Secondary Logo

Share this article on:

Part I

Minimum Quality Threshold in Preclinical Sepsis Studies (MQTiPSS) for Study Design and Humane Modeling Endpoints

Zingarelli, Basilia*; Coopersmith, Craig M.; Drechsler, Susanne; Efron, Philip§; Marshall, John C.; Moldawer, Lyle§; Wiersinga, W. Joost||; Xiao, Xianzhong**; Osuchowski, Marcin F.; Thiemermann, Christoph††

doi: 10.1097/SHK.0000000000001243
Review Articles
Editor's Choice

ABSTRACT Preclinical animal studies are mandatory before new treatments can be tested in clinical trials. However, their use in developing new therapies for sepsis has been controversial because of limitations of the models and inconsistencies with the clinical conditions. In consideration of the revised definition for clinical sepsis and septic shock (Sepsis-3), a Wiggers-Bernard Conference was held in Vienna in May 2017 to propose standardized guidelines on preclinical sepsis modeling. The participants conducted a literature review of 260 most highly cited scientific articles on sepsis models published between 2003 and 2012. The review showed, for example, that mice were used in 79% and euthanasia criteria were defined in 9% of the studies. Part I of this report details the recommendations for study design and humane modeling endpoints that should be addressed in sepsis models. The first recommendation is that survival follow-up should reflect the clinical time course of the infectious agent used in the sepsis model. Furthermore, it is recommended that therapeutic interventions should be initiated after the septic insult replicating clinical care. To define an unbiased and reproducible association between a new treatment and outcome, a randomization and blinding of treatments as well as inclusion of all methodological details in scientific publications is essential. In all preclinical sepsis studies, the high standards of animal welfare must be implemented. Therefore, development and validation of specific criteria for monitoring pain and distress, and euthanasia of septic animals, as well as the use of analgesics are recommended. A set of four considerations is also proposed to enhance translation potential of sepsis models. Relevant biological variables and comorbidities should be included in the study design and sepsis modeling should be extended to mammalian species other than rodents. In addition, the need for source control (in case of a defined infection focus) should be considered. These recommendations and considerations are proposed as “best practices” for animal models of sepsis that should be implemented.

*Department of Pediatrics, Division of Critical Care Medicine, Cincinnati Children's Hospital Medical Center, College of Medicine, University of Cincinnati, Cincinnati, Ohio

Emory University School of Medicine, Atlanta, Georgia

Ludwig Boltzmann Institute for Experimental and Clinical Traumatology in the AUVA Research Center, Vienna, Austria

§Sepsis and Critical Illness Research Center, University of Florida College of Medicine, Gainesville, Florida

Keenan Research Centre for Biomedical Science, St. Michael's Hospital, University of Toronto, Toronto, Canada

||Division of Infectious Diseases, Center for Experimental and Molecular Medicine, The Academic Medical Center, University of Amsterdam, Amsterdam, The Netherlands

**Xiangya School of Medicine, Central South University, Chagnsha, Hunan, China

††The William Harvey Research Institute, Barts and London School of Medicine & Dentistry, Queen Mary University of London, London, United Kingdom

Address reprint requests to Basilia Zingarelli, MD, PhD, Department of Pediatrics, Division of Critical Care Medicine, Cincinnati Children's Hospital Medical Center, Cincinnati, OH. E-mail: Basilia.Zingarelli@cchmc.org; Co-correspondence: Christoph Thiemermann, MD, PhD, The William Harvey Research Institute, Barts and London School of Medicine & Dentistry, Queen Mary University of London, London, United Kingdom. E-mail: c.thiemermann@qmul.ac.uk

Received 20 April, 2018

Revised 16 May, 2018

Accepted 26 July, 2018

The Austrian Science Fund T707-B13 (SD, MFO); The William Harvey Research Foundation (CT); NWO VIDI (no.: 91716475) and Horizon 2020: MC-ITN “European Sepsis Academy” (WJW); National Institutes of Health R01 GM067202 and GM115973 (BZ); The National Institute of General Medical Sciences GM072808, GM104323, GM109779, and GM113228 (CMC).

The authors report no conflicts of interest.

Back to Top | Article Outline

INTRODUCTION

Sepsis is defined as life-threatening organ dysfunction caused by a dysregulated host response to infection (1). It is the most important cause of morbidity and mortality in patients admitted to intensive care units (ICU) with a significant cost impact in health care worldwide (2). Over the last decade, basic science research has identified fundamental molecular processes involved in the pathophysiology of the dysregulated metabolic, inflammatory, and immune responses. Despite this knowledge growth, investments in drug development and multiple clinical trials, no new effective therapies have been introduced to clinical practice. The treatment of the patient still relies on supportive care and antimicrobial agents (3). Although we cannot underestimate inherent issues within clinical trials (4, 5), there is increasing skepticism about the usefulness of animal models for predicting responses in clinical sepsis (6). One prominent reason of the inability of industry- and government-sponsored clinical trials to validate results from the majority of animal studies should be attributed to methodological challenges in preclinical study design that poorly correlates with the clinical condition of sepsis.

An initiative to develop guidance on how to improve the quality and efficiency of preclinical studies was undertaken by the international Wiggers-Bernard Conference, held in May 2017 in Vienna. As the basis for the conference discussions, participants conducted a literature review of the 260 most highly cited scientific articles on sepsis models published between 2003 and 2012. The objective of the conference was to identify limitations of preclinical sepsis models and to propose a set of guidelines, defined as the “Minimum Quality Threshold in Pre-Clinical Sepsis Studies” (MQTiPSS; 7), to enhance translational relevance of the models. Concrete examples specifically related to experimental design, procedures, and ethical endpoints are provided throughout the guidelines presented in this paper. It is expected that these guidelines will be used in conjunction with the more general and mandatory rules of a national legislation of a country in which research is conducted. It is important to note that these recommendations and considerations are proposed to assist in the design of the most appropriate animal sepsis model(s) and should be tailored to the specific hypothesis of the investigation.

Overall, the Wiggers-Bernard initiative has generated three joint publications (8, 9) to serve as an MQTiPSS guideline for establishing the basic conditions in modeling of sepsis to improve their translational relevance. The current part I paper makes specific recommendations for preclinical models of sepsis within the areas of study design and humane modeling endpoints. The goal of the conference was to create quality thresholds for future studies so that findings in those two particular areas are more clinically applicable and the studies themselves are better comparable across laboratories and/or species.

Back to Top | Article Outline

METHODS

The Wiggers-Bernard Conferences on Shock, Sepsis and Organ Failure is an expert opinion exchange platform for international scientists organized by the Ludwig Boltzmann Institute of Experimental and Clinical Traumatology in the AUVA Research Center (LBI Trauma), Vienna, Austria (http://trauma.lbg.ac.at/en). The conference series was named after two outstanding scientists, one from the “New World” (Dr. Carl Wiggers) and one from the “Old World” (Dr. Claude Bernard) who devoted their careers to critical care medicine and experimental sciences. LBI Trauma is responsible for the topic selection, whereas the Austrian Society of Advancement of Research in Shock and Tissue Engineering provides sponsorship for each Wiggers-Bernard Conference.

To address the deficits regarding management guidelines and standardization in the field of preclinical sepsis research, in May 2017 LBI Trauma organized the 9th iteration of the Wiggers-Bernard Conferences titled “Pre-clinical Modeling in Sepsis: Exchanging Opinions and Forming Recommendations.” The key goal of the conference was to identify and publish essential elements that should be included in preclinical sepsis studies and defined by the MQTiPSS descriptor (10). A total of 31 experts from 12 countries, including 5 members of the Sepsis-3 definitions task force (1), were invited to participate in the initiative based on their experience in experimental, clinical, and translational research.

The initiative consisted of three phases: 3-month preparatory phase where participants performed a systematic review of the 260 top cited publications from 2003 to 2012 and identified the key modeling topics to be discussed; discussions in Vienna (2 days), during which the participants drafted a list of guidelines; and postconference refinement of the created works.

The preparatory phase review was conducted using ISI Web of Knowledge database (using the query: “sepsis model”). The 260 most cited papers (the citation range 50–743; referenced over 29,000 times in aggregate) featuring a total of 374 animal studies were identified. The time frame was subjectively defined as 10 consecutive years beginning with 2003 as the year of publication of the second iteration of sepsis definitions (11). The results of that survey pertinent to the topics covered in this paper are collated in Tables 1 and 3. As the first analysis showed that mice were used in 79% of the 2003 to 2012 papers, a secondary smaller search was performed and included all 2013 to 2017 studies (total of 190; irrespective of the number of citations) with mouse sepsis models only (using the query: “sepsis AND mice”); to compare to selected endpoints reviewed in the main review that spanned 2003 to 2012. Both analyses were used during the meeting. Overall, the preparatory phase aimed at identification of the most important concepts in animal sepsis modeling to be addressed at the Viennese Wiggers-Bernard Conference. All participants were allocated into six specific thematic Working Groups (WGs): Study Design, Humane Modeling, Infection Type, Organ Failure/Dysfunction, Fluid Resuscitation, and Antimicrobial Therapy Endpoints.

Table 1

Table 1

During the conference phase, each WG separately drafted a set of guideline points that were subsequently subjected to general discussion and streamlined either for further refinement in WGs or dismissal (day 1). After improvements, the proposed points were subjected to voting by all participants to reach consensus (day 2). Overall, the Wiggers-Bernard Conference participants reached consensus on 29 points; 20 at “recommendation” strength and 9 at “consideration” strength (the WG-1/2 points are listed in Tables 2 and 4). Following the format used by the Sepsis-3 task force (12), at least 2/3 (over 65%) of the votes were required for approval of a proposed point. All consensus points were reached either unanimously or with no more than two abstentions per point (i.e., Recommendation 8). The “recommendation” strength indicates virtually unanimous agreement among the 31 participants, regarding both the content and the need for rapid implementation. Issues that require additional discussion (in the opinion of the participants) before final recommendations could be made were classified as considerations.

Table 2

Table 2

Table 3

Table 3

Table 4

Table 4

During the postconference phase, the arguments to be included in the final MQTiPSS publications were finalized through teleconferences and electronic-based discussion among WGs using a modified Delphi method. Finally, a writing committee (formed at the conference) together with all participants developed an Executive Summary for MQTiPSS (7) and three full-size publications (8, 9). Each (of the three) publication focuses on two related WGs; the current part I paper provides detailed discussion on the guideline points for Study Design and Humane Modeling Endpoints.

Back to Top | Article Outline

CHAPTER 1: STUDY DESIGN

An ideal preclinical animal model should accurately reproduce the human disease. Although the complexity of human sepsis and its phenotypes precludes creation of a single ideal model, a standardization of defined model systems appears feasible and should be considered (13). We are convinced that adequately designed animal models of sepsis and other diseases can be useful tools, including the discovery and development of new therapeutic interventions (14). Therefore, it is important to elucidate the criteria, which must be fulfilled to obtain meaningful animal-to-human translation.

The premeeting review of the animal studies provided evidence of bias and numerous methodological limitations of animal research in sepsis. In Table 1, we identified several challenges in the study design, experimental conduct, and reporting that can impede successful translation of the findings from animal research to patients. For example, although survival was reported as a primary endpoint in 43% of the animal sepsis studies, the majority of experiments had a brief follow-up. Given the frequent late mortality and long-term sequelae in septic patients (15), such a brief monitoring in many preclinical studies is not justified by the prolonged course of clinical sepsis. Another shortcoming is the mismatch of therapeutic interventions between animal studies and septic patients. Only in 36% of the animal studies the experimental therapy was given after the onset of sepsis. In most cases, the timing of those interventions was chosen subjectively and not dictated by symptoms and/or disease severity. Of concern is also a low inclusion of biological variables and comorbidities in the study design; only 5% of the reviewed studies featured any type of comorbidity. Although the choice of healthy, inbred animals of same sex, age, and weight limits the baseline variability in preclinical models, it simultaneously prohibits replication of the heterogeneity encountered in the patient population. Promising preclinical findings obtained in those simplistic models should be validated in more complex experiments that take into consideration modifying risk factors of morbidity and lethality.

The above study design shortcomings are additionally aggravated by insufficient reporting of the methodological details. In the reviewed top-cited papers, we identified several inadequacies in describing details on animals, methods, and materials used in the experiments—all of which can potentially confound the interpretation of the study results and impede experimental reproducibility. Inadequate reporting also prohibits verification whether proper tools for reducing bias were used, i.e., randomization for group allocation and blinding of outcome assessment. Scientific rigor demands that scientific reports provide accurate and sufficient details on the methodology to enable replication of the findings by other investigators to prove their validity (16). For a successful translatability of animal models, it is paramount that rigor is observed in preclinical sepsis research.

Back to Top | Article Outline

Specific recommendations for study design

The conference discussed several specific recommendations for preclinical models of sepsis. In the current part I paper, the recommendations and considerations from the Study Design Endpoints working group are numbered consecutively beginning with recommendation 1 and continue in the next chapter (Humane Modeling Endpoints) and the two subsequent companion papers (Part II and III).

Back to Top | Article Outline

Recommendation 1: survival follow-up should reasonably reflect the clinical time course of the sepsis model

Although animal models will never fully recapitulate human illness, it is paramount to adapt them to reflect the changing nature of the studied disease. Historically, animal sepsis models used a relatively high mortality rate (17), which reflected the high lethality of multiple organ failure (MOF) (18). As a result of multiple international initiatives to improve the implementation of evidence-based medicine in the ICU, the epidemiology of sepsis has evolved: early in-hospital mortality has decreased and many high-acuity patients survive, generating a new patient phenotype of “chronic critical illness” (CCI) (19). For example, recent prospective longitudinal cohort studies of sepsis/septic shock revealed that early inpatient mortality from refractory shock and MOF is now below 5% (20, 21). Other studies have demonstrated that the initial 28-day sepsis mortality is approximately 20%, but this increases to nearly 35% at 6 months (15). In addition, the long-term CCI morbidity can be dismal—after 6 months, a significant portion of these patients have poor function and cognition and are discharged to nonhospital inpatient facilities rather than home (15, 20, 21). Of the latter, mortality is almost 40% at 6 months (20, 21).

The clinical need for a long-term focus is poorly met by typical short-term animal sepsis studies. For example, only 10% of the studies we reviewed used monitoring exceeding 14 days (Table 1). Thus, we recommend that the survival follow-up should reasonably reflect the clinical time course of the infectious agent used in the model or the patient population being studied. For example, a shorter monitoring period for meningitis would be appropriate given the acute clinical course of the human disease (22). There are appropriate abdominal, urinary, and pulmonary models with high early mortalities that can study important aspects of the early mammalian response to severe infection (17). However, if the research goal is to replicate the clinical trajectory of most sepsis patients in developed nations, a longer monitoring period is more appropriate as acute mortality with sepsis is becoming rare. Researchers need to develop models of persistent chronic immunodysregulated conditions after sepsis, as this is now the predominant human phenotype (23–25). Although rarely performed, due to complexity and costs, modeling of chronic sepsis that features persistent immunoinflammatory deficits and late mortality is achievable (26, 27). As further discussed in part III companion paper (9), fluid resuscitation, antibiotics, and management of source control (see also Consideration c) are important interventions to mimic the current clinical therapy and are necessary to prevent early high mortality rates. Such a modeling shift, however, requires a concurrent development of humane endpoints appropriately tailored for that type of animal sepsis research (see Chapter 2).

It is still unclear what the equivalent number of hours or days in a mouse/rat are when compared with human time points, as there is a temporal mismatch between the species (17). For example, 1 h in mice/rats is equivalent to approximately 40 h in humans (assuming the lifespan of 2 vs. 80 years). However, the 1 h vs. 40 h recalculation formula should not be used reflexively as acute response between rodents and man bear many temporal similarities. For example, intravenous lipopolysaccharide (LPS) stimulation in human volunteers (28, 29), mice (30), rats (31), and pigs (32) leads to a virtually identical time-based response in the acute release of circulating inflammatory cytokines. Although some researchers have determined certain equations to relate different species (i.e., mouse with man) (33, 34), variations persist when considering weaning, puberty, and senescence (33, 35). In addition, there are other differences in the timing and magnitude of the sepsis response in both species (17). Therefore, researchers may never be able to definitely state, one week after cecal ligation and puncture (CLP) in a mouse is the same as one month for a septic human in the ICU.” However, it is unlikely that a murine model with 80% to 100% mortality in the first 48 to 72 h accurately represents the biology of patients who become CCI, or subsequently develop the Persistent Inflammation Immunosuppression Catabolism Syndrome (20, 21).

Back to Top | Article Outline

Recommendation 2: therapeutic interventions should be initiated after the septic insult replicating clinical care.

To mimic the clinical scenario, it is instrumental to administer any therapeutic agent to be tested after the induction of sepsis. Animal models have been utilized for the initial testing of potentially effective therapies for decades, but one can conclude that there is a large inconsistency between animal and human trials (36, 37). The application of pretreatment instead of posttreatment has been an important shortcoming in numerous studies that has hindered the extrapolation of animal data to patients (36, 37). Although the onset of experimental sepsis is known in animal models, patients never present at “time zero” and their infection develops for a significant time before clinical identification. Furthermore, it should be emphasized that sepsis itself will have a profound impact on the metabolic, cardiovascular, immunological, and other responses in an animal model (23–25, 36). These, in turn, can have considerable impact on the therapeutic intervention that is evaluated. In this respect, it is essential to extrapolate treatment-related findings from the specific models toward the specific clinical scenario they attempt to recapitulate (e.g., CLP representing polymicrobial peritonitis).

There are some points of contention concerning this recommendation. There are many examples of pharmacological agents, which have been positively evaluated in an animal sepsis model using a proper posttreatment approach, but which yielded negative results in large human clinical trials (38). Well-documented examples include the use of recombinant tissue factor pathway inhibitor (tifacogin) (39, 40), anti-Toll like receptor (TLR)-4 strategies (41–43), and interleukin-1 receptor blockade (44, 45). Also, the issue of posttreatment is not simply time, but more the evolution of organ dysfunction and the processes that could result in death. Compared with patients, these trajectories can be divergent in animal models. Thus, a therapeutic intervention should not be solely based on the vector of time but should also account for the phenotype of the sepsis pathophysiology at the time of the intervention.

This further emphasizes the point that this specific recommendation is just part of the presented broader set of recommendations aiming to better mimic the clinical scenario and enhancing the translational power of the sepsis model used. In fact, it would not be entirely surprising if the abovementioned treatment strategies will eventually be demonstrated to work in more precisely defined subsets of septic patients (36, 46). In addition, it should be acknowledged that—depending on the objective of any particular study—pretreatment can be reasonable, e.g., in multihit models simulating secondary infections or as prophylaxis. Also, pretreatment is valuable if the goal is to understand disease pathogenesis rather than to predict treatment efficacy. These points, however, should be explicitly defined in the methods.

In summary, from a clinical translation standpoint, when testing novel therapies, treatments should mimic the clinical management of the patients, i.e., given after the onset of sepsis. Efficacy of experimental drugs should be compared with or used in addition to minimum standard care of sepsis, i.e., fluid resuscitation and antibiotics (outlined in part III paper; 9).

Back to Top | Article Outline

Recommendation 3: we recommend that the treatment be randomized and blinded when feasible

Methodological shortcomings in animal experimentation introduce bias and may distort study conclusions. Systematic analyses of preclinical studies demonstrate shortcomings in randomization and blinding. For example, in 2009, the National Centre for the Replacement, Refinement and Reduction of Animals in Research (NC3Rs) reported that only 12% of studies performed randomization and 14% used blinding (out of 271 surveyed studies) (47) and similar deficiencies were reported by others (48, 49). Although we did not determine randomization/blinding in our review of preclinical sepsis studies, others reported difficulty in appraising the risk of bias secondary to lack of randomization, allocation concealment, and blinding (50). In the critical care field, Ramirez et al. (49) demonstrated presence of randomization only in 22% and blinding in 33% of examined cardiovascular model studies. It cannot be excluded, however, that some of those studies used randomization/blinding without disclosing it. Interestingly, the lowest use of randomization (17%) was reported in mouse-based experiments (49)—the species whose size enables repetitive high-power testing.

Lack of proper randomization and blinding in critical care studies may overestimate treatment benefits both in human trials (51) and animal models (52). An analysis of abstracts presented at the annual emergency medicine meetings revealed that nonrandomized and/or unblinded studies were more likely to report positive outcomes (odds ratio 5.2; 95% confidence interval, 2.0–13.5) (53). Failure to randomize and/or blind were key factors behind the inability to reproduce landmark preclinical findings in anticancer, cardiovascular, and amyloid lateral sclerosis therapies (54, 55). Some constraints in blinding are unavoidable and should be recognized in some study types, e.g., when testing new devices.

Promising animal treatment studies often constitute a launching platform for human testing. Thus, to eliminate dissemination of misleading data, the methodological rigor of randomization and blinding must be applied in preclinical experiments, whenever study design allows that. As an ultimate goal, to strengthen the translation bridge between bench and bedside, the preclinical testing should approach the quality of clinical trials. The recent multicenter preclinical randomized controlled trial verifying efficacy of anti-CD49d treatment against stroke (56) demonstrates that this is feasible and could be adapted for sepsis research.

Back to Top | Article Outline

Recommendation 4: provide as much information as possible (e.g., ARRIVE guidelines) on the model and methodology, to enable reproducibility

Although experimental reproducibility is key in evidence-based science (16), preclinical studies are burdened by methodological underreporting with estimates for irreproducibility ranging from 75% to 90% (57). Holman et al. (58) showed that underreporting precluded identification of animal attrition in over 60% of articles in stroke and cancer. Publication analysis of three high-impact critical care journals revealed poor methodological reporting of study design and ethical intervention in animal studies (59, 60). Poor transparency impedes replication and cross-comparison of animal studies including sepsis. The NIH has recently launched a training initiative to address this problem (www.nih.gov/research-training/rigor-reproducibility).

Our recommendation may appear redundant in view of various existing guidelines promoting transparency reporting, e.g., Animals in Research: Reporting In Vivo Experiments (ARRIVE) (61), journal checklists (e.g., EMBO Press Checklist) (62), and Transparency Openness Promotion (TOP; https://cos.io/top) initiative by Nature. Compliance to these guidelines is key for reproducibility. Unfortunately, using the ARRIVE example, the recent analysis of preclinical studies demonstrated their low compliance with the ARRIVE and poor improvement in reporting quality (63, 64). The underlying reasons are mixed: disinclination/neglect of the authors to provide complete methodology, space limitations by the journals, and lax enforcement at the peer-review process and publication. It is possible that guidelines specifically tailored to individual research areas and endorsed by their professional bodies will have more impact and enable better enforcement. Sepsis research should follow the existing examples: the American Heart Association released recommendations on design, execution, and reporting of animal studies in atherosclerosis (65) and the Stroke journal has recently issued a second checklist edition for experimental stroke models (66). The latter example demonstrates a success of such a focused approach: reporting standards improved in animal studies submitted to Stroke after implementation of the first checklist (67). Implementation of best reporting practices should also include full disclosure of the originally posited study objective(s) to communicate the rationale behind the experimental design. Use of the journal supplementary section to provide a detailed methodological description should be encouraged. This absence of detail is not trivial; despite widely endorsed CONSORT guidelines (www.consort-statement.org), analysis of 67 clinical trials by COMpare Trial Project identified severe discrepancies between final clinical trial reports and their entry protocols (e.g., 357 unplanned outcomes added, 354 planned outcomes not reported) (68). The preclinical field is much less controlled for such inconsistencies and more efforts should be made to improve the reporting practices. The high-quality reporting standards will not be achieved without strong enforcement mechanisms.

Back to Top | Article Outline

Consideration (a): consider replication of the findings in models that include comorbidity and or other biological variables (i.e., age, sex, diabetes, cancer, immunosuppression, genetic background, and others)

Advanced age, chronic obstructive disease, cancer, chronic renal disease, chronic liver disease, diabetes, and immunosuppression constitute known risk factors in sepsis (69) and influence the degree of infection/injury as compared with the same insults in healthy young adults (69–75). Although young mice are valid for specific types of basic science sepsis research, the results of such works are limited in their ability to be directly translated to septic humans (4, 17). In preclinical studies, the use of healthy inbred animals of the same sex, age, and weight is frequent as it limits baseline variability (17). However, human patients are “outbred,” have variable ages, sex and weight, individual comorbidities, and have different causes of sepsis. All of these will affect the host response and influence the morbidity and mortality of the septic patient. Host genetic factors are also relevant to the variability in sepsis susceptibility and outcomes (69).

Sepsis pathophysiology is extremely complex (25, 36, 76, 77). Although there is value in studying the mammalian response to severe infection in standardized rodent models, researchers should consider repeating their work in modified animal models that more closely recapitulate the human condition/variability before directly translating their findings to patients (17, 36). We encourage development of a large family of sepsis models that represent options in which sepsis phenotypes may present and fluctuate, for example, validating the work in a model that features a modifying risk of morbidity and lethality (e.g., aging, sex, diabetes, cancer, immunosuppression, genetic background). This also includes two-hit models in which sepsis is modified by a defined critical care condition (e.g., trauma) and/or secondary infection (78–80). For sepsis, age constitutes one of the key modifiers given the demographic characteristic of septic patients (typically >65 years old) and associated age-related comorbidities (81). Our review of preclinical sepsis studies reported that less than 1% of experiments used appropriately aged animals (82). Regarding biological variables, outbred mice feature an immune system that is more comparable to humans, providing a tool to improve the translatability of sepsis research to human patients (83). Furthermore, nonrodent sepsis models in species whose biology is more similar to humans can be conducted to determine how applicable rodent work is to human biology (17). Based on our current understanding of sepsis pathophysiology, failure to properly integrate the abovementioned factors into experimental designs of animal studies likely limits the translational potential of the preclinical results.

Back to Top | Article Outline

Consideration (b): in addition to rodents (mice and rats), consider modeling sepsis also in other (mammal) species

Due to the varied nature of sepsis, it is unlikely that models that involve one species will be able to mimic all aspects of the clinical and biological complexity of the disease that are encountered in humans (36). Therefore, the authors believe researchers should consider modeling sepsis in other mammalian species in addition to rodents. This consideration does not intend to immediately compel investigators into performing repetitions of their studies across multiple species, especially if studies in rodents are well validated and government agencies (e.g., United States Food and Drug Administration [FDA] and European Medicine Agency [EMA]) do not require such a step. However, as for most basic science research, it is important to note that rodents are by far the most commonly used species for modeling sepsis (84). The reasons for robust use of mice and rats include high fecundity; accelerated life cycle; low maintenance; well-characterized genome; inbred, outbred, and transgenic strains; widespread availability as well as reagents used to study them; and the creation of “humanized” mice (17). Our literature review (Table 1) shows that 79% of the sepsis studies used mice and 94% used rodents. However, we need to consider that rodent models have several significant inherent limitations (84, 85). For example, mice have a higher resistance to the systemic inflammatory response associated with infection (17); due to the high resilience of mice against infections, 10E7–9 Escherichia coli or Staphylococcus aureus are needed to affect mice; this would correspond to 3.5 × 10E12 bacteria in humans (86, 87). In this context, a rabbit model may be more appropriate for S. aureus-induced sepsis (88). Another example is the blunted response of mice to bacterial products, such LPS—the lethal dose in mice is approximately 1,000 times greater than the estimated lethal dose in humans (17). Other differences between humans and mice also need to be taken into consideration. The composition of murine leukocytes in whole blood is dissimilar to that of adult humans, for both innate and adaptive immunity (17).

Thus, a mouse does not necessarily represent the complex systemic background of the septic response in humans and narrow (i.e., in a single species) preclinical testing of given phenomena could mask numerous effects (17). Given these concerns, validation of preclinical sepsis findings in more than one single species can enhance its translational potential. This can include rabbit, porcine, bovine, and nonhuman primate models (84, 89). Furthermore, other species may be more appropriate in specific sepsis models due to their physiology and pathophysiology being more similar to humans. It should be noted, though, that to date these animals have also not been successful in the clinical application of biological response modifiers in humans (17). Finally, cost and the absolute necessity for the humane treatment of these research animals can limit what can be conducted by individual laboratories (17). However, those issues should not preclude attempted advancement or optimization of animal sepsis research modeling.

Back to Top | Article Outline

Consideration (c): consider need for source control

“Ubi pus, ibi evacua”; when there is a collection of pus in the body causing sepsis the evacuation of it is the most important aspect of its management. The Surviving Sepsis Campaign guidelines recommend that source control should be implemented as soon as medically and logistically practical after the diagnosis is made (3). Consequently, prompt removal of intravascular access devices that are a potential source of sepsis is recommended after other vascular access has been established (3). In humans, source control within 6 to 12 h after diagnosis seems to be sufficient in most cases (3, 90, 91). The sepsis guidelines mention the following foci of infection readily amenable to source control: intra-abdominal abscesses, gastrointestinal perforation, ischemic bowel, cholangitis, cholecystitis, pyelonephritis associated with obstruction or abscess, necrotizing soft tissue infection, other deep space infection (e.g., empyema or septic arthritis), and implanted device infections (3). How do these insights translate to the design of a preclinical model of sepsis?

Most literature on this subject is derived from the CLP model. The ligated and punctured cecum can be excised at various intervals to serve as a source control model of sepsis (92). Source control measurements in that model have been associated with resolution of the inflammatory process (93). Nonetheless, it should be acknowledged that source control adds complexity to the model which could interfere with other endpoint parameters. In addition, the timing of excision and drainage is of importance. An early excision for source control can be associated with no mortality, whereas delayed intervention can lead to increased mortality or no effect on the clinical course. Finally, many septic patients die with an unidentified but existing focus of infection (94), thus a retained abscess in an animal model (e.g., after CLP) recapitulates a realistic no-source-control clinical scenario. In summary, the committee recommends researchers to consider the use of source control in an animal model of sepsis, when appropriate, to be consistent with the management of human sepsis.

Back to Top | Article Outline

CHAPTER 2: HUMANE MODELING

Our desire to establish humane endpoints relates to our aim to promote good care and welfare practices in preclinical sepsis experimentation worldwide. The current rules for experimental animal welfare in sepsis studies differ among countries, although these differences are declining as more United States and international organizations are voluntarily seeking accreditation by Association for the Assessment and Accreditation of Laboratory Animal Care International (AAALAC). Furthermore, many journals go beyond local ethics committee approval and adhere to animal welfare recommendations promulgated by the Guide for the Care and Use of Laboratory Animals (8th edition), published by the National Research Council (USA) (95). Given that animal sepsis models display a relative high burden of suffering, precise monitoring, effective analgesic control, and death-as-an-endpoint are frequently discussed. This paper aims to instigate a long-term process that eventually leads to an optimal standardization of humane practices in animal sepsis modeling. For example, the emphasis should be on improving the ability to detect indicators of sepsis-related morbidity and mortality, and on challenging assumptions that mortality as an endpoint is “inevitable,” yet retaining compatibility with human sepsis studies, which continue to rely on the death endpoint and include patients with comorbidities. Numerous humane endpoints can be refined and perceptions about the ability to predict impending death are constantly changing due to technological improvements (e.g., biomarker screening from small blood samples, noninvasive microchip monitoring of vitals).

Humane endpoints in sepsis are best used in conjunction with prospective planning for their use (i.e., not ad hoc to address welfare concerns as they arise). In designing an experiment, the researcher should clearly specify the expected experimental outcome (and efficacy endpoints for drug intervention studies), adequately justify the needs for a given outcome to prove the hypothesis, and precisely delineate all tools used for eliminating/reducing animal suffering. Our review of the 260 preclinical sepsis studies demonstrates that the welfare-related elements are typically not reported (Table 3). For example, in over 90% of the reviewed studies no euthanasia criteria were defined/mentioned, whereas in less than 10% of the studies the use of analgesia was disclosed. Specific criteria that will allow recognition of when the experimental outcomes have been met should be identified when planning the study and noninvasive techniques including imaging, behavioral, or physiological monitoring (e.g., via biotelemetry) can be useful in reaching this goal. It must also be recognized that it is not always necessary for an animal sepsis model to share all features of the human sepsis pathophysiology. It may be sufficient that the animal model recapitulates one specific but relevant element of the human disease (e.g., cardiac dysfunction, acute lung, kidney injury). Overall, development of uniform and justifiable humane endpoint guidelines for preclinical sepsis experiments would aid in facilitating approval for necessary and clinically translatable studies with professional regulators as well as public opinion concerned with the ethical use of animals in research.

Back to Top | Article Outline

Specific recommendations for Humane Modeling

The conference discussed several specific recommendations for preclinical models of sepsis to advance the use of these models. The following recommendations and considerations from the Humane Modeling Endpoints working group are numbered consecutively from the preceding chapter and start with recommendation 5.

Back to Top | Article Outline

Recommendation 5: The development and validation of standardized criteria to monitor the well-being of septic animals is recommended

A laboratory animal should be able to exercise natural behavior without experiencing distress. Such an environment can be provided for rodents and rabbits (96, 97), but not as easily for large mammals (98) and nonhuman primates (99). Majority of experimental procedures impair the animal well-being, but sepsis studies produce a significant degree of suffering. To classify the magnitude of the impact on well-being, development and validation of monitoring criteria for septic animals is necessary (100, 101). The selected well-being criteria need to be frequently monitored and should encompass animal behavior as well as clinical examination (100, 102). Few scientific publications propose specific evaluation protocols (103, 104); they focus on the assessment of the sepsis severity rather than the animal welfare itself. For example, a mouse clinical assessment score for sepsis (M-CASS) allows staging the severity of pneumonia (103) by evaluating several clinical and behavioral parameters. Our literature search failed to reveal any standardized scores for the monitoring of animal well-being and/or sepsis progress in large mammals.

Modern technology can enhance the noninvasive monitoring capability in animal experimentation. Implantable biotelemetry devices are used for monitoring physiology and, in sepsis, disease severity (e.g., heart rate, body temperature, mobility) in mice (105–107). Recently, Lewis et al. (108) demonstrated a large-scale utility of biotelemetry monitoring for fluid resuscitation and antimicrobial treatment in CLP mice. In vivo wireless monitoring of cardiovascular endpoints has been successfully tested in pigs (109), dogs, and nonhuman primates (110). Continuous body temperature monitoring using noninvasive infrared light is another alternative (111). However, disadvantages exist: biotelemetry devices are relatively expensive, require a surgical intervention, which may alter the response to the sepsis insult, and might necessitate specific housing (112). Alternative monitoring techniques such as echocardiography (113), blood pressure, and heart rate assessments (114) are also possible, but require expertise and additional procedures for the animals, such as anesthesia and restraint.

Initial well-being assessment criteria can be simple; it is important to first instigate a positive reception for such practices and create a framework that enables its quality standardization and further technical development. As the first step, we recommend focusing on systematic recordings of behavioral changes (e.g., food intake, vocalization, mobility, social interactions) and clinical symptoms (e.g., body weight, respiratory, and temperature changes) (103, 104, 115). Preclinical laboratories already use many of these endpoints and their arrangement into a standardized well-being protocol should not be arduous. The next step will require adjustments of the evaluation criteria to meet the “welfare demands” of more complex sepsis models (e.g., comorbidity, two-hit models of secondary infections, chronic sepsis). Comorbidities typically alter both behavior and clinical parameters, e.g., an overweight diabetic mouse is less active compared to a healthy mouse (116) and weight gain in a chronically septic mouse is a sign of recovery, not deterioration as in acute sepsis (117). A routine use of standardized well-being scores in septic animals has the advantage to mimic the bedside monitoring of the septic patient and can serve as additional efficacy or adverse effect variable to complement nonmortality secondary endpoints such as assessment of organ dysfunction. Thus, monitoring of well-being scores can be tailored to the respective sepsis model to account for variations in pathophysiologic responses secondary to changes in environment, strain, sex, and comorbidities.

Back to Top | Article Outline

Recommendation 6: The development and validation of standardized criteria for euthanasia of septic animals is recommended (exceptions possible)

Current legislation for animal experimentation in the United States (95), Japan (118) China (119), and European Union (EU) (120) allows but discourages inclusion of death as an endpoint. Some EU countries (e.g., the United Kingdom) and individual research institutions (e.g., Vlaams Instituut for Biotechnologie, Belgium) have voluntarily implemented ban on using death as endpoint. In critical care animal and human studies, death remains a frequently used parameter; its replacement with surrogates is not always justified and may be misleading. The key concern is that “preemptive” euthanasia (i.e., dictated by the ban) or euthanasia based on commonly used humane endpoints is either uninformative or the outcome assumptions can be imprecise. For example, Nemzek et al. (121) demonstrated that only 56% of CLP mice with a body temperature below 30°C died. Thus, liberal euthanasia cutoffs in preclinical sepsis can distort data subsequently impairing translatability of animal findings to patients (115, 121). In addition, predictive imprecision of surrogate endpoints may preclude identification of unexpected life-saving effects by some therapies. Currently, many investigators assume their favorite surrogate endpoint, such as reduction of organ dysfunction predicts an increase in survival; such an approach should not be followed until a given surrogate marker has been validated to precisely predict death or long-term survival.

The above controversies underline the need for developing precise and standardized criteria for euthanasia in sepsis research (122) to ensure an acceptable combination of experimental design quality and ethical practices. Development of defined cutoff(s) for euthanasia in septic animals is inherently linked with R-5 given that the animals must first deteriorate (i.e. decreased well-being) to the moribund state (defined by R-6). The two R-5 and R-6 recommendations should be viewed as a continuous monitoring paradigm transitioning from a set of behavioral/clinical descriptors (R-5) in nonlethal sepsis to a precise decision-making tool (R-6) for euthanasia in animals approaching the moribund state. Thus, the key welfare issue predominantly arises from the distress preceding the moribund state; it is currently unclear to what extent (if at all) unresponsive and/or comatose animals experience pain (122). Euthanasia of animals that reach “a dying state” eliminates spontaneous deaths but does not eliminate their distress experienced during progression to that state (123, 124). In the ethical context, endpoints identifying moribund animals can never be considered humane enough (115); they constitute a trade-off between a need for investigative confidence and relief from unnecessary suffering. A tight synchronization/use of both R-5 and -6 should enhance the latter without jeopardizing the former. A reliable R-5 (well-being) score will automatically strengthen the informational quality and precision of R-6. This, in turn, will potentially facilitate identification and implementation of the irreversible “dying state” cutoffs at earlier stage(s) of sepsis.

In the technical context, the existing criteria for euthanasia in septic rodents (103, 104, 121) and pigs (124) are typically based on changes in behavior, body weight and temperature; telemetric devices can further refine the above approach (105, 109, 110). Blood biomarker measurements are another alternative as outcome predictor in septic mice (125, 126). Compared with the clinically based criteria, biomarkers are advantageous as relatively early predictors of mortality, thus preventing the deterioration of animals to the moribund state. However, they require repeated blood sampling (127), which produce distress (128). In addition, current biomarker-based assays are not completely precise (126, 129), are technically challenging and preclude the monitoring of late sepsis.

Several elements require consideration for creation of effective preclinical euthanasia criteria. First, noninvasive clinical and behavioral descriptors (as discussed in R-5) appear to be a good starting platform. Recent works in mice provide several candidates for defining the moribund state (121) and demonstrate how their combinations can be effectively applied for ‘euthanasia decision-making’ (103, 104). For example, body temperature changes are indicative of sepsis severity (130, 131) and are an independent predictor of outcome (132, 133). In large septic mammals, the blood glucose monitoring was reported as useful outcome predictor (134). Second, disease-specific parameters should be integrated into the euthanasia criteria depending on the type of the sepsis model used (e.g., severe dyspnea, respiratory alterations in pneumosepsis) (103, 104). Finally, the chosen euthanasia criteria have to be validated before use in each laboratory separately, for every sepsis model, species/strains, age, and sex. Strong interlaboratory and animal variability precludes automatic adaptation of euthanasia protocols across research laboratories.

Back to Top | Article Outline

Recommendation 7: Analgesics recommended for surgical sepsis should be consistent with ethical considerations

A principle of animal welfare is that any procedure expected to cause pain in humans is considered likely to cause pain in animals and should be alleviated through appropriate care and pain management (e.g., analgesia). Regardless of international regulatory differences, surgical sepsis is always rated as causing the most severe grade of distress, assuming the animal recovers consciousness after surgery.

The use of pre- and/or postoperative pain medicine is rarely reported in preclinical sepsis studies (115, 135). In our Wiggers-Bernard review, analgesics were used in 30 experiments, not used in 19 and not reported in 329 experiments, despite CLP being the leading sepsis model. This is consistent with a recent report where only 15% of the analyzed publications used analgesics in experimental sepsis (60). Although some (or many) of the manuscripts not reporting actually used analgesics, it is likely that many studies did not use analgesics in surgical sepsis. There are two possibilities for why investigators have historically withheld analgesia in surgical sepsis—the belief that animals cannot feel pain and/or do not feel pain based upon lack of signs such as vocalization, and the concern that analgesics would alter critical endpoints. The first supposition is incorrect; mice and rats demonstrate pain via changes in facial expression (136) and they also have subtle behavioral changes following surgery (137). This can be alleviated by analgesics, and trained personnel can distinguish rodents that received postsurgical pain medicine compared to those that did not. However, mice do not typically have a vocal response to a painful procedure, and mice may vocalize at frequencies above the range of human hearing (138).

The second often-quoted reason for withholding analgesia is that analgesics cause alterations in the inflammatory response and coagulation (139–141). It is important to acknowledge that different analgesics have different side effects, which may limit the utility of some classes of drugs in sepsis research. For instance, nonsteroidal anti-inflammatory drugs are associated with anti-inflammatory effects via inhibition of prostaglandins and may also be associated with renal impairment and bleeding (142). Similarly, mu-agonists such as morphine have immune-modulating effects and can cause respiratory depression (143). However, opioids that act as kappa-receptor agonists and mu-receptor antagonists have been demonstrated to be safe and effective without causing significant immunomodulation. Specifically, numerous studies have demonstrated the efficacy/safety of buprenorphine and tramadol (144, 145). Although buprenorphine adversely may impact mortality in male (but not female) septic mice, this can be prevented by dose reduction (146). Furthermore, buprenorphine treatment results in minimal differences in inflammatory parameters although neutrophil counts are transiently decreased in male mice (146). In addition, continuous infusion of nalbuphine, another opioid agonist/antagonist, has been used in rodent models of CLP and fecal slurry (147, 148).

Importantly, although analgesics can alter the inflammatory profile, pain, in and of itself, may also affect disease outcome and experimental variability (115). Thus, from both an ethical and experimental standpoint, the use of analgesics should be standard and reported in surgical sepsis models. Exceptions—if they exist—should be rare, should be experimentally demonstrated, and cannot be justified by the catch-all phrase that “analgesics alter the host response.”

Back to Top | Article Outline

Consideration (d): Consider analgesics for nonsurgical sepsis

The data are less clear for animals in which sepsis is induced via a nonsurgical approach. Sepsis clearly causes encephalopathy in patients. Many septic patients in the ICU appear to be in pain, although it is difficult to separate the impact of the underlying disease from interventions meant to support septic patients (mechanical ventilation, pressor support via large bore invasive catheters). Guidelines for the management of critically ill patients state that “adult medical, surgical and trauma ICU patients routinely experience pain, both at rest and with routine ICU care” and recommend intravenous opioids as the first-line drug class of choice to treat nonneuropathic pain in critically ill patients (not specific to sepsis) (149). In the absence of clear data suggesting the degree to which laboratory animals with sepsis from a nonsurgical source experience pain, investigators should weigh the benefits of analgesia versus the potential side effects of analgesia. Implementation of rigorous pain-oriented monitoring of septic rodents (and larger species) subjected to nonsurgical sepsis protocols may likely provide the necessary evidence regarding the absence/presence of pain as well as its potential magnitude. It is possible that the emerging evidence will support a uniform implementation of analgesics in all septic models regardless of the experimental origin of sepsis.

Back to Top | Article Outline

SUMMARY

This Part I manuscript details the recommendations and considerations of the two working groups from the Wiggers-Bernard conference. Analysis of the top-cited preclinical sepsis papers showed substantial shortcomings regarding both the use and reporting on the study design and humane modeling elements. Due to multiple inconsistencies with the clinical conditions, inadequate modeling protocols are at least partly responsible for failures in developing effective therapies for septic patients. Given the disease burden, the highest standards of animal welfare must be implemented in all preclinical sepsis studies. The two working groups made specific recommendations about the rigors of study design and adequate humane modeling of sepsis in animals. We hope that these recommendations and considerations will serve to bring a level of standardization to preclinical models of sepsis and ultimately improve the translation of preclinical findings. We acknowledge that new challenges based on new information from the clinical and bench studies will continue to arise. A close collaborative work between basic scientists and clinicians is critical for a thoughtful (re)interpretation of any existing and newly posited principles.

Back to Top | Article Outline

Acknowledgments

The Part I paper was created by two Working Groups: Study Design (B. Zingarelli head; PE, LM, MFO, and WJW participants) and Humane Modeling Endpoints (C. Thiemermann head; CC, SD, JM, and XX participants). In addition, MFO served as coordinator of the 9th Wiggers-Bernard initiative.

Back to Top | Article Outline

REFERENCES

1. Singer M, Deutschman CS, Seymour CW, Shankar-Hari M, Annane D, Bauer M, Bellomo R, Bernard GR, Chiche JD, Coopersmith CM, et al. The Third International Consensus Definitions for Sepsis and Septic Shock (Sepsis-3). JAMA 2016; 315:801–810.
2. Vincent JL. Increasing awareness of sepsis: World Sepsis Day. Crit Care 2012; 1:152.
3. Rhodes A, Evans LE, Alhazzani W, Levy MM, Antonelli M, Ferrer R, Kumar A, Sevransky JE, Sprung CL, Nunnally ME, et al. Surviving Sepsis Campaign: International Guidelines for Management of Sepsis and Septic Shock: 2016. Crit Care Med 2017; 45:486–552.
4. Opal SM, Dellinger RP, Vincent JL, Masur H, Angus DC. The next generation of sepsis clinical trial designs: what is next after the demise of recombinant human activated protein C? Crit Care Med 2014; 42:1714–1721.
5. Prescott HC, Calfee CS, Thompson BT, Angus DC, Liu VX. Toward smarter lumping and smarter splitting: rethinking strategies for sepsis and acute respiratory distress syndrome clinical trial design. Am J Respir Crit Care Med 2016; 194:147–155.
6. Seok J, Warren HS, Cuenca AG, Mindrinos MN, Baker HV, Xu W, Richards DR, McDonald-Smith GP, Gao H, Hennessy L, et al. Inflammation and Host Response to Injury, Large Scale Collaborative Research Program. Genomic responses in mouse models poorly mimic human inflammatory diseases. Proc Natl Acad Sci USA 2013; 110:3507–3512.
7. Osuchowski MF, Ayala A, Bahrami S, Bauer M, Boros M, Cavaillon JM, Chaudry I, Coopersmith CM, Deutschmann C, Drechsler S, et al. Minimum Quality Threshold in Pre-Clinical Sepsis Studies (MQTiPSS): An International Expert Consensus initiative for Improvement of Animal Modeling in Sepsis. Shock 2018; 50:377–380.
8. Libert C, Ayala A, Bauer M, Cavaillon JM, Deutschmann C, Frostell C, Kozlov AV, Wang P, Osuchowski MF, Remick DG. Part II: Minimum Quality Threshold in Pre-Clinical Sepsis Studies (MQTiPSS) for Types of Infections and Organ Dysfunction Endpoints. Shock 2019; 51:23–32.
9. Hellman J, Bahrami S, Boros M, Chaudry I, Fritsch G, Gozdzik W, Inoue S, Radermacher P, Singer M, Osuchowski MF, et al. Part III: Minimum Quality Threshold in Pre-Clinical Sepsis Studies (MQTiPSS) for fluid resuscitation and antimicrobial therapy endpoints. Shock 2019; 51:33–43.
10. Osuchowski MF, Thiemermann C, Remick DG. Sepsis-3 on the block: what does it mean for preclinical sepsis modeling? Shock 2017; 47:658–660.
11. Levy MM, Fink MP, Marshall JC, Abraham E, Angus D, Cook D, Cohen J, Opal SM, Vincent JL, Ramsay G. SCCM/ESICM/ACCP/ATS/SIS: 2001 SCCM/ESICM/ACCP/ATS/SIS International Sepsis Definitions Conference. Crit Care Med 2003; 31:1250–1256.
12. Shankar-Hari M, Phillips GS, Levy ML, Seymour CW, Liu VX, Deutschman CS, Angus DC, Rubenfeld GD, Singer M. Sepsis Definitions Task Force: Developing a New Definition and Assessing New Clinical Criteria for Septic Shock: For the Third International Consensus Definitions for Sepsis and Septic Shock (Sepsis-3). JAMA 2016; 315:775–787.
13. Remick DG, Ayala A, Chaudry I, Coopersmith CM, Deutschman C, Hellman J, Moldawer L, Osuchowski MF. Premise for standardized sepsis models. Shock 2019; 51:4–9.
14. Coen D. Oxford TB vaccine study calls into question selective use of animal data. BMJ 2018; 360:j5845.
15. Yende S, Austin S, Rhodes A, Finfer S, Opal S, Thompson T, Bozza FA, LaRosa SP, Ranieri VM, Angus DC. Long-term quality of life among survivors of severe sepsis: analyses of two international trials. Crit Care Med 2016; 44:1461–1467.
16. Baker M. 1,500 scientists lift the lid on reproducibility. Nature 2016; 533:452–454.
17. Stortz JA, Raymond SL, Mira JC, Moldawer LL, Mohr AM, Efron PA. murine models of sepsis and trauma: can we bridge the gap? ILAR J 2017; 58:90–105.
18. Moore FA, Moore EE. Evolving concepts in the pathogenesis of postinjury multiple organ failure. Surg Clin North Am 1995; 75:257–277.
19. Sauaia A, Moore EE, Johnson JL, Chin TL, Banerjee A, Sperry JL, Maier RV, Burlew CC. Temporal trends of postinjury multiple-organ failure: still resource intensive, morbid, and lethal. J Trauma Acute Care Surg 2014; 76:582–592.
20. Stortz JA, Murphy TJ, Raymond SL, Mira JC, Ungaro R, Dirain ML, Nacionales DC, Loftus TJ, Wang Z, Ozrazgat-Baslanti T, et al. Evidence for persistent immune suppression in patients who develop chronic critical illness after sepsis. Shock 2018; 49:249–258.
21. Stortz JA, Mira JC, Raymond SL, Loftus TJ, Ozrazgat-Baslanti T, Wang Z, Ghita GL, Leeuwenburgh C, Segal MS, Bihorac A, et al. Benchmarking clinical outcomes and the immunocatabolic phenotype of chronic critical illness after sepsis in surgical intensive care unit patients. J Trauma Acute Care Surg 2018; 84:342–349.
22. Mook-Kanamori B, Geldhoff M, Troost D, van der Poll T, van de Beek D. Characterization of a pneumococcal meningitis mouse model. BMC Infect Dis 2012; 8 12:71.
23. Venet F, Monneret G. Advances in the understanding and treatment of sepsis-induced immunosuppression. Nat Rev Nephrol 2018; 14:121–137. 28.
24. Hotchkiss RS, Karl IE. The pathophysiology and treatment of sepsis. N Engl J Med 2003; 348:138–150.
25. Hotchkiss RS, Monneret G, Payen D. Sepsis-induced immunosuppression: from cellular dysfunctions to immunotherapy. Nat Rev Immunol 2013; 13:862–874.
26. Osuchowski MF, Craciun F, Weixelbaumer KM, Duffy ER, Remick DG. Sepsis chronically in MARS: systemic cytokine responses are always mixed regardless of the outcome, magnitude, or phase of sepsis. J Immunol 2012; 189:4648–4656.
27. Pugh AM, Auteri NJ, Goetzman HS, Caldwell CC, Nomellini V. A murine model of persistent inflammation. Immune suppression, and catabolism syndrome. Int J Mol Sci 2017; 18 8:E1741.
28. Branger J, van den Blink B, Weijer S, Madwed J, Bos CL, Gupta A, Yong CL, Polmar SH, Olszyna DP, Hack CE, et al. Anti-inflammatory effects of a p38 mitogen-activated protein kinase inhibitor during human endotoxemia. J Immunol 2002; 168:4070–4077.
29. Ramakers BP, Riksen NP, van den Broek P, Franke B, Peters WH, van der Hoeven JG, Smits P, Pickkers P. Circulating adenosine increases during human experimental endotoxemia but blockade of its receptor does not influence the immune response and subsequent organ injury. Crit Care 2011; 15:R3.
30. Remick DG, Newcomb DE, Bolgos GL, Call DR. Comparison of the mortality and inflammatory response of two models of sepsis: lipopolysaccharide vs. cecal ligation and puncture. Shock 2000; 13:110–116.
31. Liu D, Zeng BX, Shang Y. Decreased expression of peroxisome proliferator-activated receptor gamma in endotoxin-induced acute lung injury. Physiol Res 2006; 55:291–299.
32. Nielsen JS, Larsson A, Rix T, Nyboe R, Gjedsted J, Krog J, Ledet T, Tønnesen E. The effect of activated protein C on plasma cytokine levels in a porcine model of acute endotoxemia. Intensive Care Med 2007; 33:1085–1093.
33. Dutta S, Sengupta P. Men and mice: relating their ages. Life Sci 2016; 152:244–248.
34. Turnbull IR, Wlzorek JJ, Osborne D, Hotchkiss RS, Coopersmith CM, Buchman TG. Effects of age on mortality and antibiotic efficacy in cecal ligation and puncture. Shock 2003; 19:310–313.
35. Miller RA, Nadon NL. Principles of animal use for gerontological research. J Gerontol A Biol Sci Med Sci 2000; 55:B117–B123.
36. Iskander KN, Osuchowski MF, Stearns-Kurosawa DJ, Kurosawa S, Stepien D, Valentine C, Remick DG. Sepsis: multiple abnormalities, heterogeneous responses, and evolving understanding. Physiol Rev 2013; 93:1247–1288.
37. Angus DC. The search for effective therapy for sepsis: back to the drawing board? JAMA 2011; 306:2614–2615.
38. Fink MP, Warren HS. Strategies to improve drug development for sepsis. Nat Rev Drug Discov 2014; 13:741–758.
39. Opal SM, Palardy JE, Parejo NA, Creasey AA. The activity of tissue factor pathway inhibitor in experimental models of superantigen-induced shock and polymicrobial intra-abdominal sepsis. Crit Care Med 2001; 29:13–17.
40. Abraham E, Reinhart K, Opal S, Demeyer I, Doig C, Rodriguez AL, Beale R, Svoboda P, Laterre PF, Simon S, et al. OPTIMIST Trial Study Group: efficacy and safety of tifacogin (recombinant tissue factor pathway inhibitor) in severe sepsis: a randomized controlled trial. JAMA 2003; 290:238–247.
41. Takashima K, Matsunaga N, Yoshimatsu M, Hazeki K, Kaisho T, Uekata M, Hazeki O, Akira S, Iizawa Y, Ii M. Analysis of binding site for the novel small-molecule TLR4 signal transduction inhibitor TAK-242 and its therapeutic effect on mouse sepsis model. Br J Pharmacol 2009; 157:1250–1262.
42. Rice TW, Wheeler AP, Bernard GR, Vincent JL, Angus DC, Aikawa N, Demeyer I, Sainati S, Amlot N, Cao C, et al. A randomized, double-blind, placebo-controlled trial of TAK-242 for the treatment of severe sepsis. Crit Care Med 2010; 38:1685–1694.
43. Opal SM, Laterre PF, Francois B, LaRosa SP, Angus DC, Mira JP, Wittebole X, Dugernier T, Perrotin D, Tidswell M, et al. ACCESS Study Group: Effect of eritoran, an antagonist of MD2-TLR4, on mortality in patients with severe sepsis: the ACCESS randomized trial. JAMA 2013; 309:1154–1162.
44. Alexander HR, Doherty GM, Buresh CM, Venzon DJ, Norton JA. A recombinant human receptor antagonist to interleukin 1 improves survival after lethal endotoxemia in mice. J Exp Med 1991; 173:1029–1032.
45. Opal SM, Fisher CJ Jr, Dhainaut JF, Vincent JL, Brase R, Lowry SF, Sadoff JC, Slotman GJ, Levy H, Balk RA, et al. Confirmatory interleukin-1 receptor antagonist trial in severe sepsis: a phase III, randomized, double-blind, placebo-controlled, multicenter trial. The Interleukin-1 Receptor Antagonist Sepsis Investigator Group. Crit Care Med 1997; 25:1115–1124.
46. Shakoory B, Carcillo JA, Chatham WW, Amdur RL, Zhao H, Dinarello CA, Cron RQ, Opal SM. Interleukin-1 receptor blockade is associated with reduced mortality in sepsis patients with features of macrophage activation syndrome: reanalysis of a prior phase III trial. Crit Care Med 2016; 44:275–281.
47. Kilkenny C, Parsons N, Kadyszewski E, Festing MF, Cuthill IC, Fry D, Hutton J, Altman DG. Survey of the quality of experimental design, statistical analysis and reporting of research using animals. PLoS One 2009; 4:e7824.
48. Hirst JA, Howick J, Aronson JK, Roberts N, Perera R, Koshiaris C, Heneghan C. The need for randomization in animal trials: an overview of systematic reviews. PLoS One 2014; 9:e98856.
49. Ramirez FD, Motazedian P, Jung RG, Di Santo P, MacDonald ZD, Moreland R, Simard T, Clancy AA, Russo JJ, Welch VA, et al. Methodological rigor in preclinical cardiovascular studies: targets to enhance reproducibility and promote research translation. Circ Res 2017; 120:1916–1926.
50. Lamontagne F, Briel M, Duffett M, Fox-Robichaud A, Cook DJ, Guyatt G, Lesur O, Meade MO. Systematic review of reviews including animal studies addressing therapeutic interventions for sepsis. Crit Care Med 2010; 38:2401–2408.
51. Odgaard-Jensen J, Vist GE, Timmer A, Kunz R, Akl EA, Schünemann H, Briel M, Nordmann AJ, Pregno S, Oxman AD. Randomisation to protect against selection bias in healthcare trials. Cochrane Database Syst Rev 2011; 4:MR000012.
52. Macleod MR, Lawson McLean A, Kyriakopoulou A, Serghiou S, de Wilde A, Sherratt N, Hirst T, Hemblade R, Bahor Z, Nunes-Fonseca C, et al. Risk of bias in reports of in vivo research: a focus for improvement. PLoS Biol 2015; 13:e1002273.
53. Bebarta V, Luyten D, Heard K. Emergency medicine animal research: does use of randomization and blinding affect the results? Acad Emerg Med 2003; 10:684–687.
54. Begley CG, Ellis LM. Drug development: Raise standards for preclinical cancer research. Nature 2012; 483:531–533.
55. Perrin S. Preclinical research: make mouse studies work. Nature 2014; 507:423–425.
56. Llovera G, Hofmann K, Roth S, Salas-Pérdomo A, Ferrer-Ferrer M, Perego C, Zanier ER, Mamrak U, Rex A, Party H, et al. Results of a preclinical randomized controlled multicenter trial (pRCT): anti-CD49d treatment for acute brain ischemia. Sci Transl Med 2015; 7:299ra121.
57. Begley CG, Ioannidis JP. Reproducibility in science: improving the standard for basic and preclinical research. Circ Res 2015; 116:116–126.
58. Holman C, Piper SK, Grittner U, Diamantaras AA, Kimmelman J, Siegerink B, Dirnagl U. Where have all the rodents gone? The effects of attrition in experimental research on cancer and stroke. PLoS Biol 2016; 14:e1002331.
59. Bara M, Joffe AR. The methodological quality of animal research in critical care: the public face of science. Ann Intensive Care 2014; 4:26.
60. Bara M, Joffe AR. The ethical dimension in published animal research in critical care: the public face of science. Crit Care 2014; 18:R15.
61. Kilkenny C, Browne WJ, Cuthill IC, Emerson M, Altman DG. Improving bioscience research reporting: the ARRIVE guidelines for reporting animal research. PLoS Biol 2010; 8:e1000412.
62. Pulverer B. Transparent, reproducible data. EMBO J 2014; 33:2597.
63. Enserink M. Sloppy reporting on animal studies proves hard to change. Science 2017; 357:1337–1338.
64. Baker D, Lidster K, Sottomayor A, Amor S. Two years later: journals are not yet enforcing the ARRIVE guidelines on reporting standards for pre-clinical animal studies. PLoS Biol 2014; 12:e1001756.
65. Daugherty A, Tall AR, Daemen MJAP, Falk E, Fisher EA, García-Cardeña G, Lusis AJ, Owens AP 3rd, Rosenfeld ME, Virmani R. American Heart Association Council on Arteriosclerosis; Thrombosis and Vascular Biology; and Council on Basic Cardiovascular SciencesRecommendation on design, execution, and reporting of animal atherosclerosis studies: a scientific statement from the American Heart Association. Circ Res 2017; 121:e53–e79.
66. Vahidy F, Schäbitz WR, Fisher M, Aronowski J. Reporting standards for preclinical studies of stroke therapy. Stroke 2016; 47:2435–2438.
67. Minnerup J, Zentsch V, Schmidt A, Fisher M, Schäbitz WR. Methodological quality of experimental stroke studies published in the Stroke Journal: Time trends and effect of the basic science checklist. Stroke 2016; 47:267–272.
68. Goldacre B, Drysdale H, Powell-Smith A, Dale A, Milosevic I, Slade E, Hartley P, Marston C, Mahtani K, Heneghan C: The COMPare Trials Project. Available at: www.COMPare-trials.org, 2016.
69. Mayr FB, Yende S, Angus DC. Epidemiology of severe sepsis. Virulence 2014; 5:4–11.
70. Nacionales DC, Gentile LF, Vanzant E, Lopez MC, Cuenca A, Cuenca AG, Ungaro R, Li Y, Baslanti TO, Bihorac A, et al. Aged mice are unable to mount an effective myeloid response to sepsis. J Immunol 2014; 192:612–622.
71. Inata Y, Kikuchi S, Samraj RS, Hake PW, O’Connor M, Ledford JR, O’Connor J, Lahni P, Wolfe V, Piraino G, et al. Autophagy and mitochondrial biogenesis impairment contribute to age-dependent liver injury in experimental sepsis: dysregulation of AMP-activated protein kinase pathway. FASEB J 2018; 32:728–741.
72. Fox AC, Robertson CM, Belt B, Clark AT, Chang KC, Leathersich AM, Dominguez JA, Perrone EE, Dunne WM, Hotchkiss RS, et al. Cancer causes increased mortality and is associated with altered apoptosis in murine sepsis. Crit Care Med 2010; 38:886–893.
73. Inoue S, Nakamura H, Otake K, Saito H, Terashita K, Sato J, Takeda H, Tomoike H. Impaired pulmonary inflammatory responses are a prominent feature of streptococcal pneumonia in mice with experimental emphysema. Am J Respir Crit Care Med 2003; 167:764–770.
74. Koh GC, Peacock SJ, van der Poll T, Wiersinga WJ. The impact of diabetes on the pathogenesis of sepsis. Eur J Clin Microbiol Infect Dis 2012; 31:379–388.
75. Drechsler S, Weixelbaumer K, Raeven P, Jafarmadar M, Khadem A, van Griensven M, Bahrami S, Osuchowski MF. Relationship between age/gender-induced survival changes and the magnitude of inflammatory activation and organ dysfunction in post-traumatic sepsis. PLoS One 2012; 7:e51457.
76. Hotchkiss RS, Moldawer LL, Opal SM, Reinhart K, Turnbull IR, Vincent JL. Sepsis and septic shock. Nat Rev Dis Primers 2016; 2:16045.
77. Angus DC, van der Poll T. Severe sepsis and septic shock. N Engl J Med 2013; 369:840–851.
78. Al-Chalabi A, Matevossian E, von Thaden A, Schreiber C, Radermacher P, Huber W, Perez Ruiz de Garibay A, Kreymann B. Evaluation of an ADVanced Organ Support (ADVOS) system in a two-hit porcine model of liver failure plus endotoxemia. Intensive Care Med Exp 2017; 5:31.
79. Suzuki T, Shimizu T, Szalay L, Choudhry MA, Rue LW 3rd, Bland KI, Chaudry IH. Androstenediol ameliorates alterations in immune cells cytokine production capacity in a two-hit model of trauma-hemorrhage and sepsis. Cytokine 2006; 34:76–84.
80. Drechsler S, Weixelbaumer KM, Redl H, van Griensven M, Bahrami S, Osuchowski MF. Experimentally approaching the ICU: monitoring outcome-based responses in the two-hit mouse model of posttraumatic sepsis. J Biomed Biotechnol 2011; 2011:357926.
81. Milbrandt EB, Eldadah B, Nayfield S, Hadley E, Angus DC. Toward an integrated research agenda for critical illness in aging. Am J Respir Crit Care Med 2010; 182:995–1003.
82. Starr ME, Saito H. Sepsis in old age: review of human and animal studies. Aging Dis 2014; 5:126–136.
83. Beura LK, Hamilton SE, Bi K, Schenkel JM, Odumade OA, Casey KA, Thompson EA, Fraser KA, Rosato PC, Filali-Mouhim A, et al. Normalizing the environment recapitulates adult human immune traits in laboratory mice. Nature 2016; 532:512–516.
84. Osuchowski MF, Remick DG, Lederer JA, Lang CH, Aasen AO, Aibiki M, Azevedo LC, Bahrami S, Boros M, Cooney R, et al. Abandon the mouse research ship? Not just yet!. Shock 2014; 41:463–475.
85. Masopust D, Sivula CP, Jameson SC. Of mice, dirty mice, and men: using mice to understand human immunology. J Immunol 2017; 199:383–388.
86. Blanchet C, Jouvion G, Fitting C, Cavaillon JM, Adib-Conquy M. Protective or deleterious role of scavenger receptors SR-A and CD36 on host resistance to Staphylococcus aureus depends on the site of infection. PLoS One 2014; 9:e87927.
87. Chiang N, Fredman G, Bäckhed F, Oh SF, Vickery T, Schmidt BA, Serhan CN. Infection regulates pro-resolving mediators that lower antibiotic requirements. Nature 2012; 484:524–528.
88. Reizner W, Hunter JG, O’Malley NT, Southgate RD, Schwarz EM, Kates SL. A systematic review of animal models for Staphylococcus aureus osteomyelitis. Eur Cell Mater 2014; 27:196–212.
89. Reisz JA, Wither MJ, Moore EE, Slaughter AL, Moore HB, Ghasabyan A, Chandler J, Schaub LJ, Fragoso M, Nunns G, et al. All animals are equal but some animals are more equal than others: plasma lactate and succinate in hemorrhagic shock—a comparison in rodents, swine, nonhuman primates, and injured patients. J Trauma Acute Care Surg 2018; 84:537–541.
90. Azuhata T, Kinoshita K, Kawano D, Komatsu T, Sakurai A, Chiba Y, Tanjho K. Time from admission to initiation of surgery for source control is a critical determinant of survival in patients with gastrointestinal perforation with associated septic shock. Crit Care 2014; 18:R87.
91. Bloos F, Thomas-Rüddel D, Rüddel H, Engel C, Schwarzkopf D, Marshall JC, Harbarth S, Simon P, Riessen R, Keh D, et al. MEDUSA Study Group,Impact of compliance with infection management guidelines on outcome in patients with severe sepsis: a prospective observational multi-center study. Crit Care 2014; 18:R42.
92. Ping W, Chaudry IH. Schein M, Marshall JC. Experimental models of source control. Springer, Source Control. Berlin, Heidelberg: 2003.
93. Nakagawa NK, Jukemura J, Aikawa P, Nogueira RA, Poli-de-Figueiredo LF, Sannomiya P. In vivo observation of mesenteric leukocyte-endothelial interactions after cecal ligation/puncture and surgical sepsis source control. Clinics (Sao Paulo) 2007; 62:321–326.
94. Torgersen C, Moser P, Luckner G, Mayr V, Jochberger S, Hasibeder WR, Dünser MW. Macroscopic postmortem findings in 235 surgical intensive care patients with sepsis. Anesth Analg 2009; 108:1841–1847.
95. National Research CouncilGuide for the Care and Use of Laboratory Animals. 8th ed.Washington, DC: The National Academies Press; 2011.
96. Gaskill BN, Karas AZ, Garner JP, Pritchett-Corning KR. Nest building as an indicator of health and welfare in laboratory mice. J Vis Exp 2013; 82:51012.
97. Baumans V. Environmental enrichment for laboratory rodents and rabbits: requirements of rodents, rabbits, and research. ILAR J 2005; 46:162–170.
98. Swindle MM, Makin A, Herron AJ, Clubb FJ Jr, Frazier KS. Swine as models in biomedical research and toxicology testing. Vet Pathol 2012; 49:344–356.
99. Tardif SD, Coleman K, Hobbs TR, Lutz C. IACUC review of nonhuman primate research. ILAR J 2013; 54:234–245.
100. Hawkins P, Morton DB, Burman O, Dennison N, Honess P, Jennings M, Lane S, Middleton V, Roughan JV, Wells S, et al. UK Joint Working Group on Refinement BVAAWF/FRAME/RSPCA/UFAWA guide to defining and implementing protocols for the welfare assessment of laboratory animals: eleventh report of the BVAAWF/FRAME/RSPCA/UFAW Joint Working Group on Refinement. Lab Anim 2011; 45:1–13.
101. Nemzek JA, Hugunin KM, Opp MR. Modeling sepsis in the laboratory: merging sound science with animal well-being. Comp Med 2008; 58:120–128.
102. Burkholder T, Foltz C, Karlsson E, Linton CG, Smith JM. Health evaluation of experimental laboratory mice. Curr Protoc Mouse Biol 2012; 2:145–165.
103. Huet O, Ramsey D, Miljavec S, Jenney A, Aubron C, Aprico A, Stefanovic N, Balkau B, Head GA, de Haan JB, et al. Ensuring animal welfare while meeting scientific aims using a murine pneumonia model of septic shock. Shock 2013; 39:488–494.
104. Shrum B, Anantha RV, Xu SX, Donnelly M, Haeryfar SMM, McCormick JK, Mele T. A robust scoring system to evaluate sepsis severity in an animal model. BMC Res Notes 2014; 7:233.
105. Lewis A, Zuckerbraun B, Griepentrog J, Zhang X, Rosengart M. Reducing animal use with a biotelemetry-enhanced murine model of sepsis. Sci Rep 2017; 7:6622.
106. Lewis AJ, Yuan D, Zhang X, Angus DC, Rosengart MR, Seymour CW. Use of biotelemetry to define physiology-based deterioration thresholds in a murine cecal ligation and puncture model of sepsis. Crit Care Med 2016; 44:e420–e431.
107. Osuchowski MF, Craciun FL, Schuller E, Sima C, Gyurko R, Remick DG. Untreated type 1 diabetes increases sepsis-induced mortality without inducing a prelethal cytokine response. Shock 2010; 34:369–376.
108. Lewis AJ, Griepentrog JE, Zhang X, Angus DC, Seymour CW, Rosengart MR. Prompt administration of antibiotics and fluids in the treatment of sepsis: A murine trial. Crit Care Med 2018; 46:e426–e434.
109. Bechsgaard T, Honge JL, Nygaard H, Jensen MO. In vivo wireless monitoring system of cardiovascular force data. Cardiovasc Eng Technol 2015; 6:2–7.
110. Cordes JS, Heyen JR, Volberg ML, Poy N, Kreuser S, Shoieb AM, Steidl-Nichols J. Validation and utility of the PhysioTel™ Digital M11 telemetry implant for cardiovascular data evaluation in cynomolgus monkeys and Beagle dogs. J Pharmacol Toxicol Methods 2016; 79:72–79.
111. Rothe P, Sommerfeld O, Queissner CH, Otto GP, Sossdorf M, Richter A, Claus RA. Continuous non-invasive infrared monitoring in animal research during infectious diseases. Infection 2015; 43:S67–S68.
112. Hawkins P. Refining housing, husbandry and care for animals used in studies involving biotelemetry. Animals (Basel) 2014; 4:361–373.
113. Chen J, Chiazza F, Collino M, Patel NS, Coldewey SM, Thiemermann C. Gender dimorphism of the cardiac dysfunction in murine sepsis: signalling mechanisms and age-dependency. PLoS One 2014; 9 6:e100631.
114. Zhao X, Ho D, Gao S, Hong C, Vatner DE, Vatner SF. Arterial pressure monitoring in mice. Curr Protoc Mouse Biol 2011; 1:105–122.
115. Lilley E, Armstrong R, Clark N, Gray P, Hawkins P, Mason K, López-Salesansky N, Stark AK, Jackson SK, Thiemermann C, et al. Refinement of animal models of sepsis and septic shock. Shock 2015; 43:304–316.
116. Ostler JE, Maurya SK, Dials J, Roof SR, Devor ST, Ziolo MT, Periasamy M. Effects of insulin resistance on skeletal muscle growth and exercise capacity in type 2 diabetic mouse models. Am J Physiol Endocrinol Metab 2014; 306:E592–E605.
117. Osuchowski MF, Welch K, Yang H, Siddiqui J, Remick DG. Chronic sepsis mortality characterized by an individualized inflammatory response. J Immunol 2007; 179:623–630.
118. Science Council of Japan: Guidelines for Proper Conduct of Animal Experiments, 2006.
119. National Standard of the People's Republic of China (GB/T 35892-2018): Laboratory Animal Guideline for Ethical Review of Animal Welfare, 2018.
120. Directive 2010/63/EU of the European Parliament and of the Council of 22 September 2010 on the protection of animals used for scientific purpose.
121. Nemzek JA, Xiao HY, Minard AE, Bolgos GL, Remick DG. Humane endpoints in shock research. Shock 2004; 21:17–25.
122. Toth LA. Defining the moribund condition as an experimental endpoint for animal research. ILAR J 2000; 41:72–79.
123. Franco NH, Correia-Neves M, Olsson IA. How “humane” is your endpoint? Refining the science-driven approach for termination of animal studies of chronic infection. PLoS Pathog 2012; 8:e1002399.
124. Olsen HG, Kjelgaard-Hansen M, Tveden-Nyborg P, Birck MM, Hammelev KP, Vegge A, Aalbæk B, Leifsson PS, Jensen HE, et al. Modelng severe Staphylococcus aureus sepsis in conscious pigs: are implications for animal welfare justified? BMC Res Notes 2016; 9:99.
125. Osuchowski MF, Connett J, Welch K, Granger J, Remick DG. Stratification is the key: inflammatory biomarkers accurately direct immunomodulatory therapy in experimental sepsis. Crit Care Med 2009; 37:1567–1573.
126. Remick DG, Bolgos GR, Siddiqui J, Shin J, Nemzek JA. Six at six: interleukin-6 measured 6 h after the initiation of sepsis predicts mortality over 3 days. Shock 2002; 17:463–467.
127. Weixelbaumer KM, Raeven P, Redl H, van Griensven M, Bahrami S, Osuchowski MF. Repetitive low-volume blood sampling method as a feasible monitoring tool in a mouse model of sepsis. Shock 2010; 34:420–426.
128. Moore ES, Cleland TA, Williams WO, Peterson CM, Singh B, Southard TL, Pasch B, Labitt RN, Daugherity EK. Comparing phlebotomy by tail tip amputation, facial vein puncture, and tail vein incision in C57BL/6 mice by using physiologic and behavioral metrics of pain and distress. Am Assoc Lab Anim Sci 2017; 56:307–317.
129. Raeven P, Drechsler S, Weixelbaumer KM, Bastelica D, Peiretti F, Klotz A, Jafarmadar M, Redl H, Bahrami S, Alessi MC, et al. Systemic inhibition and liver-specific over-expression of PAI-1 failed to improve survival in all-inclusive populations or homogenous cohorts of CLP mice. J Thromb Haemost 2014; 12:958–969.
130. Drechsler S, Weixelbaumer KM, Weidinger A, Raeven P, Khadem A, Redl H, van Griensven M, Bahrami S, Remick D, Kozlov A, et al. Why do they die? Comparison of selected aspects of organ injury and dysfunction in mice surviving and dying in acute abdominal sepsis. Intensive Care Med Exp 2015; 3:48.
131. Miao P, Kong Y, Ma Y, Zeng H, Yu Z. Hypothermia predicts the prognosis in colon ascendens stent peritonitis mice. J Surg Res 2013; 181:129–135.
132. Laitano O, Van Steenbergen D, Mattingly AJ, Garcia CK, Robinson GP, Murray KO, Clanton TL, Nunamaker EA. Xiphoid surface temperature predicts mortality in a murine model of septic shock. Shock 2018; 50:226–232.
133. Trammell RA, Toth LA. Markers for predicting death as an outcome for mice used in infectious disease research. Comp Med 2011; 61:492–498.
134. Zhou H, van der Windt DJ, Dons EM, Rigatti LH, Echeverri GJ, Bottino R, Wijkstrom M, Wagner R, Cooper DK. A syndrome of severe hypoglycemia and acidosis in young immunosuppressed diabetic monkeys and pigs-association with sepsis. Transplantation 2012; 94:1187–1191.
135. Marshall JC, Deitch E, Moldawer LL, Opal S, Redl H, van der Poll T. Preclinical models of shock and sepsis: what can they tell us? Shock 2005; 24 (Suppl. 1):1–6.
136. Langford DJ, Bailey AL, Chanda ML, Clarke SE, Drummond TE, Echols S, Glick S, Ingrao J, Klassen-Ross T, Lacroix-Fralish ML, et al. Coding of facial expressions of pain in the laboratory mouse. Nat Methods 2010; 7:447–449.
137. Wright-Williams SL, Courade JP, Richardson CA, Roughan JV, Flecknell PA. Effects of vasectomy surgery and meloxicam treatment on faecal corticosterone levels and behaviour in two strains of laboratory mouse. Pain 2007; 130:108–118.
138. Williams WO, Riskin DK, Mott AK. Ultrasonic sound as an indicator of acute pain in laboratory mice. J Am Assoc Lab Anim Sci 2008; 47:8–10.
139. Jeger V, Hauffe T, Nicholls-Vuille F, Bettex D, Rudiger A. Analgesia in clinically relevant rodent models of sepsis. Lab Anim 2016; 50:418–426.
140. Griffin MJ, Letson HL, Dobson GP. Buprenorphine analgesia leads to coagulopathy and increased plasma fibrinogen in healthy rats: implications for small animal research. Shock 2017; 48:78–84.
141. Anderson SL, Duke-Novakovski T, Singh B. The immune response to anesthesia: part 2 sedatives, opioids, and injectable anesthetic agents. Vet Anaesth Analg 2014; 41:553–566.
142. Narver HL. Nalbuphine, a non-controlled opioid analgesic, and its potential use in research mice. Lab Anim 2015; 44:106–110.
143. Breslow JM, Monroy MA, Daly JM, Meissler JJ, Gaughan J, Adler MW, Eisenstein TK. Morphine, but not trauma, sensitizes to systemic Acinetobacter baumannii infection. J Neuroimmune Pharmacol 2011; 6:551–565.
144. Albuszies G, Radermacher P, Vogt J, Wachter U, Weber S, Schoaff M, Georgieff M, Barth E. Effect of increased cardiac output on hepatic and intestinal microcirculatory blood flow, oxygenation, and metabolism in hyperdynamic murine septic shock. Crit Care Med 2005; 33:2332–2338.
145. Hugunin KM, Fry C, Shuster K, Nemzek JA. Effects of tramadol and buprenorphine on select immunologic factors in a cecal ligation and puncture model. Shock 2010; 34:250–260.
146. Cotroneo TM, Hugunin KM, Shuster KA, Hwang HJ, Kakaraparthi BN, Nemzek-Hamlin JA. Effects of buprenorphine on a cecal ligation and puncture model in C57BL/6 mice. J Am Assoc Lab Anim Sci 2012; 51:357–365.
147. Jeger V, Arrigo M, Hildenbrand FF, Muller D, Jirkof P, Hauffe T, Seifert B, Arras M, Spahn DR, Bettex D, et al. Improving animal welfare using continuous nalbuphine infusion in a long-term rat model of sepsis. Intensive Care Med Exp 2017; 5:23.
148. Kimmoun A, Louis H, Al KN, Delemazure J, Dessales N, Wei C, Marie PY, Issa K, Levy B. Beta1-adrenergic inhibition improves cardiac and vascular function in experimental septic shock. Crit Care Med 2015; 43:e332–e340.
149. Barr J, Fraser GL, Puntillo K, Ely EW, Gelinas C, Dasta JF, Davidson JE, Devlin JW, Kress JP, Joffe AM, et al. Clinical practice guidelines for the management of pain, agitation, and delirium in adult patients in the intensive care unit. Crit Care Med 2013; 41:263–306.
Keywords:

Animal welfare; best practices; preclinical models; sepsis; study design

© 2019 by the Shock Society