (Supplementary Figs. 21–23), suggesting a reaction pathway that is mechanistically distinct to the two electron elimination-addition pathway through dehydroalanine41,42, including the phosphine-mediated disulfide contraction chemistry for the formation of thioether conjugates reported by Davis and co-workers43. Notably, the selenoether linkage of 3 was shown to be completely stable to a range of basic, acidic, and biologically relevant reducing conditions, as well as human plasma, as confirmed by analytical HPLC and mass spectrometry (Supplementary Figs. 24–26). Taken together, these experiments provide clear evidence that each of the components are essential for the transformation, and that the reaction likely proceeds through a distinct photocatalytic manifold which we have termed the photocatalytic diselenide contraction (PDC). Furthermore, the demonstrated stability of the resultant selenoether functionality opens the possibility of implementing the PDC reaction for the generation of high value conjugates with therapeutic potential.
A Optimization of the PDC dimerization reaction on [H2N-USPGYS-NH2]2 model peptide 1. Site-specific PDC dimerization of B Gephyrin Binding Peptide 3a diselenide 9; C Prostate-Specific Membrane Antigen (PSMA) Binding Peptide diselenide 10; D CXCL1451-77 diselenide 11 to afford the reductively stable selenoether-linked peptide dimers 6–8. Analytical HPLC and ESI-MS of the purified selenoether products data are inset. E Observation of selanylphosphonium 14 when CaM (K148U) diselenide 12 was submitted to optimized PDC conditions. HRMS data inset showing [M + 10H+]10+ ions of the deselenized CaM (A148) (13) as the major product together with selanylphosphonium adduct 14. PTA = 1,3,5-triaza-7-phosphaadamantane, MeCN acetonitrile, AU absorbance units. Created with BioRender.com.
Site-specific dimerization of selenopeptides via PDC
With optimized conditions for the PDC transformation in hand, we next sought to demonstrate the utility of the methodology for the rapid and efficient generation of three selenoether-linked homo-dimeric target peptides that are known to exhibit improved activity in dimeric form; these included gephyrin-binding peptide 3a76 (GBP3a) (6), prostate-specific membrane antigen binding peptide77 (PSMABP) (7) and a peptide derived from the C-terminal region of the CXC chemokine ligand 14, CXCL1451-77 (8)78. Following synthesis of the diselenide dimer peptides 9–11 by solid-phase peptide synthesis (Supplementary Figs. 27–29), each was subjected to the optimized PDC conditions (vide supra) and led to excellent conversions to the corresponding selenoether-linked dimers, 6–8 (isolated yields: 51–65% following reverse-phase HPLC purification, Fig. 1B–D, Supplementary Figs. 30–35). To probe the limits of this PDC dimerization methodology, we next subjected a recombinant calmodulin (CaM) protein diselenide dimer (12), bearing a Lys-148 to Sec mutation [CaM (K148U)], to the PDC conditions (Fig. 1E). This selenoprotein was expressed using a Sec-incorporating amber-suppression platform in the evolved Sec-dependent E. coli β_UU3-T7 strain and employing an engineered tRNASec, based on recent reports by Ellington and co-workers (see Supplementary Figs. 36–39)79,80. Interestingly, when CaM (K148U) diselenide (12) was subjected to the optimized PDC conditions, instead of dimerization, we observed near-exclusive deselenization of Sec-148 to Ala to afford 13, together with a species corresponding to a selanylphosphonium adduct of CaM (K148U) (14) (Fig. 1E, Supplementary Figs. 40 and 41). We hypothesized that this PTA adduct was a genuine intermediate in the PDC reaction pathway and therefore sought to capitalize on this finding to systematically interrogate the mechanism of the reaction using photophysical and computational experiments.
Probing the mechanism of the PDC transformation using photophysical and computational experiments
To interrogate the mechanism of the reaction, we employed photoluminescence (PL) spectroscopy, cyclic voltammetry (CV), and quantum chemical calculations. We probed the first steps of the mechanism through time-resolved PL spectroscopy. Specifically, time-correlated single-photon counting (TCSPC) experiments were conducted whereby photoexcitation of [Ir(dF(CF3)ppy)2(dtbpy)] (5) at 415 nm was performed in argon-sparged 1:1 v/v H2O:MeCN (as per the typical PDC reaction conditions). PTA (4) was added to a final concentration of 10 mM, with the photocatalyst concentration ranging from 2.5–250 μM. The PL kinetics of these solutions were monitored at different wavelengths spanning the entire PL spectrum of 5 from 430–630 nm. Plotting of the wavelength-dependent PL intensity for different delays of the laser pulse from the TCSPC data revealed that the emission spectra of the photocatalyst 5 showed no observable variation over the entire time window (0.01–0.30 µs) at different concentrations of 5, consistent with it not partaking in direct covalent chemistry with the phosphine (Supplementary Figs. 42 and 43). Interestingly, the PL kinetics at each wavelength showed a clear dependence on the presence of PTA (4) (Fig. 2B). Specifically, upon addition of phosphine, the PL lifetime of the photocatalyst was diminished at least by a factor of two with a concomitant decrease in PL intensity. This suggests a non-radiative decay mechanism involving the PTA substrate leading to quenching of the photoexcited state of the photocatalyst. By comparing the PL kinetics of solutions with different molar equivalents of the photocatalyst and PTA, we inferred that an excess of PTA is needed for significant change in the PL dynamics of the photocatalyst, consistent with our experimental observations (Supplementary Figs. 44 and 45). This observed quenching of the photocatalyst by PTA is likely due to an electron transfer event between the photocatalyst and PTA, in agreement with previous reports81. Moreover, CV experiments confirmed that PTA (4) undergoes more facile single electron oxidation than the diselenide species in the reaction mixture, further supporting phosphine oxidation as the initial step of the reaction (Supplementary Figs. 46 and 47). In conjunction with our synthetic experimental observations, we proposed that the PDC reaction was initiated via a single-electron oxidation of the phosphine, PTA (4, I), mediated by the photoexcited photocatalyst, [Ir(dF(CF3)ppy)2(dtbpy)]* (5*), to afford phosphine radical cation I•+ (Fig. 2A). It follows that this species could then intercept a diselenide substrate to yield the observed selanylphosphonium intermediate II+ and an equivalent of selanyl radical III•.
A Proposed mechanism for the PDC reaction that converts diselenides to selenoethers. B Normalized photoluminescence (PL) counts of photocatalyst [Ir(dF(CF3)ppy)2(dtbpy)] (5) (c = 2.5 μM and 10 μM) in argon-sparged 1:1 v/v H2O:MeCN over a period of 3 μs monitored at 470 nm (excitation wavelength 415 nm) with or without PTA (4) (0 mM and 10 mM). C Changes in the PL intensity of 5-carboxytetramethylrhodamine (TAMRA)-derivatized selenocystamine (15) in the presence of [Ir(dF(CF3)ppy)2(dtbpy)] (5) and PTA (4) monitored at 615 nm (excitation wavelength 550 nm). D Top: B3PW91-GD3(BJ)/6-311 + G(2df,p)//B3PW91-GD3(BJ)/6-31 + G(d,p) computed Gibbs free energy profile in kcal/mol (SMD MeCN solvent, 298.15 K) including main and competitive pathways for [N-Boc-l-Sec-OtBu]2; bottom: sensitivity of activation barriers for heterolytic deselenization to steric effects. PTA = 1,3,5-triaza-7-phosphaadamantane, Arb. Units arbitrary units, SET single electron transfer.
We also sought to probe the second step of our proposed mechanism using time-resolved PL spectroscopy. To this end, we synthesized selenocystamine derivatized with a 5-carboxytetramethylrhodamine (TAMRA) fluorophore (15). TAMRA was specifically chosen due to its red-shifted absorption spectrum relative to [Ir(dF(CF3)ppy)2(dtbpy)] (5), thus allowing for selective photoexcitation to monitor the PL response from the diselenide. The fluorescent TAMRA-labelled diselenide 15 was selectively excited with a 500 nm laser pulse (pulse width ~200 ps, repetition rate −80 MHz) in the presence of PTA (4) and/or [Ir(dF(CF3)ppy)2(dtbpy)] (5) and with continuous background LED irradiation at 450 nm to promote the PDC dimerization (Fig. 2C). The PL kinetics of 15 were monitored at different emission wavelengths over the course of continuous UV irradiation spanning 1–20 min. A subtle broadening and red shift of the steady-state emission spectra of 15 was observed throughout the course of the reaction as revealed by changes in the intensity and spectral shape of the emission profile (Fig. 2C, Supplementary Figs. 48–50). These results support the notion that, after initial oxidation, PTA (4) undergoes chemical reaction with the peptide diselenide, which in and of itself has no or minimal interaction with the photocatalyst, [Ir(dF(CF3)ppy)2(dtbpy)] (5), to generate the highly electrophilic selanylphosphonium II+. To close the photocatalytic cycle, we propose that an equivalent of nucleophilic selenolate anion III− could be generated through single-electron reduction of selanyl radical III•, which could facilitate selenoether V formation through nucleophilic attack on the carbon center α to the Se-P bond of the activated selanylphosphonium II+ via a hypothetical transition state (TS-IV). This process would lead to the formation of a thermodynamically favourable π-bond between Se and P and the extrusion of phosphine selenide VI, that is observed by both mass spectrometry and 31P NMR spectroscopy following PDC reactions (Supplementary Fig. 51). Given that phosphine reagents can undergo SN2 attack on diselenides in the absence of light, that would also generate phosphine selenide VI (through an alternative deselenization pathway), we conducted a 31P NMR time study in which PTA (4) was incubated with [H2N-USPGYS-NH2]2 dimer (1) in D2O. This investigation confirmed that there is no background reaction to generate phosphine selenide VI over the timescale of the PDC reaction (up to 60 min); PTA oxide was the only species that could be observed (Supplementary Fig. 52).
Having established a working hypothesis for the mechanism of the PDC transformation and corroborated the feasibility of the first two proposed steps by time-resolved PL spectroscopy, we next sought to further probe the mechanistic hypothesis using quantum chemical calculations. We used density functional theory (DFT) calculations at the B3PW91-GD3(BJ)/6-311 + G(2df,p)//B3PW91-GD3(BJ)/6-31 + G(d,p) level of theory82,83,84,85, with barriers for electron-transfer estimated using protocols described previously by Houk and Buchwald86, Vaissier87 and a hybrid approach (used in Fig. 2D), obtaining similar conclusions (Supplementary Figs. 53–62, Supplementary Tables 5–8, Supplementary Data 1–2). An [N-Boc-l-Sec-OtBu]2 amino acid diselenide system was studied to generate energy profiles, since its structure emulates the peptide-like environments employed experimentally, showing activation barriers accessible at room temperature (Fig. 2A, D).
The long-lived T1 triplet state of catalyst 5 formed following photoexcitation is 56.6 kcal/mol above its ground state. Single-electron oxidation of PTA (I) by 5* is computed to occur favourably (ΔG = −8.0 kcal/mol) with a small barrier, in line with the experimental PL spectroscopy data (Fig. 2B). Subsequently, the reaction of radical cation I•+ and diselenide is barrierless and exergonic by 6.1 kcal/mol, forming a selanyl phosphonium cation and selanyl radical (II+ and III•). We considered a SH2 homolytic substitution pathway involving these species to form the Se-C bond (via the transition state TS-VII), however, the barrier is unfavorable (ΔG‡ = 29.4 kcal/mol). In contrast, back electron transfer from the catalyst to reduce the selanyl radical III• to selenolate anion III− is computed to be more facile (ΔG‡ = 2.6 kcal/mol) and highly exergonic. From the selanyl phosphonium/selenolate ion-pair, SN2 nucleophilic substitution can occur at the α-carbon center to form the contracted product (through TS-IV) or at selenium center to reform the diselenide starting material (TS-VIII). Other pathways were considered, however they did not significantly affect the kinetics of the reaction. This reaction network was used to generate a microkinetic model for the conversion of a model substrate, dipentafluorobenzyl diselenide (see Supplementary Figs. 63–64)88. Comparison of simulated concentration profiles against experiment are consistent with the proposed mechanism and support the observed accumulation of phosphine selenide VI over the course of the reaction. We next interrogated the influence of sterics at the site of diselenide contraction to help rationalize the inability of the PDC conditions to dimerize the CaM (K148U) diselenide dimer protein 12 (Fig. 2D). Computationally, we found that the barrier for the heterolytic deselenization step (TS-IV) does not change significantly if there are relatively small substituents on the other side of the diselenide (ΔG‡ from 17.2 to 17.8 kcal/mol when a Me is replaced with a tBu group). However, two sterically demanding substituents cause a substantial increase in barrier height (ΔG‡ of 25.4 kcal/mol); this potentially explains why CaM (K148U) 12 could not be dimerized under PDC conditions. Importantly however, these computational studies raised the exciting possibility that the PDC reaction could be applied to the rapid and site-selective functionalization of large selenoproteins using smaller diselenides.
Site-specific functionalization of selenoproteins via PDC
Based on the computational studies above, we envisaged carrying out the kinetically driven formation of an asymmetric protein-small molecule diselenide by adding an excess of a small molecule diselenide to a protein diselenide. Contraction of this asymmetric diselenide under PDC conditions could then be carried out to execute rapid and site-specific protein functionalization at Sec. The feasibility of the late-stage functionalization strategy was first validated on model peptides, which pleasingly led to quantitative peptide functionalization within 5 min using slightly modified PDC conditions to those used for dimerization (see Supplementary Figs. 65–71). Importantly, the chemoselectivity of the transformation was also demonstrated on a model peptide containing a Sec and two Cys residues, with exclusive functionalisation observed at the Sec residue as demonstrated by mass spectrometry (see Supplementary Figs. 72 and 73).
Motivated by these results on peptidic systems, we turned our attention to the late-stage functionalization of the recombinant CaM (K148U) diselenide dimer protein 12. To this end, 12 was first mixed with super-stoichiometric amounts of a synthetic hexaethylene glycol diselenide ([Se-PEG6]2; 16). This led to exclusive formation of the CaM-PEG6 asymmetric diselenide 17 after mixing as judged by HPLC-MS analysis (Fig. 3). Addition of PTA (4) (66 equiv.) and 10 mol% [Ir(dF(CF3)ppy)2(dtbpy)]PF6 (5) and LED irradiation at 450 nm led to clean contraction to the desired PEG6-functionalized CaM (K148U) 18 in 5 min (91% conversion, Supplementary Figs. 74 and 75). The PEG6-CaM (K148U) selenoether conjugate 18 generated from a multi-milligram PDC reaction was submitted directly (without purification) to a crystallization screen (Supplementary Fig. 76). A crystal diffracted to 1.95 Å resolution by X-ray crystallography (Supplementary Fig. 77 and Supplementary Table 9), with the refined structure of 18 nearly identical to ligand-bound conformations of CaM published in the protein databank, thus confirming the retention of higher order secondary and tertiary structural features. Importantly, this highlights the biocompatibility of the PDC conditions (see Fig. 3 for solved protein structure). While electron density surrounding the PEG6 selenoether modification could not to be resolved, the presence of a Se atom in this structure was confirmed through X-ray absorption at the Se edge (Kα; E = ~1152 deV) (Supplementary Fig. 78).
Functionalization of a CaM (K148U) diselenide 12 with [PEG6-Se]2 (16) to afford PEG6-modified CaM (K148U) 18; mass spectra of the asymmetric diselenide 17 formed from mixing 12 and 16 (A) and subsequent photocatalytic contraction to afford 18 (B) are shown as insets. MALDI-TOF spectra of crude desalted reaction mixtures after PDC functionalisation with C biotin-PEG5- (19), D mPEG17- (20), E GalNAc- (21), F (Me)2NCH2CH2- (22), G AcHNCH2CH2- (23), H PropionylHNCH2CH2- (24), and I SuccHNCH2CH2- (25) are also inset. Reaction conversions were calculated through averaging integrations of HRMS-derived extracted ion chromatograms of the [M + 11H+]11+, [M + 10H+]10+ and [M + 9H+]9+ charge states and errors are reported as the standard deviation of the integration of these three ion peaks for a single experiment (see Supplementary Information). Ribbon structure used depicts the X-ray crystal structure solved for 18 (PDB: 7T2Q); PTA 1,3,5-triaza-7-phosphaadamantane, MeCN acetonitrile, Gnd.HCl guanidinium hydrochloride, NaPi sodium phosphate. Created with BioRender.com.
Having established conditions for the rapid functionalization of CaM (K148U) diselenide (12) with PEG6, we next explored the scope of the PDC functionalization chemistry using a diverse library of PTM mimics, PEG oligomers and purification handles (see Supplementary Figs. 79–103 for small molecule diselenide characterization). Gratifyingly, reaction with larger diselenides ([Biotin-PEG5-Se]2 and [mPEG17-Se]2) under the optimized PDC conditions led to clean site-specific functionalization of CaM (K148U) (12) within 5 min to afford conjugates 19 and 20 (Fig. 3, Supplementary Figs. 104–107). CaM (K148U) (12) could also be rapidly and efficiently modified with PTMs including N-acetylgalactosamine (α-GalNAc) (21), and mimics of Lys dimethylation (22), acetylation (23), propionylation (24) and succinylation (25) (Fig. 3, Supplementary Figs. 108–117). Pleasingly, in all the cases, functionalization of CaM (K148U) (12) was accomplished within 5 min following treatment with the corresponding diselenides (see Supplementary Information for synthetic details), PTA (4) and irradiation at 450 nm, with excellent conversions (80–97%). Taken together, these examples showcase the utility of the PDC methodology for the simple, fast and efficient installation of PTM mimics and designer modifications such as PEGylation and affinity handles to proteins in a chemo- and regioselective manner.
Having demonstrated the rapid and efficient functionalization of an expressed protein bearing the 21st amino acid, Sec, we next sought to assess the utility of the PDC technology for the C-terminal functionalization of an expressed protein, namely human ubiquitin. To this end, a gene encoding the full-length ubiquitin sequence was fused to the Mycobacterium xenopi DNA Gyrase A intein and a chitin-binding domain. Following expression in E. coli, the fusion protein was immobilized on chitin beads and the target ubiquitin acyl hydrazide 26 liberated by treatment with aqueous hydrazine (Fig. 4, Supplementary Figs. 118 and 119). Acetylacetone (acac)-based activation and treatment with selenocystamine then provided ubiquitin diselenide dimer 27 (via initial selenoester formation and a rapid Se-to-N acyl shift89, Supplementary Fig. 120). In addition, a Cys mutant of ubiquitin (K48C) was generated bearing a C-terminal selenocystamine moiety (using the same intein-fusion approach used for the wild-type protein) to assess the chemoselectivity of PDC functionalization in the presence of Cys (Supplementary Fig. 121). To explore PDC-functionalization at the C-terminus of ubiquitin diselenide 27, we selected a range of reagents, including [PEG6-Se]2, [mPEG17-Se]2 and [Biotin-PEG5-Se]2. Pleasingly, reaction under the optimized photocatalytic conditions afforded the C-terminally functionalized ubiquitin bearing PEG6 (28), mPEG17 (29), and PEG5-biotin (30) with 88% to quantitative conversions in 5–10 min and with very high crude purities (Fig. 4, Supplementary Figs. 122–127). Purification by reverse-phase HPLC then provided each of the conjugates in 40–71% isolated yield. Pleasingly, the Cys-containing mutant, ubiquitin (K48C), also underwent chemo- and regioselective functionalization at the C-terminal diselenide moiety with [PEG6-Se]2 diselenide (16) under modified PDC conditions, whereby the amount of phosphine [PTA (4)] was reduced to 18 molar equivalents to prevent deleterious desulfurization of the Cys residue (Supplementary Fig. 128). Finally, to explore the conjugation of larger structures to the C-terminus of 27, we synthesized a Sec-(PEG4)2-Arg8 diselenide dimer peptide as an example of a cell penetrating peptide motif90 (see Supplementary Fig. 129 for synthesis). Pleasingly, treatment of ubiquitin diselenide 27 with this larger peptidic diselenide under optimized PDC conditions led to clean conversion to the selenoether-linked conjugate 31 within 5 min and was isolated in good yield following purification by reverse-phase HPLC (Fig. 4, Supplementary Figs. 130 and 131). Finally, a selenopeptide derived from the histone protein H2AX91 (see Supplementary Fig. 132 for synthesis) was also fused to the C-terminus of ubiquitin via PDC in excellent yield to afford selenoether-linked conjugate 32, which represents a stable structural mimic of ubiquitin linked to a Lys side chain within a polypeptide (Fig. 4, Supplementary Figs. 133 and 134). Taken together, these examples of asymmetric protein-peptide coupling, a transformation that would be difficult to achieve using existing bioconjugation methods, lay the foundation for expanding the scope of the PDC manifold toward a wide range of other high value peptide–protein conjugates in the future, for example antibody-drug conjugates bearing cytotoxic payloads.
Conversion of ubiquitin acyl hydrazide 26 to ubiquitin diselenide 27 and MALDI-TOF spectra of crude desalted reaction mixtures after C-terminal functionalization with A PEG6- (28), B mPEG17- (29), C Biotin-PEG5- (30), D Arg8-(PEG4)2-Ala- (31) and E H2AX- (32) under optimized PDC conditions. Reaction conversions were calculated through averaging integrations of HRMS-derived extracted ion chromatograms of the [M + 9H+]9+, [M + 8H+]8+ and [M + 7H+]7+ charge states and errors are reported as the standard deviation of the integration of these three ion peaks for a single experiment (see Supplementary Information); acac acetylacetone, TCEP tris-carboxyethylphosphine, DPDS diphenyl diselenide, Gnd.HCl guanidinium hydrochloride, HEPES = 4-(2-hydroxyethyl)−1-piperazineethanesulfonic acid, PTA 1,3,5-triaza-7-phosphaadamantane, MeCN acetonitrile, NaP sodium phosphate, Quant. quantitative conversion, Yield isolated yield of modified protein following reverse-phase HPLC purification. Created with BioRender.com.
In summary, we have discovered a synthetic transformation called the photocatalytic diselenide contraction (PDC) that enables the rapid and efficient conversion of diselenides to stable selenoethers with the formal extrusion of a selenium atom. The mild PDC conditions (comprising an iridium photocatalyst, a phosphine and blue LED irradiation) enabled fast and clean conversion of several Sec-containing diselenide dimer peptides to selenoether dimers within 5 min, however, larger protein diselenide dimers could not be similarly dimerized. Detailed interrogation of the proposed reaction pathway by PL spectroscopy and DFT calculations was used to substantiate the proposed mechanism of this reaction, and provided key insight into a PDC reaction pathway for the site-selective functionalization of proteins through the contraction of asymmetric protein-small molecule diselenides. The feasibility and utility of this late-stage functionalization chemistry was demonstrated through the site-specific modification of selenocalmodulin and the C-terminal modification of ubiquitin with a diverse array of small molecule diselenides, including examples with larger polypeptide chains. By virtue of the chemoselectivity and regioselectivity of the PDC transformation at diselenides (including at the side chain of the very rare 21st proteinogenic amino acid Sec) we envisage that the PDC methodology will find widespread utility in the generation of modified proteins and therapeutically valuable protein conjugates in the future.
Methods
Ethics
All procedures involving the collection of blood from healthy donors were approved by the University of Sydney Human Research Ethics Committee (HREC, Project 2014/244) and all studies conformed to the principles outlined in the Declaration of Helsinki. Written informed consent was obtained from all human research participants.
General PDC conditions for peptide dimerization
Peptide diselenide (1 eq.) was dissolved in a solution of [Ir(dF(CF3)ppy)2(dtbpy)]PF6 (1 mol%). in either 1:1 v/v MeCN:H2O or 1:1 v/v MeCN:1 M Gnd.HCl, 0.02 M NaPi, pH 7.0 buffer, to a final peptide concentration of 2.5–10 mM. This solution was then used to dissolve PTA (4 eq.), and the reaction mixture irradiated with 450 nm LED light for 4–6 min. Aliquots were taken at 0 min and 5 min following irradiation for analysis of reaction progression by UPLC-MS and UPLC. The crude reaction mixture was then purified by reverse-phase HPLC to afford selenoether-linked peptide dimers following lyophilization.
General PDC conditions for protein functionalization
Protein diselenide (1 eq.), small molecule diselenide (32 eq.), PTA (66 eq.), and [Ir(dF(CF3)ppy)2(dtbpy)]PF6 (10 mol% relative to protein diselenide) were dissolved in 1:1 v/v MeCN:1 M Gnd.HCl, 0.02 M NaPi, pH 7.0 buffer, to give a final protein concentration of 0.5 mM. The reaction mixture was then irradiated with 450 nm LED light for 5 min. Aliquots were taken at 0 min and 5 min for analysis of reaction progression by MALDI-TOF MS and LC-HRMS. Isolated yields of functionalized ubiquitin proteins were obtained after crude reaction mixtures were purified by reverse-phase HPLC and lyophilized.
Reporting summary
Further information on research design is available in the Nature Portfolio Reporting Summary linked to this article.
Data availability
Thermochemical data (Supplementary Data 1) and molecular coordinates from computational mechanistic studies (Supplementary Data 2), and the PDB validation report for 7T2Q are provided with this manuscript as Supplementary Data Sets. The thermochemical data (obtained with the GoodVibes software, https://github.com/bobbypaton/GoodVibes) and molecular coordinates from computational mechanistic studies are also available in Zenodo (https://doi.org/10.5281/zenodo.7224862). The mass spectrometry proteomics data have been deposited to the ProteomeXchange Consortium via the PRIDE partner repository with the dataset identifier PXD037525. Data is available from the corresponding authors upon request.
Code availability
The AQME program (https://github.com/jvalegre/aqme) was used to carry out the conformational sampling in computational studies. The CSV input file and Jupyter Notebook workflow used are available in Zenodo: https://doi.org/10.5281/zenodo.7224862.
References
Walsh, C. T., Garneau-Tsodikova, S. & Gatto, G. J. Jr Protein posttranslational modifications: the chemistry of proteome diversifications. Angew. Chem. Int. Ed. 44, 7342–7372 (2005).
Spicer, C. D. & Davis, B. G. Selective chemical protein modification. Nat. Commun. 5, 4740 (2014).
Hoyt, E. A., Cal, P. M. S. D., Oliveira, B. L. & Bernardes, G. J. L. Contemporary approaches to site-selective protein modification. Nat. Rev. Chem. 3, 147–171 (2019).
Sletten, E. M. & Bertozzi, C. R. From mechanism to mouse: a tale of two bioorthogonal reactions. Acc. Chem. Res. 44, 666–676 (2011).
Leader, B., Baca, Q. J. & Golan, D. E. Protein therapeutics: a summary and pharmacological classification. Nat. Rev. Drug Discov. 7, 21–39 (2008).
Ravasco, J. M. J. M., Faustino, H., Trindade, A. & Gois, P. M. P. Bioconjugation with maleimides: a useful tool for chemical biology. Chem. Eur. J. 25, 43–59 (2019).
Beck, A., Goetsch, L., Dumontet, C. & Corvaïa, N. Strategies and challenges for the next generation of antibody–drug conjugates. Nat. Rev. Drug Discov. 16, 315–337 (2017).
Wang, L., Brock, A., Herberich, B. & Schultz, P. G. Expanding the genetic code of Escherichia coli. Science 292, 498–500 (2001).
Neumann, H., Wang, K., Davis, L., Garcia-Alai, M. & Chin, J. W. Encoding multiple unnatural amino acids via evolution of a quadruplet-decoding ribosome. Nature 464, 441–444 (2010).
Dunkelmann, D. L., Willis, J. C., Beattie, A. T. & Chin, J. W. Engineered triply orthogonal pyrrolysyl–tRNA synthetase/tRNA pairs enable the genetic encoding of three distinct non-canonical amino acids. Nat. Chem. 12, 535–544 (2020).
Chung, C. Z., Amikura, K. & Söll, D. Using genetic code expansion for protein biochemical studies. Front. Bioeng. Biotechnol. 8, 598577 (2020).
Yang, Y. et al. Hybrid mass spectrometry approaches in glycoprotein analysis and their usage in scoring biosimilarity. Nat. Commun. 7, 13397 (2016).
Bondalapati, S., Jbara, M. & Brik, A. Expanding the chemical toolbox for the synthesis of large and uniquely modified proteins. Nat. Chem. 8, 407–418 (2016).
Kulkarni, S. S., Sayers, J., Premdjee, B. & Payne, R. J. Rapid and efficient protein synthesis through expansion of the native chemical ligation concept. Nat. Rev. Chem. 2, 0122 (2018).
Conibear, A. Deciphering protein post-translational modifications using chemical biology tools. Nat. Rev. Chem. 4, 674–695 (2020).
Kent, S. B. H. Total chemical synthesis of proteins. Chem. Soc. Rev. 38, 338–351 (2009).
Conibear, A., Watson, E. E., Payne, R. J. & Becker, C. F. W. Native chemical ligation in protein synthesis and semi-synthesis. Chem. Soc. Rev. 47, 9046–9068 (2018).
Hackenberger, C. P. R. & Schwarzer, D. Chemoselective ligation and modification strategies for peptides and proteins. Angew. Chem. Int. Ed. 47, 10030–10074 (2008).
Agouridas, V. et al. Native chemical ligation and extended methods: mechanisms, catalysis, scope, and limitations. Chem. Rev. 119, 7328–7443 (2019).
Thompson, R. E. & Muir, T. W. Chemoenzymatic semisynthesis of proteins. Chem. Rev. 120, 3051–3126 (2019).
Koniev, O. & Wagner, A. Developments and recent advancements in the field of endogenous amino acid selective bond forming reactions for bioconjugation. Chem. Soc. Rev. 44, 5495–5551 (2015).
deGruyter, J. N., Malins, L. R. & Baran, P. S. Residue-specific peptide modification: a chemist’s guide. Biochemistry 56, 3863–3873 (2017).
Adusumalli, S. R. et al. Chemoselective and site-selective lysine-directed lysine modification enables single-site labeling of native proteins. Angew. Chem. Int. Ed. 59, 10332–10336 (2020).
Matos, M. J. et al. Chemo- and regioselective lysine modification on native proteins. J. Am. Chem. Soc. 140, 4004–4017 (2018).
Deng, J.-R. et al. Chemoselective and photocleavable cysteine modification of peptides and proteins using isoxazoliniums. Commun. Chem. 2, 93 (2019).
Zhang, C. et al. π-Clamp-mediated cysteine conjugation. Nat. Chem. 8, 120–128 (2016).
Chen, L. et al. In-depth structural charcaterization of Kadcyla® (ado-trastuzumab emtansine) and its biosimilar candidate. mAbs 8, 1210–1223 (2016).
Davis, B. G., Lloyd, R. C. & Jones, J. B. Controlled site-selective glycosylation of proteins by a combined site-directed mutagenesis and chemical modification approach. J. Org. Chem. 63, 9614–9615 (1998).
Gamblin, D. P. et al. Glyco-SeS: selenenylsulfide-mediated protein glycoconjugation—a new strategy in post-translational modification. Angew. Chem. Int. Ed. 43, 828–833 (2004).
Gamblin, D. P. et al. Glycosyl phenylthiosulfonates (Glyco-PTS): novel reagents for glycoprotein synthesis. Org. Biomol. Chem. 1, 3642–3644 (2003).
Tessier, R. et al. “Doubly orthogonal” labeling of peptides and proteins. Chem 5, 2243–2263 (2019).
Tessier, R. et al. Ethynylation of cysteine residues: from peptides to proteins in vitro and in living cells. Angew. Chem. Int. Ed. 59, 10961–10970 (2020).
Byrne, S. A. et al. Late-stage modification of peptides and proteins at cysteine with diaryliodonium salts. Chem. Sci. 12, 14159–14166 (2021).
Kasper, M.-A. et al. Cysteine-selective phosphonamidate electrophiles for modular protein bioconjugations. Angew. Chem. Int. Ed. 58, 11625–11630 (2019).
Gianatassio, R. et al. Strain-release amination. Science 351, 241–246 (2016).
Griffiths, R. C. et al. Site-selective installation of Nϵ-modified sidechains into peptide and protein scaffolds via visible-light-mediated desulfurative C-C bond formation. Angew. Chem. Int. Ed. 61, e202110223 (2022).
Bottecchia, C. et al. Visible-light-mediated selective arylation of cysteine in batch and flow. Angew. Chem. Int. Ed. 56, 12702–12707 (2017).
Cohen, D. T., Zhang, C., Pentelute, B. L. & Buchwald, S. L. An umpolung approach for the chemoselective arylation of selenocysteine in unprotected peptides. J. Am. Chem. Soc. 137, 9784–9787 (2015).
Hanaya, K. et al. Rapid nickel(II)-promoted cysteine S-arylation with arylboronic acids. Chem. Commun. 55, 2841–2844 (2019).
Messina, M. S. et al. Organometallic gold(III) reagents for cysteine arylation. J. Am. Chem. Soc. 140, 7065–7069 (2018).
Wright, T. H. et al. Posttranslational mutagenesis: a chemical strategy for exploring protein side-chain diversity. Science 354, aag1465 (2016).
Josephson, B. et al. Light-driven post-translational installation of reactive protein side chains. Nature 585, 530–537 (2020).
Bernardes, G. J. L. et al. From disulfide- to thioether-linked glycoproteins. Angew. Chem. Int. Ed. 47, 2244–2247 (2008).
Lin, S. et al. Redox-based reagents for chemoselective methionine bioconjugation. Science 355, 597–602 (2017).
Taylor, M. T., Nelson, J. E., Suero, M. G. & Gaunt, M. J. A protein functionalization platform based on selective reactions at methionine residues. Nature 562, 563–568 (2018).
Kim, J. et al. Site-selective functionalization of methionine residues via photoredox catalysis. J. Am. Chem. Soc. 142, 21260–21266 (2020).
Vantourout, J. C. et al. Serine-selective bioconjugation. J. Am. Chem. Soc. 142, 17236–17242 (2020).
Li, B. X. et al. Site-selective tyrosine bioconjugation via photoredox catalysis for native-to-bioorthogonal protein transformation. Nat. Chem. 13, 902–908 (2021).
Kim, K., Fancy, D. A., Carney, D. & Kodadek, T. Photoinduced protein cross-linking mediated by palladium porphyrins. J. Am. Chem. Soc. 121, 11896–11897 (1999).
Sato, S. & Nakamura, H. Ligand‐directed selective protein modification based on local single‐electron‐transfer catalysis. Angew. Chem. Int. Ed. 52, 8681–8684 (2013).
Ichiishi, N. et al. Protecting group free radical C–H trifluoromethylation of peptides. Chem. Sci. 9, 4168–4175 (2018).
Bloom, S. et al. Decarboxylative alkylation for site-selective bioconjugation of native proteins via oxidation potentials. Nat. Chem. 10, 205–211 (2018).
Bandyopadhyay, A., Cambray, S. & Gao, J. Fast and selective labeling of N-terminal cysteines at neutral pH via thiazolidino boronate formation. Chem. Sci. 7, 4589–4593 (2016).
Faustino, H., Silva, M. J. S. A., Veiros, L. F., Bernardes, G. J. L. & Gois, P. M. P. Iminoboronates are efficient intermediates for selective, rapid and reversible N-terminal cysteine functionalisation. Chem. Sci. 7, 5052–5058 (2016).
Rosen, C. B. & Francis, M. B. Targeting the N terminus for site-selective protein modification. Nat. Chem. Biol. 13, 697–705 (2017).
Qin, T. et al. Nickel-catalyzed barton decarboxylation and giese reactions: a practical take on classic transforms. Angew. Chem. Int. Ed. 56, 260–265 (2017).
Li, C. et al. Decarboxylative borylation. Science 356, aam7355 (2017).
Cheng, W.-M., Shang, R. & Fu, Y. Photoredox/brønsted acid co-catalysis enabling decarboxylative coupling of amino acid and peptide redox-active esters with N-heteroarenes. ACS Catal. 7, 907–911 (2017).
Sletten, E. M. & Bertozzi, C. R. Bioorthogonal chemistry: fishing for selectivity in a sea of functionality. Angew. Chem. Int. Ed. 48, 6974–6998 (2009).
Kolb, H. C., Finn, M. G. & Sharpless, K. B. Click chemistry: diverse chemical function from a few good reactions. Angew. Chem. Int. Ed. 40, 2004–2021 (2001).
Plass, T., Milles, S., Koehler, C., Schultz, C. & Lemke, E. A. Genetically encoded copper-free click chemistry. Angew. Chem. Int. Ed. 50, 3878–3881 (2011).
Blackman, M. L., Royzen, M. & Fox, J. M. Tetrazine ligation: fast bioconjugation based on inverse-electron-demand Diels–Alder reactivity. J. Am. Chem. Soc. 130, 13518–13519 (2008).
Lang, K. et al. Genetic encoding of bicyclononynes and trans-cyclooctenes for site-specific protein labeling in vitro and in live mammalian cells via rapid fluorogenic Diels–Alder reactions. J. Am. Chem. Soc. 134, 10317–10320 (2012).
Saxon, E. & Bertozzi, C. R. Cell surface engineering by a modified Staudinger reaction. Science 287, 2007–2010 (2000).
Prescher, J. A., Dube, D. H. & Bertozzi, C. R. Chemical remodelling of cell surfaces in living animals. Nature 430, 873–877 (2004).
Driscoll, D. M. & Copeland, P. R. Mechanism and regulation of selenoprotein synthesis. Annu. Rev. Nutr. 23, 17–40 (2003).
Metanis, N. & Hilvert, D. Harnessing selenocysteine reactivity for oxidative protein folding. Chem. Sci. 6, 322–325 (2015).
Mousa, R., Dardashti, R. N. & Metanis, N. Selenium and selenocysteine in protein chemistry. Angew. Chem. Int. Ed. 56, 15818–15827 (2017).
Levengood, M. R. & van der Donk, W. A. Dehydroalanine-containing peptides: preparation from phenylselenocysteine and utility in convergent ligation strategies. Nat. Protoc. 1, 3001–3010 (2006).
Liu, J., Chen, Q. & Rozovsky, S. Utilizing selenocysteine for expressed protein ligation and bioconjugations. J. Am. Chem. Soc. 139, 3430–3437 (2017).
Pedzisa, L., Li, X., Rader, C. & Roush, W. R. Assessment of reagents for selenocysteine conjugation and the stability of selenocysteine adducts. Org. Biomol. Chem. 14, 5141–5147 (2016).
Cohen, D. T. et al. A chemoselective strategy for late-stage functionalization of complex small molecules with polypeptides and proteins. Nat. Chem. 11, 78–85 (2019).
Zhao, Z., Shimon, D. & Metanis, N. Chemoselective copper-mediated modification of selenocysteines in peptides and proteins. J. Am. Chem. Soc. 143, 12817–12824 (2021).
Harpp, D. N. & Gleason, J. G. Preparation and mass spectral properties of cystine and lanthionine derivatives. Novel synthesis of L-lanthionine by selective desulfurization. J. Org. Chem. 36, 73–80 (1971).
Takaguchi, Y., Suzuki, S., Mori, T., Motoyoshiya, J. & Aoyama, H. Synthesis, characterization, and controlling morphology of an aryl ether dendrimer containing a dichalcogenide bond as the core. Bull. Chem. Soc. Jpn 73, 1857–1860 (2000).
Maric, H. M. et al. Design and synthesis of high-affinity dimeric inhibitors targeting the interactions between gephyrin and inhibitory neurotransmitter receptors. Angew. Chem. Int. Ed. 54, 490–494 (2015).
Aggarwal, S., Singh, P., Topaloglu, O., Isaacs, J. T. & Denmeade, S. R. A dimeric peptide that binds selectively to prostate-specific membrane antigen and inhibits its enzymatic activity. Cancer Res. 66, 9171–9177 (2006).
Tanegashima, K. et al. Dimeric peptides of the C-terminal region of CXCL14 function as CXCL12 inhibitors. FEBS Lett. 587, 3770–3775 (2013).
Thyer, R., Robotham, S. A., Brodbelt, J. S. & Ellington, A. D. Evolving tRNASec for efficient canonical incorporation of selenocysteine. J. Am. Chem. Soc. 137, 46–49 (2015).
Thyer, R. et al. Custom selenoprotein production enabled by laboratory evolution of recoded bacterial strains. Nat. Biotechnol. 36, 624–631 (2018).
Wu, C., Chen, H.-F., Wong, K.-T. & Thompson, M. E. Study of ion-paired iridium complexes (soft salts) and their application in organic light emitting diodes. J. Am. Chem. Soc. 132, 3133–3139 (2010).
Frisch, M. J. et al. Gaussian 16, Revision C.01. Gaussian 16, Revision C.01, (Gaussian, Inc., Wallingford, CT, 2016).
Luchini, G., Alegre-Requena, J., Funes-Ardoiz, I. & Paton, R. GoodVibes: automated thermochemistry for heterogeneous computational chemistry data. F1000Research 9, 291 (2020).
Heverly-Coulson, G. S. & Boyd, R. J. Systematic study of the performance of density functional theory methods for prediction of energies and geometries of organoselenium compounds. J. Phys. Chem. A 115, 4827–4831 (2011).
Pearson, J. K., Ban, F. & Boyd, R. J. An evaluation of various computational methods for the treatment of organoselenium compounds. J. Phys. Chem. A 109, 10373–10379 (2005).
Jones, G. O., Liu, P., Houk, K. N. & Buchwald, S. L. Computational explorations of mechanisms and ligand-directed selectivities of copper-catalyzed ullmann-type reactions. J. Am. Chem. Soc. 132, 6205–6213 (2010).
Vaissier, V., Barnes, P., Kirkpatrick, J. & Nelson, J. Influence of polar medium on the reorganization energy of charge transfer between dyes in a dye sensitized film. Phys. Chem. Chem. Phys. 15, 4804–4814 (2013).
Besora, M. & Maseras, F. Microkinetic modeling in homogeneous catalysis. Wiley Interdiscip. Rev. Comput. Mol. Sci. 8, e1372 (2018).
Kulkarni, S. S. et al. Expressed protein selenoester ligation. Angew. Chem. Int. Ed. 61, e202200163 (2022).
Schneider, A. F. L., Kithil, M., Cardoso, M. C., Lehmann, M. & Hackenberger, C. P. R. Cellular uptake of large biomolecules enabled by cell-surface-reactive cell-penetrating peptide additives. Nat. Chem. 13, 530–539 (2021).
Qian, S. et al. Quantitative analysis of ubiquitinated proteins in human pituitary and pituitary adenoma tissues. Front. Endocrinol. 10, 328 (2019).
Acknowledgements
The authors thank Mr Stephen Byrne, Dr Ian Luck and Dr Cody Szczepina at The University of Sydney for their assistance with MALDI-TOF mass spectrometry, NMR spectroscopy and liquid chromatography, respectively. We would also like to thank Prof Andrew Ellington and Dr Ross Thyer (College of Natural Sciences, The University of Texas at Austin) for providing the cell lines and plasmids for the expression of His6-MBP-TEV-CaM (K148U), and for helpful discussions. Finally, we would like to thank Dr Chandrika Deshpande (Sydney Analytical, The University of Sydney) and Dr Daniel Clayton (School of Chemistry, The University of Sydney) for their assistance with the recombinant expression of His6-MBP-TEV-CaM (K148U), Dr Daniel Ford (School of Chemistry, The University of Sydney) for performing the plasma stability studies, and Dr Lara Malins (Australian National University) and Dr Anastasios Polyzos (University of Melbourne) for kindly providing the 4-CzIPN and [Ir(dF(Me)ppy)2(dtbbpy)]PF6 photocatalysts, respectively. We thank SydneyMS for providing some of the mass spectrometers used in this study. Figures 1, 3a and 4a were created with BioRender.com. The authors would like to acknowledge funding from the National Health and Medical Research Council (Investigator Grant APP1174941 to R.J.P.), the Australian Research Council Centre of Excellence for Exciton Science (CE170100026 to A.S. and G.L.) and the John A. Lamberton Research Scholarship (to L.J.D.). R.S.P. acknowledges support from the NSF (CHE-1955876) and computational resources from the RMACC Summit supercomputer supported by the National Science Foundation (ACI-1532235 and ACI-1532236), the University of Colorado Boulder and Colorado State University, and the Extreme Science and Engineering Discovery Environment (XSEDE) through allocation TG-CHE180056. J.V.A.-R. acknowledges support from XSEDE through allocation TG-CHE200033. S.H. and C.F.W.B. gratefully acknowledge support from the Austrian Science Fund (FWF) through SFB 79. L.C.G. acknowledges support from the Texas Advanced Computing Center at The University of Texas at Austin as part of the Frontera Fellowships Program, funded by NSF Award (#1818253).
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L.J.D. and R.J.P. conceived the research project. L.J.D. and S.S.K. designed and performed all photocatalytic diselenide contraction reactions. A.M.G., S.S.K., E.E.W., and A.R.N. designed and performed the syntheses of all small molecule diselenides. J.V.A.-R., L.C.G., and R.S.P. designed, performed and analyzed all quantum chemical calculations. A.S., L.J.D., and G.L. designed, performed and analyzed all time-resolved photoluminescence spectroscopy experiments. A.S.M. performed cyclic voltammetry, 31P NMR time course experiments and selenoether stability experiments. L.J.D., A.P.W., D.vR., and T.H. performed the expression of CaM (K148U). K.P., L.J.D., and J.P.M. performed crystallization trials and K.P. performed X-ray crystallography. G.N., S.H., and C.F.W.B. expressed and characterized the wildtype and K48C ubiquitin-acyl hydrazide proteins. N.P. performed MALDI-TOF mass spectrometry. M.L. performed high-resolution mass spectrometry and proteomics. L.J.D., J.V.A.-R., R.S.P., and R.J.P. prepared the manuscript with assistance from all authors.
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Dowman, L.J., Kulkarni, S.S., Alegre-Requena, J.V. et al. Site-selective photocatalytic functionalization of peptides and proteins at selenocysteine. Nat Commun 13, 6885 (2022). https://doi.org/10.1038/s41467-022-34530-z
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DOI: https://doi.org/10.1038/s41467-022-34530-z
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