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Ulyanova V, Nadyrova A, Dudkina E, Kuznetsova A, Ahmetgalieva A, Faizullin D, Surchenko Y, Novopashina D, Zuev Y, Kuznetsov N, Ilinskaya O. Structural and Functional Differences between Homologous Bacterial Ribonucleases. Int J Mol Sci 2022; 23:ijms23031867. [PMID: 35163789 PMCID: PMC8837141 DOI: 10.3390/ijms23031867] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [What about the content of this article? (0)] [Affiliation(s)] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/25/2021] [Revised: 01/28/2022] [Accepted: 02/04/2022] [Indexed: 02/04/2023] Open
Abstract
Small cationic guanyl-preferring ribonucleases (RNases) produced by the Bacillus species share a similar protein tertiary structure with a high degree of amino acid sequence conservation. However, they form dimers that differ in conformation and stability. Here, we have addressed the issues (1) whether the homologous RNases also have distinctions in catalytic activity towards different RNA substrates and interactions with the inhibitor protein barstar, and (2) whether these differences correlate with structural features of the proteins. Circular dichroism and dynamic light scattering assays revealed distinctions in the structures of homologous RNases. The activity levels of the RNases towards natural RNA substrates, as measured spectrometrically by acid-soluble hydrolysis products, were similar and decreased in the row high-polymeric RNA >>> transport RNA > double-stranded RNA. However, stopped flow kinetic studies on model RNA substrates containing the guanosine residue in a hairpin stem or a loop showed that the cleavage rates of these enzymes were different. Moreover, homologous RNases were inhibited by the barstar with diverse efficiency. Therefore, minor changes in structure elements of homologous proteins have a potential to significantly effect molecule stability and functional activities, such as catalysis or ligand binding.
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Affiliation(s)
- Vera Ulyanova
- Department of Microbiology, Institute of Fundamental Medicine and Biology, Kazan (Volga Region) Federal University, 420008 Kazan, Russia; (A.N.); (E.D.); (A.A.); (Y.S.); (O.I.)
- Correspondence:
| | - Alsu Nadyrova
- Department of Microbiology, Institute of Fundamental Medicine and Biology, Kazan (Volga Region) Federal University, 420008 Kazan, Russia; (A.N.); (E.D.); (A.A.); (Y.S.); (O.I.)
| | - Elena Dudkina
- Department of Microbiology, Institute of Fundamental Medicine and Biology, Kazan (Volga Region) Federal University, 420008 Kazan, Russia; (A.N.); (E.D.); (A.A.); (Y.S.); (O.I.)
| | - Aleksandra Kuznetsova
- Institute of Chemical Biology and Fundamental Medicine, Siberian Branch of the Russian Academy of Sciences, 630090 Novosibirsk, Russia; (A.K.); (D.N.); (N.K.)
| | - Albina Ahmetgalieva
- Department of Microbiology, Institute of Fundamental Medicine and Biology, Kazan (Volga Region) Federal University, 420008 Kazan, Russia; (A.N.); (E.D.); (A.A.); (Y.S.); (O.I.)
| | - Dzhigangir Faizullin
- Kazan Institute of Biochemistry and Biophysics, FRC Kazan Scientific Center of RAS, 420111 Kazan, Russia; (D.F.); (Y.Z.)
| | - Yulia Surchenko
- Department of Microbiology, Institute of Fundamental Medicine and Biology, Kazan (Volga Region) Federal University, 420008 Kazan, Russia; (A.N.); (E.D.); (A.A.); (Y.S.); (O.I.)
| | - Darya Novopashina
- Institute of Chemical Biology and Fundamental Medicine, Siberian Branch of the Russian Academy of Sciences, 630090 Novosibirsk, Russia; (A.K.); (D.N.); (N.K.)
| | - Yuriy Zuev
- Kazan Institute of Biochemistry and Biophysics, FRC Kazan Scientific Center of RAS, 420111 Kazan, Russia; (D.F.); (Y.Z.)
| | - Nikita Kuznetsov
- Institute of Chemical Biology and Fundamental Medicine, Siberian Branch of the Russian Academy of Sciences, 630090 Novosibirsk, Russia; (A.K.); (D.N.); (N.K.)
| | - Olga Ilinskaya
- Department of Microbiology, Institute of Fundamental Medicine and Biology, Kazan (Volga Region) Federal University, 420008 Kazan, Russia; (A.N.); (E.D.); (A.A.); (Y.S.); (O.I.)
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Mascuch SJ, Fakhretaha-Aval S, Bowman JC, Ma MTH, Thomas G, Bommarius B, Ito C, Zhao L, Newnam GP, Matange KR, Thapa HR, Barlow B, Donegan RK, Nguyen NA, Saccuzzo EG, Obianyor CT, Karunakaran SC, Pollet P, Rothschild-Mancinelli B, Mestre-Fos S, Guth-Metzler R, Bryksin AV, Petrov AS, Hazell M, Ibberson CB, Penev PI, Mannino RG, Lam WA, Garcia AJ, Kubanek J, Agarwal V, Hud NV, Glass JB, Williams LD, Lieberman RL. A blueprint for academic laboratories to produce SARS-CoV-2 quantitative RT-PCR test kits. J Biol Chem 2020; 295:15438-15453. [PMID: 32883809 PMCID: PMC7667971 DOI: 10.1074/jbc.ra120.015434] [Citation(s) in RCA: 22] [Impact Index Per Article: 5.5] [Reference Citation Analysis] [What about the content of this article? (0)] [Affiliation(s)] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/29/2020] [Revised: 08/24/2020] [Indexed: 01/09/2023] Open
Abstract
Widespread testing for the presence of the novel coronavirus severe acute respiratory syndrome coronavirus 2 (SARS-CoV-2) in individuals remains vital for controlling the COVID-19 pandemic prior to the advent of an effective treatment. Challenges in testing can be traced to an initial shortage of supplies, expertise, and/or instrumentation necessary to detect the virus by quantitative RT-PCR (RT-qPCR), the most robust, sensitive, and specific assay currently available. Here we show that academic biochemistry and molecular biology laboratories equipped with appropriate expertise and infrastructure can replicate commercially available SARS-CoV-2 RT-qPCR test kits and backfill pipeline shortages. The Georgia Tech COVID-19 Test Kit Support Group, composed of faculty, staff, and trainees across the biotechnology quad at Georgia Institute of Technology, synthesized multiplexed primers and probes and formulated a master mix composed of enzymes and proteins produced in-house. Our in-house kit compares favorably with a commercial product used for diagnostic testing. We also developed an environmental testing protocol to readily monitor surfaces for the presence of SARS-CoV-2. Our blueprint should be readily reproducible by research teams at other institutions, and our protocols may be modified and adapted to enable SARS-CoV-2 detection in more resource-limited settings.
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Affiliation(s)
- Samantha J. Mascuch
- School of Biological Sciences, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Sara Fakhretaha-Aval
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Jessica C. Bowman
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Minh Thu H. Ma
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Gwendell Thomas
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Bettina Bommarius
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, Georgia, USA
- School of Chemical and Biomolecular Engineering, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Chieri Ito
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Liangjun Zhao
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Gary P. Newnam
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Kavita R. Matange
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Hem R. Thapa
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Brett Barlow
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Rebecca K. Donegan
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Nguyet A. Nguyen
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Emily G. Saccuzzo
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Chiamaka T. Obianyor
- School of Chemical and Biomolecular Engineering, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Suneesh C. Karunakaran
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Pamela Pollet
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | | | - Santi Mestre-Fos
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Rebecca Guth-Metzler
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Anton V. Bryksin
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Anton S. Petrov
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Mallory Hazell
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Carolyn B. Ibberson
- School of Biological Sciences, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Petar I. Penev
- School of Biological Sciences, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Robert G. Mannino
- Wallace H. Coulter Department of Biomedical Engineering, Georgia Institute of Technology and Emory University, Atlanta, Georgia, USA
| | - Wilbur A. Lam
- Wallace H. Coulter Department of Biomedical Engineering, Georgia Institute of Technology and Emory University, Atlanta, Georgia, USA
- Institute for Electronics and Nanotechnology, Georgia Institute of Technology, Atlanta, Georgia, USA
- Aflac Cancer and Blood Disorders Center, Children's Healthcare of Atlanta, Atlanta, Georgia, USA
- Department of Pediatrics, Emory University School of Medicine, Atlanta, Georgia, USA
| | - Andrés J. Garcia
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, Georgia, USA
- School of Mechanical Engineering, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Julia Kubanek
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Vinayak Agarwal
- School of Biological Sciences, Georgia Institute of Technology, Atlanta, Georgia, USA
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Nicholas V. Hud
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Jennifer B. Glass
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, Georgia, USA
- School of Earth and Atmospheric Sciences, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Loren Dean Williams
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, Georgia, USA
| | - Raquel L. Lieberman
- School of Chemistry and Biochemistry, Georgia Institute of Technology, Atlanta, Georgia, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, Georgia, USA
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3
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Mascuch SJ, Fakhretaha-Aval S, Bowman JC, Ma MTH, Thomas G, Bommarius B, Ito C, Zhao L, Newnam GP, Matange KR, Thapa HR, Barlow B, Donegan RK, Nguyen NA, Saccuzzo EG, Obianyor CT, Karunakaran SC, Pollet P, Rothschild-Mancinelli B, Mestre-Fos S, Guth-Metzler R, Bryksin AV, Petrov AS, Hazell M, Ibberson CB, Penev PI, Mannino RG, Lam WA, Garcia AJ, Kubanek JM, Agarwal V, Hud NV, Glass JB, Williams LD, Lieberman RL. A blueprint for academic labs to produce SARS-CoV-2 RT-qPCR test kits. medRxiv 2020:2020.07.29.20163949. [PMID: 32766604 PMCID: PMC7402063 DOI: 10.1101/2020.07.29.20163949] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [What about the content of this article? (0)] [Affiliation(s)] [Abstract] [Key Words] [Grants] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Indexed: 01/25/2023]
Abstract
Widespread testing for the presence of the novel coronavirus SARS-CoV-2 in individuals remains vital for controlling the COVID-19 pandemic prior to the advent of an effective treatment. Challenges in testing can be traced to an initial shortage of supplies, expertise and/or instrumentation necessary to detect the virus by quantitative reverse transcription polymerase chain reaction (RT-qPCR), the most robust, sensitive, and specific assay currently available. Here we show that academic biochemistry and molecular biology laboratories equipped with appropriate expertise and infrastructure can replicate commercially available SARS-CoV-2 RT-qPCR test kits and backfill pipeline shortages. The Georgia Tech COVID-19 Test Kit Support Group, composed of faculty, staff, and trainees across the biotechnology quad at Georgia Institute of Technology, synthesized multiplexed primers and probes and formulated a master mix composed of enzymes and proteins produced in-house. Our in-house kit compares favorably to a commercial product used for diagnostic testing. We also developed an environmental testing protocol to readily monitor surfaces across various campus laboratories for the presence of SARS-CoV-2. Our blueprint should be readily reproducible by research teams at other institutions, and our protocols may be modified and adapted to enable SARS-CoV-2 detection in more resource-limited settings.
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Affiliation(s)
- Samantha J Mascuch
- School of Biological Sciences, Georgia Institute of Technology, Atlanta, GA, USA
| | - Sara Fakhretaha-Aval
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Jessica C Bowman
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, GA, USA
| | - Minh Thu H Ma
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Gwendell Thomas
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Bettina Bommarius
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, GA, USA
- School of Chemical & Biomolecular Engineering, Georgia Institute of Technology, Atlanta, GA, USA
| | - Chieri Ito
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Liangjun Zhao
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, GA, USA
| | - Gary P Newnam
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Kavita R Matange
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Hem R Thapa
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Brett Barlow
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Rebecca K Donegan
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Nguyet A Nguyen
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Emily G Saccuzzo
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Chiamaka T Obianyor
- School of Chemical & Biomolecular Engineering, Georgia Institute of Technology, Atlanta, GA, USA
| | - Suneesh C Karunakaran
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Pamela Pollet
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | | | - Santi Mestre-Fos
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Rebecca Guth-Metzler
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Anton V Bryksin
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, GA, USA
| | - Anton S Petrov
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Mallory Hazell
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
| | - Carolyn B Ibberson
- School of Biological Sciences, Georgia Institute of Technology, Atlanta, GA, USA
| | - Petar I Penev
- School of Biological Sciences, Georgia Institute of Technology, Atlanta, GA, USA
| | - Robert G Mannino
- Wallace H. Coulter Department of Biomedical Engineering, Georgia Institute of Technology and Emory University, Atlanta, GA, USA
| | - Wilbur A Lam
- Wallace H. Coulter Department of Biomedical Engineering, Georgia Institute of Technology and Emory University, Atlanta, GA, USA
- Institute for Electronics and Nanotechnology, Georgia Institute of Technology, Atlanta, GA, USA
- Aflac Cancer and Blood Disorders Center, Children's Healthcare of Atlanta, Atlanta, GA, USA
- Department of Pediatrics, Emory University School of Medicine, Atlanta, GA, USA
| | - Andrés J Garcia
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, GA, USA
- School of Mechanical Engineering, Georgia Institute of Technology, Atlanta, GA, USA
| | - Julia M Kubanek
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, GA, USA
| | - Vinayak Agarwal
- School of Biological Sciences, Georgia Institute of Technology, Atlanta, GA, USA
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, GA, USA
| | - Nicholas V Hud
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, GA, USA
| | - Jennifer B Glass
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, GA, USA
- School of Earth & Atmospheric Sciences, Georgia Institute of Technology, Atlanta, GA, USA
| | - Loren Dean Williams
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, GA, USA
| | - Raquel L Lieberman
- School of Chemistry & Biochemistry, Georgia Institute of Technology, Atlanta, GA, USA
- Petit Institute for Bioengineering and Biosciences, Georgia Institute of Technology, Atlanta, GA, USA
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Abstract
Electrochemical aptamer-based (E-AB) sensors offer advantageous analytical detection abilities due to their rapid response time (seconds to minutes), specificity to a target, and selectivity to function in complex media. Ribonucleic acid (RNA) aptamers employed in this class of sensor offer favorable binding characteristics resulting from the ability of RNA to form stable tertiary folds aided by long-range intermolecular interactions. As a result, RNA aptamers can fold into three-dimensional structures more complex than those of their DNA counterparts and consequently exhibit better binding ability to target analytes. Unfortunately, RNA aptamers are susceptible to degradation by nucleases, and for this reason, RNA-based sensors are scarce or require significant sample pretreatment before use in clinically relevant media. Here, we combine the usefulness of a collagen I hydrogel membrane with entrapped ribonuclease inhibitors (RI) to protect small molecule RNA E-AB sensors from endogenous nucleases in complex media. More specifically, the biocompatibility of the naturally polymerized hydrogel with encapsulated RI promotes the protection of an aminoglycoside-binding RNA E-AB sensor up to 6 h, enabling full sensor function in nuclease-rich environments (undiluted serum) without the need for prior sample preparation or oligonucleotide modification. The use of collagen as a biocompatible membrane represents a general approach to compatibly interface E-AB sensors with complex biological samples.
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Affiliation(s)
- Mirelis Santos-Cancel
- Department of Chemistry and Biochemistry, University of Maryland Baltimore County (UMBC), Baltimore, Maryland 21250
| | - Ryan J. White
- Department of Chemistry and Biochemistry, University of Maryland Baltimore County (UMBC), Baltimore, Maryland 21250
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Cong X, Cremer C, Nachreiner T, Barth S, Carloni P. Engineered human angiogenin mutations in the placental ribonuclease inhibitor complex for anticancer therapy: Insights from enhanced sampling simulations. Protein Sci 2016; 25:1451-60. [PMID: 27110669 DOI: 10.1002/pro.2941] [Citation(s) in RCA: 10] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [What about the content of this article? (0)] [Affiliation(s)] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/14/2016] [Accepted: 04/20/2016] [Indexed: 01/29/2023]
Abstract
Targeted human cytolytic fusion proteins (hCFPs) represent a new generation of immunotoxins (ITs) for the specific targeting and elimination of malignant cell populations. Unlike conventional ITs, hCFPs comprise a human/humanized target cell-specific binding moiety (e.g., an antibody or a fragment thereof) fused to a human proapoptotic protein as the cytotoxic domain (effector domain). Therefore, hCFPs are humanized ITs expected to have low immunogenicity. This reduces side effects and allows long-term application. The human ribonuclease angiogenin (Ang) has been shown to be a promising effector domain candidate. However, the application of Ang-based hCFPs is largely hampered by the intracellular placental ribonuclease inhibitor (RNH1). It rapidly binds and inactivates Ang. Mutations altering Ang's affinity for RNH1 modulate the cytotoxicity of Ang-based hCFPs. Here we perform in total 2.7 µs replica-exchange molecular dynamics simulations to investigate some of these mutations-G85R/G86R (GGRRmut ), Q117G (QGmut ), and G85R/G86R/Q117G (GGRR/QGmut ). GGRRmut turns out to perturb greatly the overall Ang-RNH1 interactions, whereas QGmut optimizes them. Combining QGmut with GGRRmut compensates the effects of the latter. Our results explain the in vitro finding that, while Ang GGRRmut -based hCFPs resist RNH1 inhibition remarkably, Ang WT- and Ang QGmut -based ones are similarly sensitive to RNH1 inhibition, whereas Ang GGRR/QGmut -based ones are only slightly resistant. This work may help design novel Ang mutants with reduced affinity for RNH1 and improved cytotoxicity.
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Affiliation(s)
- Xiaojing Cong
- Computational Biophysics, German Research School for Simulation Sciences (Joint Venture of RWTH Aachen University and Forschungszentrum Jülich), Jülich, 52428, Germany
- Computational Biomedicine Section, Institute for Advanced Simulations - 5 (IAS-5), Jülich, 52428, Germany, Forschungszentrum Jülich
- Computational Biomedicine Section, Institute for Neuroscience and Medicine - 9 (INM-9), Jülich, 52428, Germany, Forschungszentrum Jülich
| | - Christian Cremer
- Department of Experimental Medicine and Immunotherapy, Institute for Applied Medical Engineering, University Hospital RWTH Aachen, Aachen, 52074, Germany
| | - Thomas Nachreiner
- Department of Experimental Medicine and Immunotherapy, Institute for Applied Medical Engineering, University Hospital RWTH Aachen, Aachen, 52074, Germany
| | - Stefan Barth
- Institute of Infectious Disease and Molecular Medicine (IDM), Faculty of Health Sciences, University of Cape Town, Cape Town, 7925, South Africa
- South African Research Chair in Cancer Biotechnology, Department of Integrative Biomedical Sciences, Faculty of Health Sciences, University of Cape Town, 7925, Cape Town, South Africa
| | - Paolo Carloni
- Computational Biophysics, German Research School for Simulation Sciences (Joint Venture of RWTH Aachen University and Forschungszentrum Jülich), Jülich, 52428, Germany
- Computational Biomedicine Section, Institute for Advanced Simulations - 5 (IAS-5), Jülich, 52428, Germany, Forschungszentrum Jülich
- Computational Biomedicine Section, Institute for Neuroscience and Medicine - 9 (INM-9), Jülich, 52428, Germany, Forschungszentrum Jülich
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Sica F, Pica A, Merlino A, Russo Krauss I, Ercole C, Picone D. The multiple forms of bovine seminal ribonuclease: structure and stability of a C-terminal swapped dimer. FEBS Lett 2013; 587:3755-62. [PMID: 24140346 DOI: 10.1016/j.febslet.2013.10.003] [Citation(s) in RCA: 7] [Impact Index Per Article: 0.6] [Reference Citation Analysis] [What about the content of this article? (0)] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/13/2013] [Accepted: 10/07/2013] [Indexed: 11/20/2022]
Abstract
Bovine seminal ribonuclease (BS-RNase) acquires an interesting anti-tumor activity associated with the swapping on the N-terminal. The first direct experimental evidence on the formation of a C-terminal swapped dimer (C-dimer) obtained from the monomeric derivative of BS-RNase, although under non-native conditions, is here reported. The X-ray model of this dimer reveals a quaternary structure different from that of the C-dimer of RNase A, due to the presence of three mutations in the hinge peptide 111-116. The mutations increase the hinge peptide flexibility and decrease the stability of the C-dimer against dissociation. The biological implications of the structural data are also discussed.
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Abstract
Onconase (ONC) is an amphibian member of the bovine pancreatic ribonuclease (RNase A) superfamily that exhibits innate antitumoral activity. ONC has been granted both orphan-drug and fast-track status by the U.S. Food and Drug Administration for the treatment of malignant mesothelioma, and is poised to become the first chemotherapeutic agent based on a ribonuclease. Investigations into the mechanism of ribonuclease-based cytotoxicity have elucidated several important determinants for cytotoxicity, including efficient deliverance of ribonucleolytic activity to the cytosol and preservation of conformation stability. Nevertheless, the most striking similarity between ONC and bovine seminal ribonuclease, another naturally cytotoxic ribonuclease, is their insensitivity to inhibition by the potent cytosolic ribonuclease inhibitor protein (RI). RI typically binds to its ribonuclease ligands with femtomolar affinity--an extraordinary feat considering the modest sequence identity among the bound ribonucleases. Mammalian ribonucleases such as RNase A or its human homologue, RNase 1, have the potential to be more attractive chemotherapeutic agents than ONC owing to their higher catalytic activity, low potential for immunogenicity, favorable tissue distribution, and high therapeutic index, but are limited by their sensitivity to RI. These non-toxic mammalian ribonucleases can be transformed into potent cytotoxins by engendering them with RI-evasion using protein engineering strategies such as site-directed mutagenesis, multimerization, fusion to a targeting moiety, and chemical modification. In several instances, these engineered ribonucleases exhibit greater cytotoxicity in vitro than does ONC. Herein, we review the biochemical characteristics of RIribonuclease complexes and progress towards the development of mammalian ribonuclease-based chemotherapeutics through the elicitation of RI-evasion.
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Affiliation(s)
| | - Ronald T. Raines
- Address correspondence to this author at the Department of Biochemistry, University of Wisconsin–Madison, 433 Babcock Drive, Madison, WI 53706-1544, USA; Tel: (608) 262-8588; Fax: (608) 262-3453;
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8
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Matoušek J, Kim JS, Souček J, Rìha J, Ribó M, Leland PA, Raines RT. Ribonucleases endowed with specific toxicity for spermatogenic layers. Comp Biochem Physiol B Biochem Mol Biol 1997; 118:881-888. [PMID: 21399757 PMCID: PMC3055560 DOI: 10.1016/s0305-0491(97)00278-2] [Citation(s) in RCA: 6] [Impact Index Per Article: 0.2] [Reference Citation Analysis] [What about the content of this article? (0)] [Affiliation(s)] [Abstract] [Key Words] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/25/2022]
Abstract
Bovine seminal ribonuclease (BS-RNase) is a dimer in which the subunits are cross-linked by disulfide bonds between Cys31 of one subunit and Cys32 of the other. Dimeric BS-RNase is resistant to ribonuclease inhibitor (RI), a protein endogenous to mammalian cells, and is toxic to a variety of cell types. Monomeric BS-RNase (like its homolog, RNase A) is bound tightly by RI and is not cytotoxic. The three-dimensional structure of the RI·RNase A complex suggests that carboxymethylation of C32S BS-RNase (to give MCM31) or C31S BS-RNase (MCM32) could diminish affinity for RI. We find that MCM31 and MCM32 are not only resistant to RI, but are also aspermatogenic to mice. In contrast to the aspermatogenic activity of dimeric BS-RNase, that of MCM31 and MCM32 is directed only at spermatogenic layers. Intratesticular injection of MCM31 or MCM32 affects neither the diameter of seminiferous tubules nor the weight of testes. Also in contrast to wild-type BS-RNase, MCM31 and MCM32 are not toxic to other cell types. Direct immunofluorescence reveals that MCM31 and MCM32 bind only to spermatogonia and primary spermatocytes. This cell specificity makes MCM31 and MCM32 of potential use in seminoma therapy and contraception.
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Affiliation(s)
- Josef Matoušek
- Institute of Animal Physiology and Genetics, Academy of Sciences of the Czech Republic, 277 21 Liběchov, Czech Republic
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