Cryptococcus neoformans is the leading cause of death by fungal meningoencephalitis; however, treatment options remain limited. Here we report the construction of 264 signature-tagged gene-deletion strains for 129 putative kinases, and examine their phenotypic traits under 30 distinct in vitro growth conditions and in two different hosts (insect larvae and mice). Clustering analysis of in vitro phenotypic traits indicates that several of these kinases have roles in known signalling pathways, and identifies hitherto uncharacterized signalling cascades. Virulence assays in the insect and mouse models provide evidence of pathogenicity-related roles for 63 kinases involved in the following biological categories: growth and cell cycle, nutrient metabolism, stress response and adaptation, cell signalling, cell polarity and morphology, vacuole trafficking, transfer RNA (tRNA) modification and other functions. Our study provides insights into the pathobiological signalling circuitry of C. neoformans and identifies potential anticryptococcal or antifungal drug targets.
Cryptococcus neoformans is the leading cause of fungal meningoencephalitis and is responsible for over a million infections and 600,000 deaths annually on a global scale1. This pathogenic yeast is ubiquitously distributed in diverse natural environments. It is considered to be a cosmopolitan fungal pathogen that utilizes a wide variety of living hosts ranging from lower eukaryotes to animals, suggesting broad distribution in the environment under conditions that lead to the production of spores and desiccated yeast cells that are both documented to be infectious propagules2. Nevertheless, treatment of systemic cryptococcosis remains challenging because only limited therapeutic options are available3. In addition to its clinical importance, C. neoformans is regarded as an ideal fungal model system for basidiomycetes, which have been diverging for at least 500 million years from their last common ancestor shared with the ascomycetes, owing to the availability of completely sequenced and well-annotated genome databases, a classical genetic dissection method through sexual differentiation, efficient methods of reverse and forward genetics, and a variety of heterologous host model systems4.
Extensive research efforts have been made over several decades to understand the mechanisms underlying the pathogenicity of C. neoformans. Besides efforts to analyse the functions of individual genes and proteins, recent large-scale functional genetic analyses have provided comprehensive insights into the overall biological circuitry of C. neoformans5,6,7. However, a complete picture of the pathobiological networks of C. neoformans remains elusive, mainly because functions of kinases, which have a central role in signalling and metabolic pathways, have not been fully characterized on a genome-wide scale. In general, kinases have pivotal roles in growth, cell cycle control, differentiation, development, the stress response and many other cellular functions, affecting ∼30% of cellular proteins by phosphorylation8. Furthermore, kinases are considered to be the second largest protein class for drug targets in clinical trials as their inhibition is readily possible by small molecules or antibodies9. The systematic functional profiling of kinases in human fungal pathogens is in high demand to identify virulence-related kinases that could be further developed as antifungal drug targets.
In this study, we performed systematic functional profiling of the kinome networks in C. neoformans by constructing a high-quality library of 264 signature-tagged gene-deletion strains through homologous recombination methods for 129 putative kinases, and examining their phenotypic traits under 30 distinct in vitro conditions, including growth, differentiation, stress responses, antifungal resistance and virulence-factor production. Furthermore, we investigated their virulence and infectivity potential in insect and murine host models. This phenotypic data set is freely accessible to the public through the Cryptococcus kinome database (http://kinase.cryptococcus.org). The data presented in this study provides insights into the pathobiological signalling circuitry of C. neoformans and may help development of novel therapies for cryptococcosis targeting unique virulence-related kinases.
Identification of kinases in C. neoformans
To select the putative kinase genes in the genome of C. neoformans var. grubii (H99 strain), we surveyed a curated annotation of kinases in the H99 genome database provided by the Broad Institute (http://www.broadinstitute.org/annotation/genome/cryptococcus_neoformans) and the JEC21 genome database within the database of the National Center for Biotechnology Information. For each gene that had a kinase-related annotation, we performed protein domain analyses using Pfam (http://pfam.xfam.org/) to confirm the presence of kinase domains and to exclude the genes with annotations such as phosphatases or kinase regulators. Through this analysis, we retrieved 183 putative kinase genes in C. neoformans (Supplementary Data 1). The phylogenetic relationship is shown in Fig. 1a.
The 183 putative kinases were classified into 19 different families based on their sequence and structure similarities (Fig. 1b), as suggested previously10. The protein kinase family is the most dominant one (120) followed by P-loop kinase (16), lipid kinase (10), ribokinase-like kinase (9), GHMP kinase (6) and other small molecule kinases. Eukaryotic protein kinase superfamilies are further classified into eight conventional protein kinase groups (ePKs) and five atypical groups (aPKs)11. ePKs include the protein kinase A, G, and C group (AGC), the calcium and calmodulin-regulated kinase group (CAMK), the casein kinase 1 group (CK1), a group of cyclin-dependent kinases (CDKs), mitogen-activated protein kinases (MAPK), glycogen synthase kinases and CDK-like kinases (CMGC), the receptor guanylate cyclase group (RGC), a group of sterile kinase (STE), the tyrosine kinase group (TK) and the tyrosine kinase-like group (TKL). The aPKs include the phosphatidylinositol 3-kinase-related kinase group (PIKK), the ribosome biogenesis kinase group (RIO), the pyruvate dehydrogenase kinase group (PDHK), and histidine kinase (HisK). To classify the C. neoformans protein kinases based on these criteria, we queried their amino acid sequences in the Kinomer v.1.0 database (http://www.compbio.dundee.ac.uk/kinomer/), which systematically classifies eukaryotic protein kinases based on a hidden Markov model12. Although seven hybrid HisKs (Tco1–7) were not classified by the Kinomer database, we classified them here as HisK in aPKs. The C. neoformans protein kinases consist of 87 ePKs (18 AGC, 22 CAMK, 2 CK1, 24 CMGC, 18 STE, 3 TKL) and 18 aPKs (2 PDHK, 7 PIKK, 2 RIO, 7 HisK) (Fig. 1c). Based on our kinase domain predictions, two other major human fungal pathogens, Candida albicans and Aspergillus fumigatus, appeared to contain 188 and 269 kinases, respectively (Supplementary Data 2). Among pathogenic fungal protein kinases, CMGC, CAMK, STE and AGC kinases appear to be the most common clades (Fig. 1c).
Construction of the C. neoformans kinase mutant library
To gain insights into the biological functions of Cryptococcus kinome networks, we aimed to construct gene-deletion mutants for each kinase and to functionally characterize them. Among the kinases analysed here, mutants for 22 kinases (TCO1, TCO2, TCO3, TCO4, TCO5, TCO7, SSK2, PBS2, HOG1, BCK1, MKK1/2, MPK1, STE11, STE7, CPK1, PKA1, PKA2, HRK1, PKP1, IRE1, SCH9, and YPK1) constructed previously were functionally characterized in part by our prior reports13,14,15,16,17,18,19,20,21,22. For the remaining 161 kinases, we attempted to construct gene-deletion mutants by using large-scale homologous recombination and by analysing their in vitro and in vivo phenotypic traits. We successfully generated 264 gene deletion mutants representing 129 kinases (including those that were previously reported) (Supplementary Data 3).
For the remaining 54 kinases, we were not able to generate mutants even after repeated attempts at gene disruption (more than four attempts, Supplementary Data 1). In many cases, we either could not isolate a viable transformant, observed the retention of a wild-type allele along with the disrupted allele (potentially aneuploidy) or incorrect genotypes were obtained. Among these, 36 (67%) are orthologous to kinases that are essential for the growth of Saccharomyces cerevisiae (26 genes), Schizosaccharomyces pombe (32 genes) or Neurospora crassa (7 genes, Supplementary Data 1). Notably, two genes (MPS1 and PIK1) that are known to be essential in S. cerevisiae were successfully deleted in C. neoformans, suggesting the presence of functional divergence in some kinases between ascomycete and basidiomycete fungi or the presence of functionally redundant kinases in C. neoformans.
Systematic phenotypic profiling of C. neoformans kinome
With this high-quality library of kinase mutants, we performed in vitro phenotypic analyses under 30 distinct growth conditions covering five major phenotypic classes: growth, differentiation, stress responses and adaptations, antifungal drug resistance and production of virulence factors (Supplementary Data 4).
To gain insights into the functional and regulatory connectivity among kinases, we attempted to group kinases by phenotypic clustering through Pearson correlation analysis (Fig. 2). The rationale behind this was that a group of kinases in a given signalling pathway tended to cluster together in terms of shared phenotypic traits. For example, mutants in three-tier MAPK cascades should cluster together because they exhibit almost identical phenotypic traits. In fact, we found that the three-tier kinase mutants in the cell wall integrity MAPK, the high osmolarity glycerol response (HOG) MAPK, and the pheromone-responsive MAPK pathways were clustered together based on their shared functions (Fig. 2). Therefore, groups of kinases clustered together by this analysis are highly likely to function in the same or related signalling cascades.
We identified several hitherto uncharacterized kinases that are functionally correlated with these known signalling pathways. First, we identified CNAG_06553, encoding a protein orthologous to yeast Gal83 that is one of three possible β-subunits of the Snf1 kinase complex controlling the transcriptional changes under glucose derepression in S. cerevisiae23,24. In C. neoformans, Snf1 functions have been previously characterized25. Here we provide several lines of experimental evidence showing that Gal83 is likely to function in association with Snf1 in C. neoformans. First, the in vitro phenotypic traits of the gal83Δ mutant were almost equivalent to those of the snf1Δ mutant (Fig. 2; Supplementary Fig. 1). Both snf1Δ and gal83Δ mutants exhibited increased susceptibility to fludioxonil and increased resistance to organic peroxide. Second, growth defects in the snf1Δ mutant in media containing alternative carbon sources (for example, potassium acetate, sodium acetate and ethanol) were also observed in gal83Δ mutants (Supplementary Fig. 1). Therefore, Gal83 is likely to be one of the possible β-subunits of the Snf1 kinase complex in C. neoformans.
We also identified several kinases that potentially work upstream or downstream of the target of rapamycin (TOR) kinase complex. Although we were not able to disrupt Tor1 kinase, which has been suggested to be essential in C. neoformans26, we found three kinases (Ipk1, Ypk1 and Gsk3) that are potentially related to Tor1-dependent signalling cascades clustered together. Recently, Lev et al.27 proposed that Ipk1 could be involved in the production of inositol hexaphosphate (IP6) based on its limited sequence homology to S. cerevisiae Ipk1. In mammals, inositol polyphosphate multikinase produces IP6, a precursor of 5-IP7 that inhibits Akt activity and thereby decreases mTORC1-mediated protein translation and increases GSK3β-mediated glucose homeostasis and adipogenesis28. In S. cerevisiae, Ypk1 is the direct target of TORC2 by promoting autophagy during amino acid starvation29. In C. neoformans, Ypk1, which is a potential downstream target of Tor1, is involved in sphingolipid synthesis and deletion of YPK1 resulted in a significant reduction in virulence30. Reflecting the essential role of Tor1, all of the mutants—ipk1Δ, ypk1Δ, and gsk3Δ—exhibited growth defects, particularly at high temperature (Fig. 2).
Unravelling the pathogenic kinome networks in C. neoformans
We performed two large-scale in vivo animal studies: a wax moth-killing virulence assay and a signature-tagged mutagenesis (STM)-based murine infectivity assay. We found 35 virulence-related kinases in insect killing assays (Supplementary Fig. 2) and 58 infectivity-related kinases in STM-based murine infectivity assays (Supplementary Fig. 3). Among these kinases, 30 (denoted in the negative side of the STM graphs) were co-identified by both assays (Fig. 3a), whereas 5 and 28 kinases were specifically identified by the insect killing and STM-based murine assays, respectively (Fig. 3a,b). In total, we discovered 63 kinase mutants apparently involved in the pathogenicity of C. neoformans.
Supporting the quality of our data, 19 known virulence-related kinases were rediscovered by our study (kinases listed in black in Fig. 3a), including Mpk1 (refs 31, 32), Hog1 (ref. 15), Pka1 (ref. 33), Ire1 (ref. 22), Ypk1 (refs 17, 30) and Snf1 (ref. 25). Chang et al.34 demonstrated that Gsk3 is required for the virulence of serotype D C. neoformans (B3501A) in a murine model system. We found that Gsk3 is also required for the virulence of serotype A C. neoformans (H99S). Although not previously reported, deletion mutants of kinases functionally connected to these known virulence-related kinases were also found to be attenuated in virulence or infectivity. These include bck1Δ and mkk1/2Δ mutants (related to Mpk1) and the gal83Δ mutant (related to Snf1) (Fig. 2). Notably, 44 kinases have been for the first time identified to be involved in the pathogenicity of C. neoformans.
For the 63 pathogenicity-related kinases in C. neoformans, we analysed phylogenetic relationships among orthologs, if any, in fungal species and other eukaryotic kingdoms (Fig. 4a), and compared our large-scale virulence data of C. neoformans with those of other fungal pathogens. A large-scale kinome analysis was performed for the pathogenic fungus Fusarium graminearum, which causes scab in wheat plants, and 42 virulence-related protein kinases were identified35. Twenty-one were involved in the pathogenicity of both types of fungi (Fig. 4b). In another human fungal pathogen C. albicans, genome-wide pathogenic kinome analysis has not been performed and yet 25 kinases are known to be involved in the virulence of C. albicans, based on information from the Candida genome database (http://www.candidagenome.org/) (Supplementary Data 2). Six were involved in the pathogenicity of both C. neoformans and C. albicans (Fig. 4b). Notably, four kinases (Sch9, Pka1, Hog1 and Mpk1) appear to be core-virulence kinases as they are involved in the virulence of all three fungal pathogens.
IPK1 (CNAG_01294), encoding a protein similar to inositol 1,3,4,5,6-pentakisphosphate 2-kinase from plants, is either not present or distantly related to those in ascomycete fungi and humans, and is considered a potential anti-cryptococcal target because inositol pyrophosphates and polyphosphates are critical for metabolic adaptation to host environments and the pathogenicity of C. neoformans27,36. Here we found that, in addition to lacking virulence, the ipk1Δ mutants exhibited pleiotropic phenotypes. Deletion of IPK1 increased capsule production, but reduced melanin and urease production. Its deletion also rendered cells to be defective in sexual differentiation and hypersensitive to high temperature and multiple stresses, and enhances susceptibility to multiple antifungal drugs (Supplementary Fig. 4).
Biological functions of pathogenicity-related kinases
We employed a genome-scale co-functional network for C. neoformans, CryptoNet (http://www.inetbio.org/cryptonet)17 to search for proteins functionally linked to the pathogenicity-related kinases, and thus construct a functional network of the pathogenicity-related kinome of C. neoformans. We did this by using previously reported information on C. neoformans and the Gene Ontology terms of corresponding kinase orthologs and its interacting proteins in S. cerevisiae and other fungi (Fig. 5). This analysis suggested that pathogenicity-related kinases have a role in a variety of different biological and physiological processes, as shown in Fig. 5 and Supplementary Data 5.
Among pathogenicity-related kinases, kinases involved in the cell cycle and growth control were identified most frequently. These include CDC7, MPS1, PIK1, CDC2801, MEC1, BUD32, and CKA1. Cdc7 is an essential catalytic subunit of the Dbf4-dependent protein kinase that is required for firing of the replication of origin throughout the S phase in S. cerevisiae37. Cdc7 in C. neoformans has a kinase domain at the C terminus (292–669 aa) and an extended N-terminal region (Supplementary Fig. 5a). Deletion of the whole-kinase domain was not feasible, suggesting that Cdc7 is likely to be an essential gene in C. neoformans (Supplementary Data 1). However, we were able to construct partial CDC7 deletion mutants by disrupting the N-terminal region and part of the kinase domain (1–418 aa) (Supplementary Fig. 5b). Unexpectedly, the remaining kinase domain (419–669 aa) was still expressed in this strain (Supplementary Fig. 5c).
The partial CDC7 deletion strain exhibited severe growth defects and high susceptibility to genotoxic and membrane-destabilizing agents (Fig. 6a) and was highly defective in urease production (Fig. 6b). All of these pleiotropic roles of Cdc7 are likely to affect the virulence of C. neoformans. Summarizing these findings, the whole-kinase domain of Cdc7 is essential for the growth and pathogenicity of C. neoformans.
Unexpectedly, two kinases that are essential in S. cerevisiae, Mps1 and Pik1, were successfully disrupted and shown to be involved in the virulence of C. neoformans. Mps1 is an essential cell cycle protein required for spindle pole body duplication and spindle checkpoint in S. cerevisiae38. The C. neoformans mps1Δ mutant exhibited growth defects (particularly at host temperature) and increased susceptibility to cell wall/membrane-perturbing agents (Fig. 6c), and was defective in melanin production (Fig. 6d). Collectively, these defects may cause the attenuated virulence in the mps1Δ mutants. Pik1 is a phosphatidylinositol 4-kinase that is known to control cytokinesis of S. cerevisiae39. Although the pik1Δ mutant did not exhibit growth defects, it exhibited increased susceptibility to cell membrane, osmotic and oxidative stresses (Fig. 6e) and defects in melanin production (Fig. 6f), which may affect the virulence of C. neoformans. To further validate the role of Cdc7, Mps1 and Pik1, we generated complemented strains by re-integrating the wild-type gene into its native locus, and confirmed that all of their mutant phenotypes were restored (Fig. 6a–f).
CNAG_00415, which was previously named Cdc2801 (ref. 5), is homologous to S. cerevisiae Cdc28 that is an essential CDK1 family protein (BLASTp score 226.5, e-value: 3e−63). However, the closest Cdc28 orthologue in C. neoformans is CNAG_01664 (BLASTp score 384.2, e-value: 1e−110), which was here named Cdc28. Given that we were not able to disrupt CDC28 (Supplementary Data 1), Cdc28 could be an essential gene in C. neoformans. Although deletion of CDC2801 did not affect the normal growth, the cdc2801Δ mutant was highly sensitive to flucytosine, which hampers RNA and DNA synthesis, suggesting that Cdc2801 might be involved in cell cycle control or DNA damage repair (Fig. 6g and Supplementary Fig. 5d). Furthermore, the cdc2801Δ mutant was highly defective in capsule and melanin production (Fig. 6h,i), which may affect infectivity.
Mec1 is required for cell cycle checkpoint, telomere maintenance and silencing and DNA damage repair in S. cerevisiae40. Reflecting these roles, deletion of MEC1 increased cellular sensitivity to genotoxic agents in C. neoformans (Supplementary Fig. 5e). Deletion of MEC1 did not cause any lethality or growth defects in C. neoformans (Fig. 6g), as was the case in C. albicans41. Cka1 and Cka2 are catalytic α-subunits of protein kinase CK2, which have essential roles in growth and proliferation of S. cerevisiae; deletion of both kinases causes lethality42. C. neoformans appears to have a single protein (CKA1) that is orthologous to both Cka1 and Cka2. Deletion of CKA1 severely affected the growth of C. neoformans (Fig. 6g). Notably, the cka1Δ mutant showed elongated, swollen, abnormal cell morphology, which is comparable to, but rather distinct from that of two kinase mutants in the RAM pathway (cbk1Δ and kic1Δ) showing mostly elongated pseudohyphal growth (Fig. 6j). Cbk1 and Kic1 control the cellular polarity and morphology of C. neoformans43. Our insect-killing and STM-based murine infectivity assays revealed the involvement of Cbk1 and Kic1 in virulence and infectivity, respectively (Fig. 3).
Bud32 is also required for growth, potentially through involvement of tRNA modification. In S. cerevisiae, Bud32 is a component of the highly conserved KEOPS/EKC protein complex that is required for N6-threonylcarbamoyladenosine (t6A) tRNA modification44. The bud32Δ mutants exhibited defective growth under basal and most of the stress conditions (Supplementary Fig. 6a), produced smaller amounts of capsule, melanin and urease (Fig. 6k,l and Supplementary Fig. 6b), and were defective in mating (Supplementary Fig. 6c). However, the bud32Δ mutant exhibited an increased resistance to fluconazole (Fig. 6m). Interestingly, we found that deletion of BUD32 abolished the induction of ERG11 upon sterol depletion by fluconazole treatment (Fig. 6n), suggesting a potential role of Bud32 in ergosterol gene expression and sterol biosynthesis in C. neoformans.
Kinases involved in nutrient metabolism are also involved in the pathogenicity of C. neoformans. In S. cerevisiae, Arg5,6 is synthesized as a single protein and is subsequently processed into two separate enzymes for biosynthesis of ornithine, an arginine intermediate45. Consistent with this, we found that the arg5,6Δ mutant was auxotrophic for arginine (Supplementary Fig. 7a). In S. cerevisiae, MET3 encodes an enzyme required for biosynthesis of homocysteine, cysteine and methionine46,47. Indeed, the met3Δ mutant was found to be auxotrophic for both methionine and cysteine (Supplementary Fig. 7b). Notably, arg5,6Δ and met3Δ mutants did not exhibit growth defects in nutrient-rich media, but exhibited severe growth defects at high temperature and under various stress conditions (Supplementary Fig. 7c), which may contribute to their virulence defects.
Retrograde vacuole trafficking affects fungal pathogenicity
In the rice blast fungus, Magnaporthe oryzae, retromer mediating retrograde protein trafficking is critical for autophagy-dependent plant infection48. In C. neoformans, the ESCRT complex-mediated vacuolar sorting process is involved in virulence because some virulence factors such as capsule and melanin need to be secreted49,50. However, the role of endosome-to-Golgi retrograde transport in the virulence of C. neoformans has not previously been characterized. Here we discovered that deletion of CNAG_02680, encoding a VPS15 orthologue involved in the vacuolar sorting process, significantly reduced virulence (Fig. 7a). This result is consistent with the finding that mutation of VPS15 also attenuates virulence of C. albicans51, strongly suggesting that the role of Vps15 in fungal virulence is evolutionarily conserved. In S. cerevisiae, Vps15 constitutes the vacuolar protein sorting complex (Vps15/30/34/38) that mediates endosome-to-Golgi retrograde protein trafficking52.
Similar to the vps15Δ null mutant in C. albicans51, the C. neoformans vps15Δ mutant also exhibited highly enlarged vacuole morphology (Fig. 7b). Defects in retrograde vacuole trafficking can cause extracellular secretion of an endoplasmic reticulum (ER)-resident chaperon protein, Kar2 (ref. 51). Supporting this, we found that vps15Δ mutants were highly susceptible to ER stress agents, such as dithiothreitol (DTT) and tunicamycin (TM) (Fig. 7c). Growth defects at 37 °C strongly attenuated the virulence and infectivity of the vps15Δ mutant (Fig. 7d). This high temperature sensitivity of the vps15Δ mutant may result from increased cell wall and membrane instability (Fig. 7d). In C. albicans, impaired retrograde transport in the vps15Δ mutant also causes cell wall stress, activating the calcineurin signalling pathway by transcriptionally upregulating CRZ1, CHR1 and UTR2 (ref. 51). In C. neoformans, however, we did not observe such activation of signalling components in the calcineurin pathway of the vps15Δ mutant (Fig. 7e). Expression levels of CNA1, CNB1, CRZ1 and UTR2 in the vps15Δ mutant were equivalent to those in the wild-type strain. In C. neoformans, cell wall integrity is also governed by the unfolded protein response (UPR) pathway22. Previously we demonstrated that activation of the UPR pathway through Ire1 kinase results in an unconventional splicing event in HXL1 mRNA, which subsequently controls an ER stress response and adaptation22. Notably, we found that cells with the VPS15 deletion were more enriched with spliced HXL1 mRNA (HXL1s) under basal conditions than the wild-type strain, indicating that the UPR pathway may be activated instead of the calcineurin pathway in C. neoformans when retrograde vacuole trafficking is perturbed (Fig. 7f).
Unknown pathogenicity-related kinases in C. neoformans
Eight of the 63 pathogenicity-related kinases did not appear to have apparent orthologs in model yeasts and were thereby named virulence-related kinase (Vrk1) or infectivity-related kinase 1–7 (Irk1–7) (Figs 2,3). Particularly, we paid attention to Vrk1 (CNAG_06161) because its deletion reduced the virulence of C. neoformans in the insect host model (Supplementary Fig. 3) and diminished infectivity in the murine host model (Fig. 3a). Surprisingly, deletion of VRK1 increased cellular resistance to hydrogen peroxide and capsule production (Fig. 8a,b), which may enhance the virulence potential of C. neoformans. In contrast, increased 5-flucytosine resistance and fludioxonil susceptibility were observed in the vrk1Δ mutant (Fig. 8a). Based on our phenome clustering data, Vrk1 was not clearly grouped with other kinases (Fig. 2), suggesting that Vrk1 may constitute a novel pathogenic kinase network in C. neoformans.
To gain further insight into the regulatory mechanism of Vrk1, we performed comparative phosphoproteomic analysis of the wild-type and vrk1Δ strains to identify Vrk1-specific phospho-target proteins. A total of 823 phosphopeptides corresponding to 380 non-redundant phosphorylated proteins were qualitatively identified by label-free liquid chromatography–tandem mass spectrometry (LC–MS/MS) (Supplementary Data 6). Among these, 29 phosphorylated peptides, which exhibited more than a 1.5-fold difference in the normalized relative phosphopeptide abundance between wild-type and vrk1Δ strains with statistical significance (P<0.05 by Student’s t-test), were considered as potential Vrk1 substrate (Supplementary Data 6), corresponding to the 23 non-redundant proteins. Only 14 of these have known yeast orthologues (Supplementary Data 6 and Fig. 8c).
To gain further insight into Vrk1-dependent functional networks, we used CryptoNet to search for any proteins that were functionally linked to the 23 Vrk1-regulated target proteins and Vrk1 itself, and constructed the correlation networks for those proteins (Supplementary Data 5). Of these, 15 proteins did not have meaningful connections with any known proteins, but eight proteins (Ebp2, Fun12, Rrp5, Sui1, Crn1, Nap1, Htb1 and Top1) were found to be functionally connected. Among a variety of potential biological functions connected to Vrk1 and its substrates, translation and ribosomal RNA processing were mostly over-represented, suggesting that Vrk1 could be involved in the protein translation process, either directly or indirectly.
In this study, we attempted to functionally analyse the C. neoformans kinome web, which is predicted to consist of 183 kinases. We constructed 264 signature-tagged mutant strains representing 129 kinases to systematically analyse their in vitro and in vivo phenotypic traits in C. neoformans. The success level for mutant construction (129 out of 183 (70%)) was lower than that for transcription factors that we previously reported (155 out of 178 (87%))(ref. 6), probably because among fungi, kinases are generally much more evolutionarily conserved than transcription factors, and a greater number of essential or growth-related genes appeared to exist (Supplementary Data 7; Supplementary Fig. 8).
Our systematic analysis revealed that C. neoformans appears to have a significantly redundant set of essential kinases, but also contain a distinct set of essential kinases. This is not unexpected finding based on other systematic fungal kinome analyses. Even in two different very well validated strains of S. cerevisiae (S288C and Σ1278b), marked differences in which genes are essential are observed53. Furthermore, several kinases essential in Aspergillus nidulans (Wee1, NimA, Vps15 and Cka1) are not essential in N. crassa54,55. Among these, Vps15 and Cka1 were also not essential in C. neoformans, although deletion of these genes resulted in growth defects, while Wee1 (CNAG_03171) and NimA (CNAG_04148) orthologs appeared to be essential in C. neoformans (Supplementary Data 1). In addition, Ire1 is not essential in C. neoformans, A. fumigatus, S. pombe and S. cerevisiae, although it is essential in A. nidulans, A. niger and F. graminearum.
Here we showed that CDC7 is likely to be essential in C. neoformans, but partial deletion of the gene region encoding the N terminus (1–418 aa) was feasible and led to the reduced virulence. C. neoformans Cdc7 has a kinase domain at the C terminus and an extended N-terminal region, which is distinct from S. cerevisiae Cdc7 having a similar kinase domain with a very short N-terminal region (Supplementary Fig. 5a). The extended N-terminal region of C. neoformans Cdc7 is longer than that of other fungal Cdc7 orthologues (Supplementary Fig. 5a), although its biological meaning remains unknown. At this point, it remains unclear how the truncated kinase domain of CDC7 in the partial CDC7 deletion strain is expressed. Due to the N-terminal deletion, the closest promoter region for expression of the C-terminal truncated kinase domain is the constitutively active ACT1 promoter in the NAT selection marker (980 bp upstream; Supplementary Fig. 5b). In fact, our quantitative reverse transcription PCR (qRT–PCR) analysis showed that expression levels of the undeleted C-terminal region of CDC7 in the partial CDC7 deletion strain were higher than those in the wild-type strain (Supplementary Fig. 5c), suggesting that the distant ACT1 promoter may induce expression of the C-terminally truncated kinase domain of CDC7. However, it needs to be further characterized whether such a truncated transcript of CDC7 may be properly translated or not.
Mps1 and Pik1 do not appear to be universally essential in all fungi. Despite the essential role of Mps1 in S. cerevisiae38, Mps1 orthologue, Mph1, is not essential in S. pombe because it is required for the spindle assembly checkpoint, but not for spindle pole body duplication56. Therefore, Mps1 may also have non-essential roles in C. neoformans like in S. pombe. The Pik1 kinase is essential in S. cerevisiae and S. pombe by controlling cytokinesis as well as protein secretion and vacuole trafficking57. PIK1 has been successfully deleted and shown to be involved in virulence of C. neoformans58. Pik1 orthologs are not found in Aspergillus, suggesting that the essential role of Pik1 may vary among fungi54. In A. nidulans, Stt4 is proposed to replace the essential role of Pik1 (ref. 54). C. neoformans contains a single ortholog (CNAG_04335) for Stt4 and we have failed to obtain its deletion mutants, suggesting that Stt4 may replace the essential role of Pik1 in C. neoformans.
Although the current study is the first genome-wide functional kinome study in a human fungal pathogen, similar studies have been performed in non-pathogenic filamentous fungal models (N. crassa55 and A. nidulans54,59) and a plant pathogenic filamentous fungus (F. graminearum35). One common phenotypic trait analysed in this and other studies is the role of developmental processes. We found that a total of 42 kinases were involved in the filamentous growth of C. neoformans during mating and that some of these have common roles in the developmental process in other fungi (Supplementary Fig. 9). Such common fungal developmental regulators include kinases in the HOG and pheromone-responsive MAPK pathways (Hog1, Ste7 and Ste11) and Kic102. The role of the two MAPK pathways in the fungal developmental process has already been reported60. However, we first reported here the role of Kic102 in the filamentous growth of C. neoformans. Deletion of KIC102 significantly increased the filamentous growth of C. neoformans (Supplementary Fig. 10), suggesting that Kic102 is a major negative regulator of the developmental process of the pathogen. In contrast, Kic102 orthologues function as positive regulators in developmental processes of other fungi, including A. nidulans54,59, F. graminearum35 and N. crassa55. Therefore, Kic102 and its orthologues appear to play divergent roles in the developmental process among fungi.
Phenotypic clustering of kinases based on collected phenome database revealed several novel kinases. However, there are two major limitations in this phenotypic clustering analysis. First, kinases that are oppositely regulated in the same pathway cannot be clustered. Second, a kinase that regulates a subset of phenotypes governed by a signalling pathway may not be clustered with its upstream kinases; this is the case of the Hog1-regulated kinase 1 (CNAG_00130; Hrk1). Although we previously demonstrated that Hrk1 is regulated by Hog1 (ref. 19), Hrk1 and Hog1 are not clustered together as Hrk1 regulates only subsets of Hog1-dependent phenotypes. Phospholipid flippase kinase 1 (Fpk1) is another such example. In S. cerevisiae, Fpk1 is inhibited by direct phosphorylation by Ypk1 (ref. 61); as expected, Fpk1 and Ypk1 were not clustered together (Fig. 2). To address the functional correlation between Fpk1 and Ypk1, we performed epistatic analyses by constructing and analysing FPK1 overexpression strains constructed in the ypk1Δ and wild-type strain backgrounds. Surprisingly, overexpression of FPK1 partly restored normal growth, resistance to some stresses and amphotericin B in ypk1Δ mutants (Supplementary Fig. 10). These results suggest that Fpk1 could be one of the downstream targets of Ypk1 and may be positively regulated by Ypk1 in C. neoformans.
In addition, we identified 63 pathogenicity-related kinases, which cover a wide range of biological functions of C. neoformans. Current therapeutic options for treatment of cryptococcosis are highly limited owing to problems of incomplete drug efficacy, cytotoxicity and emergence of drug resistant strains for clinically available antifungal drugs3,62. Therefore, the development of novel therapeutic targets and agents is in high demand. From this perspective, pathogenicity-related kinases are very attractive because kinases are highly favoured ‘druggable’ targets in past and on-going clinical trials9. Our comprehensive in vitro phenome data provide significant clues regarding how the pathogenicity-related kinases affect the virulence of C. neoformans (Supplementary Table 1). Of the 63 pathogenicity-related kinases, 30 were required for growth at the host’s physiological temperature, 52 were involved in the production of at least one of three major virulence factors (capsule, melanin and urease), and 57 were are involved in stress responses and adaptation, suggesting that these phenotypic traits are highly correlated with the pathogenicity of C. neoformans. Notably, 28 of these play pleiotropic roles in thermotolerance, virulence factor production, and stress responses. However, the in vitro phenotypic traits of four kinases (Irk2, Irk3, Psk201 and Dak202A) did not reflect their roles in pathogenicity. The irk2Δ mutant showed increased urease production and the irk3Δ mutant did not exhibit any discernible in vitro phenotypes. The psk201Δ mutant showed increased capsule production. Furthermore, the dak202AΔ mutant displayed increased production of capsule and melanin and resistance to oxidative stresses. Therefore, the four kinases could have specific in vivo roles during host infection by C. neoformans.
Based on antifungal drug susceptibility analysis of the mutant kinase library, a total 46, 50 and 43 kinases exhibited either increased or decreased susceptibility to amphotericin B, fluconazole or flucytosine, respectively, which are clinically available antifungal drugs (Supplementary Table 2). Of the pathogenicity-related kinases, we identified 32 kinases whose deletion affected susceptibility to amphotericin B, 33 to fluconazole, and 31 to flucytosine, respectively. Particularly, the following eight kinases appeared to promote resistance to all three antifungal drugs: Ypk1, Vps15, Gsk3, Utr1, Ipk1, Ire1, Cbk1 and Cdc7. Interestingly, they all promoted the pathogenicity of C. neoformans (Fig. 3), suggesting that these eight kinases could be targeted for development of both monotherapy and combination therapy with known antifungal drugs. Therefore, our kinome analysis of C. neoformans reveals potential narrow- and broad-spectrum anticryptococcal and antifungal drug targets.
Animal care and all experiments were conducted in accordance with the ethical guidelines of the Institutional Animal Care and Use Committee of Yonsei University. The Yonsei University Institutional Animal Care and Use Committee approved all of the vertebrate studies.
Construction of the C. neoformans kinase mutant library
Kinase mutant strains were constructed in the C. neoformans serotype A H99S strain63,64 background. For gene-deletion through homologous recombination, gene-disruption cassettes containing the nourseothricin-resistance marker (NAT; nourseothricin acetyl transferase) with indicated signature-tagged sequences (Supplementary Data 8) were generated by using conventional overlap PCR or NAT split marker/double-joint (DJ) PCR strategies as previously reported18,26. All primers used in this study are listed in Supplementary Data 8. In the first round of PCR, the 5′- and 3′-flanking regions for the targeted kinase genes were amplified with primer pairs L1/L2 and R1/R2, respectively, by using H99S genomic DNA as a template. For the overlap PCR, the whole NAT marker was amplified with the primers M13Fe (M13 forward extended) and M13Re (M13 reverse extended) by using a pNAT-STM plasmid containing the NAT gene with each unique signature-tagged sequence. For the split marker/DJ-PCR, the split 5′- and 3′-regions of the NAT marker were amplified with primer pairs M13Fe/NSL and M13Re/NSR, respectively, with the plasmid pNAT-STM. In the second round of overlap PCR, the kinase gene-disruption cassettes were amplified with primers L1 and R2 by using the combined first round PCR products as templates. In the second round of split marker/DJ-PCR, the 5′- and 3′-regions of NAT-split gene-disruption cassettes were amplified with primer pairs L1/NSL and R2/NSR, respectively, by using combined corresponding first round PCR products as templates. For transformation, the H99S strain was cultured overnight at 30 °C in the 50 ml yeast extract-peptone-dextrose (YPD) medium, pelleted and re-suspended in 5 ml of distilled water. Approximately 200 μl of the cell suspension was spread on YPD solid medium containing 1 M sorbitol and further incubated at 30 °C for 3 h. The PCR-amplified gene disruption cassettes were coated onto 600 μg of 0.6 μm gold microcarrier beads (Bio-Rad) and biolistically introduced into the cells by using particle delivery system (PDS-100, Bio-Rad). The transformed cells were further incubated at 30 °C for recovery of cell membrane integrity and were scraped after 4 h. The scraped cells were transferred to the selection medium (YPD solid plate containing 100 μg ml−1 nourseothricin; YPD+NAT). Stable nourseothricin-resistant (NATr) transformants were selected through more than two passages on the YPD+NAT plates. All NATr strains were confirmed by diagnostic PCR with each screening primer listed in Supplementary Data 8. To verify accurate gene deletion and the absence of any ectopic integration for each gene-disruption cassette, Southern blot analysis was performed for all of the kinase mutants. To validate a mutant phenotype and to exclude any unlinked mutational effects, we constructed more than two independent deletion strains for each kinase mutant. Some kinases that had been previously reported by others were independently deleted here with unique signature-tagged markers to perform parallel in vitro and in vivo phenotypic analysis (Supplementary Data 8). When two independent kinase mutants exhibited inconsistent phenotypes (known as inter-isolate inconsistency), we attempted to generate more than three mutants.
Construction of mutant complemented strains
To confirm the phenotypes observed in the pik1Δ, mps1Δ and cdc7Δ mutants, the corresponding complemented strains were generated. To generate mps1Δ::MPS1 complemented strains, a DNA fragment containing the promoter, terminator, and open reading frame (ORF) of MPS1 was amplified using primer pair B7488/J343 and cloned into pGEM-T-easy vector to generate the plasmid pGEM-MPS1. After sequencing to identify a clone with no errors, the MPS1 insert was subcloned into the plasmid pJAF12 containing the neomycin/G418-resistant marker (NEO) to generate the plasmid pJAF12-MPS1. The NdeI-digested linearized pJAF12-MPS1 was biolistically introduced into the mps1Δ mutants (YSB3632 and YSB3633). To generate the cdc7Δ::CDC7 complemented strains, a genomic fragment of the CDC7 gene containing the promoter, ORF, and terminator, was amplified by using the primer pair J331/J332. The amplified CDC7 gene product was cloned into a plasmid pGEM-T-easy vector to generate the plasmid pGEM-CDC7. After sequencing to determine any errors, the CDC7 gene insert was subcloned into the plasmid pJAF12 to generate the plasmid pJAF12-CDC7. The pJAF12-CDC7 was linearized by restriction digestion with NsiI and was biolistically introduced into the cdc7Δ mutants (YSB2911 and YSB2912). To construct the pik1Δ::PIK1 complemented strains, a DNA fragment containing the promoter, terminator, and ORF of PIK1 was cloned as follows. The promoter and 5′-exon region of PIK1 was amplified using the primer pair B7507/J339. The 3′-exon region of PIK1 and terminator was amplified using the primer pair J338/J340. Each amplified DNA fragment was cloned into plasmid pGEM-T-easy vector to generate the plasmids pGEM-PIK1L and pGEM-PIK1R, respectively. After sequencing, the KpnI-digested 3′-exon region of PIK1 and terminator was subcloned into pGEM-PIK1L to produce the plasmid pGEM-PIK1LR. The PIK1 gene insert was subcloned using NotI into the plasmid pJAF12 to generate the plasmid pJAF12-PIK1. The AatII-digested linearized pJAF12-PIK1 was then biolistically introduced into the pik1Δ mutants (YSB1493). A diagnostic PCR was then performed to confirm the targeted integration of each linearized plasmid into the corresponding native locus.
Construction of FPK1 overexpression strains
To construct the FPK1 constitutive overexpression strain, the native promoter of FPK1 was replaced with histone H3 promoter using an amplified homologous recombination cassette (Supplementary Fig. 10a). Primer pairs L1/OEL2 and OER1/PO were used for amplification of the 5′-flaking region and 5′-coding region, respectively, of FPK1 in the first round of PCR. The NEO-H3 promoter region was amplified with the primer pair B4017/B4018. At the second-round PCR, the 5′ region of the PH3:FPK1 cassette was amplified by DJ-PCR using the mixed templates of the 5′-flaking region of FPK1 and the NEO-H3 promoter region with the primer pair L1/GSL (primers are listed in Supplementary Data 8). The 3′-region of the PH3:FPK1 cassette was similarly amplified by using the mixed templates of the 3′-flaking region of FPK1 and the NEO-H3 promoter region with a primer pair GSR/PO. Then, the combined split PH3:FPK1 cassettes were introduced into the wild-type strain H99S and the ypk1Δ mutant (YSB1736) by biolistic transformation. Stable transformants selected on YPD medium containing G418 were screened by diagnostic PCR with a primer pair (SO/B79). The correct genotype was verified by Southern blotting using a specific probe amplified by PCR with primers L1/PO. Overexpression of FPK1 was verified by northern blot analysis using a specific northern blot probe amplified by PCR with primers NP1 and PO (Supplementary Fig. 10b,c).
Growth and chemical susceptibility test
To analyse the growth and chemical susceptibility of the kinase mutant library, C. neoformans cells grown overnight at 30 °C were serially diluted tenfold (1 to 104) and spotted on YPD plates containing the indicated concentrations of chemical agents as follows: sorbitol for osmotic stress and NaCl and KCl for cation/salt stresses under either glucose-rich (YPD) or glucose-starved (YPD without dextrose; YP) conditions; hydrogen peroxide (H2O2), tert-butyl hydroperoxide (an organic peroxide), menadione (a superoxide anion generator), diamide (a thiol-specific oxidant) for oxidative stress; cadmium sulphate (CdSO4) for toxic heavy metal stress; methyl methanesulphonate and hydroxyurea for genotoxic stress; sodium dodecyl sulphate (SDS) for membrane destabilizing stress; calcofluor white and Congo red for cell wall destabilizing stress; TM and DTT for ER stress and reducing stress; fludioxonil, fluconazole, amphotericin B, flucytosine for antifungal drug susceptibility. Cells were incubated at 30 °C and photographed post-treatment from day 2 to day 5. To test the growth rate of each mutant at distinct temperatures, YPD plates spotted with serially diluted cells were incubated at 25, 30, 37, and 39 °C, and photographed after 2–4 days.
To examine the mating efficiency of each kinase mutant, the MATα kinase mutant was co-cultured with serotype A MAT a wild-type strain KN99a as a unilateral mating partner. Each α and a strain was cultured in YPD medium at 30 °C for 16 h, pelleted, washed and resuspended with distilled water. The resuspended α and a cells were mixed at equal concentrations (107 cells per ml) and 5 μl of the mixture was spotted on V8 mating media (pH 5). The mating plate was incubated at room temperature in the dark for 7 to 14 days and was observed weekly.
In vitro virulence-factor production assay
Capsule production was examined qualitatively by India ink staining as previously described14. To measure the capsule production levels quantitatively by Cryptocrit, each kinase mutant was grown overnight in YPD medium at 30 °C, spotted onto Dulbecco’s Modified Eagle’s solid medium, and incubated at 37 °C for 2 days for capsule induction. The cells were scraped, washed with phosphate buffered saline (PBS), fixed with 10% of formalin solution, and washed again with PBS. The cell concentration was adjusted to 3 × 108 cells per ml for each mutant and 50 μl of the cell suspension was injected into microhaematocrit capillary tubes (Kimble Chase) in triplicates. All tubes were placed in an upright vertical position for 3 days to precipitate cells by gravity. The packed cell volume ratio was measured by calculating the ratio of the lengths of the packed cell phase to the total phase (cells plus liquid phases). The relative packed cell volume ratio was calculated by normalizing the packed cell volume ratio of each mutant with that of the wild-type strain. Statistical differences in relative packed cell volume ratios were determined by one-way analysis of variance tests employing the Bonferroni correction method by using the Prism 6 (GraphPad) software. To examine melanin production, each kinase mutant was grown overnight in YPD medium at 30 °C; 5 μl of each culture was spotted on Niger seed media containing 0.1% or 0.2% glucose, incubated at 37 °C and photographed after 3–4 days. For kinase mutants showing growth defects at 37 °C, the melanin and capsule production were assessed at 30 °C. To examine urease production, each kinase mutant was grown in YPD medium at 30 °C overnight, washed with distilled water, and an equal number of cells (5 × 104) was spotted onto Christensen’s agar media. The plates were incubated for 2–3 days at 30 °C and photographed.
The insect-based in vivo virulence assay
For each tested C. neoformans strain, we randomly selected a group of 15 Galleria mellonella caterpillars in the final instar larval stage with a body weight of 200–300 mg, which arrived within 7 days from the day of shipment (Vanderhorst Inc.). Each C. neoformans strain was grown overnight at 30 °C in YPD liquid medium, washed three times with PBS, pelleted and resuspended in PBS at equal concentrations (106 cells per ml). A total of 4,000 C. neoformans cells in a 4-μl volume per larva was inoculated through the second to last prolegs by using a 100-μl Hamilton syringe equipped with a 10 μl-size needle and a repeating dispenser (PB600-1, Hamilton). PBS was injected as a non-infectious control. Infected larvae were placed in petri dishes in a humidified chamber, incubated at 37 °C, and monitored daily. Larvae were considered dead when they showed a lack of movement upon touching. Larvae that pupated during experiments were censored for statistical analysis. Survival curves were illustrated using the Prism 6 software (GraphPad). The Log-rank (Mantel-Cox) test was used for statistical analysis. We examined two independent mutant strains for each kinase mutant.
The STM-based murine infectivity assay
For the high-throughput murine infectivity test, a group of kinase mutant strains with the NAT selection marker containing 45 unique signature-tags (a total of four groups) was pooled. The ste50Δ and hxl1Δ mutants were used as virulent and avirulent control strains respectively, as previously reported6,22. Each group of the kinase mutant library was grown at 30 °C in YPD medium for 16 h separately and washed three times with PBS. The concentration of each mutant was adjusted to 107 cells per ml and 50 μl of each sample was pooled into a tube. For preparation of the input genomic DNA of each kinase mutant pool, 200 μl of the mutant pool was spread on YPD plate, incubated at 30 °C for 2 days, and scraped. For preparation of the output genomic DNA samples, 50 μl of the mutant pool (5 × 105 cells per mouse) was infected into seven-week-old female A/J mice (Jackson Laboratory) through intranasal inhalation. The infected mice were sacrificed with an overdose of Avertin 15 days post-infection, their lungs were recovered and homogenized in 4 ml PBS, spread onto the YPD plates containing 100 μg ml−1 of chloramphenicol, incubated at 30 °C for 2 days, and scraped. Total genomic DNA was extracted from scraped input and output cells by the cetyltrimethyl ammonium bromide DNA extraction method. Quantitative PCR was performed with the tag-specific primers listed in Supplementary Data 8 using MyiQ2 Real-Time PCR detection system (Bio-Rad). The STM score was calculated as previously described6. Briefly, relative changes in genomic DNA amounts were calculated by the 2−ΔΔCT method to determine the STM score. The mean fold changes in input verses output samples were calculated in Log score (Log2 2−(Ct,Target−Ct,Actin)output−(Ct,Target−Ct,Actin)input). We monitored two independent mutants for each kinase.
To visualize vacuole morphology, the wild-type H99S strain and vps15Δ strains (YSB1500 and YSB1501) were cultured in liquid YPD medium at 30 °C for 16 h. FM4–64 dye (Life Technologies) was added to each culture at a final concentration of 10 μM and further incubated at 30 °C for 30 min. The cells were pelleted by centrifugation, resuspended with fresh liquid YPD medium, and further incubated at 30 °C for 30 min. The cells were pelleted again, washed three times with PBS, and resuspended in 1 ml of PBS. On the glass slide, 10 μl of the cells and 10 μl of mounting solution (Biomeda) were mixed and spotted. The glass slides were observed by confocal microscope (Olympus BX51 microscope).
TiO2 enrichment-based phosphoproteomics
To identify the phosphorylated targets of Vrk1 on a genome-wide scale, the H99S and vrk1Δ mutant strains were incubated in YPD liquid medium at 30 °C for 16 h, sub-cultured into 1 l of fresh YPD liquid medium, and further incubated at 30 °C until it approximately reached an optical density at 600 nm (OD600) of 0.9. Each whole-cell lysate was prepared with lysis buffer containing 50 mM Tris-Cl (pH 7.5), 1% sodium deoxycholate, 5 mM sodium pyrophosphate, 0.2 mM sodium orthovanadate, 50 mM sodium fluoride (NaF), 0.1% sodium dodecyl sulphate, 1% Triton X-100, 0.5 mM phenylmethylsulfonyl fluoride and 2.5 × protease inhibitor cocktail solution (Merck Millipore). The protein concentration of each cell lysate was estimated using a Pierce BCA protein kit (Life Technologies). Sulfhydryl bonds between cysteine residues in protein lysates were reduced by incubating 10 mg of total protein lysate with 10 mM DTT at room temperature for 1 h and then alkylated with 50 mM iodoacetamide in the dark at room temperature for 1 h. These samples were treated again with 40 mM DTT at room temperature for 30 min and digested using trypsin (Sequencing grade trypsin, Promega) at an enzyme: substrate ratio of 1:50 (w/w) with overnight incubation at 37 °C. The trypsin-digested protein lysates were then purified with Sep-Pak C18 columns (Waters Corporation), lyophilized and stored at −80 °C. Phosphopeptides were enriched using TiO2Mag Sepharose beads (GE Healthcare) and lyophilized for LC–MS/MS. Mass spectrometric analyses were performed using a Q Exactive Hybrid Quadrupole-Orbitrap mass spectrometer (Thermo Scientific) equipped with Dionex U 3000 RSLC nano high-performance liquid chromatography system, a nano-electrospray ionization source and fitted with a fused silica emitter tip (New Objective). All phosphopeptide samples were reconstituted in solution A (water/acetonitrile (98:2, v/v), 0.1% formic acid), and then injected into an LC-nano electrospray ionisation-MS/MS system. Samples were first trapped on a Acclaim PepMap 100 trap column (100 μm i.d. × 2 cm, nanoViper C18, 5 μm particle size, 100 Å pore size, Thermo Scientific) and washed for 6 min with 98% solution A at a flow rate of 4 μl min−1, and then separated on an Acclaim PepMap 100 capillary column (75 μm i.d. × 15 cm, nanoViper C18, 3 μm particle size, 100 Å pore size, Thermo Scientific) at a flow rate of 400 nl min−1. Peptides were analysed with a gradient of 2 to 35% solution B (water/acetonitrile (2:98, v/v), 0.1% formic acid) over 90 min, 35 to 90% over 10 min, followed by 90% for 5 min, and finally 5% for 15 min. Resulting peptides were electrosprayed through a coated silica tip (PicoTip emitter) at an ion spray voltage of 2,000 eV. MS/MS spectra were searched against the C. neoformans var. grubii H99S protein database (http://www.uniprot.org) using the MASCOT (version 2.4, Matrixscience) search algorithms through the Proteome Discoverer platform (version 1.4, Thermo Scientific) for assigning peptides. The MS and MS/MS tolerance was set at 15 p.p.m. and 0.8 Da, respectively. The PhosphoRS node was used to calculate individual site probabilities for phosphorylated peptides. The following search parameters were applied: cysteine carbamidomethylation as fixed modifications, methionine oxidation and serine/threonine/tyrosine phosphorylation as variable modifications, and two missed trypsin cleavages were allowed to identify the peptide. Peptide identification was filtered by a 1% false discovery rate cut-off. PhosphoRS probability score ≥0.75 threshold was used to confirm the site of phosphorylation. Spectral counts were used to estimate relative phosphopeptide abundance between the wild-type and vrk1Δ mutant strains. The data were further normalized by dividing each ratio (vrk1Δ per wild-type) by the median value of the ratio of each LC–MS/MS run, resulting in normalized relative phosphopeptide abundance. The Student’s t-test was used to assess the statistically significant difference between the samples.
ER stress assay
To monitor the ER stress-mediated UPR induction, the H99S and vps15Δ mutant strains were incubated in YPD at 30 °C for 16 h, sub-cultured into fresh YPD liquid medium, and further incubated at 30 °C until they reached the early-logarithmic phase (OD600=0.6). The cells were treated with 0.3 μg ml−1 TM for 1 h. The cell pellets were immediately frozen with liquid nitrogen and then lyophilized. Total RNAs were extracted using easy-BLUE (Total RNA Extraction Kit, Intron Biotechnology) and subsequently complementary DNA (cDNA) was synthesized using an MMLV reverse transcriptase (Invitrogen). HXL1 splicing patterns (UPR-induced spliced form of HXL1 (HXL1S) and unspliced form of HXL1 (HXL1U)) were analysed by PCR using cDNA samples of each strain and primers (B5251 and B5252) listed in Supplementary Data 8.
To measure the expression level of ERG11, the H99S strain and bud32Δ mutants were incubated in liquid YPD medium at 30 °C for 16 h and sub-cultured into fresh liquid YPD medium. When the cells reach the early-logarithmic phase (OD600=0.6), the culture was divided into two samples: one was treated with fluconazole for 90 min and the other was not treated. The cell pellets were immediately frozen with liquid nitrogen and then lyophilized. Total RNA was extracted and northern blot analysis was performed with the total RNA samples for each strain. For qRT–PCR analysis of genes involved in the calcineurin pathway, the H99S strain and vps15Δ mutants were incubated in liquid YPD medium at 30 °C for 16 h and were sub-cultured into fresh liquid YPD medium until they reach to the early-logarithmic phase (OD600=0.8). The cells were then pelleted, immediately frozen with liquid nitrogen, and lyophilized. After total RNA was extracted, cDNA was synthesized using RTase (Thermo Scientific). CNA1, CNB1, CRZ1, UTR2 and ACT1-specific primer pairs (B7030 and B7031, B7032 and B7033, B7034 and B7035, B7036 and B7037, B679 and B680, respectively) (Supplementary Data 8) were used for qRT–PCR.
The kinase phenome clustering
In vitro phenotypic traits of each kinase mutant were scored with the following qualitative scale: −3 (strongly sensitive or defective), −2 (moderately sensitive or defective), −1 (weakly sensitive or defective), 0 (wild-type-like), +1 (weakly resistant or enhanced), +2 (moderately resistant or enhanced) and +3 (strongly resistant or enhanced). The excel file containing the phenotype scores of each kinase mutant was loaded by Gene-E software (http://www.broadinstitute.org/cancer/software/GENE-E/) and then kinase phenome clustering was drawn using one minus Pearson correlation.
Cryptococcus kinome web-database
For public access to the phenome and genome data for the C. neoformans kinase mutant library, the Cryptococcus Kinase Phenome Database was developed (http://kinase.cryptococcus.org/). Genome sequences of the H99 strain were downloaded from Broad Institute (http://www.broadinstitute.org/annotation/genome/cryptococcus_neoformans/MultiHome.html), and incorporated into the standardized genome data warehouse in the Comparative Fungal Genomics Platform database (CFGP 2.0; http://cfgp.snu.ac.kr/)65. Classification of kinases was performed by using the hidden Markov model-based sequence profiles of SUPERFAMILY (version 1.73; ref. 66). A total of 64 family identifiers belonging to 38 superfamilies were used to predict putative kinases (Supplementary Table 3). In addition, the sequence profiles of Kinomer (version 1.0; refs 11, 12) and the Microbial Kinome67 were used to supplement the kinase prediction. Information from genome annotation of C. neoformans var. grubii H99 and protein domain predictions of InterProScan68 was also adopted to capture the maximal extent of possible kinase-encoding genes. For each gene, results from the eight bioinformatics programs are also provided to suggest clues for gene annotations. In addition, results from SUPERFAMILY, Kinomer and Microbial Kinome were displayed for supporting robustness of the prediction. If a gene has an orthologue in C. neoformans var. neoformans JEC21, a link to the KEGG database was also provided. Finally, transcript expression and phenotype screening data are shown along with the above-mentioned information. To browse genomic data in context to important biological features, the Seoul National University genome browser (SNUGB; http://genomebrowser.snu.ac.kr/)69 was integrated into the Cryptococcus kinase phenome database. In kinase browser, a direct link to the SNUGB module was provided for each gene. The Cryptococcus kinase phenome database was developed by using MySQL 5.0.81 (source code distribution) for database management and PHP 5.2.6 for web interfaces. The web-based user interface is served through the Apache 2.2.9 web server.
All the data related to mutant construction were deposited in the publicly accessible C. neoformans kinome database (http://kinase.cryptococcus.org) that we constructed for the current study. All kinase mutant strains were deposited in the Korean Culture Collection of Microorganisms in Korea (http://www.kccm.or.kr/) and in the Center of Host-Microbial Interactions at Duke University in USA. Other data that support the findings of this study are available from the corresponding author on request.
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We thank Chaeyoon Baek, Hanseul Yang, Taehoon Kim, Sora Lee, Dasom Han, Dong-Yun Choi, Sanghun Kim, Seungyeol Lee, So-Yeon Shin, Aeri Yoo, Yong In Jeong, Yongjae Song, Won Bin Lee, Won Il Chae, Jihwan Lee, Changho Lee, Taehyung Kim and Hanna Na for their technical assistance in constructing the kinase mutant library. This work was supported by National Research Foundation of Korea grants (no. 2010–0029117, 2015R1A2A1A15055687) from MEST, the Strategic Initiative for Microbiomes in Agriculture and Food funded by Ministry of Agriculture, Food and Rural Affairs (916006-2), and the Brain Korea 21 (BK21) PLUS program (to Y.-S.B.). This work was also supported in part by a NIH/NIAID R01-AI050438-10 grant to J.H. and a project fund (C35703) to J.S.C. from Korea Basic Science Institute.
The authors declare no competing financial interests.
Supplementary Figures 1-10, Supplementary Tables 1-3 and Supplementary References (PDF 5237 kb)
List of Cryptococcus neoformans kinases (XLSX 250 kb)
List of the pathogenic fungal kinases predicted based on the kinase domain database search (XLSX 72 kb)
Pathogenicity-related kinases in Cryptococcus neoformans. (XLSX 19 kb)
Complete phenome heat map of C. neoformans kinases (XLSX 55 kb)
Raw data of the network analysis from Cryptonet (XLSX 222 kb)
Detailed information regarding phosphopeptides identified in wide-type and/or vrk1Δ mutant strain of Cryptococcus neoformans (XLSX 521 kb)
BLAST matrix analysis of Cryptococcus neoformans kinases (XLSX 190 kb)
List of primers used for constructing kinase mutant library. (XLSX 96 kb)
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Lee, K., So, Y., Yang, D. et al. Systematic functional analysis of kinases in the fungal pathogen Cryptococcus neoformans. Nat Commun 7, 12766 (2016). https://doi.org/10.1038/ncomms12766
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