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Water bath is more efficient than hot air oven at thermal inactivation of coronavirus

Virology Journal volume 20, Article number: 84 (2023) Cite this article

Abstract

Background

Thermal inactivation is a conventional and effective method of eliminating the infectivity of pathogens from specimens in clinical and biological laboratories, and reducing the risk of occupational exposure and environmental contamination. During the COVID-19 pandemic, specimens from patients and potentially infected individuals were heat treated and processed under BSL-2 conditions in a safe, cost-effective, and timely manner. The temperature and duration of heat treatment are optimized and standardized in the protocol according to the susceptibility of the pathogen and the impact on the integrity of the specimens, but the heating device is often undefined. Devices and medium transferring the thermal energy vary in heating rate, specific heat capacity, and conductivity, resulting in variations in efficiency and inactivation outcome that may compromise biosafety and downstream biological assays.

Methods

We evaluated the water bath and hot air oven in terms of pathogen inactivation efficiency, which are the most commonly used inactivation devices in hospitals and biological laboratories. By evaluating the temperature equilibrium and viral titer elimination under various conditions, we studied the devices and their inactivation outcomes under identical treatment protocol, and to analyzed the factors, such as energy conductivity, specific heat capacity, and heating rate, underlying the inactivation efficiencies.

Results

We compared thermal inactivation of coronavirus using different devices, and have found that the water bath was more efficient at reducing infectivity, with higher heat transfer and thermal equilibration than a forced hot air oven. In addition to the efficiency, the water bath showed relative consistency in temperature equilibration of samples of different volumes, reduced the need for prolonged heating, and eliminated the risk of pathogen spread by forced airflow.

Conclusions

Our data support the proposal to define the heating device in the thermal inactivation protocol and in the specimen management policy.

Background

Specimen from patients and healthy volunteers often carry, or are contaminated with, known and unknown pathogens. A large number of victims acquired hepatitis and immunodeficiency syndrome through contaminated needle injections, blood transfusions, or dialysis before the implementation of mandatory screening for the respective viral pathogens in medical practices [1, 2]. Laboratory staffs who processing specimens occupationally became exposed to infectious agents and acquired infections through accidental contact with pathogenic bacteria, viruses, parasites, and fungi [3, 4]. The pathogens in medical waste without inactivation or sterilization could persist in the environment for an extended period of time and posed a threat to public health [5, 6]. During the pandemic of COVID-19, WHO and other authorities established guidelines for the processing of specimens and disposal of medical wastes to reduce the risk of exposure of hospital staff and the public to SARS-CoV-2 [7, 8]. Inactivation of specimens has been a mandatory procedure to protect hospital staff and the environment from contamination and spread of pathogens.

Various methods are recommended to inactivate pathogens in specimens, including chemical and physical, depending on the convenience, effectiveness, and compatibility with downstream biological processing. For example, formaldehyde was commonly used to eliminate pathogen infectivity while preserving cell morphology, which was often recommended for pathological and morphological diagnostics [9]. However, formaldehyde potentially altered protein structure, and was not recommended for diagnostic purposes depending on the nature of protein [10]. Detergents and Trizol were commonly used for inactivation and nucleic acid extraction, but had to be removed from samples to minimize the impact on downstream processing [11]. Chemical inactivation, such as fixation and denaturation, was not preferred for samples for immunological and nucleic acid based diagnostics because of the potential alteration of the antigenic epitopes critical for immunoassays and fragmentation of nucleic acids for polymerase chain reaction [12]. Physical inactivation mainly uses radiation and thermal energy to eliminate pathogen infectivity. Ultraviolet radiation has been used to inactivate viruses by altering viral protein structure and nucleic acids, but required considerable protection from occupational exposure, optimization of dose and exposure time [13], and the effectiveness was negated by the presence of protein in the sample [14]. Gamma irradiation has been used to inactivate a variety of pathogens. However, the accessibility, cost, and potential radioactive hazard limit its application. Thermal inactivation is the most convenient, cost-effective, and effective approach applicable to a variety of samples, such as plasma, urine, feces, nasopharyngeal, and oropharyngeal samples for serological, immunological and biochemical analysis and pathogen identification. Thermal energy denatures nucleic acids and randomly alters the structure and conformation of proteins, preventing attachment, fusion, and replication of pathogens and impairing the infectivity [15, 16], and has been used to inactivate various pathogens including viruses, bacteria, and fungi [17,18,19]. Thermal energy can also inactivate enzymes, denature protein structure, alter bioactivity, and oxidize molecules critical to diagnostics. Excessive energy could lead to false test results, particularly in samples with trace amounts of target biomarkers [20]. Although it is the most common approach to reduce pathogen infectivity with limited impact on the sample [15, 21, 22], thermal inactivation needs to be optimized to balance pathogen inactivation and sample integrity.

The Optimal temperature and duration of heat exposure depend on the intrinsic properties of the pathogen, the nature of the sample, and the downstream biological assay. For example, the titer of Middle East Respiratory Syndrome virus diminished by 4log10 in 25 min at 56℃. However, at 65℃, this decrease was achieved within 1 min [23]. The titer of SARS coronavirus diminished by 4log10 at 56 °C in 15 min [14]. Above 95 °C, the SARS-CoV-2 RNA copies and detection rate decreased significantly [24]. Prolonged exposure to excessive thermal treatment also altered the diagnostic assessment of antibodies [18, 25] and RNAs [21]. Optimized temperature and minimized exposure to heat reduce the adverse effects on samples and ensure the accuracy of assays. The WHO recommended 56 °C for 30 min for SARS-Cov-2 inactivation [7, 26]. This combination of temperature and duration has been adapted and proven safe without significantly affecting biological markers or viral nucleic acid detection [18, 24]. The efficiency of thermal inactivation also depended on the heating device and thermal energy transfer medium, which had different heating rates, thermal conductivity, and specific heat capacities [27]. However, these key factors are often neglected or not defined in most inactivation protocols and guidelines. For example the World Health Organization (WHO), the Centers for Disease Control and Prevention (CDC, USA), and the Chinese Center for Disease Control and Prevention did not define heating devices in their guidelines for COVID-19 specimen inactivation [7, 28]. To investigate how the heating device, heat transfer medium, and specimen container affected the efficiency of pathogen inactivation, we compared the inactivation efficiency of water bath and forced-air oven that have been commonly used in hospitals and biological laboratories, using transmissible gastroenteritis virus of swine (TGEV) as a model pathogen. TGEV is pathogenic to pigs but safe for humans, which can be handled outside a BSL-3 facility. TGEV, like SARS-CoV-2, SARS-CoV, and other coronaviruses, is a member of the coronaviridae family, and shares most structural features with SARS-CoV-2. Both are enveloped, single-stranded positive sense RNA viruses. Both virions are approximately spherical particles of about 100–160 nm in diameter and contain 4 structural proteins, spike (S), envelope (E), membrane (M), and nucleocapsid (N). The S, E, and M are membrane proteins. The N encapsulates the viral genome and packages it into a ribonucleoprotein [29, 30]. The S proteins, which are key to virus binding to the receptor and infecting the host cell, are structurally similar to other coronaviruses [31]. These common features made TGEV and other human coronaviruses indistinguishable in structure and components, and made the TGEV an excellent model for studying sensitivity and stability to antiviral agents [32, 33]. In fact, TGEV has been used as a surrogate for SARS CoV and SARS-CoV-2 for susceptibility testing to biocidal agents and harsh environments [34, 35]. Our comparison will provide a technical reference for the establishments of a thermal inactivation protocol, which could be critical for virus inactivation efficiency, diagnostic accuracy, and biosafety.

Methods

Thermal equilibrium assessment

Conical tubes filled with pure water sample were precooled to 8 ℃ and placed in a water bath (Shanghai Yiheng Scientific Instrument, China) or a dry air oven with forced airflow (Memmert, Germany) that were preheated to 56 ℃. The temperatures of samples were probed and recorded continuously at a frequency of every second with a digital thermometer SSN-11E (range: -40 to 125℃/-40 to -257℉; sensitivity: 0.1 ± 0.5℃/0.2 ± 0.5℉, YOWEXA, China). For consistency, the probe was immersed 30 mm below the sample surface and in the center of the tube without contacting the tube wall.

Virus and cell line

Transmissible gastroenteritis virus (TGEV) and the porcine intestinal columnar epithelial cell line (IPEC-J2) were kindly provided by Dr. Zhiwen Xu, Sichuan Agricultural University, China. IPEC-J2 cells were cultured in Dulbecco’s modified Eagle’s medium (DMEM, Thermo Fisher Scientific, MA) supplemented with 10% fetal bovine serum (Thermo Fisher Scientific, MA). Viral stocks were prepared by infecting 80% confluent layers of IPEC-J2 cells with 5 MOI of TGEV in 75 cm2 flasks. After incubation at 37℃ for 1 h in 5 mL 2% FBS DMEM medium, the flask was supplemented with 15 mL of 2% FBS DMEM medium and cultured for another 24–48 h. Cells were collected, lysed by freeze-thawing, and spun at 3,000 g for 15 min. Supernatants were collected, aliquoted, and stored at -80℃ as virus stock. Virus titers were determined by the 50% tissue culture infectious doses (TCID50) assay [36]. Briefly, IPEC-J2 cells were seeded into a 96-well plates at 2 × 104 cells/well. After reaching 80% confluence, the wells were infected with 100 µL of ten-fold serially diluted TGEV in eight replicates and cultured at 37 °C for 1 h. The wells were replenished with 100 µL of DMEM medium supplemented with 2% FBS, and incubated for another 48–72 h at 37 °C. The number of cytopathic wells in each dilution was counted. Virus titers were calculated by the Reed-Muench method and expressed as TCID50.

Virus thermal inactivation

TGEV stocks at 10 × 106.16 TCID50 in 1 mL each were added into 1.5 mL conical microcentrifuge tubes and precooled to 4 °C. The tubes were placed in a preheated water bath at 56℃ or a dry air oven with forced airflow. At the indicated time intervals, the tubes were removed and quenched on ice. Samples were then subject to limited dilution and the virus titers were assessed by plaque assay as described above.

Statistical analysis

Data were analyzed with GraphPad Prism 6.0 (GraphPad, La Jolla, CA, USA).

Results

Water bath has higher heating rates than air oven

To compare the heating rates of thermal inactivation devices, pure water samples in 50 mL conical polypropylene tubes were precooled to 8 ℃, loaded on a rack, and placed in a water bath or air oven, which are the most commonly used in hospital and biology laboratories, where the thermal energy is conducted by water or by forced airflow, respectively. The forced airflow increases the air velocity and distributes the heat evenly within the oven. In the water bath, the sample height matched the level of the heating water in the tank. The sample temperature was probed and recorded in real time at a frequency of every second. The dynamics of the temperature equilibrium over time are shown in Fig. 1, and were analyzed with the Dissemination-One Phase Exponential Decay. The K-value represents the heating rates. The result shows that water bath has significantly higher heating rate than air oven, and samples in water bath need less time than those in air oven to reach 56 °C from 8 °C initial temperature.

Fig. 1
figure 1

Heating rates of water bath and air oven. Pure water samples in conical tubes were precooled to 8 ℃ and placed into water bath and air oven. The temperature was monitored and recorded with a digital thermometer in real time and at a frequency of every second. The heating rate (K) was calculated with Dissociation - One phase Exponential Decay with GraphPad Prism. Data are representative of 3 independent experiments

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Effect of sample volume and container on the heating rate

Sample volume had a different effect on thermal equilibrium in the water bath and air oven. In the water bath, increasing the sample volume but matching the height to the level of the heating water did not increase the time lapse to 56 °C (Fig. 2b). This was consistent with the observation shown in Fig. 1, where the heating rate K was maintained consistent with the increase in sample volume. In the air oven, increasing the sample volume increased the time lapse to 56 °C. The time lapses between 20 mL and 30 mL, 30 mL and 40 mL were significantly different. Details of the time lapse to 56 °C are shown in Table 1.

Fig. 2
figure 2

Effect of sample height, volume, and container diameter on duration to 56 °C. (a) Conical tubes filled with 10 mL pure water sample in each were precooled to 8 ℃ and placed in a water bath preheated to 56 ℃. The sample height matched the level of heating water, or kept higher or lower than the level of heating water in scales respectively. The height difference was expressed as Δ. The time lapse of the sample to 56 ℃ was presented as mean ± SD from 3 independent experiments. (b) Conical tubes were filled with pure water sample in different volume were precooled to 8 ℃ and placed in water bath and air oven preheated to 56 ℃. The time lapse of water sample to 56 ℃ was shown. (c) Containers with indicated diameter were filled with 40 mL of pure water sample and precooled to 8 ℃. After being placed in water bath or air oven preheated to 56 ℃, the time lapse of water sample to 56 ℃ was shown. Data in (b) and (c) were representative of 3 independent experiments and analyzed by linear regression

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Table 1 Time lapse of specimen to 56 ℃
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In water bath inactivation, the sample height may not always match the level of heating water level in routine practice, and the difference would affect the thermal equilibrium. Our study showed that samples with a height above the level of heating water needed extra time to 56 °C, and the extended time correlated with the difference in heights (Δ). As shown in Fig. 2a, the sample with a height higher than the heating water in 40 mm needed an additional 41.07 min to 55 °C compared with the sample with a height matching the heating water, and failed to reach 56 °C as the pre-set heating water temperature even when the duration was extended to more than 85 min.

Increasing the diameter of the sample container increases the distance of heat energy transferred to the center of the sample but increases the contact area with the heating medium if the sample volume is kept constant. We tested containers with diameters of 23, 28, and 45 mm filled with 40 mL of samples, and found that increasing the diameter of the container slightly decreased the time to 56 °C in the water bath, but slightly increased the time to 56 °C in the air oven, although the differences were not significant (Fig. 2c). Samples in each container tested required additional time to reach 56 °C in the air oven compared to the water bath.

Water bath is more efficient at TGEV inactivation than air oven

Samples containing TGEV 10e6.16 TCID50 in each tube were placed in a water bath or air oven that were preheated to 56 °C, removed at the indicated time intervals, quenched on ice, and assessed for virus titer. Both inactivation data were analyzed by linear regression curves in a logarithmic plot of virus titer versus inactivation time (Fig. 3). The best-fit line is shown in dot line with a coefficient of -1.961and − 0.162 for water bath and air oven respectively. We found that the virus titer diminished more quickly and significantly in the water bath than in the air oven. A 4 Log10 reduction, representing a 99.99% inactivation, required 17.77 min in the water bath but 27.33 min in the air oven. After 26 min, the virus titer dropped below the detection limit of 10e1TCID50 /mL by water bath inactivation, while the titer remained at 10e2.44 TCID50 /mL by air oven treatment. After 30 min, 10e1.74 TCID50 /mL remained in the air oven inactivated sample.

Fig. 3
figure 3

Efficiency of pathogen inactivation by water bath and air oven. TGEV in 1 mL was precooled to 8 ℃ and placed into 56 ℃ water bath or air oven respectively, removed at the indicated time intervals, and quenched on ice. Virus titers were assessed and expressed as TCID50. The dot line in blue and red showed the best-fit pattern of water and air oven inactivation by linear regression analysis respectively. The gray line represents the lower limit of detection at 10e1TCID50 /mL. Data are representative of 3 independent experiments and presented as mean ± SD. The low limit of detection for viral cytopathic effect was 10e1 TCID50 /mL

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Discussion

Our study demonstrates that water bath is more efficient than air oven in thermal inactivation of pathogenic microorganisms, and eliminates the infectivity in a timely and consistent manner. In addition, the water bath reduces the risk of prolonged heat exposure and the spread of pathogens by forced airflow, and is energy efficient. This efficiency is less likely to vary with changes in sample volume, providing convenience and quality assurance in the daily practice of clinical and biological laboratories. The mechanism underlying the efficiency is the advantages of thermal conductivity, specific heat capacity, and heating rate of the water bath over the air oven. Assurance of pathogen inactivation guarantees biosafety; minimization of heat exposure reduces alternation to specimen, especially to critical biomarkers, thus, improving the quality of diagnosis. Water bath is recommended for routine processing of infectious specimens. Our evaluation highlights an often overlooked but critical issue for biosafety and diagnostics, and demonstrates the importance of defining the inactivation device in protocols and guidelines of specimen management.

Incomplete pathogen inactivation compromises biosafety; overheating damages integrity of sample and alters assay results. Prolonged heating has been a temptation to ensure inactivation with low efficiency devices. During the pandemic of COVID-19, thermal inactivation provided a convenient and rapid approach to allow specimens to be processed in BSL-2 facilities. However, evaluation found that heat treatment altered the quantity of SARS-CoV-2 RNA and reduced the sensitivity of pathogen identification, particularly for those with low viral loads [20]. A water bath at 56 °C for 30 min reduced 48.55% of nucleocapsid gene copies and 56.40% of ORF1ab gene copies; an air oven at 80 °C for 20 min reduced 50–60% of SARS-CoV-2 RNA copies. After autoclaving at 121 °C for 20 min or boiling at 100 °C for 20 min, no viral RNA could be detected in the samples [26]. A study found that 56 °C for 30 min or 60 °C for 60 min had little effect on the detection of viral RNA in specimens with viral loads > 6 Log10 TCID50, but reduced the quantity of RNA by at least 4 Log10 TCID50, while 92 °C for 15 min reduced viral RNA to a level below the detection limit of conventional quantitative PCR [21]. Thermal inactivation of sera samples also had a negligible impact on IgG binding capacity [18] and significantly reduced the neutralizing activity against SARS-CoV-2 [21]. Heat treatment at 56 °C for 60 min decreased thyroid-stimulating hormone, aspartate aminotransferase, and pancreatic amylase in plasma by 23–30% compared with no treatment, and damaged creatine kinase, myoglobin, alanine aminotransferase, γ-glutamyl transferase, lactate dehydrogenase, alkaline phosphatase, and the blood coagulation indicators. In contrast, thyroxine was increased by 2.4 folds by 30 min of thermal treatment [37]. The temperature and duration of heating must be minimized to balance pathogen inactivation with the nature of the specimen. Increasing the heating rate can reduce the risk of heating damage and minimize the negative impact on downstream diagnostics without compromising the biosafety.

The mechanism underlying water bath efficiency is the thermal conductivity, specific heat capacity, and heating rate. Thermal energy transfer through water is 20 times faster than that through air, and the specific heat capacity of water is 4.23 times higher than that of air. A high heating rate rapidly denatured nucleic acids and altered protein structure of pathogens [38], leading to a high inactivation efficiency [39]. The heating rate also has a profound effect on host cells harboring viral pathogens. Thermodynamic reaction and physiochemistry showed the development of thermal tolerance below the breakpoint under the slope of the Arrhenius plot [40], and demonstrated that thermal tolerance developed to a greater extent at slow heating rates [41,42,43]. A high heating rate also resulted in additional sensitization of pathogens to heat thus a quick reduction in infectivity. For a heating rate of 20 °C /minute to 14.7 °C /second, there was a more than 10-fold increase in inactivation efficiency [44]. In contrast, decreasing the heating rate from 10 °C/minute to 2 °C /minute increased heat resistance and resulted in incomplete inactivation [45]. It was hypothesized that a response to heat stress, such as upregulation of heat shock protein, could be induced by slow heating, leading to adaption to heat treatment. Our data also showed that the air oven required approximately 10 min more than the water bath to achieve a 4Log10 reduction in TGEV. Forced air circulation may facilitate the thermal energy exchange between the sample and hot air, but the heat transfer and specific heat capacity limited the heating rate of air oven. In addition, water bath has no forced airflow and circulation, thus, is safer to the environment. Water bath is preferred for routine processing of infectious specimen.

The efficiency of the water bath also ensures a consistent inactivation outcome. In routine clinical practice, especially during the pandemic, specimens were of various volume sizes and in overwhelming quantity. The high workload challenged the processing speed, capacity, and biosafety. The dynamics of thermal equilibria varied with specimens of different volume by air oven treatment, suggesting uncertainty of inactivation outcome. Prolonged hot air treatment was a temptation to ensure biosafety but compromised the integrity of specimen and the downstream diagnostics. This uncertainty can be averted by using a water bath as the preferred method. Our data showed that thermal equilibria did not vary with specimens in different volumes, nor with different types of containers tested. Water bath is preferred for efficient inactivation with consistent inactivation outcome.

Our study has limitations. We used a TGEV model to study the efficiency of sample inactivation by water bath and air oven, and to address concerns about biosafety and diagnostic quality of COVID-19 specimens. We did not evaluate this study using SARS-CoV-2 as a biosafety precaution although both viruses share most of the component and structural features, and TGEV has been used as a model to explore the stability of coronaviruses to harsh treatment. We focused on viral samples in the fluid state, which are the most common in clinical and biological laboratories. Our conclusion may not be applicable to specimen in solid and dry states and inactivated with other devices such as hot steam. Protein, salt, and other components in specimens may affect thermal inactivation, and protect pathogens by reducing the susceptibility to heat. For instance, SARS-CoV survived longer in PBS than in dechlorinated tap water [46]. Proteolytic enzymes increased the susceptibility of enteric viruses to thermal inactivation by cleaving viral proteins and exposing viral RNA [47]. Protein in the sample medium provided protection against SARS-CoV. With 20% protein, infectivity was reduced by less than 2Log10 after 30 min at 56 °C, leaving a residual infectivity. The sample had to be treated at 60 °C for 30 min for complete inactivation [48]. Our conclusion needs to be evaluated in a wide range of applications.

Conclusions

Heating device has a significant impact on inactivation efficiency and biosafety. Water bath is relatively superior in thermal conductivity, specific heat capacity and heating rate, and confers the efficiency of thermal inactivation of infectious specimen.; Air oven has advantage of capacity and convenience, and can process specimens in bulk but needs prolonged duration relative to water bath for completion of inactivation. In general, water bath offers a balance of convenience, effectiveness, biosafety, environment friendliness, energy conservation, and sample integrity for specimen inactivation, as well as the consistency of inactivation outcomes. The advantages of water bath inactivation may be applicable to the inactivation of other pathogenic microorganisms. Our study supports the proposal of defining the heating device in standard protocols and guidelines for the thermal inactivation of specimens with a defined temperature and duration to ensure the biosafety and accuracy of diagnostics.

Data Availability

The datasets used and/or analyzed during the current study are available from the corresponding author on reasonable request.

Abbreviations

COVID-19:

Corona Virus Disease 2019

SARS-CoV-2:

Severe acute respiratory syndrome coronavirus 2

SARS-CoV:

Severe acute respiratory syndrome coronavirus

PCR:

Polymerase chain reaction

WHO:

World Health Organization

CDC:

USA Centers for Disease Control and Prevention, USA

TGEV:

Transmissible gastroenteritis virus of swine

IPEC-J2:

Porcine intestinal columnar epithelial cell line

TCID50:

50% tissue culture infective doses

Δ:

The difference in heights

K:

The heating rate

References

  1. Trépo C, Chan HL, Lok A. Hepatitis B virus infection. Lancet. 2014;384(9959):2053–63.

    Article  PubMed  Google Scholar 

  2. Chen SL, Zhao HR, Zhao CY, Zhang YQ, Li BJ, Bai GY, Liang L, Lu XL. Eighteen-year follow-up report of the surveillance and prevention of an HIV/AIDS outbreak amongst plasma donors in Hebei Province, China. BMC Infect Dis. 2015;15:316.

    Article  PubMed  PubMed Central  Google Scholar 

  3. Peng H, Bilal M, Iqbal H. Improved biosafety and biosecurity measures and/or strategies to tackle laboratory-acquired infections and related risks. Int J Environ Res Public Health. 2018;15(12):2697.

    Article  PubMed  PubMed Central  Google Scholar 

  4. Normile D. Infectious diseases. Mounting lab accidents raise SARS fears. Science. 2004;304(5671):659–61.

    Article  CAS  PubMed  Google Scholar 

  5. Kampf G, Todt D, Pfaender S, Steinmann E. Persistence of coronaviruses on inanimate surfaces and their inactivation with biocidal agents. J Hosp Infect. 2020;104(3):246–51.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  6. van Doremalen N, Bushmaker T, Morris DH, Holbrook MG, Gamble A, Williamson BN, Tamin A, Harcourt JL, Thornburg NJ, Gerber SI, Lloyd-Smith JO, de Wit E, Munster VJ. Aerosol and surface stability of SARS-CoV-2 as compared with SARS-CoV-1. N Engl J Med. 2020;382(16):1564–7.

    Article  PubMed  Google Scholar 

  7. WHO. Preparing to work with SARS-CoV-2: in supplement to WHO laboratory biosafety guidance related to coronavirus disease (COVID-19). 2021.

  8. WHO. Laboratory biosafety guidance related to coronavirus disease (COVID-19). 2020.

  9. Möller L, Schünadel L, Nitsche A, Schwebke I, Hanisch M, Laue M. Evaluation of virus inactivation by formaldehyde to enhance biosafety of diagnostic electron microscopy. Viruses. 2015;7(2):666–79.

    Article  PubMed  PubMed Central  Google Scholar 

  10. Gard S. Inactivation of poliovirus by formaldehyde theoretical and practical aspects. Bull Wld Hlth Org. 1957;17(6):979–89.

    CAS  Google Scholar 

  11. Patterson EI, Prince T, Anderson ER, Casas-Sanchez A, Smith SL, Cansado-Utrilla C, et al. Methods of inactivation of SARS-CoV-2 for downstream biological assays. J Infect Dis. 2020;222(9):1462–7.

    Article  CAS  PubMed  Google Scholar 

  12. Sagripanti JL, Hülseweh B, Grote G, Voss L, Böhling K, Marschall HJ. Microbial inactivation for safe and rapid diagnostics of infectious samples. Appl Environ Microbiol. 2011;77(20):7289–95.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  13. Ravanat JL, Douki D, Cadet J. Direct and indirect effects of UV radiation on DNA and its components. J Photochem Photobiol B. 2001;63(1–3):88–102.

    Article  CAS  PubMed  Google Scholar 

  14. Darnell ME, Taylor DR. Evaluation of inactivation methods for severe acute respiratory syndrome coronavirus in noncellular blood products. Transfusion. 2006;46(10):1770–7.

    Article  PubMed  PubMed Central  Google Scholar 

  15. Loveday EK, Hain KS, Kochetkova I, Hedges JF, Robison A, Snyder DT, et al. Effect of inactivation methods on SARS-CoV-2 virion protein and structure. Viruses. 2021;13(4):562.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  16. Lee YN, Chen LK, Ma HC, Yang HH, Li HP, Lo SY. Thermal aggregation of SARS-CoV membrane protein. J Virol Methods. 2005;129(2):152–61.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  17. Hemati M, Soosanabadi M, Ghorashi T, Ghaffari H, Vahedi A, Sabbaghian E, et al. Thermal inactivation of COVID-19 specimens improves RNA quality and quantity. J Cell Physiol. 2021;236(7):4966–72.

    Article  CAS  PubMed  Google Scholar 

  18. Hu X, Zhang R, An T, Li Q, Situ B, Ou Z, et al. Impact of heat-inactivation on the detection of SARS-CoV-2 IgM and IgG antibody by ELISA. Clin Chim Acta. 2020;509:288–92.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  19. Kampf G, Voss A, Scheithauer S. Inactivation of coronaviruses by heat. J Hosp Infect. 2020;105(2):348–9.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  20. Pan Y, Long L, Zhang D, Yuan T, Cui S, Yang P, Wang Q, Ren S. Potential false-negative nucleic acid testing results for severe Acute Respiratory Syndrome Coronavirus 2 from thermal inactivation of samples with low viral loads. Clin Chem. 2020;66(6):794–801.

    Article  PubMed  Google Scholar 

  21. Pastorino B, Touret F, Gilles M, de Lamballerie X, Charrel RN. Heat inactivation of different types of SARS-CoV-2 samples: what protocols for biosafety, molecular detection and serological diagnostics? Viruses. 2020;12(7):735.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  22. Batéjat C, Grassin Q, Manuguerra J-C, Leclercq I. Heat inactivation of the severe Acute Respiratory Syndrome Coronavirus 2. J Biosaf Biosecur. 2021;3(1):1–3.

    Article  PubMed  PubMed Central  Google Scholar 

  23. Leclercq I, Batéjat C, Burguière AM, Manuguerra JC. Heat inactivation of the Middle East respiratory syndrome coronavirus. Influenza Other Respir Viruses. 2014;8(5):585–6.

    Article  PubMed  PubMed Central  Google Scholar 

  24. Pastorino B, Touret F, Gilles M, de Lamballerie X, Charrel RN. Evaluation of heating and chemical protocols for inactivating SARS-CoV-2. bioRxiv preprint. 2020. https://doi.org/10.1101/2020.04.11.036855.

    Article  Google Scholar 

  25. Lin J, Dai W, Li W, Xiao L, Luo T, Guo Y, et al. Potential false-positive and false-negative results for COVID-19 IgG/IgM antibody testing after heat-inactivation. Front Med (Lausanne). 2021;7:589080.

    Article  PubMed  Google Scholar 

  26. Chen H, Wu R, Xing Y, Du Q, Xue Z, et al. Influence of different inactivation methods on severe acute respiratory syndrome coronavirus 2 RNA copy number. J Clin Microbiol. 2020;58(8):e00958–20.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  27. Wang S, Tang J, Cavalieri RP. Modeling fruit internal heating rates for hot air and hot water treatments. Postharvest Biol Tec. 2001;22:257–70.

    Article  CAS  Google Scholar 

  28. CDC(US). Biosafety in microbiological and biomedical laboratories(6th Edition). 2020;484–501.

  29. Neuman BW, Buchmeier MJ. Supramolecular architecture of the coronavirus particle. Adv Virus Res. 2016;96:1–27.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  30. Yao H, Song Y, Chen Y, Wu N, Xu J, Sun C, et al. Molecular architecture of the SARS-CoV-2 virus. Cell. 2020;183(3):730–8e13.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  31. Turoňová B, Sikora M, Schürmann C, Hagen WJ, Welsch S, Blanc FE, et al. In situ structural analysis of SARS-CoV-2 spike reveals flexibility mediated by three hinges. Science. 2020;370(6513):203–8.

    Article  PubMed  PubMed Central  Google Scholar 

  32. Casanova LM, Jeon S, Rutala WA, Weber DJ, Sobsey MD. Effects of air temperature and relative humidity on coronavirus survival on surfaces. Appl Environ Microbiol. 2010;76(9):2712–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  33. Tatzber F, Wonisch W, Balka G, Marosi A, Rusvai M, Resch U, et al. Coating with hypertonic saline improves virus protection of filtering facepiece manyfold-benefit of salt impregnation in times of pandemic. Int J Environ Res Public Health. 2021;18(14):7406.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  34. Hatanaka N, Yasugi M, Sato T, Mukamoto M, Yamasaki S. Hypochlorous acid solution is a potent antiviral agent against SARS-CoV‐2. J Appl Microbiol. 2022;132(2):1496–502.

    Article  CAS  PubMed  Google Scholar 

  35. Cantero M, Carlero D, Chichón FJ, Martín-Benito J, De Pablo PJ. Monitoring SARS-CoV-2 surrogate TGEV individual virions structure survival under harsh physicochemical environments. Cells. 2022;11(11):1759.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  36. Reed LJ, Muench H. A simple method of estimating 50% endpoints. Am J Hyg. 1938;27(20):493–7.

    Google Scholar 

  37. Hersberger M, Nusbaumer C, Scholer A, Knöpfli V, von Eckardstein A. Influence of practicable virus inactivation procedures on tests for frequently measured analytes in plasma. Clin Chem. 2004;50(5):944–6.

    Article  CAS  PubMed  Google Scholar 

  38. Laude H. Thermal inactivation studies of a coronavirus, transmissible gastroenteritis virus. J Gen Virol. 1981;56(Pt 2):235–40.

    Article  CAS  PubMed  Google Scholar 

  39. Esteban MD, Huertas JP, Fernández PS, Palop A. Effect of the medium characteristics and the heating and cooling rates on the nonisothermal heat resistance of Bacillus sporothermodurans IC4 spores. Food Microbiol. 2013;34(1):158–63.

    Article  PubMed  Google Scholar 

  40. Dewhirst M. Thermal dosimetry. In: Seegenscluniedt MH, Fessenden P, Vernon C, editors. Thermo-radiotherapy and thermochemotherapy. Berlin: Springer-Verlag; 1995. pp. 123–36.

    Chapter  Google Scholar 

  41. Gerner EW. Thermal dose and time-temperature factors for biological responses to heat shock. Int J Hyperthermia. 1987;3(4):319–27.

    Article  CAS  PubMed  Google Scholar 

  42. Herman TS, Gerner EW, Magun BE, Stickney D, Sweets CC, White DM. Rate of heating as a determinant of hyperthermic cytotoxicity. Cancer Res. 1981;41(9 Pt 1):3519–23.

    CAS  PubMed  Google Scholar 

  43. Dewhirst M, Gross JF, Sim D. Effects of heating rate on normal and tumor microcirculation. In: Diller K, Roemer R, editors. Heat and Mass transfer in the Microcirculation of Thermally Significant Vessels. New York: American Society of Mechanical Engineers; 1986. pp. 75–80.

    Google Scholar 

  44. Huertas JP, Aznar A, Esnoz A, Fernández PS, Iguaz A, Periago PM, Palop A. High heating rates affect greatly the inactivation rate of Escherichia coli. Front Microbiol. 2016;7:1256.

    Article  PubMed  PubMed Central  Google Scholar 

  45. Conesa R, Andreu S, Fernández PS, Esnoz A, Palop A. Nonisothermal heat resistance determinations with the thermoresistometer Mastia. J Appl Microbiol. 2009;107(2):506–13.

    Article  CAS  PubMed  Google Scholar 

  46. Wang XW, Li JS, Jin M, Zhen B, Kong QX, Song N, et al. Study on the resistance of severe acute respiratory syndrome-associated coronavirus. J Virol Methods. 2005;126(1–2):171–7.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  47. Ward RL, Knowlton DR, Winston PE. Mechanism of inactivation of enteric viruses in fresh water. Appl Environ Microbiol. 1986;53(3):450–9.

    Article  Google Scholar 

  48. Rabenau HF, Cinatl J, Morgenstern B, Bauer G, Preiser W, Doerr HW. Stability and inactivation of SARS coronavirus. Med Microbiol Immunol. 2005;194(1–2):1–6.

    Article  CAS  PubMed  Google Scholar 

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Acknowledgements

We thank Dr. Zhiwen Xu, Sichuan Agricultural University, China, for kindly providing Transmissible gastroenteritis virus (TGEV) and porcine intestinal columnar epithelial cell line (IPEC-J2).

Funding

This study was supported by West China Hospital (HX-2019-nCoV-17), Sichuan Science and Technology Program (2020YFS0008; 2020YFQ0022), and National Natural Science Foundation (81671551).

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Authors and Affiliations

  1. Laboratory of Infectious Diseases and Vaccine, West China School of Medicine, West China Hospital, Sichuan University, 88 Keyuan S. Rd, Chengdu, 610041, China

    Xinxia Gu, Ting Cao, Jun Mou & Jie Liu

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  1. Xinxia Gu
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  2. Ting Cao
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  3. Jun Mou
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  4. Jie Liu
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Contributions

XG performed the experiments, analyzed and interpreted data, wrote the manuscript draft. TC & JM analyzed and interpreted data, provided assistance in the procurement and resources. JL designed the study, wrote and edited the manuscript, supervised the experiment, acquired the funding source.

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Correspondence to Jie Liu.

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Gu, X., Cao, T., Mou, J. et al. Water bath is more efficient than hot air oven at thermal inactivation of coronavirus. Virol J 20, 84 (2023). https://doi.org/10.1186/s12985-023-02038-7

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Virology Journal

ISSN: 1743-422X