jin rongsheng uc irvine manufacturer

Structure and function of bacterial toxins and receptors; synaptic proteins; protein complexes; protein-protein and protein-ligand interactions; X-ray crystallography; high-throughput screening

Our research group is dedicated to understand the molecular basis of human diseases using structural biology, which allows us to visualize how proteins function or malfunction at the atomic level. Our current research is focused on three areas: (1) exploring the molecular mechanisms underlying the toxic and therapeutic functions of botulinum neurotoxins (BoNTs), which will help to develop effective anti-BoNT strategies and improve clinical applications of BoNT; (2) characterizing the structures of Clostridium difficile (C. diff) toxins (TcdA and TcdB) and their interactions with host receptors, and understanding how they contribute to the disease of Clostridium difficile infection (CDI) that tops the CDC’s list of urgent threats; (3) advancing mechanistic understanding of ion channels, receptors, and signaling molecules in the nervous system, which will facilitate the design and improvement of therapeutic agents for the treatment of some psychological and neurological disorders. We are also developing cutting-edge small molecule high-throughput screening (HTS) assays based on our understanding of the structure and function of these disease-related proteins, which may lead to novel chemical probes and/or drug candidates for basic research and therapeutic application.

Lam, K. H., Guo, Z., Krez, N., Matsui, T., Perry, K., Weisemann, J., Rummel, A., Bowen, M. E. & Jin, R. A viral-fusion-peptide-like molecular switch drives membrane insertion of botulinum neurotoxin A1. Nat Commun 9, 5367 (2018) doi: 10.1038/s41467-018-07789-4.

Chen, P., Tao, L., Liu, Z., Dong, M. & Jin, R. Structural insight into Wnt signaling inhibition by Clostridium difficile toxin B. FEBS J (2018) doi: 10.1111/febs.14681.

Chen, P., Tao, L., Wang, T., Zhang, J., He, A., Lam, K. H., Liu, Z., He, X., Perry, K., Dong, M*. & Jin, R*. Structural basis for recognition of frizzled proteins by Clostridium difficile toxin B. Science 360, 664-669 (2018) (*corresponding authors) doi: 10.1126/science.aar1999. PMCID: PMC6231499

Lam, K. H., Sikorra, S., Weisemann, J., Maatsch, H., Perry, K., Rummel, A., Binz, T. & Jin, R. Structural and biochemical characterization of the protease domain of the mosaic botulinum neurotoxin type HA. Pathog Dis 76 (2018) doi: 10.1093/femspd/fty044. PMCID: PMC5961070

Silva, D. A., Stewart, L., Lam, K. H., Jin, R. & Baker, D. Structures and disulfide cross-linking of de novo designed therapeutic mini-proteins. FEBS J 285, 1783-1785 (2018) doi: 10.1111/febs.14394. PMCID: PMC6001749

Lam, K. H., Qi, R., Liu, S., Kroh, A., Yao, G., Perry, K., Rummel, A. & Jin, R. The hypothetical protein P47 of Clostridium botulinum E1 strain Beluga has a structural topology similar to bactericidal/permeability-increasing protein. Toxicon 147, 19-26 (2018) doi: 10.1016/j.toxicon.2017.10.012. PMCID: PMC5902665

Chevalier, A., Silva, D.A., Rocklin, G.J., Hicks, D.R., Vergara, R., Murapa, P., Bernard, S.M., Zhang, L., Lam, K.H., Yao, G., Bahl, C.D., Miyashita, S.I., Goreshnik, I., Fuller, J.T., Koday, M.T., Jenkins, C.M., Colvin, T., Carter, L., Bohn, A., Bryan, C.M., Fernández-Velasco, D.A., Stewart, L., Dong, M., Huang, X., Jin, R., Wilson, I.A., Fuller, D.H. & Baker, D. Massively parallel de novo protein design for targeted therapeutics. Nature 550(7674):74-79 (2017) doi: 10.1038/nature23912. PMCID: PMC5802399

Yao, G., Lam, K.H., Weisemann, J., Peng, L., Krez, N., Perry, K., Shoemaker, C.B., Dong, M., Rummel, A. & Jin, R. A camelid single-domain antibody neutralizes botulinum neurotoxin A by blocking host receptor binding. Sci Rep. 7;7(1):7438. (2017) doi: 10.1038/s41598-017-07457-5. PMCID: PMC5547058

Yao, G., Lam, K.H., Perry, K., Weisemann, J., Rummel, A. & Jin, R. Crystal Structure of the Receptor-Binding Domain of Botulinum Neurotoxin Type HA, Also Known as Type FA or H. Toxins (Basel) 9, 93 (2017) doi: 10.3390/toxins9030093. PMCID: PMC5371848

Yao, G., Zhang, S., Mahrhold, S., Lam, K. H., Stern, D., Bagramyan, K., Perry, K., Kalkum, M., Rummel, A.*, Dong, M.* & Jin, R.* N-linked glycosylation of SV2 is required for binding and uptake of botulinum neurotoxin A. Nat Struct Mol Biol 23 (7):656-662 (2016) (*corresponding authors) doi: 10.1038/nsmb.3245. PMCID: PMC5033645

Lee, K., Lam, K. H., Kruel, A. M., Mahrhold, S., Perry, K., Cheng, L. W., Rummel, A. & Jin, R. Inhibiting oral intoxication of botulinum neurotoxin A complex by carbohydrate receptor mimics. Toxicon 107, 43-49 (2015) doi: 10.1016/j.toxicon.2015.08.003. PMCID: PMC4658216

Lam, K.H. & Jin, R. Architecture of the botulinum neurotoxin complex: a molecular machine for protection and delivery. Current Opinion in Structural Biology 31:89-95 (2015) doi: 10.1016/j.sbi.2015.03.013. PMCID: PMC4476938

Lam, K.H., Yao, G. & Jin, R. Diverse binding modes, same goal: The receptor recognition mechanism of botulinum neurotoxin. Progress in Biophysics and Molecular Biology 117(2-3):225-31 (2015) doi: 10.1016/j.pbiomolbio.2015.02.004. PMCID: PMC4417461

Lam, T.I., Stanker, L.H., Lee, K., Jin, R. & Cheng, L.W. Translocation of botulinum neurotoxin serotype A and associated proteins across the intestinal epithelia. Cellular Microbiology 17(8):1133-1143 (2015) doi: 10.1111/cmi.12424. PMCID: PMC4610714

Matsui, T.*, Gu, S., Lam, K.H., Carter, L.G., Rummel, A., Mathews, II. & Jin, R.* Structural Basis of the pH-Dependent Assembly of a Botulinum Neurotoxin Complex. J. Mol. Biol. 426(22):3773-3782 (2014) doi: 10.1016/j.jmb.2014.09.009. (*corresponding authors) PMCID: PMC4252799

Lee, K., Zhong, X., Gu, S., Kruel, A.M., Dorner, M.B., Perry, K., Rummel, A., Dong, M. & Jin, R. Molecular basis for disruption of E-cadherin adhesion by botulinum neurotoxin A complex. Science 344(6190):1405-1410 (2014) doi: 10.1126/science.1253823. PMCID: PMC4164303

Lee, K., Lam, K.H., Kruel, A.M., Perry, K., Rummel, A. and Jin, R. High-resolution crystal structure of HA33 of botulinum neurotoxin type B progenitor toxin complex. Biochem. Biophys. Res. Commun. 446(2):568-573 (2014) doi: 10.1016/j.bbrc.2014.03.008. PMCID: PMC4020412

Yao, Y., Lee, K., Gu, S., Lam, K.H. & Jin, R. Botulinum Neurotoxin A Complex Recognizes Host Carbohydrates through Its Hemagglutinin Component, Toxins (Basel) 6(2):624-635 (2014) doi: 10.3390/toxins6020624. PMCID: PMC3942755

Lee, K., Gu, S., Jin, L., Le, T.T.N., Cheng, L.W., Strotmeier, J., Kruel, A.M., Yao, G., Perry, K., Rummel, A.* & Jin, R.* Structure of a Bimodular Botulinum Neurotoxin Complex Provides Insights into Its Oral Toxicity. PLoS Pathog. 9(10): e1003690 (2013) doi:10.1371/journal.ppat.1003690. (*corresponding authors) PMCID: PMC3795040

Zong, Y. and Jin, R. Structural mechanisms of the agrin-LRP4-MuSK signaling pathway in neuromuscular junction differentiation. Cell. Mol. Life Sci. 70(17):3077-88 (2013) doi: 10.1007/s00018-012-1209-9. PMCID: PMC4627850

Gu, S. and Jin, R. Assembly and function of the botulinum neurotoxin progenitor complex. Curr. Top. Microbiol. Immunol. 364:21-44 (2013) doi: 10.1007/978-3-642-33570-9_2. PMCID: PMC3875173

Gu, S., Rumpel, S., Zhou, J., Strotmeier, J., Bigalke, H., Perry, K., Shoemaker, C.B., Rummel, A. & Jin, R. Botulinum neurotoxin is shielded by NTNHA in an interlocked complex. Science 335(6071):977-81 (2012) doi: 10.1126/science.1214270. PMCID: PMC3545708

Zong, Y., Zhang, B., Gu, S., Lee, K., Zhou, J., Yao, G., Figueiredo, D., Perry, K., Mei, L.* & Jin, R.* Structural basis of neuron-specific regulation of postsynaptic differentiation. Gene & Development 26:247-258 (2012) doi: 10.1101/gad.180885.111. (*corresponding authors) PMCID: PMC3278892

Yao, G., Zong, Y., Gu, S., Zhou, J., Xu, H., Mathews, II. & Jin, R. Crystal structure of the glutamate receptor GluA1 amino-terminal domain. Biochem. J. 438(2):255-63 (2011) doi: 10.1042/BJ20110801. PMCID: PMC3296483

Strotmeier, J., Gu, S., Jutzi, S., Mahrhold, S., Zhou, J., Pich, A., Eichner, T., Bigalke, H., Rummel, A.*, Jin, R.* & Binz, T*. The biological activity of botulinum neurotoxin type C is dependent upon novel types of ganglioside binding sites. Mol. Microbiol. 81(1):143-56 (2011) doi: 10.1111/j.1365-2958.2011.07682.x. Epub 2011 Jun 2. (*corresponding authors)

Strotmeier, J., Lee, K., Völker, A.K., Mahrhold, S., Zong, Y., Zeiser, J., Zhou, J., Pich, A., Bigalke, H., Binz, T., Rummel, A.* & Jin, R.* Botulinum neurotoxin serotype D attacks neurons via two carbohydrate-binding sites in a ganglioside-dependent manner. Biochem. J. 431(2):207-16 (2010) (*corresponding authors)

Jin, R.*, Singh, S.K., Gu, S., Furukawa, H., Sobolevsky, A.I., Zhou, J., Jin, Y. & Gouaux E.* Crystal structure and association behavior of the GluR2 amino-terminal domain. EMBO J. 28(12):1812-23 (2009) (*corresponding authors) PMCID: PMC2699365

Kumar, J., Schuck. P., Jin, R. & Mayer, M.L. The N-terminal domain of GluR6-subtype glutamate receptor ion channels. Nat. Struct. Mol. Biol. 16(6):631-8 (2009) PMCID: PMC2729365

Jin, R., Rummel, A., Binz, T. & Brunger, A.T. Botulinum neurotoxin B recognizes its protein receptor with high affinity and specificity. Nature 444:1092-5 (2006)

Jin, R., Clark, S., Weeks, A.M., Dudman, J.T., Gouaux, E. & Partin, K.M. Mechanism of positive allosteric modulators acting on AMPA receptors. J. Neurosci. 25(39):9027-36 (2005)

Jin, R., Junutula, J.R., Matern, H.T., Ervin, K.E., Scheller, R.H. & Brunger, A.T. Exo84 and Sec5 are competitive regulatory Sec6/8 effectors to the RalA GTPase. EMBO J. 24:2064-74 (2005)

Jin, R., Bank, T., Mayer, M. L., Traynelis, S. & Gouaux, E. Structural basis for partial agonist action at ionotropic glutamate receptors. Nat. Neurosci. 6(8):803-10 (2003)

Structure of the glucosyltransferase domain of TcdA in complex with RhoA provides insights into substrate recognition. Sci Rep. 2022 05 30; 12(1):9028.

Jahid S, Ortega JA, Vuong LM, Acquistapace IM, Hachey SJ, Flesher JL, La Serra MA, Brindani N, La Sala G, Manigrasso J, Arencibia JM, Bertozzi SM, Summa M, Bertorelli R, Armirotti A, Jin R, Liu Z, Chen CF, Edwards R, Hughes CCW, De Vivo M, Ganesan AK. PMID: 35385746; PMCID: PMC9127750.

Probing the structure and function of the protease domain of botulinum neurotoxins using single-domain antibodies. PLoS Pathog. 2022 01; 18(1):e1010169.

Chen P, Zeng J, Liu Z, Thaker H, Wang S, Tian S, Zhang J, Tao L, Gutierrez CB, Xing L, Gerhard R, Huang L, Dong M, Jin R. PMID: 34145250; PMCID: PMC8213806.

Structural Insights into Rational Design of Single-Domain Antibody-Based Antitoxins against Botulinum Neurotoxins. Cell Rep. 2020 02 25; 30(8):2526-2539.e6.

Chen P, Lam KH, Liu Z, Mindlin FA, Chen B, Gutierrez CB, Huang L, Zhang Y, Hamza T, Feng H, Matsui T, Bowen ME, Perry K, Jin R. PMID: 31308519; PMCID: PMC6684407.

The hypothetical protein P47 of Clostridium botulinum E1 strain Beluga has a structural topology similar to bactericidal/permeability-increasing protein. Toxicon. 2018 Jun 01; 147:19-26.

High-resolution crystal structure of HA33 of botulinum neurotoxin type B progenitor toxin complex. Biochem Biophys Res Commun. 2014 Apr 04; 446(2):568-73.

When the average American thinks about Botox, they imagine injections that deliver wrinkle-free foreheads and migraine relief. When Rongsheng Jin, Ph.D., professor in the Department of Physiology and Biophysics from UC Irvine’s School of Medicine, thinks about Botox, he recalls the deadly toxin it was derived from, its intricate three-dimensional structure first determined by his team and the mechanisms that can both prevent the appearance of wrinkles and kill humans.

The bacterium responsible for Botox, Clostridium botulinum (C. botulinum), and another deadly bacterium, Clostridioides difficile (C. diff), are the two main research areas of focus for Jin. In his lab, Jin and team uncover the blueprints behind these bacteria and the toxins they produce to better understand them and find ways to use their own mechanisms for good — such as improved cosmetics or potential cancer therapeutics — and to combat their deadly effects.

“We focus on the mechanism,” said Jin. “Knowing and understanding the mechanism at the molecular level is the universal approach. Once you know the blueprints of how it works, you can do so many things — you can make it better or worse.”

Jin’s lab has made significant strides in finding ways to combat C. diff infections — a Centers for Disease Control and Prevention urgent threat — which are typically contracted in hospitals and healthcare settings and has symptoms ranging from diarrhea to life-threatening colitis. One approach pursued in the Jin lab is a novel vaccine that can prevent infections and the other is a protein therapeutic that essentially tricks the toxin into binding to the drug rather than the human receptors. The latter of the two is available for licensing through UCI Beall Applied Innovation’s Research Translation Group.

“There will be no chance to develop a vaccine for this toxin because nobody is going to take it,” said Jin. “If you take the vaccine, Botox doesn’t work!”

In light of this, Jin and team have shifted their focus from a C. botulinum vaccine to exploring the use of novel antitoxins to treat infections rather than prevent them or to develop new products with improved clinical and cosmetic features.

Jin makes clear that fully understanding how a bacterial toxin looks and operates within the human body is critically important. To illustrate that point, Jin and team are currently in the early stages of exploring the use of a fragment of the deadly C. diff toxin as a cancer treatment or using C. botulinum toxin’s own tactics to develop better and safer cosmetics.

“We focus on the mechanism and then we ask two questions,” said Jin. “‘Is there anything good about this toxin that we can learn from?’ and ‘How to play on a pathogen’s weakness to defeat it?’”

SimRated is a UC Irvine (UCI) startup that provides online simulation training programs for medical procedures with a mission to improve patient safety by effectively training healthcare workers and students to perform these procedures through simulation-based training. Co-founder and CEO Dr. Cameron Ricks, clinical professor of Anesthesiology and director of the Medical Education Simulation Center at UCI’s School of Medicine, and his team have honed the program’s development and are now in revenue, reaching hundreds of students in their path to startup success.

For over a decade, Ricks has taught anesthesiology and, during his time as the director of the Medical Education Simulation Center, began to realize a potential venture in online simulation training.

“Cameron and I work toward standardizing medical education, particularly in medical simulation for increased competence and patient safety down the line,” said Beaulieu. “We have customers in high school career and technical education programs using our products to learn how to do vital signs and suturing, all the way to the other side of the continuum with advanced airway techniques for medical students.”

“We’re having fun with it; it’s an entrepreneurial adventure. It’s education for us; we’re learning, we get to interact with high school students and teachers,” said Ricks. “We also get to interact with the clinical experts who help develop the videos.”

“Education is changing and people are looking to see what’s out there and are interested in online options, especially in spaces where they may not have that primary education because having a physician or nurse come into the classroom is not always possible because these clinicians are busy,” said Ricks. “We solve that problem by coming into the classroom remotely and I think that’s part of what attracts the teachers, as well.”

Though the world’s switch to online learning has been beneficial for the startup’s impact on high school educational reach, SimRated experienced their first sale about a year and half ago. Currently, their primary clientele, high school teachers, range in location from the Bay Area to Los Angeles Unified School District and local school districts in Orange County.

Since its launch, the SimRated team has utilized UCI Beall Applied Innovation’s resources and programs to help the startup progress. Because Ricks was using his own capital to initially fund the company, Ricks consulted with licensing officers to ensure he was launching the startup through the appropriate UCI avenues. The team also took part in the I-Corps program, Applied Innovation’s market discovery program funded by the National Science Foundation, and have since joined the Wayfinder incubator, where the team remains as they move their startup forward.

“Our first customer came to because Juan Felipe [Vallejo] introduced me to an Innovation Advisor who said I should call this high school,” said Ricks. “So, I called and that was our first customer.”

Looking ahead, the team plans to study the growth of their startup, during and post-pandemic as well as expand into more high schools. SimRated also wants to move into higher education, like junior colleges and medical schools, Ricks says, each one with their own separate market and learning curves.

“My hope is one day this grows big enough that I can work for fun and stay at UCI because I enjoy it,” said Ricks. “I think I have many years until that happens, so I’m not quitting my day job anytime soon.”

A new study led by University of California, Irvine (UCI) researchers identifies two ways in which APOBEC3A— a vital enzyme that is responsible for genetic changes resulting in a variety of cancers while protecting our cells against viral infection—is controlled.

Scientists from the University of California, Irvine School of Biological Sciences have discovered how to forestall Alzheimer"s disease in a laboratory setting, a finding that could one day help in devising targeted drugs that prevent it.

Researchers from the University of California, Irvine and Harvard University have discovered how the Clostridium difficile toxin B (TcdB) recognizes the human Frizzled protein, the receptor it uses to invade intestinal cells and lead to deadly gastrointestinal infections. The findings could pave ...

Led by UCI professor of molecular biology & biochemistry Christopher C.W. Hughes, the research team successfully established multiple vascularized micro-organs on an industry-standard 96-well plate. Hughes and the study"s first author, Duc T. T. Phan, showed that these miniature tissues are much ...

A University of California, Irvine pharmacology researcher has helped create a class of inhibitory compounds that can strongly enhance the effect of anti-tumor drugs for melanoma.

UC Irvine Health researchers have developed a cost-effective one-step test that screens, detects and confirms hepatitis C virus (HCV) infections. Current blood-based HCV testing requires two steps and can be expensive, inconvenient and is not widely available or affordable globally.

Human neural stem cell treatments are showing promise for reversing learning and memory deficits after chemotherapy, according to UC Irvine researchers. In preclinical studies using rodents, they found that stem cells transplanted one week after the completion of a series of chemotherapy sessions ...

Zheng Liu, Conceptualization, Investigation, Visualization, Writing - original draft,1 Sicai Zhang, Conceptualization, Formal analysis, Investigation, Methodology, Validation, Visualization, Writing - original draft, Writing - review & editing,2 Peng Chen, Conceptualization, Methodology,1 Songhai Tian, Conceptualization, Data curation, Formal analysis, Funding acquisition, Investigation, Methodology, Project administration, Resources, Software, Supervision, Validation, Visualization, Writing - original draft, Writing - review & editing,2 Ji Zeng, Investigation, Resources,2 Kay Perry, Investigation,3 Min Dong, Conceptualization, Funding acquisition, Methodology, Project administration, Supervision, Visualization, Writing - original draft, Writing - review & editing,2 and Rongsheng Jin, Conceptualization, Data curation, Funding acquisition, Methodology, Project administration, Resources, Supervision, Validation, Visualization, Writing - original draft, Writing - review & editing1

This is an open-access article distributed under the terms of the Creative Commons Attribution-NonCommercial license, which permits use, distribution, and reproduction in any medium, so long as the resultant use is not for commercial advantage and provided the original work is properly cited.

Toxin B (TcdB) is a primary cause of Clostridioides difficile infection (CDI). This toxin acts by glucosylating small GTPases in the Rho/Ras families, but the structural basis for TcdB recognition and selectivity of specific GTPase substrates remain unsolved. Here, we report the cocrystal structures of the glucosyltransferase domain (GTD) of two distinct TcdB variants in complex with human Cdc42 and R-Ras, respectively. These structures reveal a common structural mechanism by which TcdB recognizes Rho and R-Ras. Furthermore, we find selective clustering of adaptive residue changes in GTDs that determine their substrate preferences, which helps partition all known TcdB variants into two groups that display distinct specificities toward Rho or R-Ras. Mutations that selectively disrupt GTPases binding reduce the glucosyltransferase activity of the GTD and the toxicity of TcdB holotoxin. These findings establish the structural basis for TcdB recognition of small GTPases and reveal strategies for therapeutic interventions for CDI.

TcdB (~270 kDa) contains four structurally distinct domains: an N-terminal glucosyltransferase domain (GTD), a cysteine protease domain (CPD), a central transmembrane delivery and receptor binding domain (DRBD), and a C-terminal combined repetitive oligopeptides (CROPs) domain (Fig. 1A). It is widely accepted that the toxins bind to cell surface receptors and enter cells through receptor-mediated endocytosis (2, 5–8). Acidification in the endosome triggers conformational changes in the toxins that prompt the DRBD to form a pore and deliver the GTD and the CPD across the endosomal membrane (9, 10). In the cytosol, the CPD is activated by eukaryotic-specific inositol hexakisphosphate and subsequently undergoes autoproteolysis to release the GTD, which then glucosylates small guanosine triphosphatases (GTPases) in the Rho and/or Ras families (2, 11–15).

(A) A schematic diagram showing the domain organization of TcdBVPI10463 and the design of Cdc42–GTDVPI10463 and R-Ras–GTDM68 fusion proteins. GTD, glucosyltransferase domain (marine); CPD, cysteine protease domain (wheat); DRBD, delivery and receptor binding domain (pink); CROPs, combined repetitive oligopeptides domain (green); and Cdc42/R-Ras (orange). (B and C) Cartoon representations of the Cdc42–GTDVPI10463 complex with GTDVPI10463 colored in marine and Cdc42 in orange. (D and E) Close-up views of the interfaces: GTDVPI10463 W520 loop (deep purple); GTDVPI10463 α16–17 helices (light blue); Cdc42 switch I (yellow, residue T35N shown as sticks); and Cdc42 switch II (brown). GDP and UDP are shown as yellow and light blue sticks, respectively; Mg2+ and Mn2+ are represented as green and slate spheres, respectively. (F and G) Close-up views into the extensive interactions between Cdc42 and GTDVPI10463 focusing on the switch I– and switch II–binding regions.

Small GTPases are common targets of bacterial toxins (16). These proteins are crucial molecular switches cycling between the guanosine triphosphate (GTP)–bound active state and the guanosine diphosphate (GDP)–bound inactive state, which enable the activated GTPases to interact with many of their effector proteins and regulate diverse signal transduction pathways. The GTD of TcdB glucosylates Rho/Ras proteins at a threonine residue (T35Rac1, T35Cdc42, T37Rho, and T61R-Ras) in their switch I region using UDP-glucose as a sugar donor. Glucosylation disrupts the interactions of Rho/Ras GTPases with their downstream effector proteins and therefore abolishes signal transduction, leading to alterations in the actin cytoskeleton, cell rounding, and ultimately cell death (11, 17).

TcdB variants from diverse C. difficile strains display different selectivity toward Rho or Ras family GTPases, which are linked to two distinct types of cytopathic effects (14, 18–20). For example, TcdB from strains {"type":"entrez-protein","attrs":{"text":"VPI10463","term_id":"1642177071","term_text":"VPI10463"}}VPI10463 and UK1, which effectively modifies RhoA, Rac1, and Cdc42, but not R-Ras, causes classic rounded cells with spikes that remain attached to plates (11, 12, 14). In contrast, TcdB from strains M68, VPI1470, NAP1v, and 8864 preferentially modifies R-Ras, Rac1, and Cdc42 with a lower potency, but not RhoA, which induces perfect cell rounding and detachment (13, 14, 21, 22). Rho and R-Ras GTPases are notably different in their sequences (~23% identity) and cellular functions: Rho GTPases are the master regulators of the cytoskeleton, cell polarity, microtubule dynamics, and intracellular traffic (23), while R-Ras controls the activity of integrins, cell adhesion, and vascular regeneration (24–26). The different preferences toward these two distinct GTPases by TcdB variants may contribute to the different pathogenicity in humans and animal models observed among different C. difficile strains (21, 27).

Here, we use the GTD of TcdB from strains {"type":"entrez-protein","attrs":{"text":"VPI10463","term_id":"1642177071","term_text":"VPI10463"}}VPI10463 (GTDVPI10463) and M68 (GTDM68), which display distinct GTPase preferences and cytopathic effects, as examples, and report their cocrystal structures in complex with a human Cdc42 and R-Ras, respectively. Our complementary structural and functional studies reveal a common structural basis for Rho/Ras recognition shared by TcdB variants. Furthermore, we find that the GTPase-binding interfaces in the GTD provide a flexible structural platform for TcdB variants from diverse C. difficile strains to tune their specificity toward Rho or R-Ras, which may lead to distinct cytopathic effects in host cells.

Our earlier efforts to determine the structures of the GTD in complex with Rho or Ras GTPases were hampered by the transient interactions between them, which are a common feature for most enzyme-substrate pairs. We first managed to determine a low-resolution partial structure of a RhoA–GTDVPI10463 complex at about 4-Å resolution after numerous trials of crystallization optimization and crystal diffraction screening at the synchrotron. This structure revealed the relative positioning of these two proteins with the C terminus of RhoA located in close proximity to the N terminus of the GTD, which is similar to an earlier model proposed based on mutagenesis study (12). Guided by this structure, we designed and biochemically characterized a series of tandem Rho–GTDVPI10463 fusion proteins, where the GTD was covalently linked to the C terminus of RhoA, Cdc42, or Rac1 with a flexible peptide linker without restricting their interactions. Covalent linking of two proteins increases their local concentrations and thus strengthens the protein-protein interactions (28, 29).

The best crystals were obtained using a Cdc42–GTDVPI10463 fusion protein, where GTDVPI10463 (residues M1–S542) and Cdc42 (residues I4–P182) were covalently linked via a 16–amino acid peptide linker (Fig. 1A). We also introduced a mutation in Cdc42 switch I (T35N) to prevent glucosylation to stabilize the complex (11). The best diffraction data at 2.79-Å resolution were obtained from a crystal of the Cdc42–GTDVPI10463 complex in the presence of cofactors for the GTD (UDP-glucose and Mn2+) and Cdc42 (GDP and Mg2+) (Fig. 1, B and C, and table S1). There is one pair of the Cdc42–GTDVPI10463 complex in an asymmetric unit with a total buried molecular interface of ~1539 Å2. The UDP-glucose molecule in the complex was hydrolyzed, and the electron density for the UDP moiety is well defined. However, no visible electron density was observed for the cleaved glucosyl moiety of UDP-glucose or the flexible 16-residue peptide linker.

Cdc42 in the complex adopts the classic Rho GTPase fold. Most of its interactions with GTDVPI10463 are mediated by its switch I and switch II regions (residues 30 to 40 and 59 to 73, respectively), which otherwise act as a molecular switch modulating its interactions with effector proteins. The overall structure of the Cdc42•UDP-bound GTDVPI10463 is similar to the standalone GTD in the presence of UDP and glucose [Protein Data Bank (PDB): 2BVL] (30) or a nonhydrolyzable UDP-glucose homology U2F (PDB: 5UQN) (fig. S1A) (31). We notice that a loop connecting the α20 and α21 helices (W520 loop, residues 515 to 523) of the GTD displays a large conformational change in comparison to the apo GTD in all three structures with the Cα of W520 moving ~9.6 Å (fig. S1, B and C), which is believed to be triggered by its direct interactions with UDP-glucose and Mn2+ (31–33). In the Cdc42–GTDVPI10463 complex, the conformation of this W520 loop is further stabilized by residue Y32 and the T35N mutation on the switch I of Cdc42 (Fig. 1F). In contrast, the W520 loop in the apo conformation may clash with Cdc42, suggesting that UDP-glucose binding helps the GTD to engage its substrate.

Using a similar strategy, we also successfully determined the cocrystal structure of GTDM68 in complex with R-RasT61N in the presence of UDP-glucose, GDP, Mn2+, and Mg2+ at 2.34-Å resolution (Fig. 2, A and B, and table S1). The overall architecture of the R-Ras–GTDM68 complex is very similar to the Cdc42–GTDVPI10463 complex, where GTDM68 grips R-Ras mainly through its switch I and II regions, and the W521 loop of GTDM68 (equivalent to the W520 loop of GTDVPI10463) adopts the UDP-glucose•Mn2+-bound conformation and facilitates R-Ras binding (Fig. 2, C and D, and fig. S1, D to F) (34). However, we observe a unique feature that is not observed in the Cdc42–GTDVPI10463 complex, where a region between the switch I and II of R-Ras involving residues T67, I69, R78, and D80 (termed inter-switch) is bound by GTDM68 via a loop between its α19 and α20 helices (Fig. 2E). The UDP-glucose molecule in the R-Ras–GTDM68 complex was also hydrolyzed, and we observed a clear electron density for UDP but a weak density for the hydrolyzed glucose, indicating its low occupancy.

It is well accepted that the switch I of small GTPases adopts distinct conformations in the presence of GTP or GDP, which is the structural basis underlying their functions as molecular switches. In this study, the GTD-bound Cdc42 and R-Ras were crystallized in the presence of GDP. Unexpectedly, the switch I of both Cdc42 and R-Ras displays a unique conformation upon toxin binding that is different from their classic GDP-bound conformations (Fig. 3, A and B, and fig. S2) (35). In particular, the switch I of Cdc42 and R-Ras moves away from its GDP•Mg2+-binding cleft to insert into the UDP-glucose–binding pocket of the GTD, which is stabilized by extensive protein-protein interactions between the switch I and multiple discontinuous regions in the GTD that are converged in 3D (Figs. 1F and ​and2C2C and table S2). As a result, this shift of the switch I positions the key residue T35Cdc42 and T61R-Ras, the targeted residues for glucosylation, in close proximity to the UDP-glucose–binding site in the GTD (Fig. 3, A and B). For example, N35Cdc42-T35N moves ~6.3 Å closer to the GTD and UDP, establishing hydrogen bonding with K463, S518, and S521 of the GTD and the UDP β-phosphoryl group (Fig. 1F). However, the engineered T35NCdc42 or T61NR-Ras does not have the hydroxyl group to accept the glucosyl unit from UDP-glucose, and therefore, the cleaved glucose cannot be located in the complexes. This previously unidentified conformation of the switch I likely represents an intermediate state where T35Cdc42 and T61R-Ras are primed to be glucosylated by the GTD. In contrast to this favorable GTD-binding conformation, the switch I of Rho/Ras in the GTP-bound conformation is located further away from the GTD when compared to the GDP-bound state, while the hydroxyl groups of the Thr residue—the glucosylation target—could be engaged in intramolecule hydrogen bonds in the GTP-bound forms (fig. S2, B to D) (35–39). These results thus provide the structural basis to understand prior observations that the GDP-bound Rho GTPases are the preferred substrates for TcdB than the GTP-bound forms (11).

(A) Superposition of the structures of the Cdc42•GDP–GTDVPI10463 complex, Cdc42•GDP (PDB: 1ANO, yellow), and Cdc42•GMP-PCP (β,γ-methyleneguanosine 5′-triphosphate) (PDB: 2QRZ, light blue) focusing on the switch I and II regions. GDP and GMP-PCP are shown as sticks. Residues T35 in the WT Cdc42 and T35N in the Cdc42•GDP–GTD complex are shown as sticks. (B) Structural comparison between the GTDM68-bound R-Ras and the GTDVPI10463-bound Cdc42, focusing on the switch I and II regions. Residues T61NR-Ras and T35NCdc42 are shown as sticks. (C) The glucosyltransferase activities of the selected GTDVPI10463 mutants toward the recombinant Rac1 were examined using an in vitro assay. (D and E) The cytopathic effects of the GTDVPI10463 mutants were examined using the cell-rounding assay, and the percentage of rounded cells was quantified. (F) The percentages of rounded cells at 5 hours after treatment. The data are presented as means ± SD, n = 3.

A third shared GTD-binding interface is found in a region upstream of the switch I of Cdc42 (T24TNKFP) and R-Ras (I50QSYFV) (termed pre-switch I) (Fig. 4A), whose contribution to the GTPase function is not fully appreciated. The pre-switch I of Cdc42/R-Ras is bound by two discrete regions in the GTD that form a clamp-like motif (Fig. 4, B and C). For example, the upper and lower clamps in GTDVPI10463 are composed of residues 308 to 311 and 378 to 381, respectively. Together, our structural studies reveal a common strategy by which the GTD from two distinct TcdB variants recognizes their preferred substrates mostly via their characteristic switch I, switch II, and a pre-switch I region.

(A) Amino acid sequence alignment among human Cdc42, Rac1, RhoA, and R-Ras that was prepared using MultAlin (59) and ESPript 3.0 (60), focusing on the pre-switch I, switch I, inter-switch, and switch II regions. Residue numbers for Cdc42 are shown. The secondary structures of Cdc42 and R-Ras are shown on the top and bottom, respectively. The residues in Cdc42 and R-Ras that directly interact with GTDVPI10463 or GTDM68 are highlighted with orange stars or green triangles, respectively. (B) A molecular clamp in GTDVPI10463 grips the pre-switch I of Cdc42. (C) The molecular clamp in GTDM68 selectively interacts with the pre-switch I of R-Ras. (D) Strain-specific Cdc42-binding residues in GTDVPI10463 are listed in green, while the equivalent residues in GTDM68 are listed in red. (E) Strain-specific R-Ras–binding residues in GTDM68 are listed in green, while the equivalent residues in GTDVPI10463 are listed in red. (F) The upper clamp in GTDM68 (pale cyan) is more compatible to Rac1 that has a small amino acid A27 in this region, while GTDVPI10463 (blue) could accommodate Rac1, Cdc42, and RhoA. The structures of Rac1•GDP (PDB: 5N6O, green) and RhoA•GDP (PDB: 1FTN, yellow) were superimposed to the GTDVPI10463-bound Cdc42 (orange). (G) The lower clamp of GTDVPI10463 changes its conformation to recognize the pre-switch I of Rho GTPases.

Another interesting finding is that both the Cdc42- and R-Ras–binding interfaces in the GTD are largely masked by the CPD in the context of the full-length TcdB holotoxin (PDB code: 6OQ5) (fig. S3A) (34). Therefore, the GTD is in a self-inhibited state until it is cleaved by the CPD and released from the rest of the toxin. This provides a molecular explanation for the prior observation that the glucosyltransferase activities of TcdB and TcdA increased upon autoproteolytic activation and GTD release (33). Furthermore, our structures also suggest that the main substrates of the GTD should be the membrane-anchored Rho GTPases (2, 34), because the cytosolic Rho GTPases are predominantly bound by Rho guanosine dissociation inhibitors that occupy both the switch I and II of Rho and thus prevent GTD binding (fig. S3B) (40).

We then carried out structure-based mutagenesis studies, using GTDVPI10463 as a model, to validate the structural findings and better understand the functional role of the GTD in TcdB pathogenesis. Guided by the crystal structure, we designed GTDVPI10463 variants that carry two different types of mutations: (i) mutations that weaken GTD binding to Cdc42 switch I, including GTDK463G, GTDI466G, GTDA475D, GTDI382G/I383G, GTDI382G/I383G/I466G, and GTDP471G/I491G, and (ii) mutations in the α16–17 helices that disrupt its binding with the switch II of Cdc42, including GTDI432G, GTDD433G, GTDA439D, GTDI435G/M436G, and GTDM447G/M448G. We confirmed that all these mutations did not affect GTD folding and stability based on thermal denaturation experiments (figs. S4 and S5C).

We first examined the glucosyltransferase activity of these rationally designed GTDVPI10463 mutants using an in vitro glucosylation assay that has been well established for Rac1 (Fig. 3C). This assay uses a monoclonal antibody (mAb 102) that is highly specific for the nonglucosylated Rac1 and another antibody mAb 23A8 that detects the total Rac1 regardless of their glucosylation states (41, 42). We found that GTDI432G displayed a decreased glucosyltransferase activity compared to the wild-type (WT) GTD, and the activities of GTDI466G, GTDI435G/M436G, GTDM447G/M448G, GTDI382G/I383G, GTDP471G/I491G, and GTDI382G/I383G/I466G were further reduced (Fig. 3C and fig. S5A). On the basis of these findings, we designed another two GTD mutants, GTD5MA (I382G/I383G/I466G/I435G/M436G) and GTD5MB (I382G/I383G/I466G/M447G/M448G), which carry mutations to disrupt its interactions with both the switch I and switch II of Rho GTPase. As expected, the glucosyltransferase activities of these two GTDVPI10463 mutants were almost completely abolished (Fig. 3C and fig. S5B).

We then examined the cytopathic effect of these GTD variants using a cell-rounding assay, as inactivation of Rho GTPases by TcdB damages the actin cytoskeleton and results in the characteristic cell-rounding phenotype (43). The WT GTDVPI10463 and its variants were delivered into HeLa cells using Lipofectamine CRISPRMAX reagents, and the percentage of rounded cells was examined. We found that GTDI382G/I383G, GTDI466G, GTDI382G/I383G/I466G, and GTDP471G/I491G that have disrupted interactions with the switch I of Cdc42 and GTDI435G/M436G and GTDM447G/M448G that have corrupted switch II–binding interfaces showed notably decreased toxicity. GTD5MA and GTD5MB that carry mutations in both the switch I– and switch II–binding interfaces showed more than 70% decreased toxicity 5 hours after treatment and ~60% reduction after 20 hours (Fig. 3, D to F). In comparison, our negative control, the well-studied catalytically inactive GTD-N286XN288 mutant that has a disrupted Mn2+•UDP-glucose–binding pocket, was atoxic after 20 hours post-delivery (fig. S6, A and B).

Although all the GTD mutations discussed above were designed to disrupt its binding to GTPases, some residues may also be involved in its glycohydrolase function. Therefore, we further examined the UDP-glucose hydrolase activity for all the GTD mutants using the UDP-Glo assay. We found that GTDI435G/M436G, GTDI466G, GTDI382G/I383G/I466G, GTDP471G/I491G, GTD5MA, and GTD5MB displayed decreased glycohydrolase activities, while the other mutants showed comparable activity to the WT GTD (fig. S5, D and E, and table S3). Structural analyses showed that residues I383, I466, and P471 help to accommodate the glucose moiety (30), which may account for the impaired hydrolase activities when some of these residues were mutated. However, we also observed an unexpected ~5-fold decreased glycohydrolase activity for GTDI435G/M436G, which carries mutations on the α16 helix that are far away from the UDP-glucose–binding site. These findings suggest that the in vitro glycohydrolase activity of the GTD in general is very sensitive to mutagenesis, although all the GTD mutants reported here did not affect GTD folding and stability (figs. S4 and S5C).

Our structural studies reveal four GTD-binding regions in Rho and R-Ras, including switch I, switch II, pre-switch I, and inter-switch (Fig. 4A). As Rho and R-Ras represent two distinct groups in the Ras superfamily, the primary sequences in these four GTD-binding areas are largely conserved within the Rho members but different between Rho and R-Ras (Fig. 4A and fig. S7). Accordingly, structural and sequence analysis showed that GTDVPI10463 and GTDM68 exploit unique sets of amino acids to preferentially recognize these regions on Rho or R-Ras, respectively (Fig. 4, D and E, and fig. S8).

To understand how these structural differences exemplified by GTDVPI10463 and GTDM68 are related to the evolution of diverse TcdB variants, we carried out structure-based sequence analyses among all known TcdB variants available in DiffBase, which have been classified into 12 subfamilies (B1 to B12) (fig. S8) (18). We found that all these TcdB variants could be classified into two distinct groups based on their sequences in the GTPase-binding areas. Specifically, characteristic Rho-binding residues are conserved not only in other members of the same subfamily of TcdBVPI10463 (B1) but also in members of the B2, B5, B6, B9, B10, B11, and B12 subfamilies, while the R-Ras–binding residues are highly conserved in the B3 (including M68), B4, B7, and B8 subfamilies. Therefore, TcdB seems to have branched into two distinct groups during evolution that have developed two distinct sets of amino acids in their GTPase-binding areas to selectively recognize Rho or R-Ras. We propose to name them the RhoA group and R-Ras group, respectively, based on their preferred substrates, which cause two distinct types of cytopathic effects as reported in prior studies. We envision that these signature sequences in the GTD can be used to predict substrate specificity and pathogenicity of new C. difficile clinical strains that will emerge in the future.

To experimentally verify the specific pair-wise recognition between the GTD and its preferred substrate, we first produced a series of chimeric GTD constructs by swapping the GTPase-binding modules between TcdBVPI10463 and TcdBM68 and then examined how these chimeras change their glucosyltransferase activity toward Rho or R-Ras (Fig. 5A). Specifically, we designed three groups of GTD chimeras whose switch II–, switch I–, or the inter-switch–binding areas were swapped. We confirmed that all these mutations do not affect GTD folding and stability (figs. S4 and S9C), and they are active for UDP-glucose binding and hydrolysis (fig. S9, D and E). We then examined the glucosyltransferase activity of these chimeras against Rho or R-Ras (Fig. 5). In this assay, the lysate of HeLa cells was first treated with the WT GTD and these chimeras, and the unglucosylated RhoA, Rac1/Cdc42, or R-Ras was pulled down by the RhoA effector human Rhotekin (14, 22), Rac1/Cdc42 effector human p21-activated kinase 1 (PAK1) (14, 22), or R-Ras effector Raf1 (44), respectively. Since glucosylation of Rho/R-Ras GTPases inhibits their binding to these effector proteins, the fractions of the unglucosylated RhoA, Rac1/Cdc42, or R-Ras that are pulled down by the corresponding effectors reflect the activities of the GTD variants being examined.

We found that all three GTDVPI10463 mutants carrying the M68-like switch II–binding site (GTDVPI10463-α16M68, GTDVPI10463-α17M68, and GTDVPI10463-α16/17M68) showed clearly decreased glucosyltransferase activity against three Rho GTPases when compared to the WT GTDVPI10463 (Fig. 5, B and C, and fig. S9, A and B). Meanwhile, GTDM68-α16/17VPI10463 lost its ability to modify R-Ras. However, it was almost fully active toward Rac1 and partially active toward Cdc42 but barely targeting RhoA (Fig. 5, E and F, and fig. S9, A and B). These results demonstrate that the signature sequences in the α16–17 helices of GTDVPI10463 and GTDM68 play a key role in differentiating Rho and R-Ras.

When T473 and K450 of GTDM68 that favorably interact with the switch I of R-Ras are replaced with the equivalent residue Glu on GTDVPI10463, GTDM68-T473E/K450E displayed decreased glucosyltransferase ability for R-Ras, while its activity toward Cdc42 was unchanged (Fig. 5, E and F). Nevertheless, the unexpected decrease of its activity toward Rac1 cannot be readily explained on the basis of the structure. In another test, when the R-Ras inter-switch–binding region of GTDM68 was swapped with GTDVPI10463-like residues, GTDM68-InterVPI10463 exhibited reduced activity toward R-Ras (Fig. 5). GTDM68-InterVPI10463 showed WT-like activity toward Rac1, but decreased activity against Cdc42 (Fig. 5, E and F, and fig. S9, A and B), suggesting that the inter-switch region on Rho proteins may also participate in binding with GTDM68.

Last, we examined how disrupting GTPase recognition would affect the cytopathic toxicity of the full-length TcdB. As GTDVPI10463-α16/17M68 (mutant #4 in Fig. 5) displayed a decreased glucosyltransferase activity but maintained a WT-like hydrolase activity, we incorporated this GTD mutant into the holotoxin. On the basis of the cell-rounding assay, we found that TcdBVPI10463-α16/17M68 displayed a drastically decreased cytopathic toxicity: The toxin concentration that induced 50% of the cells to become round (CR50) is ~10.8 ± 5.33 nM, which is ~180,000-fold higher than that of the WT TcdB at ~5.9 ± 2.0 × 10−2 pM (Fig. 5D). This finding demonstrates that GTPase recognition is crucial for TcdB’s cytopathic toxicity and also suggests a strategy to neutralize TcdB by pharmacologically disrupting the GTD-GTPase recognition.

Given the different substrate specificities between the RhoA and R-Ras group of GTDs, it is intriguing that Rac1 is a good substrate for both groups (21, 22) (Fig. 5A). So, how do the GTDs in the R-Ras group manage to preferentially recognize Rac1 but not the closely related Cdc42 or RhoA? Guided by the crystal structures, we found that the pre-switch I region, which is gripped by a molecular clamp in the GTD, has distinct sequences among Rho GTPases (Cdc42: T24TNK27; Rac1: T24TNA27; RhoA: S26KDQ29), while all other GTD-binding regions in switch I and II are identical within the Rho family (Fig. 4A and fig. S7). Notably, GTD in the R-Ras group has one extra Lys residue inserted in the upper clamp (e.g., K308 in GTD-M68, VPI1470, and 8864) when compared to that in the RhoA group (fig. S8). The large side chain of the inserted Lys in the upper clamp would unfavorably interact with the bulky side chains of K27Cdc42 or Q29RhoA while better tolerate A27Rac1 (Fig. 4F). We envision that this could render Rac1 as a better substrate for the GTD in the R-Ras group. When we replaced the upper clamp of GTDVPI10463 with the homologous region in GTDM68 (K308–D312) (termed GTDVPI10463-ClampM68upper; Fig. 5A), we found that this mutant effectively glucosylated Rac1 but showed decreased activity toward RhoA and Cdc42 (Fig. 5, B and C). Prior studies also found that replacing A27Rac1 with a Lys decreased the glucosyltransferase activity of TcdB in the R-Ras group, while a K27A mutation in Cdc42 showed an improved activity (45). These results suggest that a Lys insertion in the upper clamp of GTD in the R-Ras family would negatively affect Cdc42/RhoA recognition.

Structural analysis focusing on the lower clamp shows that this region in GTDVPI10463 more favorably interacts with the pre-switch I of Rac1 and Cdc42, which has a smaller residue T25Rac1 and T25Cdc42 as opposed to the bulky K27RhoA (Fig. 4G). This structural finding is consistent with prior studies showing that substitution of T25Rac1 with a RhoA-like Lys led to decreased modification of Rac1T25K by TcdB (45). Furthermore, our structural modeling based on calculation of quantitative changes in binding affinity caused by sequence variations using the MutaBind server (46) showed that the lower clamp of GTDM68 (A379–S382) may provide even better binding for Cdc42 in comparison to that of GTDVPI10463 (N378–G381) (table S4). To verify this finding, we generated another mutant of GTDVPI10463 whose upper and lower clamps were both replaced by the equivalent regions in GTDM68 (termed GTDVPI10463-ClampM68; Fig. 5A). We found that this mutant displayed a better activity against Cdc42 when compared to GTDVPI10463-ClampM68upper (Fig. 5, B and C), suggesting that the M68-like lower clamp more favorably interacts with Cdc42 than that of GTDVPI10463, which may compensate for the unfavorable interactions imposed by the M68-like upper clamp. Rac1 remained as a good substrate for both GTDVPI10463-ClampM68upper and GTDVPI10463-ClampM68 as it has smaller residues A27 and T25 in this region. In contrast, both GTDVPI10463-ClampM68upper and GTDVPI10463-ClampM68 displayed decreased activity toward RhoA, which was likely due to the bulky side chains of its Q29 and K27 that impose steric tensions to the M68-like upper and lower clamps in the GTD. These findings suggest that, for GTDM68, the favorable interactions between its clamp and the unique pre-switch I in Rac1 may outweigh the unfavorable contribution of its switch I– and switch II–binding areas that are evolved to better recognize R-Ras. Consistent with this notion, the chimera GTDM68-ClampVPI10463 showed decreased activities toward Cdc42, Rac1, and R-Ras (Fig. 5, E and F, and fig. S9, A and B). Together, our data suggest that the clamp of the GTD helps to fine-tune selectivity toward different Rho members via the pre-switch, while the Rho/R-Ras specificity is jointly determined by all GTPase-binding regions on the GTD.

Among the four structurally and functionally distinct domains of TcdB, the GTD is the “warhead” that specifically glucosylates the Rho/Ras GTPases. To better understand the function of the GTD and its contribution to the pathogenicity of TcdB, we determined the crystal structure of the GTD from two distinct TcdB variants, GTDVPI10463 and GTDM68, in complex with their preferred substrates human Cdc42 and R-Ras, respectively. These two structures reveal a common structural mechanism by which the GTD from diverse TcdB variants recognizes its substrate via the switch I, switch II, and a pre-switch region in the GTPases. Furthermore, we identified selective clustering of adaptive mutations in the GTDs that modulate their specificities toward Rho or R-Ras. On the basis of the signature sequences in the GTPase-binding sites, TcdB variants can be partitioned into two functional groups: The RhoA group includes the B1, B2, B5, B6, B9, B10, B11, and B12 subfamilies of TcdB that selectively target Rho GTPases but not R-Ras, while the B3, B4, B7, and B8 subfamilies of TcdB form the R-Ras group that effectively targets R-Ras and Rac1, Cdc42 to a less extent, but not RhoA. The different GTPase specificities of these two groups of TcdB are correlated to two distinct types of cytopathic effect (18, 47). These signature sequences in the GTD identified here can be used to predict substrate specificity and pathogenicity of C. difficile clinical strains and help inform therapeutic strategies targeting specific toxin variants.

To date, the only nonantibiotic treatment option for CDI is a mAb bezlotoxumab, which blocks TcdB binding to its receptor chondroitin sulfate proteoglycan 4 (CSPG4) via an allosteric mechanism (48, 49). However, TcdB becomes inaccessible to antibodies after entering the host cells. We found that mutations that selectively disrupt GTPases binding drastically reduced the cytopathic toxicity of TcdB holotoxin, which is consistent with prior studies showing that a glucosyltransferase-deficient TcdB mutant was atoxic in vivo (50). Therefore, the GTD is an ideal molecular target for therapeutic interventions once the toxin is inside the cells, which will directly target the root cause of disease symptoms and cellular damage. The common feature of GTD-Rho/Ras interplay revealed in these studies could inform the development of therapeutic reagents that inhibit Rho/Ras glucosylation via disrupting the GTD-GTPase recognition. Similar strategies could be applied to develop inhibitors against TcdA and other members in the family of large clostridial glucosylating toxins whose GTDs share similar structures, including Clostridium novyi α-toxin (Tcnα), Clostridium sordellii lethal and hemorrhagic toxins (TcsL and TcsH), and Clostridium perfringens toxin (TpeL) (2, 51).

Notably, TcsL (strain 1522) displays a substrate selectivity similar to that of TcdBM68 (13), and their GTD domains also share high sequence and structural similarities (32). We envision that GTDTcsL should adopt a GTDTcdB-like GTPase–binding mode. For example, the α16–17 helices on GTDTcsL may favor Ras binding over Rho subfamily because most R-Ras switch II–binding residues on GTDM68 are conserved in GTDTcsL (fig. S10A). Moreover, the α16–17 helices on GTDTcsL may be less suitable to target Rho proteins as (i) N452TcsL will abolish a cation-pi interaction formed between the corresponding K452VPI10463 and Cdc42-Y64, and (ii) residues S432, A436, and S439 of GTDTcsL may weaken the hydrophobic packing with Cdc42 L67 and L70 on switch II when compared to the GTDVPI10463-like residues (fig. S10B). A previous study showed that swapping the α17 helix between GTDTcsL and GTDVPI10463 led to a change of their substrate specificities (12). The structure analyses show that the Cdc42 switch I–binding residues on GTDVPI10463 are more conserved on GTDTcsL, when compared to the R-Ras switch I–binding residues on GTDM68 (fig. S10). However, there are many unique GTDTcsL residues on the GTPase-binding interfaces that could create GTDTcsL-specific interactions with GTPases, and the details await further studies. Therefore, the GTD of TcdB provides an important system to study pathogenic bacteria adaptation and evolution, which might facilitate how pathogens respond to environmental changes, such as host-elicited immune response, different host tissues, or use of antibiotics.

The gene encoding GTDVPI10463 (residues M1–S542) of TcdB (strain {"type":"entrez-protein","attrs":{"text":"VPI10463","term_id":"1642177071","term_text":"VPI10463"}}VPI10463) was cloned into a modified pET28a vector with a 6xHis/SUMO (small ubiquitin-like modifier, Saccharomyces cerevisiae Smt3p) tag introduced to its N terminus. Human Rac1 (M1–V182) gene was cloned into the pET28a vector with an N-terminal 7xHis tag followed by a thrombin-cleavage site. For the Cdc42T35N–GTDVPI10463 fusion protein, GTDVPI10463 was covalently linked to the C terminus of Cdc42T35N (I4–P182) through a 16–amino acid peptide linker (LEVLFQGPGTGSVDGG), and the fusion protein was cloned into the pET28a vector with an N-terminal 6xHis/SUMO tag. GTDM68 (M1–A543) of TcdB (strain M68) was expressed as described previously (52). For the R-RasT61N–GTDM68 fusion protein, GTDM68 was covalently linked to the C terminus of human R-RasT61N (P24–S201) through a 16–amino acid peptide linker (GGSGGSVDGTGSVDGG), and the fusion protein was cloned into the pET28a vector with an N-terminal 6xHis/SUMO tag. All the GTD, Cdc42–GTDVPI10463, and R-Ras–GTDM68 mutants were generated by two-step polymerase chain reaction (PCR) and verified by DNA sequencing. TcdBVPI10463 holotoxin and TcdBVPI10463-α16/17M68 were cloned into a modified pET28a vector with an N-terminal Twin-Strep tag following a PreScission protease-cleavage site and a C-terminal 6xHis tag. The full-length toxins were expressed and purified as described previously (49).

The GTD and its mutants, the covalently linked Cdc42T35N–GTDVPI10463 and R-RasT61N–GTDM68, were expressed in Escherichia coli strain BL21-Star (DE3) (Invitrogen). Bacteria were cultured at 37°C in LB medium containing kanamycin. The temperature was reduced to 18°C when optical density at 600 nm reached ~0.8. Expression was induced with 1 mM isopropyl-β-d-thiogalactopyranoside (IPTG) and continued at 18°C overnight. Rac1 was expressed using a similar protocol but with 0.1 mM IPTG induction. The cells were harvested by centrifugation and stored at −80°C until use.

Initial crystallization screening of the Cdc42T35N–GTDVPI10463 and the R-RasT61N–GTDM68 complexes in the presence of 5 mM UDP-glucose was carried out at 18°C using a Gryphon crystallization robot (Art Robbins Instruments) with commercial high-throughput crystallization screening kits from Hampton Research and Qiagen. Extensive manual optimizations were then performed at 18°C using the hanging-drop vapor-diffusion method when proteins were mixed with reservoir solution at 1:1 ratio. Streak-seeding was necessary to obtain single crystals suitable for x-ray diffraction. The best crystals for the Cdc42T35N–GTDVPI10463 complex were obtained in a mother liquor containing 0.1 M sodium cacodylate (pH 6.6), 2.4 M ammonium sulfate, and 2.5% (v/v) Jeffamine M-600 (pH 7.0), and the crystals were cryo-protected in the mother liquor supplemented with an additional 1.5 M lithium sulfate. The best crystals for the RasT61N–GTDM68 complex were grown in a condition containing 0.2 M ammonium acetate, 0.1 M sodium citrate tribasic dihydrate (pH 4.8), and 17% polyethylene glycol 4000, and the crystals were cryo-protected in the mother liquor supplemented with an additional 25% (v/v) ethylene glycerol.

The x-ray diffraction data were collected at 100 K at the NE-CAT beamline 24-ID-C, Advanced Photon Source. The data were processed with XDS software as implemented in RAPD (https://github.com/RAPD/RAPD) (53). For the Cdc42T35N–GTDVPI10463 complex, the structure was solved by molecular replacement using GTDVPI10463 (PDB: 2BVM) (30) and Cdc42 (PDB: 2WMN) (54) as the search models. One Cdc42T35N–GTDVPI10463 molecule could be positioned in the asymmetric unit using PHENIX.Phaser (55). For the R-RasT61N–GTDM68 complex, the structure was solved by molecular replacement using GTDM68 (PDB: 6OQ7) (34) and R-Ras (PDB: 2FN4) as the search models. Two R-RasT61N–GTDM68 molecules were positioned in the asymmetric unit using PHENIX.Phaser (55). The initial atomic models were refined with PHENIX.Refinement (55). Further structural modeling and refinement were carried out iteratively using COOT (56) and Phenix.Refinement (55) or Refmac5 refinement (57). All the refinement progress was monitored with the free R value using a 5% randomly selected test set. The structures were validated through the MolProbity (58). Data collection and structural refinement statistics are listed in table S1. All structure figures were prepared with PyMOL (DeLano Scientific).

For each reaction, the recombinant Rac1 (1 μM) was incubated with 10 nM GTD (WT or the mutants) and 10 μM UDP-glucose in a 20-μl buffer containing 50 mM Hepes (pH 7.5), 100 mM KCl, 2 mM MgCl2, 1 mM MnCl2, 10 μM GDP, and bovine serum albumin (0.1 mg/ml) for 60 min at room temperature. The reactions were stopped by adding 2× SDS loading buffer and boiling at 100°C. An equal amount of Rac1 from each reaction was loaded and analyzed by SDS–polyacrylamide gel electrophoresis (SDS-PAGE). Following electrophoresis, samples were transferred to nitrocellulose membranes and blocked with 5% milk/phosphate-buffered saline and 0.05% Tween 20 (PBST) and then probed with a 1/4000 dilution of the anti-Rac1 antibodies mAb 102 (BD Biosciences) or mAb 23A8 (MilliporeSigma). After an overnight incubation with the primary antibody, the blots were washed with PBST buffer and incubated with a 1/4000 dilution of an anti-mouse antibody conjugated with horseradish peroxidase for 60 min. Chemiluminescent detection was carried out using the enhanced chemiluminescence substrate kit (Thermo Fisher Scientific) and recorded on ChemiDoc Molecular Imager (Bio-Rad).

The hydrolase assay was performed following the manufacturer’s instruction (Promega). Briefly, 100 nM GTD and the mutations were incubated with 100 μM UDP-glucose in the hydrolase buffer [50 mM Hepes (pH 7.5), 100 mM KCl, 2 mM MgCl2, 1 mM MnCl2, and bovine serum albumin (0.1 mg/ml)] with a final volume of 20 μl. Reactions were allowed to proceed at room temperature for 15 or 60 min. Then, 10 μl of each reaction was added to a white, polystyrene, 96-well half-area microplate (Corning) containing 10 μl of UDP detection reagent that stopped the hydrolysis reaction. The plates were further incubated at room temperature for 1 hour, and luminescence was then recorded on a PerkinElmer multimode plate reader (EnVision 2015). To determine the kinetic parameters for the initial rate of the glycohydrolase reaction, 100 nM GTD or the mutants were incubated with varying concentrations of UDP-glucose (1.56 to 500 μM) in the hydrolase buffer for 15 min at room temperature. A UDP standard curve was established according to the manufacturer’s instructions to determine the conversion factor between the luminescence intensity and the amount of UDP product. The Km (Michaelis constant) and Vmax (maximal velocity) values were plotted against substrate UDP-glucose concentrations and fitted to the Michaelis-Menten equation. The data were obtained from three independent experiments.

Data and materials availability: Atomic coordinates and structure factors of the Cdc42T35N–GTDVPI10463 and R-RasT61N–GTDM68 complexes have been deposited in the PDB under accession codes 7S0Y and 7S0Z, respectively. The x-ray diffraction data were processed with XDS as implemented in RAPD (https://github.com/RAPD/RAPD). All data needed to evaluate the conclusions in the paper are present in the paper and/or the Supplementary Materials.

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