Phosphatidylinositol 3-kinase type 2α (PI3KC2α) is an essential member of the structurally unresolved class II PI3K family with crucial functions in lipid signaling, endocytosis, angiogenesis, viral replication, platelet formation and a role in mitosis. The molecular basis of these activities of PI3KC2α is poorly understood. Here, we report high-resolution crystal structures as well as a 4.4-Å cryogenic-electron microscopic (cryo-EM) structure of PI3KC2α in active and inactive conformations. We unravel a coincident mechanism of lipid-induced activation of PI3KC2α at membranes that involves large-scale repositioning of its Ras-binding and lipid-binding distal Phox-homology and C-C2 domains, and can serve as a model for the entire class II PI3K family. Moreover, we describe a PI3KC2α-specific helical bundle domain that underlies its scaffolding function at the mitotic spindle. Our results advance our understanding of PI3K biology and pave the way for the development of specific inhibitors of class II PI3K function with wide applications in biomedicine.
Phosphoinositide 3-kinases (PI3Ks) are a family of lipid-modifying enzymes that phosphorylate the 3′-OH group of inositol phospholipids and play key roles in physiology ranging from cell growth and metabolism to organismal development. Dysfunction of PI3K signaling is implicated in human diseases including cancer, immunodeficiency, diabetes and neurological disorders1,2,3. Mammalian PI3Ks are grouped into three classes based on their structural organization. Class I PI3Ks are receptor-activated heterodimeric enzymes with pivotal roles in cell signaling (for example, cell growth) via synthesis of phosphatidylinositol (PI) 3,4,5-trisphosphate (PI(3,4,5)P3) at the plasma membrane2,4,5,6. Isoform-specific pharmacological inhibitors of class I PI3K activity have undergone clinical development as anticancer therapeutics and for the treatment of human disorders caused by PI3K pathway hyperactivation.
Complexes of Vps34, the sole class III PI3K member, produce PI 3-phosphate (PI(3)P) in the endolysosomal system and during autophagy to regulate vesicle-mediated sorting en route to lysosomes1. Recent structural studies7,8 have enabled the development of selective Vps34 inhibitors that have been instrumental for the analysis and manipulation of class III PI3K function in autophagy and in the regulation of nutrient signaling.
The class II PI3K isoforms PI3KC2α, PI3KC2β and PI3KC2γ are unique in directly synthesizing PI 3,4-bisphosphate (PI(3,4)P2) from PI 4-phosphate (PI(4)P) at the plasma membrane and within the endolysosomal system9,10, in addition to synthesis of PI 3-phosphate (PI(3)P)11,12,13,14. The mechanistic basis for the ability of class II PI3Ks to recognize PI(4)P as a substrate to directly produce local pools of PI(3,4)P2 at defined endocytic membrane nanodomains is unknown. PI3KC2α is essential in mice13. Loss of its catalytic activity is associated with cellular defects in endocytosis15,16, angiogenesis and endothelial cell function17,18,19, regulation of blood pressure20, viral replication21,22, platelet formation23,24 and primary cilia signaling13. Abrogation of PI3KC2α activity in animal models and in humans leads to kidney cyst formation, skeletal abnormalities, neurological symptoms and cataract formation25. In addition to these catalytic roles, PI3KC2α is also required for genome stability by acting as a scaffold at the mitotic spindle during cell division26.
In contrast to class I4,6 and class III PI3Ks (refs. 4,7,8,27) that are understood in structural detail, little is known about the structural and functional architecture, and mechanism of activation of class II PI3Ks including PI3KC2α. Unlike their class I and class III relatives that are targeted to their site of action via associated subunits, class II enzymes such as PI3KC2α lack stable association with other subunits4,14 and, thus, must be activated via a distinct regulatory mechanism that so far has remained elusive. The lack of structural information on PI3KC2α and related class II PI3Ks has also greatly hampered the development of isoform-selective pharmacological inhibitors for clinical applications. Moreover, the molecular basis of the scaffolding function of PI3KC2α at the mitotic spindle via its association with the microtubule-binding protein TACC3 at kinetochore fibers to prevent aneuploidy26 is unknown.
To address these important unresolved issues, we have determined high-resolution crystal structures as well as a 4.4-Å cryogenic- electron microscopic (cryo-EM) structure of PI3KC2α in different conformational states and in the presence of nonselective small molecule inhibitors. Our results identify a hitherto unknown coincident mechanism of lipid-induced activation of PI3KC2α that is distinct from that of all other PI3Ks and can serve as a model for the entire class II PI3K family. Moreover, our structural and functional biochemical data will greatly facilitate the future development of isoform-selective PI3KC2α inhibitors with biomedical applications that range from the treatment of thrombosis28 to viral infections21,22, diabetes29 and cancer1,14.
Overall architecture of PI3KC2α
Like other members of the PI3K family1,4, PI3KC2α contains a PI3K core that consists of a Ras-binding domain (RBD) and an N-terminal C2 domain, as well as helical and kinase domains (KDs). In addition, PI3KC2α harbors the C-terminal Phox-homology (PX) and C2 domains that are unique to class II enzymes (Fig. 1a). To determine the X-ray crystal structure of PI3KC2α, we embarked on an iterative process of construct screening and optimization of various forms of PI3KC2α from different species assisted by hydrogen/deuterium exchange–mass spectrometry (HDX–MS) to identify disordered regions. A purified mouse PI3KC2α construct containing a re-engineered internal loop sequence and lacking the intrinsically disordered N-terminal region and the C-terminal C2 domain (C-C2) (Extended Data Figs. 1a,b and 2) was used to obtain the 3.3 Å crystal structure of PI3KC2αΔN+ΔC−C2 (Table 1).
The overall structure of PI3KC2αΔN+ΔC−C2 comprises a large compact multidomain kinase core that is mounted onto a helical stalk (Fig. 1b). The latter is unique to class II PI3Ks and has not been observed or predicted before in any other PI3K, that is PI3Kα−δ or Vps34 (Fig. 1c). The compact core region is flanked by the distantly located PX domain that is stabilized by contacts with a neighboring molecule in the crystal. Earlier biochemical data demonstrated an autoinhibitory role of the PX-C2 domains for PI3KC2α catalytic activity30. The release of the PX-C2 domain from the catalytic core may thus indicate that the obtained PI3KC2αΔN+ΔC−C2 crystal structure represents an active conformation of the enzyme, a hypothesis tested and corroborated below. The core region and the helical stalk comprise an N-terminal helix and five additional domains: the RBD, the N-terminal C2 domain (N-C2), the solenoid helical domain that tightly packs against the catalytic KD comprising a smaller N-terminal and a larger C-terminal lobe, and a helical bundle domain (HBD) (Fig. 1b). The helical domain in this assembly acts as the central hub that connects the conserved archetypical two-lobed KD of PI3KC2α (refs. 4,6,31) with the N-C2 domain. The globular N-terminal RBD displays a conserved α/β sandwich fold that resembles the RBD of class I PI3Ks (refs. 4,6) (Fig. 1c) and forms close contacts with the N-terminal lobe of the KD. In spite of this structural conservation, the primary sequence between the RBDs of PI3KC2α and class I PI3Ks is poorly conserved (<25%, Extended Data Fig. 2). This is consistent with the fact that class II PI3Ks including PI3KC2α functionally associate with endosomal Rab family proteins12,13 rather than with Ras, a major activator of class I PI3Kα (refs. 5,6,32).
A conserved feature of all mammalian class II PI3Ks is a sequence insertion of about 100 amino acids between the RBD and the N-C2 domain (Extended Data Fig. 2) that is absent in class I and class III enzymes (Fig. 1c). This sequence folds into a unique stalk-forming HBD comprising four helices (Fig. 1b). The HBD points away from the kinase core and is dispensable for catalytic activity (Extended Data Fig. 1c), suggesting that it exhibits a structural role as a protein interaction scaffold, as corroborated below (Fig. 6). The HBD contacts the N-terminal C2 domain via its C-terminal helices and connects to this domain via a short flexible linker. The N-C2 domain preserves an antiparallel β-sandwich topology. Based on the abundance of conserved basic residues within the disordered loop that connects β-strands 3 and 4, the N-C2 domain might associate with negatively charged membrane phospholipids. This role of the N-C2 domain is distinct from its function in Vps34, where it serves as a protein interaction hub7 (Fig. 1c).
Structural basis for PI3KC2α catalytic activity
To gain insights into the mechanism of catalysis and to enable the development of small molecule inhibitors of PI3KC2α, we determined crystal structures of the kinase core domain. Based on the PI3KC2αΔN+ΔC−C2 construct, we designed a recombinant PI3KC2αcore variant that lacks the N-terminal low complexity region and the distal PX and C-C2 domains. The HBD was substituted by a short seven residue-long linker (Fig. 1a and Extended Data Fig. 2). The 2.5-Å crystal structure of PI3KC2αcore determined in the absence or presence of Mg2+ and ATP confirmed the architecture of the PI3KC2α catalytic core (Fig. 2a, Extended Data Fig. 3a and Table 1) and revealed important insights into the catalytic mechanism (Fig. 2b,c).
The PI3KC2α KD displays a typical PI3K KD fold comprising a smaller N- and a larger C-lobe linked by a hinge (Extended Data Fig. 3b). The ATP-binding P-loop is located between strands kβ1 and kβ2, and contacts the α-phosphate via a conserved serine (S1114). The catalytic loop located between kα6 and kβ7 contains a conserved 1250DRH1252 motif, in which R1251 stabilizes the N-terminal part of the activation loop containing the 1268DFG1270 motif. H1252 within the DRH motif could act as catalytic base in lipid kinases to deprotonate the 3′-OH of the inositol substrate, a reaction aided by D1250 and D1268 (ref. 31). An atypical feature of the crystallized PI3KC2α catalytic core is the presence of only a single Mg2+ ion that is coordinated by the β- and γ-phosphates of ATP and D1146 in kα3 and D1268 in the DFG motif. In this Mg2+-bound state, N1255, that is a residue bound to a second Mg2+ ion in PI3Kγ5 and other PI3Ks4, interacts with D1250 and H1252 in the HRD motif, apparently to inhibit the catalytic function (Fig. 2c and Extended Data Fig. 3b). Hence, this conformation of PI3KC2α likely reflects an early precatalytic state. Binding of the second Mg2+ conceivably induces a conformational change of N1255 to release the HRD motif from intramolecular inhibition, thereby enabling catalysis.
Class II PI3Ks including PI3KC2α among other features are distinguished from class I and class III enzymes by their substrate selectivity, most notably their unique ability to use PI(4)P as a substrate to directly produce PI(3,4)P2 at endocytic membranes1,14, for example to facilitate endocytosis15,33. We confirmed the preference of purified recombinant PI3KC2α to synthesize PI(3,4)P2 from PI(4)P over PI(3)P synthesis from PI (Fig. 2e), in agreement with our earlier cell-based data15,16. Cellular production of PI(3,4)P2 versus PI(3)P in addition to substrate availability is likely modulated by the specific membrane environment, explaining the distinct functions of PI3KC2α at the plasma membrane and at endosomes1,14. Lipid substrate binding in PI 3-kinases is encoded within the activation loop. The primary sequence of the activation loop is highly conserved also among class II PI3Ks, suggesting that they bind their substrates via similar mechanisms (Extended Data Fig. 2). While the N-terminal part of the activation loop harboring the catalytic DFG motif is clearly resolved, the C-terminal part of the PI3KC2α activation loop containing the phospholipid headgroup-binding basic residues remains disordered. We therefore used the class I PI3Kα complexed to PI(4,5)P2 (ref. 34) as a reference to model PI(4)P headgroup binding to PI3KC2α. In this model, the 3′-OH group of inositol is oriented toward the γ-phosphate of ATP, whereas the 4-phosphate binds to a flexible positively charged surface created by K1283 and R1284 on the C-terminal activation loop (Fig. 2d). We tested this model experimentally by creating charge neutralization mutants of PI3KC2α. Consistently, we found that alanine substitution of K1283 and R1284 abrogated catalytic activity toward PI(4)P (Fig. 2f) and greatly reduced phosphorylation of PI (Extended Data Fig. 3c), whereas alanine substitution of K1283 only had very minor effects.
These data provide a firm structural basis for the unique ability of PI3KC2α and related class II PI3Ks to directly synthesize PI(3,4)P2 from PI(4)P to control its biological function and activity.
Small molecule inhibition of PI3KC2α catalytic function
Given the multiple important roles of PI3KC2α and related class II PI3Ks in cell physiology and in disease1,14, we next sought to probe the structural basis for inhibition of its catalytic activity by small molecules. Although no specific inhibitors of PI3KC2α have been identified so far, the enzyme is known to be targeted by pan-PI 3-kinase inhibitors (that is, PIK-90, Extended Data Fig. 4b)35 and by Torin-2, an ATP-competitive inhibitor of the PI3K-related kinase superfamily member mTOR36 (Extended Data Fig. 4a). To explore the determinants of inhibitor potency and specificity, we determined the structures of PI3KC2αcore bound to Torin-2 or PIK-90 and compared these to the structure of the apo-form of the enzyme (Fig. 3a). Torin-2 binds to PI3KC2α in a mode similar to mTOR (Fig. 3b and Extended Data Fig. 4c). The tricyclic benzonapththyridine ring of Torin-2 occupies the hydrophobic adenine pocket and a sulfur–pi interaction contributed by the conserved M1125 located in hydrophobic pocket II. Binding is further enabled by local small scale conformational changes of K1138 and D1268 to accommodate the amino-pyrimidine group of Torin-2 and by hydrophobic contacts of the benzotrifluoride group with M1136 and F1112 (Fig. 3b,c). The reduced half-maximum inhibitory concentration (IC50) of Torin-2 for mTOR (IC50mTOR = 2.5 nM versus IC50 PI3KC2α = 64 nM) compared to PI3KC2α is largely due to the pi–pi interaction of the tricyclic benzonapththyridine ring with W2239 inside the mTOR hinge region36, a residue not conserved in PI3KC2α (Fig. 3b and Extended Data Fig. 4c). PIK-90, which also displays profound off-target activity toward PI3KC2α (IC50PI3KC2α = 78 nM), occupies a similar position to Torin-2 in the ATP site. The imidazoquinazoline ring of PIK-90 binds to the adenine pocket via a single hydrogen bond and hydrophobic region II (Fig. 3d and Extended Data Fig. 4d), while the pyridine ring in the terminal hinge of PIK-90 targets the innermost region of the affinity pocket (Fig. 3d,e). In contrast to Torin-2, association of PI3KC2α with PIK-90 involves comparably minor conformational movements of K1138 and D1268 (Fig. 3e). We conclude that Torin-2 and PIK-90 bind to PI3KC2α via the conserved ATP-binding site common to PI3K-related kinases and PI3Ks and in a manner similar to complex formation with their target enzymes (Extended Data Fig. 4c,d), providing a structural basis for their high affinity but moderate selectivity.
Based on these data and the size and chemical composition of the catalytic site in PI3KC2α we predict that PI3KC2α should in principle be amenable to selective targeting by high-affinity small molecule inhibitors.
Conformational control of PI3KC2α activity
Unlike class I and class III PI3Ks that are activated by membrane binding of their associated subunits2,4,7,27,34, class II PI3Ks such as PI3KC2α are autoregulated by their lipid-binding distal PX and C2 domains30. To structurally dissect the mechanism of PI3KC2α autoregulation, we purified near full-length PI3KC2α only lacking the intrinsically disordered N-terminal region but containing the distal PX and C2 domains (PI3KC2αΔN) (Extended Data Fig. 1a,b). We then determined the three-dimensional (3D) structure of PI3KC2αΔN by single-particle cryo-EM (Fig. 4 and Extended Data Fig. 5). Tilted data collection followed by two-dimensional (2D) classification resulted in a reconstruction with a nominal resolution of 4.4 Å from roughly 600,000 particles (Table 2) with substantial resolution anisotropy and the highest resolution in the core domain (Extended Data Fig. 5). The cryo-EM structure of PI3KC2αΔN unequivocally showed the catalytic core of PI3KC2α, which was overlaid almost perfectly with the PI3KC2α crystal structure. Two additional EM densities were located underneath the core region: a donut-shaped density in 2D classes that adopted a barrel shape in the 3D map. This density could accommodate the previously solved crystal structure of the C-terminal C2 domain of PI3KC2α (ref. 37) (Fig. 4). A second, less well-defined density was located in the vicinity of the C-terminal lobe of the catalytic kinase core domain, which likely corresponds to the lipid-binding PX domain (Fig. 4).
As the PX domain exhibited significant flexibility within PI3KC2α, we complemented our results from single-particle cryo-EM by crosslinking–mass spectrometry (XL–MS). This analysis (Supplementary Table 2) imposed distance constraints (30 Å, measured by the Cα–Cα distance between two crosslinked residues) of the PX domain relative to the C-C2 domain and the C-terminal lobe of the kinase core domain (Extended Data Fig. 6a–c), and supported docking of the PX domain into the cryo-EM structure38. We then used the information derived from cryo-EM, XL–MS and the crystal structure of PI3KC2αcore to generate a composite 3D model of PI3KC2α. Ιn this model, only the N-terminal half of kα12 (kα12(N)) is folded whereas the remainder of it is disordered. kα12(N) interacts with the loop between kα7 and kα8 of the KD forming closed contact I. The disordered C-terminal half of kα12 provides the flexibility necessary to place the C-C2 domain in the vicinity of the RBD, where it forms another set of interactions referred to as closed contact II (Fig. 5a). These contacts precisely map to putative autoinhibitory interfaces defined earlier by HDX–MS analysis30. In particular, we had reported that mutation of 1303EKP1305 to 1303KKT1305 (that is, ‘KKT mutant’), in the kinase core domain in closed contact I, results in elevated lipid kinase activity. Moreover, HDX–MS analysis had identified a putative intramolecular interaction between the RBD and the distal PX-C2 domain module30. Our integrative structural analysis identifies this interaction as closed contact II, formed by K426, W458, D461 and D462 on the RBD. Based on these data, we hypothesized that the composite structure of PI3KC2αΔN represents an inactive conformation that is stabilized by closed contacts I and II.
We further experimentally tested this model. Affinity chromatography experiments showed that the immobilized glutathione S-transferase- (GST-)tagged C2, but not the PX domain, directly associates with PI3KC2αΔN+ΔPX−C2 but less well with a mutant version of PI3KC2α, in which the RBD binding interface with the distal C2 domain had been perturbed by mutations in the closed contact I interface (K426A, W458A, D461A, D462A; that is, the ‘RBD mutant’) (Extended Data Fig. 6d). Disruption of either closed contact I in the KKT mutant (1303EKP1305 to 1303KKT1305) or of contact II in the RBD mutant (K426A, W458A, D461A, D462A) significantly increased the PI(3,4)P2-synthesizing activity of PI3KC2α, a phenotype further augmented in a double KKT/RBD mutant of PI3KC2α, in which both inhibitory interfaces were disrupted (Fig. 5c).
As PI3KC2α transitions from the inactive closed to the active open conformation, the C2 and PX domains likely are dislodged from their positions at the RBD and kinase core, respectively, while kα12 undergoes repositioning and folding into a complete helix (Fig. 5a,b). Consistently, we observed the PX domain to be displaced from the kinase core, and closed contact I involving the N terminus of kα12 to be disrupted in the crystal structure of PI3KC2αΔN+ΔC−C2 (Fig. 1b and Extended Data Fig. 3a). Instead, in this open conformation of PI3KC2α, the kα12 helix interacts via hydrogen bonding of H1391 with the backbone of a short helical segment within the intermediate section of the activation loop (Fig. 5b). In the open conformation, the C-terminal part of the activation loop known to be crucial for lipid binding remains flexible to enable catalysis.
This mechanism is distinct from the function of kα12 in other PI3Ks. PI3Kγ uses kα12 to capture the catalytic loop in an inactive state (Extended Data Fig. 7a), whereas in VPS34, kα12 interacts with the N terminus of VPS15 to trap the activation loop7 (Extended Data Fig. 7b). Finally, conformational opening requires the lipid-binding distal C2 domain to be displaced from its inhibitory contact with the RBD. In the closed conformation, association with the RBD renders the lipid-binding surface of the C2 domain difficult to access and misaligns it with the substrate lipid-binding site in the activation loop (Extended Data Fig. 7c). Hence, we predict the distal C2 domain to be flexibly positioned away from the kinase core in the open conformation of the enzyme (Fig. 6e and below). A further prediction from this structure-based activation mechanism is that disruption of the interaction between kα12 and the activation loop in the open form should abrogate lipid kinase activity. In vitro kinase assays confirmed that the H1391A mutation in the center of the kα12-activation loop interface resulted in a complete loss of enzymatic activity (Fig. 5c). H1391 is thus required to stabilize the open catalytically active conformation of PI3KC2α.
Our combined data indicate a molecular model for the conformational control of PI3KC2α activity by large-scale rearrangements in the position of the lipid-binding PX and C2 domains that is accompanied by refolding and repositioning of the kα12 helix critical for catalysis.
Conformational control of PI3KC2α function in cells
We tested this structure-based model for the conformational activation of PI3KC2α at membranes by analyzing the PI(3,4)P2-synthesizing activity of PI3KC2α during endocytic membrane dynamics. Depletion of PI3KC2α from Cos7 cells resulted in reduced levels of PI(3,4)P2 at endocytic plasma membrane coated pits and a concomitant reduction in clathrin-mediated endocytosis of transferrin. These defects were rescued by re-expression of the small interfering RNA-resistant wild-type (WT) enzyme (Fig. 5d–f) or a mutant lacking the HBD (Fig. 6a), in agreement with its presumed scaffolding role during mitosis. In contrast, PI3KC2α mutant versions defective in PI(4)P substrate binding (K1283A,R1284A) or lacking critical hydrogen bonding via H1391 to stabilize the open conformation (H1391A) failed to restore PI(3,4)P2 levels and defective endocytosis. Conversely, conformational activation of PI3KC2α by disrupting closed contacts I and II via the combined KKT and RBD mutations led to elevated cellular PI(3,4)P2 synthesis and a gain in endocytic transferrin uptake (Fig. 5d–f). These results confirm that structural changes in the position of the lipid-binding PX and C2 domains and the kα12 helix underlie the conformational activation of PI3KC2α at membranes in vivo.
A further prediction from our combined structural and biochemical studies is that distinct structural elements mediate the catalytic roles of PI3KC2α in endocytic membrane dynamics and its noncatalytic function at the mitotic spindle1,14. The unique HBD of PI3KC2α, which points away from the KD (Figs. 1b and 4c), is dispensable for catalytic activity in vitro (Extended Data Fig. 1c) and for endocytosis in vivo (Fig. 6a). We therefore hypothesized, that the HBD might facilitate targeting of the enzyme to the mitotic spindle by associating with the microtubule-binding protein TACC3 (ref. 26). Consistently, we found that the HBD of PI3KC2α with its four antiparallel α-helices displays strong structural homology to cytoskeletal proteins, such as the focal-adhesion targeting domain of Crk-associated substrate (Cas) and to the F-actin binding domains of vinculin and α-catenin (Fig. 6b). To probe the possible function of the HBD in targeting of PI3KC2α to the mitotic spindle, we examined the subcellular localization of an N-terminally truncated PI3KC2α lacking the clathrin binding region, a mutant version thereof, in which the HBD was deleted (PI3KC2αΔN+ΔHBD), or the isolated HBD alone (PI3KC2αHBD). The HBD was sufficient for targeting to the mitotic spindle and for association with TACC3 (Fig. 6c,d), whereas deletion of the HBD abrogated the spindle localization of PI3KC2αΔN (Fig. 6c) and complex formation with TACC3 (Fig. 6d). These data uncover the unique HBD as an important structural element that underlies the scaffolding function of PI3KC2α at the mitotic spindle26. We note that while the presence of the HBD is conserved among the members of the class II PI3K subfamily, its relatively low level of sequence conservation (Extended Data Fig. 2) suggests that they interact with different protein binding partners to execute putative noncatalytic functions.
Our integrated structural analysis of PI3KC2α reveals different conformational states of the enzyme that suggest a molecular model for the local activation of PI3KC2α at endocytic membranes (Fig. 6e). In its cytosolic form, the enzyme is present in a closed inactive conformation that is stabilized by intramolecular contacts within the kinase core domain that occlude catalysis and an inhibitory interface between the RBD and the distal C2 domain, which may be further augmented by placement of the PX domain at the interface between the distal C2 and the C-terminal lobe of the kinase core domain, in agreement with our earlier biochemical data30. Clathrin-mediated recruitment15,39 and activation of PI3KC2α at endocytic membranes involves a large-scale conformational change within the single subunit enzyme that releases PI3KC2α from autoinhibition to enable local PI 3-phosphate synthesis (Fig. 5). In this active conformation, the substrate PI(4)P is bound by basic residues (that is, K1283, R1284) within the PI3KC2α activation loop (Fig. 2d–f). Of note, these residues are absent from Vps34, a PI3K that is unable to use PI(4)P as a substrate, providing a molecular explanation for the distinct catalytic activities of PI3KC2α and related class II PI3Ks (refs. 1,2,14).
The mechanism of activation of PI3KC2α is distinct from that of all other PI3Ks, in which membrane binding and catalytic activation are induced by conformational transitions in tightly associated accessory subunits (compare Fig. 1c). In class I PI3K, hydrophobic residues in the C-terminal tail of the KD not present in PI3KC2α as well as basic amino acids in the charged activation loop are only allowed to contact the membrane once the enzyme has been released from allosteric inhibition by its regulatory p85 subunit40. The class III Vps34 complex binds to membranes via the tips of two arms that is three of its four subunits: one contact is formed by the catalytic Vps34 subunit and the Vps15 myristoylation site, the other one involves the Vps30/Beclin 1 BARA domain7.
The unique mechanism of membrane binding and activation of PI3KC2α is not only interesting from a mechanistic viewpoint, but also bears important implications for our understanding of class II PI3K biology. Our structural data predict that the conformational activation and, thereby, the catalytic function of PI3KC2α is triggered by multiple coincident signals, most notably, the membrane association of its PX and C2 domains30,37. The exquisite lipid-binding specificity of these domains for PI(4,5)P2 thereby limits PI3KC2α activity to nanoscale sites enriched in PI(4,5)P2, providing a structural explanation for the observed spatiotemporal restriction of PI3KC2α-mediated synthesis of PI(3,4)P2 or PI(3)P at late-stage endocytic pits15,33,41 and the base of primary cilia13,42. Our structural and biochemical data further predict that the conformational activation of PI3KC2α, and likely other class II PI3K family members, further requires or is facilitated by complex formation of the RBD with an endocytic Rab protein12,13. Rab association would aid displacement of the distal C2 domain from the RBD and, thereby, act as a third coincidence determinant, in addition to clathrin15,39 and PI(4,5)P2 (ref. 30). The structure-based mechanism for the activation of PI3KC2α at membranes described here therefore predicts that the multiple physiological functions of PI3KC2α, for example in endocytic receptor internalization and recycling12,15,16,33, VEGF-driven angiogenesis19 and viral replication21,22, result from and are defined by the coincident interaction of PI3KC2α with PI(4,5)P2 and different Rab proteins that steer its catalytic activity to distinct nanoscale sites. Identifying the respective Rab protein underlying these activities will be key to our understanding of the physiological functions of PI3KC2α in cell physiology and disease.
Additionally to providing insights into the mechanism of PI3KC2α activation and function, our structural analysis of PI3KC2α in complex with nonselective PI3K inhibitors will undoubtedly serve as a door-opener for rational development of isoform-selective PI3KC2α inhibitors and other class II PI3K family members that may provide new therapeutic avenues for the treatment of important human diseases such as thrombosis28, viral infection21,22, diabetes29 or cancer1,14. Finally, we provide a structural basis for the scaffolding function of PI3KC2α at the mitotic spindle that involves the association of its unique HBD with the microtubule-associated kinetochore protein TACC3 (Fig. 6). These structural insights will be of relevance to develop new therapeutics to fight cancer and cancer metastasis14,26.
Oligonucleotide sequences used in this study are listed in Supplementary Table 1.
HeLa, human embryonic kidney 293T (HEK293T) and Cos7 cells were obtained from ATCC and cultured in DMEM with 4.5 g l−1 glucose (Lonza) containing 10% heat-inactivated FBS, 100 U ml−1 penicillin and 100 μg ml−1 streptomycin (Gibco). Cells were routinely tested for and devoid of mycoplasma contamination.
Cloning and mutagenesis
Complementary DNA encoding mouse PI3KC2α was synthesized from total RNA extracted from mouse brain using a gene specific primer (5′TAGATACGTTGCCGCAGTCAGCTG3′) (Supplementary Table 1) according to the SuperScript III protocol. For baculovirus-mediated expression in insect cells, cDNA encoding mouse PI3KC2αΔN (amino acids 377–1686), PI3KC2αΔN+ΔC−C2 (amino acids 377–1,539) and PI3KC2αΔN+ΔPX−C2 (amino acids 377–1,400) was amplified by PCR and cloned into pFL10His via KasI/XbaI restriction sites. Mutations were introduced by site-directed mutagenesis using PCR. Crystallization construct I, PI3KC2αΔN+ΔC−C2 contains a re-engineered internal loop with amino acids 533–544 being replaced by the amino acid sequence GSGS. In PI3KC2αcore, the HBD (amino acids 550–665) was replaced by the sequence SGAGSGA. GST-PX (amino acids 1409–1539), GST-PX-C2 (amino acids 1,409–1,686) and GST-distal C2 (amino acids 1,561–1,686) were cloned into pGEX-4T-1 using BamHI and NotI sites for expression in Escherichia coli. The siRNA-resistant enhanced green fluorescent protein- (eGFP-)PI3KC2α mutant was generated by site-directed mutagenesis PCR based on siRNA-resistant eGFP-PI3KC2α used in our earlier studies15,30.
Protein expression and purification
His10-tagged PI3KC2αΔN, PI3KCΔN+ΔC−C2, PI3KC2αcore and related mutants were expressed in Sf21 insect cells, using SF900-II serum-free media (ThermoFisher). In brief, Sf21 cells (800 ml) grown to a density of 1.5–2 × 106 cells per ml were infected with 8 ml amplified baculovirus encoding the desired construct. Cells were collected when the viability was less than 90%. Cell pellets were stored frozen at −20 °C until purification. For purification, cell pellets from each 200 ml of culture were resuspended in 35 ml of lysis buffer (50 mM Tris pH 7.2, 300 mM NaCl, 10 mM imidazole, 1 mM dithiothreitol (DTT), 0.5% Triton X-100, 1 tablet per 50 ml of protease inhibitor cocktail), sonicated for 1 min (1 s pulse on, 5 s pulse off) and centrifuged for 20 min at 87,000g. Then 50 ml of supernatant were incubated with 0.5 ml Nickel NTA beads (Sigma Inc.) on a rotating wheel for 1 h. Beads were collected in an open column, washed with 20 ml of lysis buffer, then with 30 ml of wash buffer (50 mM Tris pH 7.5, 300 mM NaCl, 20 mM imidazole, 1 mM DTT). Protein was eluted with 8 ml of elution buffer (20 mM Tris pH 7.5, 300 mM NaCl, 300 mM imidazole, 5 mM DTT). The His10-tag was released by tobacco etch virus (10 mg of protein per 0.25 mg of tobacco etch virus) cleavage overnight, while dialyzing against size-exclusion chromatography (SEC) buffer (20 mM Tris pH 7.5, 300 mM NaCl, 5 mM DTT) at 4 °C. Proteins were purified on a Superdex 200 gel filtration column at 4 °C with SEC buffer (20 mM Tris pH 7.5, 300 mM NaCl, 5 mM DTT). Proteins were concentrated to about 2.4 mg ml−1 for PI3KC2αΔN, 2.5 mg ml−1 for PI3KC2αΔN+ΔC−C2, 5 mg ml−1 for PI3KC2αcore and 1–2 mg ml−1 for other mutants. All proteins were flash frozen in liquid nitrogen and stored at −80 °C.
Crystallization of PI3KC2αΔN+ΔC−C2 and PI3KC2αcore
To obtain PI3KC2αΔN+ΔC−C2 crystals, >1,000 conditions were screened using a Crystal Gryphon robot setup (Art Robbins) with 200 nl of protein solution (2.5 mg ml−1) and 200 nl of screen solution in 96-well sitting-drop plates. Initial crystals were observed with a 50% water-diluted kit from Molecular Dimensions Morpheus E10 and E11, which originally contains 0.12 M ethylene glycol mix, 0.1 M Tris/Bicine, 40% v/v ethylene glycol, 20% w/v polyethylene glycol (PEG) 8,000 (in E10) or 40% glycerol and 20% PEG 4,000 (in E11). Optimal crystals were obtained at room temperature by microseeding in 24-well sitting-drop plates in mother liquid containing 0.1 M Tris pH 7.5, 8–9% PEG 20,000, 10% ethylene glycol and 10% formamide (for the protein complex with Torin-2:mother liquid:seed of 1:5:0.5 μl). Thin plate-shaped crystals grew into large clusters within 2–3 d. Single crystals were isolated and washed in cryogenic solution (50% fresh prepared mother liquid, 50% buffer (20 mM Tris pH 7.5, 150 mM CsI, 5 mM DTT), supplied with 10% ethylene glycol). Initial PI3KC2αcore crystals were obtained using homemade screening buffers containing 0.1 M Tris pH 7.5, 200 mM MgSO4, 10% PEG 8,000. Concentrated protein sample was filtered with 0.2-μm spin filters and final crystals were grown in 0.1 M Tris pH 7.5, 100–200 mM MgSO4, 7–10% PEG 3,350. Crystals were cryo-protected with mother liquid supplied with 10% ethylene glycol. For ligand soaking, 2 mM ATP, 1 mM Torin-2, 0.5 mM PIK-90 were prepared in cryoprotection solution and incubated with protein crystals for 30 min. Crystals were mounted in a nylon loop and flash cooled in liquid nitrogen.
Data collection, model building and refinement
Diffraction data were collected at station BL14.1 of BESSY/Helmholtz Center Berlin (HZB). Images were processed with XDSAPP43. The PI3KC2αΔN+ΔC−C2 structure was determined by molecular replacement with the PHENIX suite44 using the helical domains and KDs of PI3Kγ (PDB 1E8X) and the PX domain of PI3KC2α (2IWL) as search models. The structure was manually built using COOT and iteratively refined using Refmac45 and BUSTER46 PI3KC2αcore structures were determined by molecular replacement with PHENIX using the crystal structure of PI3KC2αΔN+ΔC−C2 as a search model. The structures were manually built using COOT47 and refined with PHENIX and BUSTER. Data collection and structure refinement statistics are summarized in Table 1. Ramachandran statistics in the order of favored, allowed, outliers for each structure are: PI3KC2αΔN+C−C2 (95.26, 4.74, 0%), PI3KC2αcore apo (96.91, 2.97, 0.12%), PI3KC2αcore in complex with ATP-Mg2+ (94.6, 5.28, 0.12%), PI3KC2αcore in complex with Torin-2 (98.76, 1.11, 0.12%) and PI3KC2αcore in complex with PIK-90 (96.78, 3.22, 0%). Structural data were deposited in the Protein Data Bank (PDB) and are available under accession numbers 7BI2, 7BI4, 7BI6 and 7BI9.
Negative stain screening of PI3KC2αΔN in buffer with different salt concentrations
Purified PI3KC2αΔN (roughly 2.4 mg ml−1, in 20 mM Tris-HCl buffer, with 300 mM NaCl at pH 7.4) was diluted to a final concentration of 0.02 mg ml−1 into buffers containing 20 mM Tris-HCl, and various concentrations of NaCl (50 to 300 mM) at pH 7.4, before being negatively stained with 2% (w/v) uranyl formate. Negatively stained images were collected using a Tecnai Spirit BioTwin transmission electron microscope (Thermo Fisher Scientific) at 120 kV at a nominal magnification of ×49,000 (2.26 Å per pixel) on a Gatan Rio CCD camera (4,000 × 4,000). The sample diluted in a buffer containing 100 mM NaCl presented a good particle distribution without showing significant aggregates. A group of images was collected at a defocus around −1.5 to −3.5 μm. Contrast transfer function (CTF) estimation was performed with CTFFIND 4.1 (ref. 48). Particles were auto-picked using Gautomatch-0.53 (https://www2.mrc-lmb.cam.ac.uk/research/locally-developed-software/zhang-software/), and 2D class averages were performed with RELION-2.0 and higher49.
Cryo-EM sample preparation of PI3KC2αΔN
Purified PI3KC2αΔN (0.8 mg ml−1 in 20 mM Tris-HCl, 100 mM NaCl at pH 7.4) were used for plunge-freezing. Double-application of 3 μl of diluted PI3KC2αΔN were applied onto freshly plasma-cleaned (NanoClean, model 1070, Fischione Instruments) QUANTIFOIL Holey Au-carbon-R2/2 specimen grids, and vitrified by plunge-freezing into liquid ethane using a Mark IV Vitrobot device (Thermo Fisher Scientific). Cryo-EM specimen prepared with different blotting conditions (blot force, blot time) were screened. Final datasets were collected from the cryo-EM grids with thinner uniform ice thickness and good particle orientation distribution.
Cryo-EM single-particle data collection of PI3KC2αΔN specimen
The cryo-EM single-particle datasets of PI3KC2αΔN were collected without and with −30° stage-tilting on a Titan Krios cryo-transmission electron microscope (Thermo Fisher Scientific) operated at 300 kV and equipped with a K3 direct electron detector (Gatan, Inc.) device at a nominal magnification of ×105,000 yielding a pixel size at the specimen of 0.837 Å per pixel in counting mode (Table 2). Videos were collected with EPU, a data collecting automation software package (Thermo Fisher Scientific), with an imaging setting of total exposure equal to 60 electrons over 50 fractions in 3 s and a defocus range between −1.5 and −2.8 μm, at the Max Planck Institute of Biophysics, Frankfurt, Germany.
Cryo-EM image processing
During data collection, all datasets were preprocessed ‘on-the-fly’ using cryoSPARC live50 running video motion correction, CTF estimation and automatic particle picking and stream 2D classification to estimate particle quality. As the streamed 2D classification showed particle features as expected, more data automated positions were defined. Once data collection was completed, all videos from both datasets were imported into cryoSPARC, processed with patch motion correction and CTF estimation, and auto-picked separately. The auto-picked particles were inspected and extracted with a box size of 260 pixels to perform particle cleaning using several rounds of 2D classification and 3D heterogeneous refinement (3D classification, if effective) with C1 symmetry, accordingly. The most homogenous particle sets after cleaning and separation from both datasets were merged, containing about 1 million particles, and taken to perform 3D homogeneous refinement and further 2D classifications as necessary. 3D variability was performed to show the heterogeneity of the PI3KC2αΔN specimen due to its flexibility. Fourier shell correlation (FSC) estimation was done both in cryosparc and Relion. Postprocessing and local resolution was estimated in RELION-3.0, and global directional resolution estimation was performed using 3DFSC (ref. 51). A detailed image processing pipeline is shown in Extended Data Fig. 5. Cryo-EM data were deposited in the PDB and are available under accession number EMD-12191. Original EM micrographs were deposited in the Electron Microscopy Public Image Archive (EMPIAR) (code EMPIAR-10665).
ADP-Glo kinase assay of PI3KC2α
Purified PI3KC2α variants were prediluted to 0.5 mg ml−1 in SEC buffer used for purification. All variants were subsequently diluted to 20 μg ml−1 in kinase buffer (5 mM HEPES/KOH, pH 7.2, 25 mM KCl, 2.5 mM Mg (OAc)2, 150 mM K-glutamate, 10 μM CaCl2, 0.2% CHAPS). Native liver PI or PI 4-phosphate (PI(4)P) were dissolved to a concentration of 400 μM with kinase buffer by water-bath sonification and then supplied with 200 μM ATP. The buffer supplied with 200 μM ATP served as a negative control. Reactions were started by mixing 5 μl of protein stock with 5 μl of substrate solution and incubated for 20 m at room temperature. The reactions were stopped by adding 10 μl of ADP-Glo reagent (Promega). After 40 min of incubation, 20 μl of Kinase Detection Reagent were added. After 20 min incubation, luminescence was read with a TECAN plate reader. IC50 measurements of Torin-2 and PIK-90 were carried out using concentration series of these compounds.
XL–MS analysis of PI3KC2αΔN
Purified PI3KC2αΔN was buffer exchanged to crosslinking buffer (20 mM BisTris-propane, pH 7.5, 300 mM NaCl) by dialysis. 1.2 mg ml−1 PI3KCαΔN was diluted into 20 mM BisTris-propane, pH 7.5, to final concentration of 0.4 mg ml−1. Crosslinking was performed by adding 0.5 μl of disuccinimidyl sulfoxide (DSSO) (stock concentration 50 mM) to 50 μl diluted PI3KC2αΔN. The reaction was performed twice for 20 min each. Samples were quenched by addition of 1 M Tris pH 7.5 (final concentration 20 mM) for 30 min. Crosslinked PI3KC2αΔN was separated by SDS–PAGE followed by in-gel tryptic digest. Crosslinked peptides were analyzed using a Thermo Scientific Dionex UltiMate 3000 system combined to an Orbitrap Fusion Lumos mass spectrometer. Cross-link acquisition was performed using a MS2-MS3 method. MS2 spectra were acquired on every selected MS1 precursor whereas MS3 acquisitions were triggered if a unique mass difference of 31.9721 was observed in the MS2 spectrum52. Data analysis was conducted using XlinkX standalone52 with the following parameters: minimum peptide length of 6; maximal peptide length of 35; missed cleavages of 3; fix modification: Cys carbamidomethyl of 57.021 Da; variable modification, Met oxidation of 15.995 Da; DSSO crosslinker 158.0038 Da (short arm 54.0106 Da and long arm 85.9824 Da); precursor mass tolerance of 10 ppm and fragment mass tolerance of 20 ppm. Results were reported at 1% false discovery rate (FDR) at the level of cross-link spectrum matches (CSM).
Model of PI3KC2αΔN
To build the model with PX and C2 domain, all of identified crosslinked sites between PX and C2 were introduced with 5–15 Å (Cβ to Cβ) distance restraints for docking of PX and C2 by HADDOCK. In total, 24 docked PX-C2 structures from six different clusters were generated. The PX-C2 domain together with PI3KC2αcore were used to fit into the EM map with Chimera. The best fitted structures were validated with the crosslinked sites between PI3KC2αcore and PX-C2 domain to obtain the final model.
GST pull down assay
GST pull down assays were performed with immobilized GST-fused PX, C2 or PX-C2 of PI3KC2α as baits. Then 10 μg of immobilized GST fusion protein was used to capture 200 μg of PI3KC2αΔN+ΔPX−C2 WT or PI3KC2αΔN+ΔPX−C2 RBD mutant in 500 μl of binding buffer (20 mM Tris, pH 7.5, 100 mM NaCl). Samples were incubated on a rotating wheel for 1 h at 4 °C, unbound material was removed by washing three times and bound proteins were eluted with 2× SDS–PAGE sample buffer. Samples were analyzed by SDS–PAGE and Coomassie blue staining.
Cells were seeded and transfected with 50 μM siRNA on day 1 using jetPRIME (Polyplus Transfection) according to the manufacturer’s instructions by reverse transfection. A second round of knockdowns was performed on day 2. Cells were plated onto a Matrigel (BD Biosciences) -coated cover slides in the morning of day 3 and transfected with eGFP-PI3KC2α constructs using jetPRIME (Polyplus Transfection) according to the manufacturer’s instructions.
Analysis of the localization of eGFP-PI3KC2α in metaphase-arrested cells
HeLa cells were synchronized in metaphase using 2 mM thymidine (Sigma-Aldrich) for 20 h, 30 μM deoxycitidine for 6 h (Sigma-Aldrich) and 50 ng ml−1 nocodazole (Sigma-Aldrich) for 12 h, followed by 2 h release in fresh medium in the presence of 20 mM MG132 (Calbiochem). HeLa cells were blocked in interphase by starvation for 16 h. Synchronized cells were transfected with plasmids encoding eGFP-PI3KC2α WT or mutants. For immunofluorescence, the cells were fixed by ice-cold methanol. HeLa cells were permeabilized with 0.1% Saponin for 10 s and then fixed in 2% paraformaldehyde (PFA) for 5 min. Staining for GFP, α-tubulin and 4,6-diamidino-2-phenylindole (DAPI) was performed, and the cells were examined with a Zeiss Observer-Z1 microscope, equipped with the Apotome, Leica TCS-II SP5 or a Leica TSC-II SP8 confocal microscope.
Coimmunoprecipitation of TACC3 and PI3KC2α
HEK293T were transfected with plasmids encoding eGFP-PI3KC2α WT or mutants, mitotically arrested 24 h post-transfection and gathered as reported in ref. 26. The following primary antibodies were used: TACC3 (Rabbit, no. 8069, Cell Signaling) and homemade GFP (Rabbit, polyclonal). Membranes probed with the indicated antibodies were then incubated with HRP-conjugated anti-Rabbit IgG light chain (1:5,000, 211-032-171, Jackson ImmunoResearch) and developed with enhanced chemiluminescence (ECL, BD).
PI(3,4)P2 detection at the plasma membrane
PI3KC2α KD Cos7 cells or PI3KC2α KD Cos7 cells re-expressing eGFP-PI3KC2α WT or mutants were grown on Matrigel (BD Biosciences)-coated eight-well glass bottom μ-slide (ibidi). Cos7 cells were washed with PBS containing 10 mM MgCl2 once and fixed in 2% PFA with 0.5% glutaraldehyde for 20 min at room temperature. Cells were washed three times with PBS and twice with PBS containing 50 mM NH4Cl. Cells were permeabilized with PBS containing 0.5% Saponin and 1% BSA for 30 min. PI(3,4)P2 antibody (Echlon catalog no. Z-P034b) and Goat anti-Mouse IgG (H + L) AF647 labeled secondary antibody (Thermo Fisher catalog no. A21237) were incubated for 2 and 1 h, respectively, in PBS buffer containing 1% BSA and 10% normal goat serum. Cells were analyzed by total internal reflection fluorescence microscopy (Nikon TI Eclipse, 488 and 561 nm laser, ×60 numerical aperture 1.49 objective and sCMOS Andor mNeo). Plasma membrane PI(3,4)P2 levels at clathrin-coated pits were quantified using ImageJ software.
Transferrin uptake and surface labeling
Cos7 cells transfected with siRNA and/or PI3KC2α (WT or mutant)-encoding plasmids or pretreated for 4 h with 0.1% dimethylsulfoxide or 20 μM PITCOIN1 were starved in serum-free DMEM media for 1 h. For transferrin uptake, cells were incubated with 25 mg ml−1 Alexa647 labeled transferrin (Molecular Probes, Invitrogen) for 10 min at 37 °C in a humidity chamber. Cells were washed twice with ice-cold PBS supplied 10 mM MgCl2 and then acid washed twice at pH 5.3 (0.2 M sodium acetate, 200 mM sodium chloride) on ice for 2 min to remove surface-bound transferrin. Cells were then washed twice more with ice-cold PBS containing 10 mM MgCl2 and fixed with 4% PFA for 45 min at room temperature. For surface labeling, cells were incubated with 25 mg ml−1 Alexa647 labeled transferrin at 4 °C for 45 min and then washed three times with ice-cold PBS (10 mM MgCl2) on ice for 1 min. Cells were fixed with 4% PFA for 45 min at room temperature. Transferrin labeling was analyzed using the Nikon Eclipse Ti microscope and ImageJ software. Internalized transferrin per cell was quantified and normalized to the amount of surface-bound transferrin determined in the same experiment as a measure for the efficiency of internalization.
All data are presented as mean ± s.e.m. and were obtained from ≥3 independent experiments with total sample numbers provided in the figure legends. Statistical significance was evaluated by Prism software (GraphPad), using one simple, two-tailed t-test with theoretical mean of 100 or one-way analysis of variance (ANOVA) test with Tukey’s multiple comparisons. Specific P values are indicated in the legends to figures. Significant differences were marked as *P < 0.05, **P < 0.01, ***P < 0.001 and ****P < 0.0001.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
Structural data were deposited in the PDB and are available under accession numbers 7BI2, 7BI4, 7BI6 and 7BI9 (X-ray crystallography) (Table 1) and EMD-12191 (cryo-EM) (Table 2). Original EM micrographs have been deposited in the EMPIAR and are available under the code EMPIAR-10665. All other data are available in the main manuscript, extended data, supplementary materials and in the source data. Materials and reagents are available from the corresponding authors upon request. Source data are provided with this paper.
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We are indebted to M.C. Wahl (Freie Universität Berlin, Berlin, Germany) for help with insect cell expression, M. Bommer (Max-Delbrück Center, Berlin, Germany) for help with data collection and processing, and D. Löwe and U. Fink (both from FMP Berlin, Germany) for technical assistance. We also thank BESSY/HZB (Berlin, Germany) staff scientists for support during data collection at beamline MX14.1. Supported by in-house funds from the FMP. Y.Z. and M.K. are supported by a Sofja Kovalevskaja Award from the Alexander von Humboldt Foundation. Y.Z. was partially supported by an IMPRES international student scholarship from the Max Planck Society. M.K. is supported by the Heisenberg Program of the Deutsche Forschungsgemeinschaft (grant no. KU 3222/3-1). O.D. acknowledges funding by the Deutsche Forschungsgemeinschaft (grant no. TRR186/A23 to O.D.).
Open access funding provided by Leibniz-Forschungsinstitut für Molekulare Pharmakologie im Forschungsverbund Berlin e.V. (FMP)
The authors declare no competing interests.
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Extended Data Fig. 1 Purification and lipid kinase activity of PI3KC2αΔN, PI3KC2αΔN+ΔC−C2, and PI3KC2αcore.
(a) Size exclusion chromatography of PI3KC2αΔN, PI3KC2αΔN+ΔC−C2 and PI3KC2αcore. Peak fractions were collected for structural analysis. (b) Coomassie Blue-stained SDS–PAGE of purified PI3KC2αΔN, PI3KC2αΔN+ΔC−C2 and PI3KC2αcore from (a). (c) In vitro kinase activity of PI3KC2αWT and PI3KC2αΔHBD using PI(4)P as a substrate. HBD deletion showed no influence on kinase activity. Data represent mean ± SD from triplicate (n = 3) experiments. One sample, 2 tailed t-test with hypothetical mean of 100, NS = non-significant.
Extended Data Fig. 2 Secondary structure of PI3KC2α and primary sequence alignment with PI3Ks.
The sequence corresponding to crystallization construct I (that is musPI3KC2αΔN+ΔC−C2) was used as template to align human PI3KC2α (hs PI3KC2α, UniProt accession: O00443.2), other human class II PI3K isoforms [PI3KC2β (UniProt accession: O00750.2), PI3KC2γ (UniProt accession: O75747.3)], human class I PI3K (PI3Kγ, UniProt accession: P48736.3), and human class III PI3K (VPS34, UniProt accession: Q8NEB9.1). The dashed lines indicate disordered linker regions. All identified secondary structural elements are color-coded as in Fig. 1a. The light grey arrow indicates the replacement of a short, disordered sequence by GSGS to improve crystallization of PI3KC2αΔN+ΔC−C2. To generate the ΔHBD construct, the HBD was replaced by the sequence SGAGSGA as indicated by the orange arrow. kα12 (N) is indicated by a black arrow.
Extended Data Fig. 3 Catalytic activity and structure of PI3KC2α.
(a) Structural superimposition of PI3KC2αΔN+ΔC−C2 (spectrum) and PI3KC2αcore (gray). The main distinctive features are the conformations of kα12 and of the activation loop. In the PI3KC2αΔN+ΔC−C2 structure, a short helical segment within the activation loop and kα12 is well defined and folded. In contrast, in the structure of PI3KC2αcore, only the N-terminal part of kα12 is folded and the short helical segment within the activation loop of PI3KC2α core is disordered. (b) Structural superimposition of the kinase domains from PI3KC2α (N-lobe: cyan; C-lobe: blue) and PI3Kγ (1E8X; wheat). Close-up view of the proposed movement of catalytic loop residues, N1255, and ATP with the appearance of a second metal ion (metal II). Wheat spheres indicate two Mg2+ ions bound to PI3Kγ, black sphere represents the single Mg2+ bound to PI3KC2α. (c) In vitro kinase activity of activation loop mutants with PI as a substrate. The K1283A and R1284A mutations greatly reduce activity. Data represent mean ± SD from triplicate (n = 3) experiments. One sample, 2 tailed t-test with hypothetical mean of 100, NS = non-significant; ∗∗p = 0.0025.
Extended Data Fig. 4 Pharmacological inhibition of mTOR kinase and PI3Kγ by Torin-2 and PIK-90.
(a,b) 2D structure and IC50 of Torin-2 (a) and PIK-90 (b) bound to PI3KC2α. (c) Binding pocket of mTOR in association with Torin-2 (pdb: 4JSX). W2239 from the hinge of mTOR kinase contributes a pi-pi interaction with Torin-2. (d) Binding pocket of PI3Kγ in complex with PIK-90 (pdb: 2CHX). The pyridine ring of PIK-90 binds to a deep cavity in the affinity pocket of PI3Kγ.
Extended Data Fig. 5 Cryo-EM structure determination of PI3KC2αΔN.
(a) Cryo-EM image processing workflow. 2.3 ×106 of particles were extracted for 2D classification. 683k particles were selected after two rounds of 2D classification. 340k selected particles from 2D classes based on datasets with 30 tilted angles were joined for a third round of 2D averaging. 601k selected particles were finally used to obtain a 3D reconstruction with a global resolution 4.35 Å. The angular distribution is represented as a heat map to indicate the distributed projections of all particles contributing to the consensus map. (b) Representative 2D classes of PI3KC2αΔN after 2 rounds of 2D averaging. (c) Local resolution of the PI3KC2αΔN EM-map shown as a heat map from 4.04 Å (blue) to 6.71 Å (red) with two different views. The central core region of PI3KC2α displays a compact helix-rich fold with the highest local resolution.
Extended Data Fig. 6 Different conformational states of PI3KC2α.
(a) PI3KC2αΔN was crosslinked with DSSO chemical crosslinker and separated by 4–15% gradient SDS-PAGE. The monomeric band of crosslinked PI3KC2αΔN indicated as dashed red square was cut out for further MS analysis. (b) Identified crosslinked peptides using DSSO as chemical crosslinker. (c) Model of PI3KC2αΔN based on the cryo-EM map without the PX domain. The PX domain was docked onto the distal C2 domain using restraints imposed by the obtained crosslinks between the PX and distal C2 domain, using the HADDOCK server. The obtained model was subsequently verified manually using all identified crosslinking sites between the kinase core, PX, and distal C2 domains and the C- to N- terminal connections between these domains. Green line: distance < 30 Å; red line; distance > 30 Å. Distant crosslinks (>30 Å) suggest different conformational states of PI3KC2α. (d) Interaction between the kinase core and lipid binding C2 domains of PI3KC2α. GST pull down assays using GST-PX, GST-C2 or GST-PX-C2 as baits to capture PI3KC2αΔN+ΔPX−C2 Wild-type (WT) or RBD mutant (K426A; W458A; D461A; D462A) versions. Samples were analyzed by SDS-PAGE and Coomassie Blue staining and quantified using ImageJ software. Binding of PI3KC2αΔN+ΔPX−C2 WT was set to 100%. Data represent SEM from triplicate (n = 3) experiments.
Extended Data Fig. 7 Comparison of the inhibitory conformations of PI3Ks.
(a) Auto-inhibited conformation of PI3Kγ (pdb: IE8X). kα12 (red) bends inward towards the catalytic pocket. (b) Auto-inhibited conformation of yeast Vps34/Vps15 in complex II (pdb: 5DFZ). The activation loop of VPS34 (yellow) is locked by kα12 (red) and the N-terminus of VPS15 (blue). (c) Auto-inhibited conformation of PI3KC2αΔN as ribbon and surface representation. The distal C2 domain binds to the RBD. The yellow and orange regions represent the catalytic pocket and the activation loop, where lipid substrates bind. The PI(4,5)P2-binding surface in the distal C2 domain is colored in blue. The locations of the lipid-binding pockets are distributed on different sides of the PI3KC2α molecule in the closed conformation.
Supplementary Table 1 and PDB validation report.
Supplementary Table 1
Source Data Fig. 2e
Statistical source data for Fig. 2e.
Source Data Fig. 2f
Statistical source data for Fig. 2f.
Source Data Fig. 5c
Statistical source data for Fig. 5c.
Source Data Fig. 5e
Statistical source data for Fig. 5e.
Source Data Fig. 5f
Statistical source data for Fig. 5f.
Source Data Fig. 6a
Statistical source data for Fig. 6a.
Source Data Fig. 6d
Unprocessed blots for Fig. 6d.
Source Data Extended Data Fig. 1a
Chromatography data for Extended Data Fig. 1a.
Source Data Extended Data Fig. 1b
Uncropped gel for Extended Data Fig. 1b.
Source Data Extended Data Fig. 1c
Statistical source data for Extended Data Fig. 1c.
Source Data Extended Data Fig. 3c
Statistical source data for Extended Data Fig. 3c.
Source Data Extended Data Fig. 6d
Statistical source data for Extended Data Fig. 6d.
Source Data Extended Data Fig. 6d
Uncropped gel for Extended Data Fig. 6d.
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Lo, WT., Zhang, Y., Vadas, O. et al. Structural basis of phosphatidylinositol 3-kinase C2α function. Nat Struct Mol Biol 29, 218–228 (2022). https://doi.org/10.1038/s41594-022-00730-w
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