Thalidomide and its derivatives lenalidomide and pomalidomide (IMiDs) are effective treatments of haematologic malignancies. It was shown that IMiDs impart gain-of-function properties to the CUL4-RBX1-DDB1-CRBN (CRL4CRBN) ubiquitin ligase that enable binding, ubiquitination and degradation of key therapeutic targets such as IKZF1, IKZF3 and CSNK1A1. While these substrates have been implicated as efficacy targets in multiple myeloma (MM) and 5q deletion associated myelodysplastic syndrome (del(5q)-MDS), other targets likely exist. Using a pulse-chase SILAC mass spectrometry-based proteomics approach, we demonstrate that lenalidomide induces the ubiquitination and degradation of ZFP91. We establish ZFP91 as a bona fide IMiD-dependent CRL4CRBN substrate and further show that ZFP91 harbours a zinc finger (ZnF) motif, related to the IKZF1/3 ZnF, critical for IMiD-dependent CRBN binding. These findings demonstrate that single time point pulse-chase SILAC mass spectrometry-based proteomics (pSILAC MS) is a sensitive approach for target identification of small molecules inducing selective protein degradation.
The ubiquitin proteasome system (UPS) constantly remodels the proteome to regulate a plethora of cellular processes1,2,3. In the UPS, ubiquitin is covalently coupled to a substrate lysine by activity of an E1 (ubiquitin activating enzyme), E2 (ubiquitin conjugating enzyme) and E3 (ubiquitin ligase) enzyme cascade. Specificity in the UPS is largely conferred by E3 ligases, of which there are more than 600 in the human genome4.
Thalidomide and its derivatives lenalidomide and pomalidomide (collectively known as IMiDs for immune-modulatory drugs), while initially marketed as sedatives found to cause severe teratogenic side effects, are widely used to treat haematologic malignancies, including multiple myeloma (MM) and 5q deletion associated myelodysplastic syndrome (del(5q) MDS)5,6,7,8. Lenalidomide binds to the ubiquitin ligase CRL4CRBN and exhibits dual activity by inhibiting CRL4CRBN from ubiquitinating endogenous substrates such as MEIS2 (refs 9, 10), while simultaneously promoting the CRL4CRBN-dependent ubiquitination and degradation of IKZF1 (Ikaros), IKZF3 (Aiolos) and Casein kinase 1 alpha (CSNK1A1)10,11,12,13,14. IKZF1 and IKZF3 have been implicated in MM anti-proliferative effects of IMiDs, and CSNK1A1 has been shown to be the efficacy target of lenalidomide in del(5q)-MDS8. Recent reports have further demonstrated that lenalidomide disrupts the ubiquitin-independent regulation of CD147 and MCT1 by CRBN15 and that glutamine synthetase (GS) is ubiquitinated by CRL4CRBN in an IMiD-independent fashion16. However, the pleiotropic effects of IMiDs and the largely unexplained adverse effects such as the profound teratogenicity and neurotoxicity suggest that other substrates likely exist. To identify novel CRL4CRBN substrates regulated by lenalidomide, we performed proteomics studies in non-hematopoietic cell lines to avoid masking of results with the dominant presence of IKZF1/3 in hematopoietic tissues.
Mass spectrometry-based methods have become standard for the identification of E3 ubiquitin ligase substrates and were successfully applied to various classes of ligases, such as the Cullin RING ligase family SCF/CRL1 (refs 17, 18, 19). However, other ligase families have proven recalcitrant to commonly used methods such as affinity-purification mass spectrometry, di-Gly proteomics or whole proteome relative quantification. Common complications for the identification of ubiquitin ligase substrates are secondary effects, such as transcriptional response or changes to translation. For profiling of protein stability-directed drugs, such as lenalidomide, most secondary effects can be reduced through relatively short drug treatments (<24 h) compared to the typical treatment times for RNAi or genetic inactivation (typically >48 h). However, faced with the challenge of relatively small changes to total protein levels, we reasoned that an approach directed at measuring changes to protein turnover in response to drug treatment would provide increased sensitivity compared to relative quantification of total protein abundance. Such a sensitive method would also be valuable to a growing field of drug development efforts directed at protein degradation20,21,22,23.
Pulse-chase experiments, performed with 35S isotope labelling or through blockade of translation by treatment with cycloheximide (CHX), are considered the gold standard method to investigate protein stability. Modern mass spectrometry combined with stable isotope labelling (SILAC) can principally be used to perform pulse-chase experiments on a proteome-wide scale, and this has been applied to interrogate global protein synthesis and decay rates24,25,26,27,28. However, such experiments typically involve multiple time points.
Here we show that direct measurement of changes in protein stability in a single time point mass spectrometry experiment is a sensitive and robust alternative to identify targets of lenalidomide. The method is based on temporally controlled incorporation of heavy amino acids by changing the growth medium (pSILAC) simultaneously with applying the desired perturbation, such as treatment with a drug. Samples are subjected to shotgun proteomics utilizing liquid chromatography coupled tandem mass spectrometry (LC-MS/MS)29. The pre-existing (light amino acid containing) and newly synthesized (heavy amino acid containing) protein species can be differentially quantified based on their characteristic mass difference to derive heavy to light (H/L) protein ratios30. In such an experimental design, and assuming constant incorporation rate, logarithmic H/L ratios should increase linearly over time. H/L protein ratios represent a quantitative measure of protein stability and differences between treated and control cells can be used to identify drug-induced changes to protein turnover, such as induced degradation of target proteins. We demonstrate that a single time point pSILAC experiment is sufficient to identify CSNK1A1 along with new substrate candidates. We further show that the zinc finger (ZnF) protein, ZFP91, a putative ubiquitin ligase31,32, is a bona fide lenalidomide-dependent CRL4CRBN substrate.
Identification of novel CRL4CRBN targets through pSILAC MS
We sought to explore a single time point pSILAC approach, which would increase the depth of proteome profiling and significantly reduce the required machine time compared to multi time point experiments. To understand the scopes and limitations of this approach, we performed a direct comparison with multi time point pSILAC and quantified the changes to total protein abundance using tandem mass tags (TMT)33.
To generate a reference data set for direct comparison, we first designed a multi time point pSILAC experiment. We used metabolic pulse labelling with heavy amino acids to measure protein turnover in growing HEK293T cells treated with 30 μM lenalidomide or dimethyl sulfoxide (DMSO) control (Fig. 1a). The high concentration of lenalidomide was chosen to achieve maximum response in a short time window and thereby aid substrate identification. HEK293T cells were chosen to bias the experiment towards targets beyond the well-studied transcription factors IKZF1 and IKZF3 that are found explicitly in hematopoietic lineages34. Cells were collected in duplicates at three time points, 6 h (T6), 10 h (T10) and 16 h (T16) post treatment with lenalidomide or DMSO and parallel metabolic labelling. To prevent arginine to proline conversion, a pervasive problem in SILAC, the cell culture medium was supplemented with excess unlabelled proline. Label swap experiments at the T6 and T10 time points were performed and analysed to exclude the possibility of SILAC label artefacts (growth medium changing from H/L isotope label on treatment, see also Supplementary Figs 1a–c and 2a–c). While we observe a small systematic offset in H/L protein ratios comparing forward to reverse experiments (most pronounced at early time points), the overall correlation between forward and reverse experiments and random spot checks suggest that label artefacts can be neglected for further analysis. Whole-cell lysates were pre-fractionated into 15 fractions by SDS–PAGE and tryptic peptides subjected to LC-MS/MS analysis on an Orbitrap VELOS platform (see Methods section). Mass spectrometry data were analysed with the MaxQuant software35. We identified 100,763 peptide sequences, which were assigned to 6,328 unique protein groups (false discovery rate <1% on peptide and protein level; requiring min one unique peptide quantified for a protein to be included).
Polypeptides synthesized after drug treatment and metabolic labelling will predominantly incorporate heavy amino acids, thus the H/L protein ratios can serve as a direct readout of protein turnover (Fig. 1b–d)24. H/L protein ratios were quantile normalized (Supplementary Fig. 2a,b) and showed high correlation coefficients across replicates and time points (around 0.9, Supplementary Fig. 2c), which reflects the expected small overall perturbation induced by the drug, and the consistent rank order of H/L protein ratios over time. Of the 6,328 unique protein groups identified, the 2,837 quantified across all time points and replicates were selected to subsequently calculate protein half-lives as previously described24. Additional quality filtering was applied to reject proteins for which the linear regression resulted in r2<0.9 for a total of 2,759 remaining protein groups (Fig. 1e). Due to the experimental design geared towards drug effects, the shortest time point was set at 6 h post treatment, compromising the ability to quantify very short-lived proteins. We hypothesized that proteins differentially degraded in a lenalidomide-dependent manner should exhibit differences in protein half-lives and would thus be candidate substrates. Comparing global protein half-lives of lenalidomide treated and control cells (Fig. 1e), we identified casein kinase 1 alpha (CSNK1A1) as the most affected protein, which we validated elsewhere11 in parallel to a study published by Krönke et al.12, who linked CSNK1A1 degradation to 5q-MDS efficacy of lenalidomide. Analysis of the full data set confirmed that the effect on CSNK1A1 is more pronounced and clearly identified at the late time point (Fig. 1f), supporting the concept of single time point measurements for target identification. To test the proposed approach of a single time point pSILAC experiment, we analysed the T16 time point (two replicates) alone by calculating moderated t-test P values using the limma package36. We included all protein groups that were identified with at least three unique peptides and quantified with more than two peptides (n=2,654). Comparison of the T16 H/L protein ratios of lenalidomide or DMSO-treated samples identifies CSNK1A1, ZFP91 and HEXB as significantly downregulated targets along with a number of proteins whose turnover is reduced on drug treatment (Fig. 1g and Supplementary Table 2).
Single time point pSILAC mass spectrometry
Next, we sought to assess the robustness of our approach by conducting a single time point experiment in a different cell line (Hct116), with four replicate measurements at 16 h post treatment, of which, two were designed as label swap experiments (see Supplementary Fig. 1a–c). Hct116 cells were treated with either 30 μM lenalidomide or DMSO control concomitant with transfer into medium containing amino acids labelled with heavy isotopes (similar to the first experiment). Cells were collected 16 h post treatment and split for pSILAC MS and RNA-seq experiments (Fig. 2a). Samples for MS analysis were pre-fractionated and subsequent analyses were performed on an Orbitrap Fusion mass spectrometer. LC-MS/MS data were processed with MaxQuant35, identifying 108,546 peptide sequences assigned to 7,759 unique protein groups (false discovery rate <1% on peptide and protein level; requiring a minimum of one unique peptide per protein). H/L protein ratios (H/L protein ratios of label swap experiments were inverted) were log2 transformed and quantile normalized (Supplementary Fig. 3a–c). We restricted our initial analysis to protein groups quantified with at least three unique peptides in all experiments (n=3,352). Comparing averaged log2 H/L protein ratios of lenalidomide treated or DMSO control samples (Pearson’s correlation coefficient of 0.99), we identified CSNK1A1 as the most strongly affected protein (Fig. 2b), which is in accordance with the pSILAC experiments in HEK293T. We next assessed the statistical significance of drug-induced changes to protein turnover, which is reflected in the difference between H/L protein ratios of DMSO and lenalidomide samples. We calculated intensity binned (10 bins of equal size) P values using the significance B approach35 (Fig. 2c), which reflects the commonly observed dependence of H/L protein variability on signal intensity. In this approach, we identified additional proteins to exhibit significantly altered H/L protein ratios, most notably ZFP91 (Fig. 2b,c and Supplementary Table 3). To exclude the possibility of the drug treatment altering RNA levels, we performed RNA-seq on the samples used for mass spectrometry. The resulting data were analysed both at the levels of exons and introns, which allows the detection of both transcriptional and post-transcriptional changes37. However, very few genes displayed a significant change in transcript levels, suggesting that transcriptional changes can still be neglected at the T16 time point (Fig. 2d). Overall, the experimental design significantly reduced the required machine time compared to multi time point experiments. Notably, CSNK1A1 and ZFP91 were both also identified by analysing forward and reverse experiments individually (two replicates each), which indicates that two replicates would be sufficient to generate a list of candidates for further validation (Supplementary Fig. 1b,c).
Comparing changes in protein stability and abundance
Next, we directly compared single time point pSILAC MS to measuring changes in total protein levels by TMT. We treated HEK293T cells for 16 h with 30 μM lenalidomide or a DMSO control (two biological replicates, consistent with the treatment for pSILAC, except that we did not exchange the growth medium for heavy amino acids). After lysis, reduction, alkylation and tryptic digest, peptides were subjected to TMT labelling, pre-fractionation and subsequent mass spectrometry analysis using a MS3 protocol on an Orbitrap Fusion mass spectrometer (see Methods section)38. Following scaling and normalization of reporter ion intensities, we performed statistical analysis by calculating moderated t-test P values using the limma package36 (Fig. 3a). While the two validated substrates CSNK1A1 and ZFP91 show induced degradation by lenalidomide, the observation, however, is not significant and neither CSNK1A1 nor ZFP91 were reliably identified as a drug target based on the TMT data set. In contrast, within the pSILAC HEK293T T16 samples as well as in the Hct116 T16 samples (see Figs 1g and 2b,c and Supplementary Fig. 1b,c), we unambiguously identify CSNK1A1 and ZFP91.
We conclude that for the target identification of small molecules that exert their effects by altering protein stability, measuring protein turnover provides a sensitive and robust alternative compared to relative quantification of changes to protein abundance.
Combining multiple data sets can further increase robustness
We next explored the potential for combining data from multiple data sets to enhance the robustness of target identification. To do so, we utilized a linear model approach as implemented in the limma package36 and frequently employed for the analysis of gene expression data (see Methods section; and Supplementary Table 1 for design matrix). This framework allows modelling of both, the general changes to log2 H/L protein ratios over time and the influence of the drug treatment on these changes. When applied to H/L protein ratios of all forward pSILAC experiments (proteins with unique peptides <3 or missing values were excluded, resulting in 3,535 proteins analysed), we find CSNK1A1 and ZFP91 as the two most significant proteins (P<0.0005 and log-fold change >±0.5), with log2 fold changes of 0.72 and 0.57, respectively (Fig. 3b, Table 1 and Supplementary Table 4). Therefore, this approach is suitable to combine data from biological replicates and together with the previous results, prompted us to further validate ZFP91 as a novel lenalidomide-induced target of CRL4CRBN.
ZFP91 is a lenalidomide-dependent CRL4CRBN substrate
ZFP91 is a ZnF protein and putative ubiquitin ligase31,32. To recapitulate our mass spectrometry results, we treated MM.1S cells with increasing concentrations of lenalidomide, thalidomide or with DMSO control and performed western blot analysis. We found a dose-dependent decrease of ZFP91 protein when treated with lenalidomide (Fig. 4a). We next examined the effect of lenalidomide on ZFP91 half-life in cells, by performing CHX chase experiments in HEK293T and SK-N-DZ cells (SK-N-DZ were selected for higher levels of CRBN9 and to validate the results in a cell line different from the cell lines used for mass spectrometry experiments). Following treatment with 50 μg ml−1 CHX and increasing concentrations of lenalidomide or thalidomide, we found that ZFP91 protein levels were largely depleted after 6 h of treatment with lenalidomide in a dose-dependent manner (Fig. 4b,c). Greater depletion was observed in SK-N-DZ cells, in accordance with the higher levels of CRL4CRBN ligase. Thalidomide in contrast had very little effect on the stability of ZFP91, similar to what has been previously observed for the ZnF proteins IKZF1 and IKZF3 (refs 13, 14, 39). We next confirmed that lenalidomide-dependent degradation of ZFP91 was abrogated by treatment with the proteasome inhibitor bortezomib (Fig. 4d, lanes 4–5) and the NEDD8-activating enzyme inhibitor MLN4924 (Fig. 4d, lanes 6–7), in line with a Cullin RING ligase and proteasome-dependent mechanism. To confirm the dependence of ZFP91 degradation on CRL4CRBN, we utilized CRISPR/Cas9 genome editing to generate two independent pools of HEK293T cells with genetic inactivation of CRBN. Treatment of these cells did not result in altered stability of ZFP91, which in contrast was readily degraded in parental HEK293T cells (Fig. 4e).
We next examined if CRL4ACRBN binds to and ubiquitinates ZFP91 in a fully recombinant system. We subjected insect cell expressed and purified ZFP91 to in vitro ubiquitination by purified recombinant CRL4ACRBN and found that in accordance with the cellular data, presence of lenalidomide promotes ubiquitination of ZFP91 in a dose-dependent manner (Fig. 5a, lanes 1–7). We further found that the close derivatives thalidomide and pomalidomide also promote the ubiquitination of ZFP91 in vitro.
This prompted us to characterize the binding of ZFP91 to CRL4ACRBN in vitro. We measured the affinity of biotinylated ZFP91 to fluorescently labelled CRL4ACRBN using time-resolved fluorescence energy transfer (TR-FRET)11. In presence of saturating concentrations of lenalidomide, we confirmed a tight association of ZFP91 with CRL4ACRBN with an apparent dissociation constant (KDapp) of 107±4 nM (Fig. 5b and Methods section). However, no binding was observed in the absence of compound. We had previously shown that CSNK1A1 and IKZF1/3 bind CRBN through a β-hairpin loop11, a structural feature also observed in GSPT1, the CRL4CRBN substrate dependent on the IMiD analogue CC885 (ref. 40). Similar to IKZF1/3, ZFP91 contains ZnF domains, and sequence comparison reveals that ZnF4 of ZFP91 (residues 400–422) shares a key glycine with ZnF2 of IKZF1 (Fig. 5c). To test if ZnF4 is responsible for binding to CRL4CRBN, we mutated ZFP91 residue histidine 418 (one of the zinc-coordinating residues) to alanine (H418A), to disrupt the structural integrity of the ZnF4 domain. To test the effect on binding, we compared IMiD-induced binding of ZFP91 wild type and H418A mutant to CRL4ACRBN. While we observe dose-dependent binding of wild-type ZFP91 to CRL4ACRBN, the H418A mutation largely disrupts binding of ZFP91 to CRL4CRBN (Fig. 5b,d). In accordance with the similarity to IKZF1/3, we found that thalidomide, lenalidomide and pomalidomide promote binding of ZFP91 to CRL4ACRBN in vitro, however, the potency of the compounds relative to each other slightly differs from what was observed for IKZF1/3 (ref. 11). Following this observation, we next sought to test if pomalidomide and thalidomide would also promote ZFP91 degradation in cells. We treated MM.1S cells with increasing concentrations of thalidomide, lenalidomide and pomalidomide and found that lenalidomide and pomalidomide promote ZFP91 degradation to a similar extent, while the effect of thalidomide is minimal (Fig. 5e). This is in accordance with what has been reported for IKZF1/3 and could be a result of thalidomide being significantly less stable in cell culture medium than lenalidomide and pomalidomide9,13,14. We conclude that ZFP91 represents a bona fide lenalidomide-induced substrate for CRL4CRBN. Based on recent structural studies of the CRBN–lenalidomide–CSNK1A1 and CRBN–CC885–GSPT1 complexes11,41, we propose that a common sequence motif exists for IMiD-dependent binding of ZnF containing substrates to CRL4CRBN (Fig. 5c).
The increasing number of small molecules directed at altering the stability and degradation of protein targets20,21,22,23,42, and natural products with potential activity towards protein stability43, require large-scale and proteome-wide methods to interrogate global on- and off-target effects. Here we introduce a novel approach to detect global changes to protein turnover in a single time point pSILAC mass spectrometry-based proteomics experiment. While it should be noted that single time point pSILAC does not report precise protein half-lives, and differences to H/L ratios can be the product of multiple effects (such as induced protein degradation/stabilization, altered translation or transcriptional effects); we demonstrate that the combination of short drug treatment and RNA-seq can largely mitigate these potential sources of false positives. The combination of pSILAC with TMT44 could further reduce the required machine time by combining replicates and multiple conditions into a single mass spectrometry experiment. However, such a strategy would likely come at the cost of sequencing depth due to necessary fragmentation of both (heavy and light) SILAC pairs to achieve TMT quantification. An alternative approach for a higher level of multiplexing could be neutron-encoded mass signatures SILAC (NeuCode-SILAC)45, which similarly to conventional SILAC can be applied in a pulsed manner.
By applying pSILAC to the potent anti-cancer therapeutic lenalidomide, we demonstrate that a single time point experiment could identify ZFP91 as novel lenalidomide-dependent CRL4CRBN substrate. ZFP91 and the known target CSNK1A1 were consistently detected as neo-substrate candidates in all single time point pSILAC experiments. While calculated protein half-lives from the multi time point experiment robustly identified CSNK1A1, ZFP91 was dropped from half-life calculation due to missing values at one of the time points. Characterization of the ZFP91 interaction with CRL4CRBN shows that a common structural motif in the ZnF4 and ZnF2 domains of ZFP91 and IKZF1/3, respectively, mediates a high-affinity interaction with a CRL4CRBN-IMiD complex. The plethora of ZnF proteins in the human proteome, together with the tolerance for amino-acid variation increases the probability that even more targets of IMiD-induced and CRL4CRBN-mediated degradation exist.
Compounds, enzymes and antibodies
Thalidomide (HY-14658), lenalidomide (HY-A0003), pomalidomide (HY-10984), MLN4924 (HY-70062) and bortezomib (HY-10227) were purchased from MedChem Express (MCE, USA). All compounds were dissolved in DMSO at various concentrations. Due to limited stability of thalidomide in aqueous solutions9, all required dilutions and cell culture media containing compounds were prepared fresh. HEK293T, SK-N-DZ, MM.1S and Hct116 cell lines were purchased from ATCC and cultured according to ATCC instructions. Cell lines were routinely tested for mycoplasma contamination using the MycoAlert detection kit (Lonza). Arginine and lysine-free cell culture medium, dialysed foetal bovine serum and amino acids for pulse-SILAC mass spectrometry were purchased from Cambridge isotope (Cambridge isotope laboratories, USA). Proteins were tested for >99% SILAC amino-acid incorporation after six–ten passages by mass spectrometry. Sequencing grade modified trypsin (V5117) was purchased from Promega (Promega, USA) and mass spectrometry grade lysyl endopeptidase from Wako (Wako Pure Chemicals, Japan). Primary and secondary antibodies used included anti-ZFP91 at 1:100–1:500 dilution (ab30970, abcam), anti-ZFP91 at 1:250–1:5,000 dilution (A303-245A, Bethyl Laboratories), anti-CRBN at 1:250 dilution (NBP1–91810, Novus), anti-GAPDH at 1:10,000 dilution (G8795, Sigma), IRDye680 Donkey anti-mouse at 1:10,000 dilution (926–68072, LiCor) and IRDye800 Goat anti-rabbit at 1:10,000 dilution (926–32211, LiCor). Ubiquitination enzymes Uba1, UbcH5a and ubiquitin were purchased from Boston Biochem.
HEK293T and Hct116 cells were cultured in L-arginine and L-lysine-free DMEM supplemented with dialysed foetal bovine serum, 2 mM L-glutamine and unlabelled L-arginine and L-lysine. Cells were grown to 40–50% confluency and the medium exchanged for DMEM supplemented with heavy L-arginine (13C6, 15N4—R10) and heavy L-lysine (13C6, 15N2—K8) to obtain heavy SILAC medium. Simultaneously, the medium was either supplemented with 30 μM lenalidomide (100 mM solution in DMSO) or the equivalent amounts of DMSO as control. Cells were incubated at 37 °C, 5% CO2 and collected at various time points by two washes with phosphate-buffered saline and direct addition of lysis buffer. If samples were split for parallel RNA-seq, cells were washed twice with phosphate-buffered saline, (Gibco) and split into two halves before lysis or RNA extraction. Total RNA was extracted using the RNeasy Mini Kit (Qiagen) following the manufacturer’s instructions.
Constructs and protein purification
Human DDB1, human CRBN, human CUL4A and mouse RBX1 were subcloned into pAC-derived vectors46 and recombinant proteins expressed as N-terminal His6 fusion proteins in Trichoplusia ni High Five insect cells using the baculovirus expression system (Invitrogen)9. Recombinant CRL4ACRBN complex was purified through sequential Ni-NTA affinity, anion exchange (poros 50HQ) and size exclusion (Superdex 200) chromatography. In vitro neddylation was carried out as described9,11, CRL4ACRBN was incubated with a reaction mixture containing Alexa488-NEDD8(M1C) at 3.8 μM, NAE/UBA1 (E1) at 50 nM, and UBC12 (E2), 1 mM ATP, 50 mM Tris pH 7.5, 100 mM NaCl, 2.5 mM MgCl2, 0.5 mM DTT and 5% (v/v) glycerol for 2 h at room temperature. Neddylated CRL4ACRBN was purified by size exclusion chromatography. Full-length human ZFP91 was obtained as synthetic codon optimized gBlock from IDT (IDT, USA) and cloned into pAC-derived vectors46. Mutant ZFP91 H418A was derived from this construct by Q5 mutagenesis (NEB, USA). Recombinant ZFP91 was expressed as N-terminal StrepII fusion protein in Trichoplusia ni High Five insect cells using the baculovirus expression system (Invitrogen). For purification of StrepII-ZFP91, cells were lysed by sonication in lysis buffer (50 mM Tris-HCl pH 8.0, 200 mM NaCl, 5 mM 2-mercaptoethanol (BME), 1 mM phenylmethylsulfonyl fluoride, 0.1% Triton X-100 and 1 × protease inhibitor cocktail (Roche). Following ultracentrifugation, the soluble fraction was passed over Strep-Tactin Sepharose (IBA) and eluted with 2.5 mM D-desthiobiotin in wash buffer (50 mM Tris-HCl, 200 mM NaCl, 5 mM BME). The affinity purified protein was diluted to 50 mM NaCl with dilution buffer (50 mM Tris-HCl pH 8.5, 0.5 mM tris(2-carboxyethyl)phosphine (TCEP)) and further purified via anion exchange chromatography (Poros 50HQ) with a linear gradient of 0–80% buffer B (50 mM Tris-HCl pH 8.5, 1 M NaCl, 0.5 mM TCEP) in buffer A (50 mM Tris-HCl pH 8.5, 25 mM NaCl, 0.5 mM TCEP) and subjected to size exclusion chromatography in 50 mM HEPES pH 7.4, 200 mM NaCl and 0.5 mM TCEP. The protein containing fractions were pooled, concentrated using ultrafiltration (Millipore) and flash frozen in liquid N2. Proteins were stored at −80 °C.
Biotinylation of ZFP91
Purified StrepII-Avi-tagged wild-type or mutant ZFP91 were biotinylated in vitro at a concentration of 5–20 μM by incubation with final concentrations of 2.5 μM BirA enzyme and 0.2 mM D-biotin in 50 mM HEPES pH 7.4, 200 mM NaCl, 10 mM MgCl2, 0.25 mM TCEP and 20 mM ATP. The reaction was incubated for 1 h at room temperature and stored at 4 °C for 14–16 h. Biotinylated proteins were purified by gel filtration chromatography and stored at −80 °C.
TR-FRET binding assay
Increasing concentrations of Alexa488-NEDD8-labelled CRL4CRBN (N8CRL4CRBN)47 were added to pre-mixed biotinylated ZFP91 at 100 nM, terbium-coupled streptavidin at 2 nM (Invitrogen) and IMiDs at 5 μM (final concentrations) in 384-well microplates (Greiner, 784076) in a buffer containing 50 mM Tris pH 7.5, 100 mM NaCl, 0.1% pluronic acid and 1% DMSO. After excitation of terbium (Tb) fluorescence at 337 nm, emission at 490 nm (Tb) and 520 nm (Alexa488) were recorded with a 70 μs delay to reduce background fluorescence and the reaction was followed over 1 h by recording 60 technical replicates of each data point using a PHERAstar FS microplate reader (BMG Labtech). The TR-FRET signal of each data point was extracted by calculating the 520/490 nm ratio. Data were analysed with GraphPad Prism 6 assuming equimolar binding of the probe to the receptor using the following equation11,47:
FIObs is the observed fluorescence intensity, and FIFree and FIBound the fluorescence intensities of the probe in its free and its bound states, respectively.
Dose response curves for IMiDs were obtained by mixing increasing concentrations of IMiD with a reservoir containing N8CRL4ACRBN at 200 nM, biotin-ZFP91 or biotin-ZFP91(H418A) at 100 nM, and Tb-Streptavidin at 2 nM. The fluorescence as 520/490 nm ratio were recorded over 1 h as 60 technical replicates of each data point using a PHERAstar FS microplate reader (BMG Labtech) and resulting data analysed with GraphPad Prism 6.
In vitro ubiquitination assays
In vitro ubiquitination was performed by mixing ZFP91 at 0.6 μM, and N8CRL4CRBN at 80 nM with a reaction mixture containing IMiDs at indicated concentrations or a DMSO control, E1 (UBA1, Boston Biochem) at 40 nM, E2 (UBCH5a, Boston Biochem) at 1.2 μM, ubiquitin at 23 μM. Reactions were carried out in 50 mM Tris pH 7.5, 30 mM NaCl, 5 mM MgCl2, 0.2 mM CaCl2, 2.5 mM ATP, 0.1% Triton X-100 and 0.1 mg ml−1 BSA, incubated for 15–30 min at 30 °C and analysed by western blot using anti-ZFP91 and anti-rabbit IRDye 800CW antibodies. Blots were scanned on a LICOR Odyssey infrared imaging system (uncropped immunoblots are provided in Supplementary Fig. 4).
HPLC and mass spectrometry
The multi time point mass spectrometry experiment consisted of two replicates each for DMSO and LENA-treated cells collected at 6 h (T6), 10 h (T10.raw data files were initially mislabelled as T8) and 16 h (T16) post treatment. One additional reverse experiment (label swap) was conducted at the T6 and T10 time points. During data analysis, we noticed a dramatically reduced MS signal for the T10 forward samples, which we believe was due to reduced peptide yields from fractionation and digest (the reverse samples processed at a different time were unaffected). These samples were removed from all downstream analysis. Since we did not aim to generate precise protein half-life values, we refrained from repeating the experiments. For the multi time point experiment, cells were lysed in RIPA buffer (50 mM Tris pH 8.0, 150 mM NaCl, 0.1% SDS, 0.5% sodium deoxycholate, 1% Triton X-100, 1 tablet per 100 ml Sigma protease inhibitor cocktail) for 30 min on ice. 200 μg of lysate was subjected to reduction, alkylation and subsequent SDS–PAGE separation. SDS–PAGE gels were fixed in fixing solution (10% v/v acetic acid and 50% v/v methanol) for 30 min and whole gel lanes cut into 15 slices of equal size. Gel pieces were individually subjected to in-gel tryptic digest. Peptides were analysed by nano liquid chromatography tandem mass spectrometry with an EASY-nLC 1,000 pump using a two-column set-up (Thermo Scientific). The acidified peptides were loaded with buffer A onto a trap column (C18 Acclaim PepMap 100 trap column 75 μm × 2 cm, 3 μm 100 Å) at a flow rate of 200 nl min−1. They were separated with a linear gradient of 2–5% buffer B in 5 min followed by 5–30% B in 150 min, 30–50% B in 30 min, 50–80% B in 5 min and by 5 min wash at 80% buffer B (buffer A: 0.1% formic acid in water, buffer B: 0.1% formic acid in acetonitrile) on a 75 μm × 25 cm Reprosil-PUR C18, 3 μm, 100 Å PicoFrit column at 60 °C mounted on a DPV ion source (New Objective) connected to an Orbitrap VELOS mass spectrometer (Thermo Scientific). The data were acquired in a mass range of m/z 350–1,300, resolution 60,000, AGC 2 × 106, maximum injection time 200 ms, dynamic exclusion 15 s for the peptide measurement in the Orbitrap, a top 20 method with CID fragmentation of the most abundant peptides at a maximum injection time 50 ms, AGC 1 × 104, NCE 35% and fragment ion measurement in the LTQ.
For the single time point pulse-SILAC experiment (two replicates per condition forward and two replicates per condition reverse for a total of four technical replicates), cells were lysed in buffer containing 0.5 M Tris pH 8.6 and 6 M GnHCl. An aliquot of 200 μg of protein lysate was reduced in 16 mM TCEP for 30 min and alkylated in 35 mM iodoacetamide for 30 min in the dark. The proteins were digested at 37 °C with lysyl endopeptidase (Wako) after dilution to ≈2 M GnHCl (with 50 mM Tris-HCl pH 7.3, 5 mM CaCl2 buffer) for 6 h, and after dilution to <1 M GnHCl with trypsin (Promega) at 37 °C overnight. The resulting peptides were desalted using 50 mg C18 solid-phase extraction cartridges (Waters) and offline fractionated into 36 fractions by high pH reversed phase chromatography on an Agilent1100 system. Between 25 and 40 μg of peptides were loaded in high pH buffer A and separated at a flow rate of 12 μl min−1 with a gradient of 2–10% high pH buffer B in 10 min followed by a linear increase from 10–35% B in 60 min, 35–100% B in 5 min followed by 5 min wash at 100% B (high pH buffer A: 20 mM ammonium formate at pH 10, high pH buffer B: 20 mM ammonium formate at pH 10 in 90% acetonitrile) on a YMC-Triart C18 0.5 × 250 mm, 12 nm × 3 μm column. The 36 fractions were pooled (fr01+fr13+fr25, fr02+fr14+fr26 and so on) to a final of 12 samples.
Peptides were analysed by nano liquid chromatography tandem mass spectrometry with an EASY-nLC 1,000 pump using a two-column set-up (Thermo Fisher Scientific). The peptides were loaded in buffer A onto a trap column (Acclaim PepMap 100, 75 μm × 2 cm, C18, 3 μm, 100 Å). They were separated, at a flow rate of 150 nl min−1 with a linear gradient of 2–6% buffer B in 8 min followed by a linear increase from 6–22% B in 88 min, 22–28% B in 16 min, 28–36% B in 8 min, 36–80% B in 4 min followed by 10 min wash at 80% B (buffer A: 0.1% formic acid in water, buffer B: 0.1% formic acid in acetonitrile) on a PepMap RSLC analytical column (50 μm × 15 cm, C18, 2 μm) at 45 °C mounted on a modified DPV ion source (New Objective) connected to an Orbitrap Fusion mass spectrometer (Thermo Scientific). The data were acquired using a mass range of m/z 350–1,600, resolution 120,000, AGC target 3 × 105, maximum injection time 100 ms, dynamic exclusion of 60 s for the peptide measurements in the Orbitrap and a cycle time of 3 s for HCD fragmentation of the most abundant peptides and fragment ion measurement in the LTQ using AGC target 1 × 102, NCE 30%, maximum injection time 250 ms.
Mass spectrometry data analysis
MaxQuant35 (versions 126.96.36.199 and 188.8.131.52 for multi time point and single time point, respectively) was used for RAW file processing and controlling peptide and protein level false discovery rates, assembling proteins from peptides, and protein quantification from peptides. Fragment ion spectra were searched against a human Uniprot database (downloaded on 13 November 2014 and 29 January 2015 for multi time point and single time point, respectively) and common contaminant proteins (included in the MaxQuant software). Carbamidomethylation (Cys) was set as a fixed modification; deamidation (Gln, Asn) and oxidation (Met) were selected as variable modifications. SILAC amino acids used for quantification were Lys8 and Arg10. The MaxQuant ProteinGroups.txt output file was imported into the R framework48 for all subsequent analyses.
Before statistical analysis proteins flagged as contaminants, reverse (decoy) proteins and proteins only identified by site were removed from the data set. H/L protein ratios (‘Ratio H/L’ columns per time point, not normalized) were quantile normalized using the limma package36 with normalization carried out separately for each time point. The quantile normalization as described elsewhere49 and implemented in the limma package has the advantage of being a complete data method without requiring a defined baseline data set. In short, n data sets of length p are turned into a matrix X with p × n dimensions, with each data set being a column. We sort each column of X to give Xsort and now assign the mean across each row of Xsort to each element of the row to give X’Sort. Next, we rearrange each column of X’Sort back to the original ordering and derive XNormalised.
Determination of protein half-lives
While we performed the linear regression fits to obtain protein half-lives, we noted several challenges for accurate determination of protein half-lives, including low number of time points, low number of replicates, inclusion of label swap data (which display a consistent rank order but a systematic offset compared to the forward experiments, see also Supplementary Fig. 3), and also the known limitations of obtaining half-lives by SILAC mass spectrometry, such as ‘light’ amino-acid recycling27. However, we demonstrate that despite these limitations the data are informative for the identification of ligase targets. Protein half-lives were obtained as previously described24. In essence, normalized and log2 transformed H/L ratios for protein groups quantified across all time points and replicates (n=2,837) were used for linear regression (log2(H/L) ∼time) for the DMSO and lenalidomide samples of each protein. Proteins that exhibited sufficient quality of both (DMSO and lenalidomide) fits (r2>0.9, total number of proteins 2,759) were used to obtain the protein decay rate constant (kdp) using the following equation24:
where m is the number of time points (ti), rti the H/L ratio of a specific protein at a given time point, and tcc is the time needed to double the total amount of protein in the experiment, which is usually set to the duration of the cell cycle. The doubling time of HEK293T cells was estimated to be ≈22 h by counting cells growing on 100 mm dishes. However, using tcc=22 h resulted in negative decay rates for a subset of proteins, indicating that in our experimental set-up the protein doubling time was longer than 22 h. We attributed this effect to the cells growing more slowly than expected during the experiment, for example, due to increasing cell densities or the effect of heavy amino acids. To accommodate for this effect, tcc was set to 100 h, which resulted in a mean protein half-life of 44.6 h similar to published estimates24. While the use of an incorrect tcc value leads to incorrect absolute protein decay rates, it does not limit the use of the inferred decay rates or protein half-lives as a relative measure in the comparison of different treatment conditions, which is the purpose in this study. Based on the decay constant, the half-life of a protein is given by24:
The derived protein half-lives were used for subsequent comparison.
Data analysis for single time point pulse SILAC
For conventional SILAC mass spectrometry, it has been shown that the distance of a ratio r measured in terms of the s.d. can serve as a robust estimate of its significance. Under the assumption of a normal distribution of the data, a P value can be calculated (significance A)35. Based on the observation that the error of H/L protein ratios is correlated to the summed intensity, P values are calculated for subsets of the data binned by intensity (significance B)35. Since the log-transformed LENA/DMSO protein ratios assume in approximation a normal distribution, we utilized this approach to assess the statistical significance of proteins.
To control for potential non-linearities in some samples, log2 H/L protein ratios were quantile normalized using the normaliseBetweenArrays function from the limma package36 (see description of quantile normalization above). Protein ratios were filtered to include only proteins quantified by at least three unique peptides (not razor) and with a minimum of two peptides (unique and razor) in every individual LC-MS/MS experiment (no missing values for protein ratios). The remaining 3,352 protein ratios were used for subsequent analysis: median of DMSO and median of lenalidomide-treated H/L protein ratios were used to calculate LENA/DMSO protein ratios (ΔH/L). The ΔH/L ratios were binned by summed intensities (10 bins of equal size) and the 15.87, 50 and 84.13 percentiles r−1, r0 and r1 were calculated for each of the bins. For each protein, a significance B P value35 was calculated with the r−1, r0 and r1 values corresponding to their intensity bin and by using the following formula:
with the error function erfc defined as: , where pnorm() is the R function for cumulative distribution function for the normal distribution. Further z is defined as the distance measured in terms of the s.d.:
A list of all significance B values is provided (see Supplementary Table 3). A P value <1 × 10−7 was selected as cutoff.
MS analysis across experiments using linear models
Log2 transformed H/L protein ratios were analysed using the limma package36 (see Supplementary Table 1 for design matrix). Intensities in mass spectrometry experiments have been found to correlate with the quality of quantification, log10 transformed intensities were therefore included as weighting factor for the linear model analysis. A list of log2 fold changes and statistical information for all protein groups is provided (see Supplementary Table 4).
Sample preparation TMT LC-MS3 mass spectrometry
Samples were prepared as previously described50 with the following modification. All solutions are reported as final concentrations. Lysis buffer (8 M Urea, 1% SDS, 50 mM Tris pH 8.5, protease and phosphatase inhibitors from Roche) was added to the cell pellets to achieve a cell lysate with a protein concentration between 2 and 8 mg ml−1. A micro-BCA assay (Pierce) was used to determine the final protein concentration in the cell lysate. Proteins were reduced and alkylated as previously described. Proteins were precipitated using methanol/chloroform. In brief, four volumes of methanol was added to the cell lysate, followed by one volume of chloroform and finally three volumes of water. The mixture was vortexed and centrifuged to separate the chloroform phase from the aqueous phase. The precipitated protein was washed with one volume of ice-cold methanol. The washed precipitated protein was allowed to air dry. Precipitated protein was resuspended in 4 M urea, 50 mM Tris pH 8.5. Proteins were first digested with LysC (1:50; enzyme:protein) for 12 h at 25 °C. The LysC digestion was diluted down to 1 M urea, 50 mM Tris pH 8.5 and then digested with trypsin (1:100; enzyme:protein) for another 8 h at 25 °C. Peptides were desalted using a C18 solid-phase extraction cartridges as previously described. Dried peptides were resuspended in 200 mM EPPS, pH 8.0. Peptide quantification was performed using the micro-BCA assay (Pierce). The same amount of peptide from each condition was labelled with TMT reagent (1:4; peptide:TMT label) (Pierce). The 10-plex labelling reactions were performed for 2 h at 25 °C. Modification of tyrosine residue with TMT was reversed by the addition of 5% hydroxyl amine for 15 min at 25 °C. The reaction was quenched with 0.5% TFA and samples were combined at a 1:1:1:1:1:1:1:1:1:1 ratio. Combined samples were desalted and offline fractionated into 24 fractions as previously described.
LC-MS3 for TMT relative quantification
Twelve of the 24 peptide fraction from the high pH reverse phase step (every other fraction) were analysed with an LC-MS3 data collection strategy38 on an Orbitrap Fusion mass spectrometer (Thermo Fisher Scientific) equipped with a Proxeon Easy-nLC 1,000 for online sample handling and peptide separations. Approximately 5 μg of peptide resuspended in 5% formic acid+5% acetonitrile was loaded onto a 100 μm inner diameter fused-silica micro capillary with a needle tip pulled to an internal diameter less than 5 μm. The column was packed in-house to a length of 35 cm with a C18 reverse phase resin (GP118 resin 1.8 μm, 120 Å, Sepax Technologies). The peptides were separated using a 180 min linear gradient from 3 to 25% buffer B (100% acetonitrile+0.125% formic acid) equilibrated with buffer A (3% acetonitrile+0.125% formic acid) at a flow rate of 400 nl min−1 across the column. The scan sequence for the Fusion Orbitrap began with an MS1 spectrum (Orbitrap analysis, resolution 120,000, 400–14,000 m/z scan range with quadrupole isolation, AGC target 2 × 105, maximum injection time 100 ms, dynamic exclusion of 60 s). ‘Top N’ (the top 10 precursors) was selected for MS2 analysis, which consisted of CID ion trap analysis (AGC 8 × 103, NCE 35, maximum injection time 150 ms), and quadrupole isolation of 0.5 Da for the MS1 scan. The top 10 fragment ion precursors from each MS2 scan were selected for MS3 analysis (synchronous precursor selection), in which precursors were fragmented by HCD prior to Orbitrap analysis (NCE 55, max AGC 1 × 105, maximum injection time 150 ms; MS2 quadrapole isolation was set to 2.5 Da, resolution 60,000).
LC-MS3 data analysis
A suite of in-house software tools (Thermo Center for Multiplexed Proteomics at Harvard Medical School) were used to for.RAW file processing and controlling peptide and protein level false discovery rates, assembling proteins from peptides, and protein quantification from peptides as previously described. MS/MS spectra were searched against a Uniprot human database (February 2014) with both the forward and reverse sequences. Database search criteria are as follows: tryptic with two missed cleavages, a precursor mass tolerance of 50 ppm, fragment ion mass tolerance of 1.0 Da, static alkylation of cysteine (57.02146 Da), static TMT labelling of lysine residues and N-termini of peptides (229.16293 Da) and variable oxidation of methionine (15.99491 Da). TMT reporter ion intensities were measured using a 0.003 Da window around the theoretical m/z for each reporter ion in the MS3 scan. Peptide spectral matches with poor quality MS3 spectra were excluded from quantification (<summed signal-to-noise across 10 channels and <0.5 precursor isolation specificity).
Samples of isolated RNA were used for library preparation using ScriptSeq v2 total RNA library preparation kit and sequenced on an Illumina HiSeq 2,500 sequencer per Illumina standards. Sequencing reads were aligned to the human genome (Bsgenome.Hsapiens.UCSC.hg19 Bioconductor package, using splicedAlignment=TRUE) and quantified at the level of genes (TxDb.Hsapiens.UCSC.hg19.knownGene Bioconductor package) using the QuasR package with default parameters51. Intronic and exonic reads were separately quantified and differentially expressed genes were identified using the edgeR Bioconductor package52 as described elsewhere37.
All RNA-seq data sets have been deposited in GEO under the accession number GSE94728. Mass spectrometry raw data files have been deposited in PRIDE Archive under the accession numbers PXD005857 and PXD005849 for the HEK293T and Hct116 experiments, respectively. The data that support the findings of this study are available from the corresponding author on request.
How to cite this article: An, J. et al. pSILAC mass spectrometry reveals ZFP91 as IMiD-dependent substrate of the CRL4CRBN ubiquitin ligase. Nat. Commun. 8, 15398 doi: 10.1038/ncomms15398 (2017).
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Financial support for this work was provided by the Dana-Farber/Novartis Drug Discovery Program (grant to E.S.F.), NIH grant NCI R01CA214608 (grant to E.S.F.), the Claudia Adams Barr Program for Innovative Cancer Research and the Linde Family Foundation (start-up funds to E.S.F.). Work in the Stadler group is funded by the MetastasiX project of the Swiss Initiative for Systems Biology (SystemsX.ch). We thank Daniel Hess for help with peptide fractionation and mass spectrometry experiments. TMT labelling and corresponding LC-MS3 mass spectrometry were performed at the Thermo Fisher Scientific Center for Multiplexed Proteomics at the Harvard Medical School.
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