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OB and JR designed the study. AB carried out cross-linking/mass spectrometry experiments. AB, MS, LF, MM, KS, OB and JR analyzed data. AB, MS, MM, KS, OB and JR wrote the manuscript.
Determining the structure of a protein by any method requires various contributions from experimental and computational sides. In a recent study, high-density cross-linking/mass spectrometry (HD-CLMS) data in combination with ab initio structure prediction determined the structure of human serum albumin (HSA) domains, with an RMSD to X-ray structure of up to 2.5 Å, or 3.4 Å in the context of blood serum. This paper reports the blind test on the readiness of this technology through the help of Critical Assessment of protein Structure Prediction (CASP). We identified between 201-381 unique residue pairs at an estimated 5% FDR (at link level albeit with missing site assignment precision evaluation), for four target proteins. HD-CLMS proved reliable once crystal structures were released. However, improvements in structure prediction using cross-link data were slight. We identified two reasons for this. Spread of cross-links along the protein sequence and the tightness of the spatial constraints must be improved. However, for the selected targets even ideal contact data derived from crystal structures did not allow modellers to arrive at the observed structure. Consequently, the progress of HD-CLMS in conjunction with computational modeling methods as a structure determination method, depends on advances on both arms of this hybrid approach.
CLMS - cross-linking/mass spectrometry
HD - high-density
NHS - N-hydroxysuccinimide
NMR - nuclear magnetic resonance
sulfo-SDA, sulfo-NHS-diazirine, sulfosuccinimidyl 4,4’-azipentanoate
FDR - false discovery rate
MBS - model-based search
HSA - human serum albumin
RMSD - root-mean-square deviation
CASP - Critical Assessment of protein Structure Prediction
Tris - tris(hydroxymethyl)aminomethane
PES - polyethersulphone
IAA - iodoacetamide
LTQ - linear trap quadrupole
MS2 - tandem MS scan
LC-MS - liquid chromatography mass spectrometry
FM - free modelling
Cross-linking/mass spectrometry (CLMS) is a well-established, low-resolution technique for revealing protein interactions in protein complexes and studying protein conformational changes 1– 16. In contrast, the use of CLMS to resolve the detailed tertiary protein structure, pioneered by Young et al. 17, is less well established. A limiting factor is the sparsity of CLMS data. For example, an earlier study from our laboratory found 0.07 links per residue 18. A possible culprit for the low data density is the NHS-ester based cross-linking chemistry used in most studies. These cross-linker reagents predominantly react with lysines, which results in linkage maps that are not sufficiently dense to define the detailed structure of proteins.
In a previous study, we showed that this limitation can be overcome by high-density cross-linking using photoactivatable cross-linkers 19. This approach uses a heterobifunctional cross-linker, sulfo-SDA, which on one side carries an NHS-ester and a photoactivatable diazirine on the other side. The diazirine group forms a reactive carbene species upon UV-light activation that can react with any amino acid. The resulting increased data density opens up the possibility of determining tertiary protein structure, which we demonstrated by recapitulating the domain structures of human serum albumin (HSA) in purified form (RMSD to crystal structure of 2.5 Å) and in its native environment, blood serum (RMSD to crystal structure 3.4 Å) 19.
This proof-of-concept study triggered three questions: Would the high-density CLMS (HD-CLMS) method perform robustly on proteins with unknown structure? Would current structure prediction experts be able to improve their predictions using HD-CLMS data? What are the current technical shortcomings of our approach?
To tackle these questions, we embarked on a blind study to evaluate the current capabilities of HD-CLMS in the context of the Critical Assessment of protein Structure Prediction (CASP) experiment. CASP evaluates the state-of-the art in protein modeling 20 by the following experiment: Can modeling groups blindly predict the structure of a protein if the structure is unknown to them? Modeling groups predict the structures of these proteins and then have their predictions assessed by independent evaluating scientists.
In CASP11, the Organizing Committee generously offered to identify suitable protein targets for us, which would be sent to our laboratory and give us the opportunity to blindly test our cross-linking method. After putting the proteins through our CLMS pipeline, the Rappsilber lab then submitted CLMS data in the form of distance restraints and these were then offered to the prediction groups as additional data that they could use in their predictions.
Here, we report the outcome of this experiment. In particular, 1) we analyzed whether the blindly generated cross-links fit the crystal structures; 2) we analyzed if CASP modeling groups were able to utilize the CLMS data in their predictions, which is discussed in detail elsewhere 21; and 3) we identified technical shortcomings of high-density cross-linking and the blind study approach taken here. Overcoming the issues of HD-CLMS might pave the way for transforming this hybrid approach into a tertiary structure determination method to complement X-ray crystallography, NMR, and cryo-EM.
A total of nine proteins were received from five labs. YaaA (PDB|5CAJ) was received from the lab of Prof. Mark Wilson (Department of Biochemistry/Redox Biology, University of Nebraska), as a frozen solution (25 mM HEPES, pH 8.2, 100 mM KCl, 6.89 mg/mL). Five proteins, 413472 (GS13694A), BACUNI_01052 (PDB|4QE0), RUMGNA_02398 (PDB|4QAN), SAV1486 (PDB|4QPV) and BACCAC_02064 (PDB|4QHW), were received from the lab of Dr. Ashley M. Deacon (Joint Center for Structural Genomics (JCSG), Stanford Synchrotron Radiation Lightsource, Stanford University). All were received as previously frozen and thawed-in-transit solutions, with all comprised of a buffer containing 20 mM tris(hydroxymethyl)aminomethane (Tris), pH 7.9, 150 mM NaCl, 0.5 mM tris(2-carboxethyl)phosphine (TCEP) and at concentrations of 2.3, 4.6, 5.2, 2.5 and 11 mg/mL, respectively. MmR495A (no structure in PDB) was received from the lab of Prof. Gaetano Montelione (Center for Advanced Biotechnology and Medicine, Rutgers University) as both a solid lyophilisate (from 20 mM NH4OAc) that had absorbed water during transit and also as a frozen solution on ice containing 10 mM Tris, pH 7.5, 100 mM NaCl, 10 mM DTT, 0.02% NaN 3. Af1502 (PDB|5A1Q) was received from the lab of Dr. Jörg Martin (Max-Planck Institute for Developmental Biology, Tübingen) as a frozen solution of 30 mM MOPS, 250 mM NaCl, 10% glycerol, pH 7.2, 16 mg/mL. Laminin (PDB|4YEQ) was received from the lab of Prof. Deborah Fass (Department of Structural Biology, Weizmann Institute of Science) as a frozen solution on ice containing PBS and 10% glycerol, 2.4 mg/mL.
Four of the six designated targets (BACUNI_01052, RUMGNA_02398, SAV1486 and BACCAC_02064) were buffer-exchanged prior to cross-linking to remove Tris from the buffer. Buffer exchange was carried out using polyethersulphone (PES) ultracentrifugation devices for concentration of small-volume protein samples, Vivaspin 500, 5000 MWCO, GE Healthcare. Protein concentration was estimated using a Nanodrop 1000 Spectrophotometer from Thermo Fisher Scientific, measuring at 280 nm.
Each target was cross-linked using sulfo-SDA, using four different cross-linker to protein ratios (2:1, 1:1, 0.5:1 and 0.25:1, w/w) and four UV activation times (15, 30, 45 and 60 minutes). Cross-linking was carried out in two-stages: firstly sulfo-SDA, dissolved in cross-linking buffer (20 mM HEPES-OH, 20 mM NaCl, 5 mM MgCl 2, pH 7.8), was added to target protein (30 µg, 1 µg/µL) and left to react in the dark for 1h at room temperature. This allowed the reaction of lysine side chain amino groups but also hydroxyl groups in serine, threonine and tyrosine side chains, with the sulfo-NHS ester component of the cross-linker. The diazirine group was then photo-activated using UV irradiation, at 365 nm, from a UVP CL-1000 UV Crosslinker (UVP Inc.). Samples were spread onto the inside of Eppendorf tube lids by pipetting (covering the entire surface of the inner lid), placed on ice at a distance of 5 cm from the tubes and irradiated for either 15, 30, 45 or 60 minutes. Following the reaction, half of each reaction condition sample was then pooled as a “mixed” sample (a total of 240 µg). The resulting cross-linked mixtures were then separated by electrophoresis using a NuPAGE 4–12% Bis-Tris gel, ran using MES running buffer and stained using Imperial Protein Stain from Thermo Scientific, a Coomassie blue stain. Protein monomer bands were excised from the gel, cut into pieces and then washed to remove Coomassie staining. Proteins were reduced with 20 mM DTT, alkylated using 55 mM IAA and digested overnight using trypsin following standard protocols 7. Trypsin/Glu-C co-digestion (in-gel trypsin digestion, overnight at 37 °C followed by addition of Glu-C for 6 hours at room temperature) was used for mixed samples of Target 1 and Target 2. In addition, in-solution Glu-C digestion was used for mixed samples of Targets 2–4. Digests were desalted using self-made C18 StageTips 22 prior to mass spectrometric analysis.
Peptides were loaded directly onto a spray emitter analytical column (75 µm inner diameter, 8 µm opening, 250 mm length; New Objectives) packed with C18 material (ReproSil-Pur C18-AQ 3 µm; Dr Maisch GmbH, Ammerbuch-Entringen, Germany) using an air pressure pump (Proxeon Biosystems) 23. Mobile phase A consisted of water and 0.1% formic acid. Mobile phase B consisted of acetonitrile and 0.1% formic acid. Peptides were loaded onto the column with 1% B at 700 nl/min flow rate and eluted at 300 nl/min flow rate with a gradient: 1 minute linear increase from 1% B to 9% B; linear increase to 35% B in 169 minutes; 5 minutes increase to 85% B. Eluted peptides were sprayed directly into a hybrid linear ion trap - Orbitrap mass spectrometer (LTQ-Orbitrap Velos, Thermo Fisher Scientific). Peptides were analyzed using a “high/high” acquisition strategy, detecting peptides at high resolution in the Orbitrap and analyzing, also in the Orbitrap, the products of their CID fragmentation. Survey scan (MS) spectra were recorded in the Orbitrap at 100,000 resolution. The eight most intense signals in the survey scan for each acquisition cycle were isolated with an m/z window of 2 Th and fragmented with collision-induced dissociation (CID) in the ion trap. 1+ and 2+ ions were excluded from fragmentation. Fragmentation (MS2) spectra were acquired in the Orbitrap at 7500 resolution. Dynamic exclusion was enabled with 90 seconds exclusion time and repeat count equal to 1.
Mass spectrometric raw files were processed into peak lists using MaxQuant version 188.8.131.52 24 using default parameters, except the setting for “Top MS/MS peaks per 100 Da” being set to 100. Peak lists were searched against a database, comprising in each case only the sequence of the protein that was being analyzed using the cross-linking software Xi ( https://github.com/Rappsilber-Laboratory/XiSearch) for identification of cross-linked peptides. Sequences were provided by the CASP Organizing Committee and are available in the supplement. Search parameters were MS accuracy, 6 ppm; MS/MS accuracy, 20 ppm; enzyme, trypsin; specificity, fully tryptic; allowed number of missed cleavages, four; cross-linker, SDA; fixed modifications, none; variable modifications, carbamidomethylation on cysteine, oxidation on methionine, SDA-loop (SDA cross-link within a peptide that is also cross-linked to a separate peptide). Other SDA modifications (including those resulting from reaction with water and ammonia) were not included in the database search. In earlier work we identified very few such modifications and including these modifications served to increase search database size and also increase false positive identifications, which we were keen to avoid here. Linkage specificity for sulfo-SDA was assumed to be at lysine, serine, threonine, tyrosine and protein N-termini at one end, with the other end having no specificity, i.e. linking to any amino acid residue. A modified target-decoy search strategy was used to estimate FDR 7, 25 (Fischer and Rappsilber, unpublished observations ). In short, unique residue pairs are scored on supporting PSMs by:
Before scoring residue pairs and applying an FDR at their level, the dataset is pre-filtered by applying an FDR-based score cut-off for PSMs and a subsequent FDR-based score cut-off for unique peptide pairs (scored the same way as residue pairs based on supporting PSMs). This provides a means to do noise filtering and can increase the number of unique residue pairs that pass a given FDR. Optimal score cut-offs are automatically defined using xiFDR: https://github.com/lutzfischer/xiFDR.
The MS data have been deposited to the ProteomeXchange Consortium via the PRIDE partner repository with the dataset identifier PXD003643 26.
We had the following objectives for participating in the CASP experiment:
To accomplish these goals, the CASP Organizing Committee identified four CASP target proteins (Tx781, Tx808, Tx767, Tx812, ranging from 204–420 residues in size) whose structures were known to the organizers but neither to our laboratory nor the participating modeling groups. Figure 1 shows the organization and timetable of the experiment.
We cross-linked the CASP11 targets with the photoactivatable cross-linker sulfo-SDA 19. We used a panel of different cross-linker to protein ratios and UV activation times to maximize the number of unique cross-links. We digested cross-linked proteins using trypsin and in some cases with trypsin/Glu-C double digestion or Glu-C alone (see Supplemental Text for details). We then subjected the peptide mixture to LC-MS/MS mass spectrometric analysis without an additional enrichment of cross-linked peptides using on average 4.2 days for acquisition. The data were searched against databases derived from the target protein sequences using Xi 27. We assess confidence using a target-decoy approach (Fischer and Rappsilber, unpublished observations). We identified cross-links at 5, 10 and 20% FDR and submitted the results to the CASP organizers who made the data available to the modeling groups. At 5% FDR, we identified from 201–381 links for the target proteins. Thus, for the CASP proteins we identified from 0.63–1.2 links per residue, which is comparable to our previous HD-CLMS study on HSA 19 ( Table 1). The percentage of links with >11 residues sequence separation, which are most important for protein modeling, were also comparable (59–73% vs 66%, Table 2). Notably, the analysis was not nearing complete detection of linked residue pairs as additional runs kept adding further unique residue pairs, as seen from saturation analysis ( Figure 2). We validated our CLMS data against the crystal structures which became available after the CASP prediction season.
|Target protein||MS acquisition
|Links per residue
at 5% FDR (number
of residue pairs)
|Links per residue at
10% FDR (number
of residue pairs)
|Links per residue at
20% FDR (number
of residue pairs)
|HSA (585 AA)||12 days||0.85 (500)||1.51 (881)||2.56 (1495)|
|Tx781 (420 AA)||4.7 days||0.73 (305)||1.06 (444)||1.35 (565)|
|Tx808 (418 AA)||4.4 days||0.63 (265)||0.68 (286)||0.82 (342)|
|Tx767 (318 AA)||4.0 days||1.20 (381)||n.d.||2.26 (718)|
|Tx812 (204 AA)||3.8 days||0.99 (201)||1.30 (265)||1.77 (360)|
|Target protein||5% FDR||5–10% FDR||10–20% FDR|
|HSA (585 AA)||330 (66%) 1||292 (77%)||511 (83%)|
|Tx781 (420 AA)||189 (62%)||100 (72%)||99 (82%)|
|Tx808 (418 AA)||155 (59%)||15 (71%)||52 (93%)|
|Tx767 (318 AA)||277 (73%)||n.d.||234 (69%)|
|Tx812 (204 AA)||146 (73%)||48 (75%)||63 (66%)|
1Number of links >11 residues apart (percentage of links >11 residues apart of all links)
Our first objective is to compare the CLMS data with the crystal structures to test the robustness of high-density cross-linking in a blind experiment.
CLMS experiments do not necessarily reflect the structure of a single conformer but instead reflect the different conformations in the ensemble. Thus, conformational flexibility has to be taken into account when translating the observed cross-links into residue-residue distances. Here we translate observed links into a 25 Å bound on the distance and hence linkable by photo-CLMS using sulfo-SDA, based on a prior analysis of HSA 19 (in this study, 25 Å is the distance at which the observed Cα-Cα distance distribution merges with the distribution obtained from decoy matches).
With the exception of the first target, Tx781, the 5% FDR lists matched near perfectly to the crystal structures (Tx808 9%, Tx767 5% and Tx812 4% links >25 Å, respectively, averaging to 6% error) ( Figure 3 and Figure 4). This deteriorated slightly when considering 10% FDR data (19%, n.d., 8%; links >25 Å, respectively, averaging to 10.7% error) and further worsened for 20% FDR data (54%, 20%, 28%; links >25 Å, respectively, averaging to 34% error). We attribute the deviation of the computed to the experimentally assessed accuracy to our still small data sets. FDR using the target-decoy approach relies on large data sets. We can see that this condition is not perfectly fulfilled here. For example, in the case of Tx808 data with 20% FDR added only links with very low score to the 10% FDR list, indicating that the data had been exhaustively matched already at 10% FDR. Note that many links are also much shorter than the upper distance bound of 25 Å ( Figure 4).
One explanation for why the crystal structure of Tx781 did not support the CLMS data to the same degree as the other proteins is that the shipping conditions were problematic. The protein arrived defrosted to the laboratory and required buffer exchange from Tris to HEPES. Both might have compromised the integrity of the protein structure. Possibly as a result of this or due to cross-linking, the protein was seen as highly aggregated on SDS-PAGE ( Figure 3a). As a further possibility, the protein may have a different structure in solution from in crystal. Our current data do not allow these possibilities to be distinguished.
A limitation of our current workflow is that we are missing a site assignment scoring and hence do not control for site assignment errors. Importantly, this does not affect the FDR estimation (decoys model well the distribution of long distance and hence likely false links) and we showed in earlier work that we were able to model HSA domains despite site assignment ambiguities 19, nevertheless it may falsely elevate the total number of reported links.
In conclusion however, we find good agreement between photo-CLMS and crystallography in this blind study. This suggests that HD-CLMS produces robust residue-residue constraint data.
Our second objective was to test hybrid modeling methods on our high-density CLMS data, on very difficult modeling targets such as those used in CASP11. The proteins in CASP11 are difficult “free modeling” targets, because even state-of-the-art fold recognition methods are unable to confidently find template structures for template-based modeling. Thus, predictors might use ab initio structure prediction, template-based modeling, or a mix of the two approaches.
A full report of this experiment from the protein modeling perspective is published elsewhere 21. For the 19 groups that participated in the CLMS-driven and the normal CASP experiment (where no CLMS data is provided), the CLMS data slightly improved the GDT_TS of the predicted models from 36.4 to 38.1 for the first and from 40.9 to 42.0 for the best-of-five submitted models. The GDT_TS is a measure for the match of the prediction to the native structure and ranges from 0 (structures completely dissimilar) to 100 (perfect match). Overall, improvement in modeling accuracy by CLMS-driven predictions is very small and the results suggest no clear improvement.
One explanation for this result is that the CASP11 target proteins were too difficult to model, for current state-of-the-art protein structure prediction methods even with accurate residue-residue restraint data. We tested this hypothesis by re-running the modeling experiments with idealized residue-residue constraints taken from the crystal structures ( Figure 5). Note that we evaluated this experiment on the evaluation domains used in CASP11, which are comprised of the partial domains of the full-length protein targets. Even in this idealized scenario, only two out of seven evaluation domains were “foldable” (GDT_TS of the best predicted structural model is 50 or higher). Since the HD-CLMS constraints are inferior to the idealized constraints, both in density and spatial resolution, this data supports our assumption that the CASP11 targets were too difficult to fold for current structure prediction algorithms.
Our third objective was to use the CASP experiment to identify any methodological shortcomings of our cross-linking approach. Our analysis of the high-density CLMS data revealed two potential issues with the current method: Uneven sequence coverage caused by uneven distribution of cleavage sites and cross-link bias against β-sheet regions.
The issue of uneven sequence coverage was most prevalent for target Tx781 ( Figure 6a). Our analysis of the tryptic digestion sites shows that the absence of observed residue pairs correlates with low frequency of tryptic cleavage sites: up to residue 180 there are 18 tryptic cleavage sites resulting in 0.11 cross-links per residue. For the remaining 224 residues, there were 31 tryptic digestion sites which results in a cross-link density of 0.69 cross-links per residue. The interplay of lysine and arginine residue positions influences whether a cross-linked peptide can be observed for mass spectrometry. For example, the resulting tryptic peptide of cross-linked K126 would be 60 residues long, which is prohibitively long for ordinary mass spectrometry analysis. From the K/R distribution, we estimate a total of 111 residues (62% of the sequence up to residue 180, 26% of the total protein sequence) are thus theoretically inaccessible via trypsin digestion.
We also tested the use of alternative proteases and double-digestion strategies to combat the issue of uneven sequence coverage ( Supplemental Table 1– Supplemental Table 4). Alternative digestion strategies including Glu-C, rather than relying on digestion by trypsin alone increased the number of cross-links ( Table 3). This was particularly striking for the N-terminal domain of Tx781. Glu-C digestion increased the cross-link density from 0.11 to 0.43 links per residue at 5% FDR for the first 180 residues. Thus, our data suggests that alternative or multiple proteases might improve the lack in cross-link density in some regions that is caused by uneven distribution of tryptic digestion sites.
|Target protein||5% FDR
identified of total
|Tx781 (420 AA)||305||119||39%|
|Of this in N-term.
|Tx808 (418 AA)||265||45||17%|
|Tx767 (318 AA)||381||111||29%|
|Tx812 (204 AA)||201||36||18%|
aAll digestion methods involving use of Glu-C (including trypsin/Glu-C co-digestion (Tx781 and Tx808), and in-solution Glu-C digestion (Tx808, Tx767 and Tx812).
Another issue that we found was an apparent bias against cross-links in β-sheet regions. An extreme example is the target Tx808, where 54% of the residues in the crystal structure have β-sheet structure. The cross-links of this protein are predominantly in the loop region ( Figure 4b). We would expect 80% of the cross-linked residue pairs to have at least one β-strand residue if cross-linking would be unbiased with regard to secondary structure. However, we find only 64% of the cross-linked residue pairs to contain a β-sheet residue (170 of 265; 5% FDR). This β-sheet bias also holds for targets Tx767 and Tx812 ( Figure 7a and b). We exclude Tx781 from analysis because of the issues discussed earlier. We hypothesized that this bias against β-sheet residues might be caused by lack of tryptic cleavage sites, but found that this would only explain the apparent lack in β-sheet cross-links for Tx767 ( Figure 7c). We next considered relative solvent accessibility (RSA) 28, 29 and whether this could explain discrepancies in expected and observed cross-link patterns. On average, β-strand residues have much lower relative solvent accessible areas in each of the targets (16–19%) as opposed to other residues (34–40%) ( Figure 7d and e). Consequently, both lack of anchoring residues, cleavage sites and lower RSA may contribute in different ratios and in different proteins to the problem of β-sheet analysis by CLMS. In addition, there is a fundamental issue concerning the use of sulfo-SDA as cross-linker ( Figure 6b). The α-carbon distance between adjacent hydrogen bonded beta strands is in the order of 5 Å 30, however the upper limit distance boundary defined by sulfo-SDA is in the range of 20 to 25 Å. This covers as much as five beta strands. Consequently, sulfo-SDA, especially at current data density, is insufficient to reveal the topology of β-strands in a β-sheet.
Our test of high-density CLMS under the auspices of CASP11 led to three major insights. HD-CLMS can be conducted in under a week and delivers highly reliable structural data on proteins in solution. Nevertheless, while sulfo-SDA proved very useful in solving the structure of the alpha-helical domains of HSA 19, HD-CLMS at large may require major developments to achieve a similar success for β-sheet proteins. Sequence coverage and spatial resolution pose a technological challenge and spell out the agenda for future developments. Finally, HD-CLMS is part of a hybrid workflow that relies on structure modeling. Future blind experiments to assess the current value of this hybrid approach need to select protein targets with structures that can be modeled at least when ideal data is available.
The mass spectrometry proteomics data have been deposited in the ProteomeXchange Consortium ( http://proteomecentral.proteomexchange.org) via the PRIDE partner repository with the dataset identifier PXD003643.
We would like to thank the CASP11 Organizing Committee ( www.predictioncenter.org/casp11/index.cgi), in particular Krzysztof Fidelis and Andriy Kryshtafovych for their coordination efforts, PDB for their cooperation in delaying the release of one target by one week and the following researchers for providing protein targets: Mark Wilson and Janani Prahlad (Department of Biochemistry/Redox Biology, University of Nebraska), Ashley M. Deacon and Qingping Xu (Joint Center for Structural Genomics (JCSG), Stanford Synchrotron Radiation Lightsource, Stanford University), Gaetano Montelione and Rong Xiao (Center for Advanced Biotechnology and Medicine, Rutgers University), Jörg Martin (Max-Planck Institute for Developmental Biology, Tübingen), Deborah Fass (Department of Structural Biology, Weizmann Institute of Science). We acknowledge the PRIDE team for the deposition of our data to the ProteomeXchange Consortium.
[version 1; referees: 1 approved, 2 approved with reservations]
This work was supported by the Wellcome Trust , , ; the NIH [1 R01 GM076706]; and the Alexander-von-Humboldt foundation through funding from the German Federal Ministry of Education and Research (BMBF).
The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Supplemental Tables 1–4. Zip file consisting of .csv supplemental tables 1 to 4. Tables are made up of lists of LC-MS runs for each of the targets 1 to 4, with the cross-linker:protein ratio and UV activation time used for the sample in each LC-MS run, as well as the protease(s) used for digestion.
Supplemental Text. Supplemental Text for "Blind testing cross-linking/mass spectrometry under the auspices of the 11 th critical assessment of methods of protein structure prediction (CASP11)".
Protein sequences of Targets 1–4. Protein sequences of the four target proteins used in the study "Blind testing cross-linking/mass spectrometry under the auspices of the 11 th critical assessment of methods of protein structure prediction (CASP11)".
The manuscript titled “Blind testing cross-linking/mass spectrometry under the auspices of the 11 th critical assessment of methods of protein structure prediction (CASP11)” by Belsom et al. describes a blind study to test a hybrid approach using cross-linking/mass spectrometry and ab initio modeling (CASP11) in structure prediction. The hybrid approach was proven to be successful on a mostly a-helical protein (HSA) previously published by the group. The new study with 4 proteins from a structural genomics center shows that the CLMS data provide limited or no improvement in modeling accuracy by CASP11. The authors attribute the difference to two major factors. One is the uneven sequence coverage by trypsin (solvable) and the other is the predominant b-sheet structure in the target proteins as opposed to mostly helical structure in HSA. While one of the proteins does have high percentage of the residues in b-sheet (54%), the other two analyzed in the paper have 22 and 37% of the residues in b-strand structure. If the method does not work with these mixed a/b proteins, it will require some major improvement to be effective in structure predication.
It should be emphasized in fact that the negative results seen here outline the specific milestones that have to be overcome.
Other flaws in the manuscript:
I have read this submission. I believe that I have an appropriate level of expertise to confirm that it is of an acceptable scientific standard, however I have significant reservations, as outlined above.
In their manuscript “Blind testing cross-linking/mass spectrometry under the auspices of the 11 th critical assessment of methods of protein structure prediction (CASP11)”, submitted for publication in Welcome Open Research, Rappsilber and coworkers have applied the high density cross-linking/mass spectrometry (HD-CLMS) method on four proteins provided by CASP. Using provided cross-linking data, they were able to generate proteins 3D models with slightly improved GDT_TS scores. While the experimental studies appear to be technically solid, authors are asked to answer following comments before indexing of the article.
We have read this submission. We believe that we have an appropriate level of expertise to confirm that it is of an acceptable scientific standard, however we have significant reservations, as outlined above.
The manuscript by Belsom et al. is an important benchmark in two ways:
The manuscript is very well written and clear. I have only two minor comments:
a. In the legend of Fig. 3b – I think the writing should be “cross-linking distances under 25Angs” and not “over 25Angs”.
b. At the top of page 9 the authors refer to “uncertainty in the site assignment”. I assume it means the uncertainty in the exact residue to which the diazarine is cross-linked to. Perhaps some clarification can be added to the text.
I have read this submission. I believe that I have an appropriate level of expertise to confirm that it is of an acceptable scientific standard.