Search tips
Search criteria 


Logo of ploscompComputational BiologyView this ArticleSubmit to PLoSGet E-mail AlertsContact UsPublic Library of Science (PLoS)
PLoS Comput Biol. 2011 May; 7(5): e1002056.
Published online 2011 May 26. doi:  10.1371/journal.pcbi.1002056
PMCID: PMC3102755

An Acidic Loop and Cognate Phosphorylation Sites Define a Molecular Switch That Modulates Ubiquitin Charging Activity in Cdc34-Like Enzymes

Sarah A. Teichmann, Editor


E2 ubiquitin-conjugating enzymes are crucial mediators of protein ubiquitination, which strongly influence the ultimate fate of the target substrates. Recently, it has been shown that the activity of several enzymes of the ubiquitination pathway is finely tuned by phosphorylation, an ubiquitous mechanism for cellular regulation, which modulates protein conformation. In this contribution, we provide the first rationale, at the molecular level, of the regulatory mechanism mediated by casein kinase 2 (CK2) phosphorylation of E2 Cdc34-like enzymes. In particular, we identify two co-evolving signature elements in one of the larger families of E2 enzymes: an acidic insertion in β4α2 loop in the proximity of the catalytic cysteine and two conserved key serine residues within the catalytic domain, which are phosphorylated by CK2. Our investigations, using yeast Cdc34 as a model, through 2.5 µs molecular dynamics simulations and biochemical assays, define these two elements as an important phosphorylation-controlled switch that modulates opening and closing of the catalytic cleft. The mechanism relies on electrostatic repulsions between a conserved serine phosphorylated by CK2 and the acidic residues of the β4α2 loop, promoting E2 ubiquitin charging activity. Our investigation identifies a new and unexpected pivotal role for the acidic loop, providing the first evidence that this loop is crucial not only for downstream events related to ubiquitin chain assembly, but is also mandatory for the modulation of an upstream crucial step of the ubiquitin pathway: the ubiquitin charging in the E2 catalytic cleft.

Author Summary

A major mechanism for promoting protein regulation in eukaryotes involves the labeling with ubiquitin molecules of target proteins. Protein ubiquitination is involved in almost all aspects of eukaryotic cellular functions and is mediated, at the molecular level, by a hierarchical cascade of three different enzymes. Among these enzymes, E2 ubiquitin-conjugating enzymes are located at the heart of the ubiquitination pathway and are key mediators of protein ubiquitination, which strongly influence the ultimate fate of the target substrates. Since several E2s have also been related to a variety of cancer and neurodegenerative disorders, increasing efforts are being devoted to the understanding of E2 regulation at the molecular level, a mandatory step for a complete understanding of the ubiquitination process. In the present contribution, we propose, by computational and biochemical investigations, a conserved mechanism of regulation by phosphorylation of the catalytic activity of a class of E2 enzymes, which plays a major role in the regulation of cell cycle progression and tumor development. Our results shed new light on and clarify molecular aspects related to one of the first steps of the ubiquitination cascade and its regulation.


A major mechanism for the promotion of protein regulation in eukaryotes involves the covalent attachment of ubiquitin (Ub), mediated by a hierarchical cascade of E1-E2-E3 enzymes [1], [2]. In particular, the E1 enzyme activates the ubiquitin in an ATP-dependent reaction and engages one of many cognate E2 ubiquitin-conjugating enzymes to initiate downstream events. Ubiquitin is covalently attached to the target protein through an isopeptide bond between the glycine in position 76 of ubiquitin and the ε-amino group of an internal lysine residue of the target protein, through the coordinate function of E3 ubiquitin-ligases. Several E2 cycles of E1-mediated ubiquitin loading/unloading lead to different polyubiquitination or monoubiquitination of the substrates. By multiple runs of reactions, ubiquitin is covalently attached to substrates to form K48-linked or K11-linked polyubiquitinated conjugates that are addressed to proteasomal degradation [3], [4], [5], [6], [7], [8]. Moreover, post-translational modification by Ub on other lysine residues, as K63, or ubiquitin-like proteins regulates several other processes, including cell division, immune responses and embryonic development [7], [9], [10], [11].

The yeast and human genomes encode for tens of E2s, allowing for a multitude of distinct events [12], [13]. E2s have been classified in 17 families, by a comprehensive phylogenetic analysis of several complete genomes [14] and have been shown to present different electrostatic potential surface properties which could be related to their specificity [15], [16]. All E2 enzymes share a conserved catalytic core domain (Ub-conjugating domain, UBC) which in many cases is the minimal sufficient unit for their activity, containing the catalytic cysteine (Figure 1) and the interaction interfaces for E1 and E3 enzymes. The 150-residues UBC domain adopts a β/α fold (Figure 1) and the highly conserved catalytic cysteine is located in a shallow cleft interacting with the Ub C-terminal tail [17]. Despite conservation of the UBC domain fold, many E2s contain sequence insertions. Yeast and mammalian Cdc34 are multi-domain E2 enzymes, which catalyze the formation of polyubiquitin chains on several proteins involved in cell-cycle regulation [18]. Yeast Cdc34 is characterized by a 12-residue insertion (residues 103–114) in the β4α2 loop of the UBC domain, which is known as the “acidic loop” [19], [20]. Interestingly, the acidic insertion also occurs in other yeast and human homologs and forms an extended and flexible loop [21]. In fact, alanine-mutations of the β4α2 acidic residues abolish polyubiquitin chain assembly in the human E2 Ube2g2 [22]. In Cdc34, mutations of the acidic residues compromise the processivity and linkage specificity of polyubiquitin chain synthesis [22], [23], [24]. However, few details are still known about the structural and functional properties of the acidic insertion. Several E2 catalytic domains have been reported to be finely regulated by post-translational phosphorylations [25], [26], [27], [28]. Cdc34 is a substrate of casein kinase 2 (CK2) [25], [26], [29], [30], [31], a highly conserved kinase essential in several different cellular processes [32]. In particular, CK2 phosphorylates yeast Cdc34 within the C-terminal [26], [31] and the catalytic domain (S130 and S167) [25]. S130 and S167 phosphorylations are required to stimulate yeast Cdc34 ubiquitin-charging activity in vitro and to complement a cdc34-2 ts mutant in vivo [25].

Figure 1
Summary structure of 3D UBC domain architecture.

In light of the above scenario, we provide the first molecular model of the regulatory mechanism mediated by CK2 phosphorylation of E2 Cdc34-like catalytic domain. In particular, we show that the acidic loop conformation is modulated by phosphorylation of two key serine residues. Our investigation strongly suggests that this regulatory mechanism is a conserved feature of Cdc34-like E2s, a crucial element for the modulation of ubiquitin charging activity.


Co-evolution of phosphorylation sites and acidic loop in Cdc34-like E2 enzymes

CK2 phosphorylation sites at S130 and S167 are functionally relevant for the ubiquitin-charging activity of yeast Cdc34 [25]. Multiple sequence and structural alignments among representative members of the different E2 families (Figure 2, Figure 1 in Text S1) show that phospho-sites corresponding to S130 and S167 of Cdc34, as well as the typical acidic consensus pattern for CK2 kinase, are strongly conserved in E2s belonging to family 3. E2 family 3 is the only family whose members show a 12/13 aminoacid insertion in the β4α2 loop (Figure 2, Figure 1 in Text S1). In the other E2 families, which lack the acidic insertion, the phospho-sites are poorly conserved, with the exception of E2 families (2, 4, 8, 12). The latter include members which are the closest homologs (percentage of identity >30%) to family 3 members and which are thus characterized by a higher degree of serine conservation (Figure 3). Interestingly, in most of the other E2 families, which lack the acidic insertion, serines are often replaced by non-phosphorylatable residues with no specific physical-chemical properties (Figure 2, Figure 1 in Text S1). These data suggest co-evolution of the phospho-sites at Cdc34 130 and 167 positions and the acidic loop in the proximity of the catalytic site in Cdc34-like E2 enzymes.

Figure 2
Multiple sequence alignment of family 3 E2s.
Figure 3
Conservation of phospho-sites and of CK2 consensus pattern.

Conformational changes of β4α2 loop modulates accessibility of the Cdc34UBC catalytic cleft

The striking co-presence of phosphorylation sites and the acidic loop only in family 3 E2 enzymes, prompted us to test the hypothesis of an interconnected structural, functional and regulatory role of these two elements. First, the dynamic properties of Cdc34 and its homologs have been investigated by multiple molecular dynamics (MD) simulations of the non-phosphorylated UBC domains (Table 1). In particular, flexibility profiles, principal component analysis (PCA) and correlation between accessibility of the catalytic cleft and other regions of the protein structure have been calculated. In this context, PCA applied to MD simulations allows the identification of the most relevant displacements of groups of residues and emphasizes the amplitude and direction of the dominant protein motions, by projecting them on a subset of principal components (eigenvectors) of the Cα atoms covariance matrix calculated from the MD conformational ensemble [33].

Table 1
Summary of MD simulations and simulated systems.

The conformational sub-states distribution in the proximity of the native-state of Cdc34UBC has been evaluated by free energy landscape (FEL) representation using as two-dimensional (2D) coordinates the first two principal components (PCs) derived by PCA (Figure 2 in Text S1), as well as from structural cluster analysis. The structural cluster analysis and the FEL representation indicate that Cdc34UBC exists in several sub-states in solution (Figure 2 in Text S1, Figure 4A). In particular, it is possible to identify five main structural ensembles (labeled A–E) which correspond to the minimum free energy basins and the most populated structural clusters from cluster analysis. These structural ensembles capture the most relevant conformational and dynamical features of Cdc34UBC. The major differences among the ensembles are related to different conformations of the β4α2 loop (Figure 4A).

Figure 4
Cdc34UBC simulations.

Interestingly, the β4α2 loop close to the E2 active site, and in particular its acidic insertion (residues 103–114) is characterized by a high conformational variability (Figure 4A), that can be described quantitatively by flexibility indexes as root mean square fluctuation (rmsf) calculated on each Cdc34UBC ensemble trajectory (Figure 4B, Figure 3 in Text S1). MD simulations of Cdc34 homologs with known 3D structure (yeast Ubc7 and human Ube2g2) (Figure 4B) confirmed that the β4α2 loop features the highest conformational freedom also in other family 3 members. These results are in good agreement with evidence from X-ray crystallographic investigations of these enzymes [34], [35], in which the regions corresponding to the acidic loop seem to be disordered and associated to high B-factor values. Moreover, recent NMR studies of free Ube2g2 [21] or Ube2g2 in complex with a domain of its E3 partner [36] suggest the possibility of conformational changes of the β4α2 loop. However, the MD simulations carried out in the present work, allow a higher sampling of the conformation accessible to the β4α2 loop, highlighting larger structural rearrangements.

Figure 5A shows solvent accessibility of the catalytic C95 side chain as a function of the distances between the C95 and the acidic insertion. Solvent accessibility increases as the acidic loop “moves away” from the active site. We refer to conformations of the β4α2 loop in proximity of - and away from - the catalytic cysteine as “closed” and “open” conformations, respectively. Since PCA makes it possible to identify amplitude and direction of relevant protein motions, the projections of the first principal component (PC1) on the 3D structure of Cdc34UBC have been analyzed. Protein motions governing PC1 are related to rearrangements and oscillations of the acidic loop over the catalytic site (Figure 5B) that make it function as a “lid” modulating the accessibility of the Ub-binding cleft.

Figure 5
Conformational variability of the acidic loop and C95 solvent accessibility.

Phosphorylation of Cdc34UBC improves accessibility of the catalytic site by displacing the acidic loop

In Cdc34UBC simulations, some residues within the acidic insert (D104, D108, E109, D111 and E113), came transiently close to the catalytic cleft (Figure 5A, Figure 6) and, therefore also to the α-helix in which S130 is located. This observation suggests that S130 phosphorylation, introducing a strongly negatively charged group, may result in electrostatic repulsion with the above-mentioned acidic residues, favoring the open conformation of the β4α2 loop. This hypothesis was tested by MD simulations of phospho-variants of the Cdc34UBC (Table 1) that were compared with simulations of the non-phosphorylated Cdc34UBC, as well as with simulations of the Cdc34UBC alanine mutants, in which the phosphorylation sites (S130 and S167) are abolished, and that have been used in biochemical and genetic experiments [25]. While alanine substitutions do not influence secondary structure content and flexibility patterns described for native Cdc34UBC (Figure 4B), flexibility profiles of Cdc34UBC-pS130 indicate that phosphorylation strongly reduces atomic fluctuations, structurally stabilizing the whole 3D architecture and in particular the acidic insertion (103–114) (Figure 7A). Phosphorylation of both S130 and S167 (Figure 4 in Text S1, Figure 7B) has comparable effects on acidic loop conformations compared to those observed for phosphorylated Cdc34UBC-pS130 (Figure 7), with a slightly higher capability of reducing protein flexibility of β4α2 loop of the double-phospho variant with respect to Cdc34UBC-pS130.

Figure 6
Mechanism of acidic loop activation by electrostatic repulsive effects.
Figure 7
Flexibility profiles of phospho-Cdc34UBC variants.

The comparison between snapshots of Cdc34UBC and phospho-Cdc34UBC simulations revealed that, in the phospho-Cdc34UBC versions, the loop is stabilized in an open conformation (Figure 8A, in blue), determining a higher solvent accessibility of the catalytic residue C95. It is worth mentioning that phospho-Cdc34 structures have an average value of C95 solvent accessibility (avSAS = 30%) comparable to the average value calculated for the 40 ns simulation of yeast Ubc1 (avSAS = 34%), a family 2 E2 lacking the acidic insertion. Interestingly, solvent accessibility values of the catalytic cysteine side-chain in native Ube2g2 NMR structure [21], as well as in Ube2g2 in complex with a domain of its E3 partner [36] are lower than 15%, indicating that phosphorylation in the Cdc34 catalytic domain promotes a more relevant outward conformational displacement of the acidic loop than previously shown (Figure 5 in Text S1).

Figure 8
Phospho-Cdc34UBC simulations.

These data are confirmed by the analysis of the motions described by the PC1 of phospho-Cdc34UBC simulations (Figure 8B). Fluctuations along PC1 are strongly reduced and the PCA analysis failed to identify the opening/closing oscillations of the acidic loop typical of Cdc34UBC, whereas a displacement of the loop toward open conformations is evident (Figure 5, ,8B8B and D). In order to assess that effects induced by S130 phoshorylation are mainly due to electrostatic repulsion between acidic residues in the loop and the negatively charged pS130, simulations of mutant Cdc34UBC variants with S130 replaced by negatively charged residues (Cdc34UBC-S130D and Cdc34UBC-S130E) have been carried out. The dynamical and structural properties of Cdc34UBC-S130D and Cdc34UBC-S130E, as well as the stabilization of the loop in an open conformation, are in agreement with data derived from phospho-Cdc34UBC simulations (Figure 7B, ,8C8C and Figure 6 in Text S1).

To quantitatively define differences in the solvent accessibility of catalytic cysteine and displacement of the acidic loop from the catalytic site, the distributions of the solvent accessibility of the catalytic C95 side chain as a function of the distances between C95 and the acidic insertion have been compared in non-phosphorylated, phospho- and S130E Cdc34UBC variants (Figure 8D). Interestingly, the distribution of C95 SAS as a function of the distance between C95 and the acidic loop (Figure 8D), in agreement with analysis of rmsf profiles (Figure 7B), highlights a slightly greater displacement toward open conformations induced by the double-phospho variants. Moreover, the analysis suggests that the mutation of serine to acidic (for example glutamate) residues has lower effects in promoting acidic loop displacement than do the phospho-variants, which is probably related to enhanced electrostatic repulsion induced by the replacement of a poly-anionic phospho-serine with a mono-anionic residue (as Asp or Glu).

Our results suggest that the activation of Ub-conjugation activity by S130 phosphorylation is triggered by electrostatic repulsive effects between the phospho-Ser and the acidic residues of the β4α2 loop, promoting an outward displacement of the loop and a competent conformation of the catalytic cleft for Ub-charging.

In vitro activation of Ub-charging activity of Cdc34 by CK2 phosphorylation requires the acidic loop

According to the above-described model, phosphorylation by CK2 of the catalytic domain of Cdc34 can induce an outward displacement of the acidic loop, promoting Ub access to the catalytic cleft. Thus, to experimentally test the model, we investigated the effect of CK2 phosphorylation on the efficiency of Ub-charging of a protein lacking the 12 residue insertion in the acidic loop (His6-Cdc34-Δ12). It is known that Cdc34-Δ12 is a functional enzyme both in vitro and in vivo [19], [37], [38]. Moreover, the deletion of the acidic loop does not significantly change the overall structure of Cdc34 catalytic domain in a 100 ns MD simulations of Cdc34-Δ12UBC (Figure 7 in Text S1). In a thiolester assay, Cdc34 migrates as a set of discrete bands, which are due to the linkage of multiple ubiquitin groups to lysine residues in Cdc34 protein. These autoubiquitination products depend upon the binding of the Ub molecule to the catalytic residue C95 [39], [40]. As previously reported [25], phosphorylation by CK2 strongly enhanced the ubiquitin-charging activity of His6-Cdc34 in a thiolester assay in vitro, mainly acting through S130 and S167 phosphorylations (Figure 9A). The Ub-charging activity of the mutant protein His6-Cdc34-Δ12 is unaffected by phosphorylation, since both the phosphorylated and unphosphorylated proteins are able to bind Ub to a comparable level (Figure 9A). To ascertain which of the many bands is the thiolester form, the samples of the thiolester assays were separated on both reducing and non reducing conditions (Figure 9B). The only species sensitive to DTT is the faster migrating band, corresponding to the Cdc34-Ub thiolester, as also reported by Banerjee et al. [39]. These results support the conclusions derived from MD investigation, indicating that the main role of CK2 phosphorylation on Cdc34UBC is to promote the displacement to an open conformation of the acidic loop and to expose the catalytic cysteine to the solvent.

Figure 9
CK2 phosphorylation does not stimulate Cdc34-ubiquitin charging activity of a His6-Cdc34-Δ12 protein.


E2 enzymes define a complex superfamily that includes 17 families [14]. They play a major role in protein ubiquitination and Ub chain assembly [12], [13]. Recently, E2s have been shown to be involved in a variety of disorders, including cancers and neurodegenerative diseases [41], [42], [43]. Accordingly, there is increasing interest in understanding their regulation at the molecular level, a mandatory pre-requisite for rational design of effective pharmacologically active molecules which target E2 function.

An acidic insertion in the loop β2α4 has been identified in the proximity of the catalytic cysteine of several E2 enzymes, including Cdc34 that plays a major regulatory role in cell cycle progression and tumor development [41], [42]. The acidic loop has been thoroughly investigated by mutagenesis experiments. In fact, mutations of acid residues in the loop abolished the polyubiquitin chain assembly, the processivity and the synthesis of a polyubiquitin chain with a correct topology [22], [23], [24]. It has been proposed that the loop is crucial for E2 downstream signaling such as interactions with E3 or correct interactions with the target substrates. Nevertheless, the 12-residue acidic insertion is not essential for yeast Cdc34 function in over-expression conditions [37] and its role in Cdc34 function remains unexplained.

In this paper, we report that the loop acts as one element of a bipartite signature structure conserved among the Cdc34-like E2 enzymes belonging to family 3 and regulates enzyme activity through a phosphorylation mechanism. The second component of the signature structure is defined by serines within the catalytic domain, corresponding to S130 and S167 of yeast Cdc34, which are phosphorylated by CK2, a highly conserved protein kinase, essential in several different cellular processes. Together these two elements define a molecular switch that modulates opening and closing of the catalytic cleft, and whose dynamics can be finely regulated by CK2 phosphorylation (see below).

In the unphosphorylated protein, the β4α2 loop has high conformational freedom (Figure 4, ,5A).5A). MD trajectories show that acidic residues of the loop came close to S130 of Cdc34 located in an α-helix forming one side of the catalytic cleft (Figure 5--6).6). These movements make the loop act as a “lid”, switching from “open” to “closed” conformations with respect to the catalytic cleft (Figure 10). The mobility of the acidic loop in Cdc34UBC and its modulation of solvent accessibility of the E2 catalytic cleft could explain the low basal Ub charging activity by unphosphorylated Cdc34 observed in vitro [25], also in agreement with the fact that the NMR structure of the human homolog Ube2g2, an E2 enzyme belonging to family 3, is characterized by conformations of the acidic insertion which in general does not provide accessibility of the catalytic cysteine [21].

Figure 10
Model of the activation mechanism of ubiquitin charging activity of Cdc34-like E2 enzymes.

Repulsive electrostatic effects between phospho-S130 and the acidic residues in the loop decrease its mobility, triggering an outward displacement of the loop and a competent conformation for Ub-charging (Figure 10). The proposed mechanism for Cdc34-like E2s activation is also in agreement with preliminary homology models of complexes between Cdc34-like enzymes and Ub, in which only open conformations of the loop are compatible with Ub interactions in the catalytic cleft (data not shown). It is in agreement as well with the previous observation that the acidic loop in a more closed conformation would result in steric clashes with the C-terminus of the ubiquitin molecule [36]. Our proposed model further predicts that if the electrostatic repulsive effects, which promote conformational changes of the loop, are abolished by mutations of the phospho-sites or of the acidic residues in the insertion, the loop cannot be stabilized in an open conformation upon phosphorylation, compromising downstream events in the Ub pathway. Consistently with this notion, while Cdc34 Ub-charging activity is modulated by CK2-dependent phosphorylation of S130 (and S167, see later) [25], ubiquitin charging activity of His6-Cdc34-Δ12 is unaffected by phosphorylation (Figure 9).

It has also to be considered, in our model, that ubiquitin-charging of E2 enzymes requires an interaction between E2 and E1 enzyme and a transfer of ubiquitin from the E1 catalytic cysteine to the E2 catalytic cysteine. In order, to strengthen our model, we derived by similarity with experimentally known E1-E2 complexes, a model of the putative complex between Uba1 E1 enzyme and Cdc34 with both open and closed conformations of the acidic loop (Figure 8 in Text S1). This qualitative model suggests that the acidic loop can be accommodated in the E1 binding cavity both in the open and closed conformation without causing steric effects, but if the loop is in a closed conformation it is likely to create a barrier between the E1 and E2 catalytic cysteines and probably prevents the transfer of Ub molecule. As it can be judged from the Cdc34-E1 model, the presence at position 130 of Cdc34 of serine or phospho-serine does not significantly affect the intermolecular interaction network at E1-E2 interface, even if further calculations will be necessary to clearly define the intermolecular interactions in details, whereas Uba1-Cdc34 model emphasizes the notion that the prominent role of S130 phosphorylation is to promote the acidic loop displacement (data not shown). Previous results showed that in vivo both S130 and S167 residues need to be mutated to alanine to make the yeast Cdc34 protein unable to complement a cdc34-2ts mutant, although evident morphological defects were observed in strains expressing Cdc34S130A (but not Cdc34S167A) [25]. Phosphorylation of S130 residue is likely to account for the most relevant conformational changes induced by the post-translational modification, whereas S167 may have additive enhancing effects as suggested by double-phosphorylated Cdc34 MD simulations. In our model, S167 is located close to the C-terminal end. As a result, constraints on S167, as well as its interactions with other protein domains are likely to be lost. A detailed computational study of the role of S167 phosphorylation will require a suitable structure of the full-length Cdc34 protein.

In a broader context, it has been established that post-translational phosphorylation is a widespread mechanism for the regulation of protein biological activity [44], [45]. In several cases, enzyme activity or protein function has been reported to be regulated by inhibitory or activatory phosphorylation events at specific protein sites. At the molecular level, these events are mediated by electrostatic repulsion between the phospho-residues and the neighboring negatively charged aminoacids [46], [47], [48], [49], [50], [51], pointing out a general and important regulatory mechanism. These mechanisms can be successfully investigated in atomic details by MD simulations [47], [52].

In conclusion, our study sheds a new and unexpected light on the role of the acidic loop in Cdc34-like E2 enzymes and provides the first evidence that this loop is crucial not only for downstream events related to Ub chain assembly [20][22], but above all for modulation of an upstream crucial step of the Ub pathway: the covalent Ub-binding of Cdc34-like E2s. The loop activation by phosphorylation of serine residues in the UBC domain is a mandatory step for an efficient Ub-charging and could also account for the proper proceeding of downstream events in the ubiquitin pathway.

Materials and Methods

Homology modeling of yeast Cdc34 and alignments

Three different models have been generated with Modeller [53] for yeast Cdc34 UBC domain (7–170 residues, Cdc34UBC) using as templates the known X-ray structures of human Ube2g2 [PDB entry 2CYX [32]], yeast Ubc7 [PDB entry 2UCZ [33]] and C. elegans Ubc7 [PDB entry 1PZV (to be published)] enzymes, sharing with yeast Cdc34 more than 40% of sequence identity (Text S2).

Multiple sequence and structural alignments of 250 sequences of E2 UBC domains from each of the known 17 E2 families [13] have been performed by ClustalW [54] and DALI [55]. E2s from families 10, 16 and 17 have been discarded, as they are not catalytically active or characterized by a non canonical fold [13]. In particular, UBC domain sequences of each E2s have been determined by intra-family sequence alignments. For each family, a sequence alignment between Cdc34 and the members of the family has also been carried out (Figure 1 in 1).

Molecular dynamics simulations

Molecular dynamics (MD) simulations were performed using GROMACS 3.3.3 ( with a modified version of GROMOS96 force field [56], [57]. The Cdc34 models (Cdc34UBC) and the 3D crystallographic structures of yeast Ubc7 and human Ube2g2, as well as of yeast Ubc1 [PDB entry 1FZY[15]] have been used as starting point for simulations. The structures were soaked in a dodechaedral box of SPC (Simple Point Charge) water molecules [58] in periodic boundary conditions (Text S2). In the simulations all the protein atoms were at a distance equal or greater than 0.6 nm from the box edges. Productive MD simulations were performed in the isothermal-isobaric (NPT) (300 K, 1 bar and 2 fs time-step). Electrostatic interactions were calculated using the Particle Mesh-Ewald (PME) summation scheme [59]. Van der Waals and Coulomb interactions were truncated at 1.0 nm and conformations stored every 4 ps. 4 independent simulations (replicas) were carried out for each non-phosphorylated Cdc34 model (Table 1), in order to improve the conformational sampling. MD multiple-replica approach has been shown to allow a wider conformational sampling than only few longer molecular dynamics simulations, if the stability of the trajectory and convergence of the analyzed properties have been carefully verified [60], [61], [62], [63]. The integration of structural cluster analysis and free energy landscape (Text S2, Figure 2 in Text S1) has been used in order to identify representative structures of Cdc34UBC close to its native-state, according to a protocol previously published [64]. In particular, an iterative procedure was pursued, collecting independent replicas for the same protein system until parameters from principal component analysis reach convergence (see below) and results from cluster analysis and free energy landscape are congruent (Text S2, Figure 2 in Text S1).

The average structures from native Cdc34UBC simulations have been used as starting structures for simulations of Cdc34UBC mutant and phospho-variants. The replicas collected for each protein and mutant variant differ for duration and number (Table 1), allowing us to collect more than 2.5 µs of simulations.

MD simulations using the same approach have been also carried out on the two Cdc34 homologs yeast Ubc7 and human Ube2g2 for which known experimental structures are available. Moreover, since an NMR structure of Ube2g2 has been released during the manuscript preparation (PDB entry 2KLY [19]), control simulations have been also carried out starting from a model of Cdc34 using the Ube2g2 NMR structure as template, allowing to confirm the collected results (data not shown).

Analysis of MD simulations

The rmsd (root mean square deviation) has been calculated with respect to the MD initial structures, both using all protein mainchain atoms (Figure 9 in Text S1) and mainchain atom of the common elements of the E2 fold (Figure 10 in Text S1). From 2 (Cdc34UBC and Ubc7) to 10 ns (mutant and phospho-Cdc34UBC) of each replica are required for convergence. For each system, the equilibrated portions of each replica were joined in macro-trajectories, representative of different directions of sampling around the starting structure. In order to carefully checked rmsd profiles stability, sample simulations have been extended to 80/100 ns, indicating that the proteins are not still in a slow equilibration phase and that the resulting trajectories can be used to investigate dynamic and structural properties.

The secondary structure content was calculated by DSSP program ( The root mean square fluctuation (rmsf) per residue from the average structure was calculated on α-carbons (Cα). In order to verify consistency of rmsf profiles, the Pearson correlation coefficient was calculated for rmsf data sets relative to replicas of the same system, collecting values higher than 0.6 (Text S2 for further details on MD analyses).

Principal Component Analysis (PCA) and Free Energy Landscape (FEL)

PCA reveals high-amplitude concerted motion in MD trajectories, through eigenvectors of the Cα mass-weighted covariance matrix of atomic positional fluctuations [33] calculated for each replica and concatenated trajectories. In our concatenated trajectories the first 3 principal components (PCs) describe more than 60% of the total motion. Cosine content of the first 20 PCs has been calculated to evaluate the conformational sampling achieved by simulations (Text S2, Figure 11 in Text S1).

Recombinant DNA techniques, genetic manipulations and purification of His6-Cdc34-Δ12

DNA manipulations and yeast transformations were carried out according to standard techniques. E. coli DH5α and BL21(DE3)[pLysE] were used in cloning experiments and for expression of recombinant proteins, respectively. CDC34-Δ12 (containing CDC34 gene with the deletion of the sequence encoding aminoacids 103–114) was cloned in pIVEX2.4a plasmid using custom designed primers. His6-Cdc34-Δ12 recombinant protein was purified as previously reported [23].

In vitro phosphorylation and thiolester assay

In vitro phosphorylation of recombinant proteins (7 µg of each purified protein) was performed as previously described [23], using 10 U of purified human CK2 (BIOMOL) in 10 mM Tris-HCl pH 7.5, 150 mM NaCl, 10 mM MgCl2, 100 µM ATP for 30 min at 30°C. CK2 phosphorylation was controlled using [γ-32P]-ATP. Both phosphorylated and not phosphorylated His6-Cdc34 and His6-Cdc34-Δ12 recombinant proteins were used in a thiolester assay. The reaction mixture contained the following in a volume of 40 µl: 50 mM Tris-HCl pH 7.5, 5 mM MgCl2, 2 mM DTT, 0.5 mM ATP, 20 ng/µl biotinylated-ubiquitin, 10 ng/µl E1 enzyme, 50 ng/µl His6-Cdc34 or His6-Cdc34-Δ12. After incubation at 37°C for the indicated time points, the reaction was stopped by the addition of sample buffer without β-mercaptoethanol (where indicated, 200 mM DTT was added). Samples were subjected to SDS-PAGE and analyzed by decoration with Horseradish-Peroxidase (HRP)-streptavidine.

Supporting Information

Text S1

This file contains the following supporting figures for this article: Figure 1. Intra-family multiple sequence alignment. In each alignment the families are indicated by ‘_x’. Figure 2. Conformational landscape explored in Cdc34UBC simulations. The free energy landscape is represented using projection of the Cdc34UBC macro-trajectory along the principal components PC1 and PC2 of the essential subspace. The free energy is given in KJ/mol and indicated by the color bar. The label A–E indicates the region corresponding to the minimum free energy basins and the most populated structural clusters from cluster analysis. Figure 3 Flexibility profiles of non-phosphorylated Cdc34UBC. Cα rmsf of ensemble trajectories of Cdc34UBC and Cdc34UBC–S130AS167A concatenated trajectories. The most persistent secondary structure during the simulations are represented schematically for each protein system. The rectangular box indicates the acidic loop. Figure 4. Flexibility profiles of phospho-Cdc34UBC–pS130pS167 simulations. Cα rmsf of ensemble trajectories of Cdc34UBC-pS130-pS167 and non-phosphorylated Cdc34UBC are compared. The most persistent secondary structure during the simulations are represented schematically for each protein system. The rectangular box indicates the acidic loop. Figure 5. 3D structural superimposition of an average structure from phospho-Cdc34UBCsimulations, free NMR and X-ray structure of Ube2g2 and Ube2g2 in complex with the gp78 region of its E3 partner. The average structure of phospho Cdc34UBC simulations is shown in blue, the NMR (PDB entry 2KLY) and X-ray (PDB entry 2CYX) structure of Ube2g2 are shown in dark and light green, respectively, the structure of Ube2g2 in complex with gp78 region of E3 partner (PDB entry 3H8K) is shown in orange. The catalytic cysteine is shown as yellow stick. Figure 6. Projection of the simulations frames along the PC1 of Cdc34UBC-S130D concatenated trajectory, indicated with different shades of grey. The rectangular box indicates the acidic loop and its aminoacidic composition. Figure 7. Root mean square fluctuation (rmsf) profiles of Cdc34UBC and Cdc34-Δ12UBC domains. Figure 8. Model of Cdc34 both in closed (A) and open (B) conformations in complex with Uba1 E1 on the base of the known crystallographic structures of E2-E1 enzymes (PDB codes: 3CMM (Uba1) and 2PX9 (Ubc9 E2 in complex with SAE2 E1) and 2NVU (Ubc12 E2 in complex with Uba3 E1 and Nedd8). Figure 9. Mainchain root mean square deviation of single replicas of each simulated protein system. Figure 10. Mainchain root mean square deviation of the structural elements of the common E2-fold (the mainchain atoms of the acidic loop are not included in the analysis) of the Cdc34 simulations. Figure 11. Cosine content along the first 20 principal components of single replicas and concatenated trajectories of different length for each simulated protein system.


Text S2

Homology modeling of Cdc34UBC to generate starting structures for molecular dynamics simulations and molecular dynamics simulations setup and analysis.



We thank M.G. Goebl for pYL27 plasmid containing CDC34-Δ12 gene, E.P. and L.D.G. thank Claudio Greco, Alberto Arrigoni and Ilaria Valimberti for fruitful discussion and technical assistance. We also thank Neil Campbell for language editing.


The authors have declared that no competing interests exist.

This work was supported by computational facilities at Cineca (Italy) to EP and LDG, by grants to PC (FAR 2008), to LA and MV from the EU-funded project UNICELLSYS ( and from MIUR (FIRB-ITALBIONET), and to LA from EU-funded Coordination Action Yeast Systems Biology Network (YSBN; Funding has been used to support data collection and analysis and the funders had no role in study design, decision to publish or preparation of the manuscript.


1. Dye BT, Schulman BA. Structural mechanisms underlying posttranslational modification by ubiquitin-like proteins. Annu Rev Bioph Biom. 2007;36:131–150. [PubMed]
2. Hochstrasser M. Ubiquitin-dependent protein degradation. Annu Rev Genet. 1996;30:405–439. [PubMed]
3. Hochstrasser M. Ubiquitin signalling: what's in a chain? Nat Cell Biol. 2004;6:571–572. [PubMed]
4. Pickart CM, Fushman D. Polyubiquitin chains: polymeric protein signals. Curr Opin Chem Biol. 2004;8:610–616. [PubMed]
5. Hicke L, Schubert HL, Hill CP. Ubiquitin-binding domains. Nat Rev Mol Cell Bio. 2005;6:610–621. [PubMed]
6. Harper JW, Schulman BA. Structural complexity in ubiquitin recognition. Cell. 2006;124:1133–1136. [PubMed]
7. Varshavsky A. The ubiquitin system. Trends Biochem Sci. 1997;22:383–387. [PubMed]
8. Matsumoto ML, Wickliffe KE, Dong KC, Yu C, Bosanac I, et al. K11-Linked Polyubiquitination in Cell Cycle Control Revealed by a K11 Linkage-Specific Antibody. Mol Cell. 2010;39:477–484. [PubMed]
9. Hershko A, Ciechanover A. The ubiquitin system. Annu Rev Biochem. 1998;67:425–479. [PubMed]
10. Kloetzel PM. Antigen processing by the proteasome. Nat Rev Mol Cell Bio. 2001;2:179–187. [PubMed]
11. Reed SI. Ratchets and clocks: the cell cycle, ubiquitylation and protein turnover. Nat Rev Mol Cell Bio. 2003;4:855–864. [PubMed]
12. van Wijk SJL, Timmers HTM. The family of ubiquitin-conjugating enzymes (E2s): deciding between life and death of proteins. FASEB J. 2010;24:981–993. [PubMed]
13. Ye Y, Rape M. Building ubiquitin chains: E2 enzymes at work. Nat Rev Mol Cell Bio. 2009;10:755–764. [PMC free article] [PubMed]
14. Michelle C, Vourc'h P, Mignon L, Andres CR. What was the set of ubiquitin and ubiquitin-like conjugating enzymes in the eukaryote common ancestor? J Mol Evol. 2009;68:616–628. [PMC free article] [PubMed]
15. Winn PJ, Zahran M, Battey JND, Zhou YX, Wade RC, et al. Structural and electrostatic properties of ubiquitination and related pathways. Front Biosci. 2007;12:3419–3430. [PubMed]
16. Burroughs AM, Jaffee M, Iyer LM, Aravind L. Anatomy of the E2 ligase fold: Implications for enzymology and evolution of ubiquitin/Ub-like protein conjugation. J Struct Biol. 2008;162:205–218. [PMC free article] [PubMed]
17. Hamilton KS, Ellison MJ, Barber KR, Williams RS, Huzil JT, et al. Structure of a conjugating enzyme-ubiquitin thiolester intermediate reveals a novel role for the ubiquitin tail. Structure. 2001;9:897–904. [PubMed]
18. DeSalle LM, Pagano M. Regulation of the G1 to S transition by the ubiquitin pathway. FEBS Lett. 2001;490:179–189. [PubMed]
19. Ptak C, Prendergast JA, Hodgins R, Kay CM, Chau V, et al. Functional and physical characterization of the cell cycle ubiquitin-conjugating enzyme CDC34 (UBC3). Identification of a functional determinant within the tail that facilitates CDC34 self-association. J Biol Chem. 1994;269:26539–26545. [PubMed]
20. Mathias N, Steussy CN, Goebl MG. An essential domain within Cdc34p is required for binding to a complex containing Cdc4p and Cdc53p in Saccharomyces cerevisiae. J Biol Chem. 1998;273:4040–4045. [PubMed]
21. Ju T, Bocik W, Majumdar A, Tolman JR. Solution structure and dynamics of human ubiquitin conjugating enzyme Ube2g2. Proteins. 2010;78:1291–1301. [PMC free article] [PubMed]
22. Li W, Tu D, Brunger AT, Ye Y. A ubiquitin ligase transfers preformed polyubiquitin chains from a conjugating enzyme to a substrate. Nature. 2007;446:333–337. [PubMed]
23. Petroski MD, Deshaies RJ. Mechanism of lysine 48-linked ubiquitin-chain synthesis by the cullin-RING ubiquitin-ligase complex SCF-Cdc34. Cell. 2005;123:1107–1120. [PubMed]
24. Gazdoiu S, Yamoah K, Wu K, Pan Z-Q. Human Cdc34 employs distinct sites to coordinate attachment of ubiquitin to a substrate and assembly of polyubiquitin chains. Mol Cell Biol. 2007;27:7041–7052. [PMC free article] [PubMed]
25. Coccetti P, Tripodi F, Tedeschi G, Nonnis S, Marin O, et al. The CK2 phosphorylation of catalytic domain of Cdc34 modulates its activity at the G1 to S transition in Saccharomyces cerevisiae. Cell Cycle. 2008;7:1391–1401. [PubMed]
26. Sadowski M, Mawson A, Baker R, Sarcevic B. Cdc34 C-terminal tail phosphorylation regulates Skp1/cullin/F-box (SCF)-mediated ubiquitination and cell cycle progression. Biochem J. 2007;405:569–581. [PubMed]
27. Oh RS, Bai X, Rommens JM. Human homologs of Ubc6p ubiquitin-conjugating enzyme and phosphorylation of HsUbc6e in response to endoplasmic reticulum stress. J Biol Chem. 2006;281:21480–21490. [PubMed]
28. Sarcevic B, Mawson A, Baker RT, Sutherland RL. Regulation of the ubiquitin-conjugating enzyme hHR6A by CDK-mediated phosphorylation. EMBO J. 2002;21:2009–2018. [PubMed]
29. Goebl MG, Goetsch L, Byers B. The Ubc3 (Cdc34) ubiquitin-conjugating enzyme is ubiquitinated and phosphorylated in vivo. Mol Cell Biol. 1994;14:3022–3029. [PMC free article] [PubMed]
30. Pyerin W, Barz T, Ackermann K. Protein kinase CK2 in gene control at cell cycle entry. Mol Cell Biochem. 2005;274:189–200. [PubMed]
31. Barz T, Ackermann K, Pyerin W. Control of methionine biosynthesis genes by protein kinase CK2-mediated phosphorylation of Cdc34. Cell Mol Life Sci. 2006;63:2183–2190. [PubMed]
32. Meggio F, Pinna LA. One-thousand-and-one substrates of protein kinase CK2? FASEB J. 2003;17:349–368. [PubMed]
33. Amadei A, Linssen AB, Berendsen HJ. Essential dynamics of proteins. Proteins. 1993;17:412–425. [PubMed]
34. Arai R, Yoshikawa S, Murayama K, Imai Y, Takahashi R, et al. Structure of human ubiquitin-conjugating enzyme E2 G2 (UBE2G2/UBC7). Acta Crystallogr F. 2006;62:330–334. [PMC free article] [PubMed]
35. Cook WJ, Martin PD, Edwards BF, Yamazaki RK, Chau V. Crystal structure of a class I ubiquitin conjugating enzyme (Ubc7) from Saccharomyces cerevisiae at 2.9 angstroms resolution. Biochemistry. 1997;36:1621–1627. [PubMed]
36. Das R, Mariano J, Tsai YC, Kalathur RC, Kostova Z, et al. Allosteric Activation of E2-RING Finger-Mediated Ubiquitylation by a Structurally Defined Specific E2-Binding Region of gp78. Mol Cell. 2009;34:674–685. [PMC free article] [PubMed]
37. Liu Y, Mathias N, Steussy CN, Goebl MG. Intragenic suppression among CDC34 (UBC3) mutations defines a class of ubiquitin-conjugating catalytic domains. Mol Cell Biol. 1995;15:5635–5644. [PMC free article] [PubMed]
38. Varelas X, Ptak C, Ellison MJ. Cdc34 self-association is facilitated by ubiquitin thiolester formation and is required for its catalytic activity. Mol Cell Biol. 2003;23:5388–5400. [PMC free article] [PubMed]
39. Banerjee A, Gregori L, Xu YP, Chau V. The bacterially expressed yeast CDC34 gene-prodcut can undergo autoubiquitination to form a multiubiquitin chain-linked protein. J Biol Chem. 1993;268:5668–5675. [PubMed]
40. Deffenbaugh AE, Scaglione KM, Zhang LX, Moore JM, Buranda T, et al. Release of ubiquitin-charged Cdc34-S similar to Ub from the RING domain is essential for ubiquitination of the SCFCdc4-bound substrate Sic1. Cell. 2003;114:611–622. [PubMed]
41. Chauhan D, Li G, Hideshima T, Podar K, Shringarpure R, et al. Blockade of ubiquitin-conjugating enzyme CDC34 enhances anti-myeloma activity of Bortezomib/Proteasome inhibitor PS-341. Oncogene. 2004;23:3597–3602. [PubMed]
42. Eliseeva E, Pati D, Diccinanni MB, Yu AL, Mohsin SK, et al. Expression and localization of the CDC34 ubiquitin-conjugating enzyme in pediatric acute lymphoblastic leukemia. Cell Growth Differ. 2001;12:427–433. [PubMed]
43. Duan X, Trent JO, Ye H. Targeting the SUMO E2 conjugating enzyme Ubc9 interaction for anti-cancer drug design. Anticancer Agents Med Chem. 2009;9:51–54. [PubMed]
44. Hunter T. The age of crosstalk: Phosphorylation, ubiquitination, and beyond. Mol Cell. 2007;28:730–738. [PubMed]
45. Salazar C, Brummer A, Alberghina L, Hofer T. Timing control in regulatory networks by multisite protein modifications. Trends Cell Biol. 2010;20:634–641. [PubMed]
46. Miranda FF, Teigen K, Thorolfsson M, Svebak RM, Knappskog PM, et al. Phosphorylation and mutations of Ser(16) in human phenylalanine hydroxylase - Kinetic and structural effects. J Biol Chem. 2002;277:40937–40943. [PubMed]
47. Groban ES, Narayanan A, Jacobson MP. Conformational changes in protein loops and helices induced by post-translational phosphorylation. PLoS Comput Biol. 2006;2:238–250. [PMC free article] [PubMed]
48. Aifa S, Frikha F, Miled N, Johansen K, Lundstrom I, et al. Phosphorylation of Thr(654) but not Thr(669) within the juxtamembrane domain of the EGF receptor inhibits calmodulin binding. Biochem Bioph Res Co. 2006;347:381–387. [PubMed]
49. Bartova I, Koca J, Otyepka M. Regulatory phosphorylation of cyclin-dependent kinase 2: insights from molecular dynamics simulations. J Mol Model. 2008;14:761–768. [PubMed]
50. Jarmula A, Fraczyk T, Cieplak P, Rode W. Mechanism of influence of phosphorylation on serine 124 on a decrease of catalytic activity of human thymidylate synthase. Bioorgan Med Chem. 2010;18:3361–3370. [PMC free article] [PubMed]
51. Adiga SP, Brenner DW. Molecular Basis for Neurofilament Heavy Chain Side Arm Structure Modulation by Phosphorylation. J Phys Chem C. 2010;114:5410–5416.
52. Narayanan A, Jacobson MP. Computational studies of protein regulation by post-translational phosphorylation. Cur Op Struct Biol. 2009;19:156–163. [PubMed]
53. Eswar N, Eramian D, Webb B, Shen M-Y, Sali A. Protein structure modeling with MODELLER. Methods Mol Biol. 2008;426:145–159. [PubMed]
54. Larkin MA, Blackshields G, Brown NP, Chenna R, McGettigan PA, et al. Clustal W and Clustal X version 2.0. Bioinformatics. 2007;23:2947–2948. [PubMed]
55. Holm L, Sander C. Protein structure comparison by alignment of distance matrices. J Mol Biol. 1993;233:123–138. [PubMed]
56. Paterlini MG, Thomas DD. The alpha-helical propensity of the cytoplasmic domain of phospholamban: a molecular dynamics simulation of the effect of phosphorylation and mutation. Biophys J. 2005;88:3243–3251. [PubMed]
57. Hollender D, Károly-Lakatos A, Forgó P, Körtvélyesi T, Dombi G, et al. Al(III)-binding ability of an octapeptide and its phosphorylated derivative. J Inorg Biochem. 2006;100:351–361. [PubMed]
58. Fuhrmans M, Sanders BP, Marrink SJ, de Vries AH. Effects of bundling on the properties of the SPC water model. Theor Chem Acc. 2010;125:335–344.
59. Darden T, York D, Pedersen L. Particle Mesh Ewald - An N.Log(N) Method For Ewald Sums In Large Systems. J Chem Phys. 1993;98:10089–10092.
60. Caves LS, Evanseck JD, Karplus M. Locally accessible conformations of proteins: multiple molecular dynamics simulations of crambin. Protein Sci. 1998;7:649–666. [PubMed]
61. Friedman R, Caflisch A. On the orientation of the catalytic dyad in aspartic proteases. Proteins. 2010;78:1575–1582. [PubMed]
62. Loccisano AE, Acevedo O, DeChancie J, Schulze BG, Evanseck JD. Enhanced sampling by multiple molecular dynamics trajectories: carbonmonoxy myoglobin 10 micros A0–>A(1-3) transition from ten 400 picosecond simulations. J Mol Graph Model. 2004;22:369–376. [PubMed]
63. Monticelli L, Sorin EJ, Tieleman DP, Pande VS, Colombo G. Molecular simulation of multistate peptide dynamics: a comparison between microsecond timescale sampling and multiple shorter trajectories. J Comput Chem. 2008;29:1740–1752. [PubMed]
64. Papaleo E, Mereghetti P, Fantucci P, Grandori R, De Gioia L. Free-energy landscape, principal component analysis, and structural clustering to identify representative conformations from molecular dynamics simulations: The myoglobin case. J Mol Graph Model. 2009;27:889–899. [PubMed]

Articles from PLoS Computational Biology are provided here courtesy of Public Library of Science