- Research article
- Open Access
In vitro effects of 6 % hydroxyethyl starch 130/0.42 solution on feline whole blood coagulation measured by rotational thromboelastometry
© The Author(s). 2016
Received: 16 January 2016
Accepted: 6 July 2016
Published: 26 July 2016
The artificial colloid, hydroxyethyl starch (HES), is recommended for intravascular volume expansion and colloid-osmotic pressure enhancement in dogs and cats. A well-known side effect of HES solutions in humans and dogs is coagulopathy. However, HES-associated coagulopathy has thus far not been investigated in cats. The goal of this study was to assess the in vitro effects of 6 % HES 130/0.42 on feline whole blood samples using rotational thromboelastometry (ROTEM). A further goal was to develop feline reference intervals for ROTEM at our institution. In this in vitro experimental study, blood samples of 24 adult healthy cats were collected by atraumatic jugular phlebotomy following intramuscular sedation. Baseline ROTEM analyses (using ex-tem, in-tem and fib-tem assays) were performed in duplicate. Additionally, ROTEM analyses were performed on blood samples after dilution with either Ringer’s acetate (RA) or 6 % HES 130/0.42 (HES) in a 1:6 dilution (i.e. 1 part solution and 6 parts blood).
Coefficients of variation of duplicate measures were below 12 % in all ex-tem assays, 3 of 4 in-tem assays but only 1 of 3 fib-tem assays. Reference intervals were similar albeit somewhat narrower than those previously published. Dilution with both solutions lead to significantly prolonged CT (in-tem), CFT (ex-tem and in-tem), and reduced MCF (ex-tem, in-tem, and fib-tem) and alpha (ex-tem and in-tem). Compared to RA, dilution with HES caused a significant prolongation of CT in fib-tem (P = 0.016), CFT in ex-tem (P = 0.017) and in-tem (P = 0.019), as well as a reduction in MCF in in-tem (P = 0.032) and fib-tem (P = 0.020), and alpha in ex-tem (P = 0.014). However, only a single parameter (CFT in ex-tem) was outside of the established reference interval after dilution with HES.
In vitro hemodilution of feline blood with RA and HES causes a small but significant impairment of whole blood coagulation, with HES leading to a significantly greater effect on coagulation than RA. Further studies are necessary to evaluate the in vivo effects and the clinical significance of these findings.
The artificial colloid, hydroxyethyl starch (HES), is recommended for the treatment of anesthesia-induced hypotension, for resuscitation and to increase colloid-osmotic pressure in cats [1, 2]. Although various doses have been recommended [3, 4], no study has thus far evaluated the side effects of HES solutions or established safe doses in cats.
Until recently, HES was widely used in human intensive care units throughout the world and was considered the artificial colloid of choice for resuscitation, especially in Europe . The physicochemical properties of modern, third generation HES solutions (i.e. HES 130/0.4 and HES 130/0.42) were aimed to improve its safety profile and minimize adverse effects, such as kidney injury, tissue storage, and coagulopathy [3, 4]. However, results of recent clinical trials showed risks related to kidney dysfunction, hemorrhage, and increased mortality in septic and critically-ill human patients [6–8]. As a result, the use of HES in humans has been restricted by international authorities . As little data is available with regards to safety in small animals, questions regarding the use of various HES solutions in veterinary medicine have arisen [3, 10].
The pathophysiology of hemostatic effects of HES is well described in several human and veterinary medical reviews [4, 11]. Indirect effects, due to hemodilution, as well as direct effects of HES molecules on components of the hemostatic system lead to an increased risk for hemorrhage [11–13]. Recent canine studies revealed a dose-dependent impairment of coagulation and platelet function with different HES products [14–18]. However, no data evaluating the effects of HES on feline hemostasis have thus far been published.
Assessment of whole blood coagulation using rotational thromboelastometry (ROTEM) has previously been evaluated in dogs and reference intervals have been established . In addition, the effects of tetrastarch solutions on canine whole blood coagulation have been evaluated [15, 18, 20]. In cats, rare studies have been performed evaluating whole blood coagulation using thromboelastography [21–25] and recently, one study, assessing reference intervals in healthy cats using ROTEM was published . To the authors’ knowledge, the effects of isotonic crystalloids or HES on feline whole blood coagulation using ROTEM have not been previously evaluated.
The objective of the present study was to assess the in vitro effects of HES 130/0.42 compared to isotonic crystalloids on ROTEM analyses in feline blood. The hypothesis was that both solutions cause impairment of whole blood coagulation due to hemodilution and that HES would impair coagulation to a greater extent than crystalloids. A secondary objective was to develop institution-specific reference intervals for ROTEM analyses in cats.
The study protocol was approved by University of Bern and the Animal Experiment Committee of the Swiss Federal Veterinary Office (No. 37/14). Informed owner consent was obtained before study enrollment. Thirty-four staff-owned cats with a minimum body weight of 3 kg and an age between 1 and 12 years old were initially enrolled in the study. Cats were included if they were deemed healthy based on history, clinical examination, unremarkable results of a CBC (Advia® 120, Siemens Healthcare Diagnostics AG, Zurich, Switzerland), biochemistry panel (Cobas® c501, Roche Diagnostics, Rotkreuz, Switzerland), and standard coagulation profile (STart 4 Hemostatis Analyzer ®, Stago CH SA, Zurich, Switzerland), including prothrombin, activated partial thromboplastin and thrombin times, and fibrinogen using the Clauss method, as well as negative results for feline immunodeficiency virus and feline leukemia virus ELISA tests (SNAP® Combo Plus FIV/FeLV, IDEXX Europe, Hoofddorp, Netherlands). In addition, cats were excluded if evidence of cardiomyopathy was detected using two-dimensional and M-mode echocardiographic examination, performed by a board-certified veterinary cardiologist (AK). Cats were also excluded if they had received any medication or vaccinations, or infusions with synthetic colloids or blood products within 4 weeks prior to study enrollment.
The HES product used in this study was a potato-derived HES with a molecular weight of 130 kDa and a molar substitution of 0.42 in a concentration of 60 g/L (6 % solution) in an electrolyte-balanced and buffered carrier solution (Tetraspan®, BBraun Melsungen AG, Melsungen, Germany). The crystalloid was a modified Ringer’s acetate (RA) solution (Ringerfundin®, BBraun Melsungen AG, Melsungen, Germany).
Three four-channel ROTEM (ROTEM®, TEM Innovations GmbH, Munich, Germany) analyzers were used to assess whole blood coagulation. The method dynamically analyses the viscoelastic properties of blood during initiation and propagation of clotting, as well as during fibrinolysis and is described in detail elsewhere . Recalcification was performed using the calcium chloride reagent provided by the manufacturer (star-tem®, Tem International GmbH, Munich, Germany). Activating reagents used were ex-tem (ex-tem®, Tem International GmbH, Munich, Germany), which triggers the extrinsic pathway using tissue factor, in-tem (in-tem®, Tem International GmbH, Munich, Germany), which triggers contact activation using ellagic acid, and fib-tem (fib-tem®, Tem International GmbH, Munich, Germany), which triggers the extrinsic pathway with platelet inhibition using cytochalasin D. Data obtained from the ROTEM analyzers were clotting time (CT, the time from activation until the onset of clotting), clot formation time (CFT, time between the onset of clotting and clot firmness with an amplitude of 20 mm) (in-tem and ex-tem only), maximum clot firmness (MCF, maximum amplitude of the curve) and alpha (α, slope of the tangent).
Blood sampling procedure
Cats were sedated by intramuscular injection of 0.3 mg/kg butorphanol (Morphasol® 10, Dr. E. Graeub AG, Bern, Switzerland), 2 mg/kg ketamine (Ketasol 100®, Dr. E. Graeub AG, Bern, Switzerland) and 0.2 mg/kg midazolam (Dormicum®, Roche Pharma Schweiz AG, Reinach, Switzerland). Blood was sampled by atraumatic phlebotomy of the jugular vein using a 21G butterfly needle. An initial 1.5 ml of blood was collected using a syringe attached to the butterfly needle in EDTA and heparin tubes (for CBC and biochemistry), followed by connection to a vacutainer system (BD Vacutainer® Push Button blood collection set, 21 G butterfly needle BD, Plymouth, United Kingdom) and filling of three 1.8 ml citrate tubes (BD Vacutainer® 1.8 ml coagulation tube, buffered trisodium citrate 3.2 %, BD, Plymouth, United Kingdom) for coagulation profiles and ROTEM analyses.
Dilutions and measurements
After a resting period of 15 min, baseline ROTEM measurements to establish reference intervals were performed in duplicate. The remaining citrated blood was diluted 1:6 (1 part study fluid and 6 parts blood) with RA and HES, respectively. The appropriate amount of blood was filled in prewarmed polypropylene tubes containing either HES or RA with a pipette. Mixing was performed by careful inverting and rolling the tube 6 times, followed by 5 min’ incubation. The dilution was selected to simulate a bolus administration of 10 ml/kg, taking into account a blood volume of approximately 62–66 ml/kg body weight in an adult cat . Three ROTEM devices were used in parallel and all measurements were started within 60 min after blood sampling. Samples for ROTEM measurements were stored at 37 °C in a thermostatic tube heater (WiseTerm Heating Block R48®; WITEG Labortechnik GmbH, Wertheim, Germany) and analyses were performed according to the manufacturer’s instructions. Run time was preset to 60 min. As blood collection and sample handling was shown to significantly affect whole blood coagulation in dogs , a single investigator (NAA) collected all samples and run all ROTEM analyses.
Data were assessed for normality using Q-Q plots and D’Agostino-Pearson tests. As some ROTEM data were normally distributed but others were not and could not be transformed to normality, nonparametric analyses were performed. A Friedman test was used to assess differences between samples. Where significant differences were found, a post-hoc analysis was performed using Wilcoxon paired-samples tests with Bonferroni correction. The coefficient of variation of baseline duplicate measurements was calculated. Double-sided reference intervals were determined based on the average of the two repeated baseline values, using the robust method (CLSI guideline C28-A3) with confidence intervals estimated by bootstrapping. All statistical analyses were performed using commercial software (MedCalc Software® version 14.10, Ostend, Belgium) and significance was set at P < 0.05 throughout.
Of the 34 cats initially enrolled, ten cats were excluded due abnormal results of echocardiographic examinations (n = 4), anemia (n = 1), increased plasma creatinine concentrations (n = 1), prolonged prothrombin time (n = 1), thrombocytopenia (n = 1), and decreased fibrinogen levels (n = 1). Only data from the remaining 24 cats were included in analyses. These were domestic shorthair cats (n = 22) and Bengal cats (n = 2). The cats had a mean age of 4.5 years (range, 1.5–11.2 years) and a mean body weight of 4.5 kg (range, 3.0–6.4 kg). Twelve cats were male (1 sexually intact, 11 castrated) and 12 were female (all spayed).
The mean (±SD) of hematologic variables included hematocrit, 31 ± 5 % (0.31 ± 0.05 L/L); platelet count, 267 ± 79 × 109/L; prothrombin time, 11.2 ± 0.6 s; activated partial thromboplastin time, 12.4 ± 1.2 s; and thrombin time, 16.9 ± 1.8 s. The median (range) of fibrinogen concentrations was 143 (102–294) mg/dL.
Reference intervals for ROTEM assays in 22 cats
lower (90 % CI)
upper (90 % CI)
lower (90 % CI)
upper (90 % CI)
lower (90 % CI)
upper (90 % CI)
Coefficients of variation (CV) of duplicate measure for ROTEM assays in 22 cats
Dilution with ringer’s acetate and HES
ROTEM analyses in feline blood samples without dilution (baseline), and samples diluted 1:6 with RA or HES
Compared to RA, dilution with HES lead to prolongation of CT fib-tem (P = 0.016), CFT ex-tem (P = 0.017) and in-tem (P = 0.019), as well as reduction of MCF in-tem (P = 0.032) and fib-tem (P = 0.020), and alpha ex-tem (P = 0.014).
Despite statistically significant differences in ROTEM assays after dilution with study solutions, the median measured value was outside of the established reference range only after dilution with HES in ex-tem CFT (Table 3).
This study demonstrates that in vitro hemodilution of feline blood with RA and HES affects whole blood coagulation measured by ROTEM, with HES leading to a greater hemostatic impairment than RA. These findings corroborate those reported in humans and in dogs [11, 15, 29]. After both solutions, ROTEM parameters showed a hypocoagulable pattern, characterized by a longer duration of clot formation and propagation time (increased CFT and decreased alpha), and lower clot stability and less stable fibrin network (decreased MCF). However, the magnitude of the observed changes was low, and only a single parameter (CFT ex-tem) was outside of the reference interval established after dilution with HES, suggesting that findings may not be of clinical relevance. In a recent study, evaluating the effects of HES 130/0.4 on canine ROTEM parameters, 25 % dilution resulted in 7 of 13 parameters being outside the of reference intervals although all parameters were within reference limits after 10 % dilution . In a similar study in dogs with the same HES preparation, 25 % dilution resulted in 4 out of 5, and 10 % dilution resulted in 2 out of 5 ROTEM parameters being significantly impaired compared to the dilutional control with saline . Several reasons may be responsible for the smaller effects on feline coagulation in the present study. Firstly, the dilution used was 1:6 (14 %) compared to 1:3 (25 %) in the aforementioned canine studies. This likely resulted in lesser coagulation impairing effects in the present study. Moreover, feline platelets are more reactive than those of other species, due to larger platelet size and higher concentrations of serotonin . Finally, the HES preparation used in the present study was a potato-derived starch in a calcium-containing carrier solution, in contrast to the waxy-maize-derived starch in calcium-free solution used in the aforementioned canine studies. This might have influenced ROTEM parameters, although only minor effects on coagulation were found when comparing calcium-containing versus calcium-free carrier HES preparations in a recent in vivo study in dogs . The reason why CFT ex-tem was apparently affected more than other parameters following dilution with HES in the present study is unclear, but similar findings were observed in canine studies at low dilutions [15, 18]. Despite the overall relatively minor effects observed, data in the present study suggest that dilution with HES has a more pronounced effect on whole blood coagulation than RA, suggesting that effects of HES are beyond that of dilution alone.
Little data on ROTEM analyses in cats are currently available. Notably, no data exist regarding the association between ROTEM parameters and clinically relevant impairment of hemostasis. Previous studies found that cats with laboratory evidence of disseminated intravascular coagulation rarely show clinical bleeding tendencies [31, 32]. The observed changes in ROTEM analysis after dilution with HES may therefore not be of clinical significance at the dose simulated in the current study.
Recently, feline reference intervals for ROTEM using ex-tem and in-tem assays, based on 55 clinically healthy European shorthair cats, were published . Reference ranges established in the present study were similar although a narrower interval was found for some of the parameters. However, reference intervals established in the present assay were based on a smaller population, and the robust method was used instead of a percentile method. Intra-assay coefficients of variation, evaluated from quadruplicate measurements, were found to be below 10 % for CT, CFT, alpha, and MCF in a previous study . In another study, intra-assay CV was below 5 % in kaolin-activated thromboelastography in 30 healthy cats . The coefficients of variation in our study were below 10 % in 7 of the 11 ROTEM parameters, but were between 10 and 25 % in another 4 parameters. However, CVs established in the present study were based on duplicate measurements in all 24 samples, but those previously published were based on quadruplicate measurements in only two samples. Moreover, although the mean of the 2 CVs was below 10 % in the previous study, the CV of one of the two samples was above 10 % in 3 assays. Lastly, evaluation of CVs using the fib-tem assay was not performed in previous studies.
Although HES-associated coagulopathy may in part be due to dilution alone, direct effects of HES on hemostatic components have been observed [4, 11]. Of these, an acquired impairment of fibrin polymerization is suggested to be most important. A sensitive parameter for monitoring fibrin polymerization with ROTEM is MCF, in particular in the fib-tem assay. In the present study, HES led to a significantly lower MCF compared to RA in both the in-tem and fib-tem assays, but the median value was still within the reference interval. Impaired platelet function is another important aspect of HES-induced coagulopathy. ROTEM parameters which are influenced by both platelet numbers and function are CFT, alpha, and MCF. A separate platelet function analysis might have added more specific information about the platelet impairing effect of HES in cats.
As previous studies have demonstrated that cardiac disease can affect coagulation in humans as well as in cats and dogs [33–36], an attempt to exclude cats with subclinical cardiomyopathy using echocardiography was made in the present study. Indeed, one former study evaluating the prevalence of cardiomyopathy in apparently healthy cats identified cardiomyopathy in 16 % of the cats . Similarly, four of the originally enrolled 34 cats were excluded based on abnormal echocardiography in the present study. As echocardiography was not performed in the previous study reporting feline reference intervals, the extent to which this may explain the wider intervals previously reported is unclear. Unfortunately, urinalysis was not performed in the present study as part of the health assessment. Although plasma urea and creatinine concentrations were within reference ranges, early renal disease may have gone unnoticed. Furthermore, cats were not evaluated for hemotropic mycoplasmas or Cytauxzoon felis infection.
The study has some limitations. Firstly, all cats underwent sedation to ensure atraumatic jugular venipuncture and to harvest the required amount of blood for all analyses without interruption of blood flow. A previous study in cats found that ketamine may slightly increase prothrombin time and partial thromboplastin time after intravenous administration in combination with diazepam . However, the observed changes were small and likely not of clinical relevance . Another study showed differences in kaolin-activated thromboelastographic tracings between non-sedated cats and those sedated with butorphanol and midazolam, with the latter having a mild increase in the rapidity of clot formation . Neither reaction time nor maximum amplitude was significantly affected in the sedated cats. Therefore, the authors of that study suggested that the effects on thromboelastographic variables may not be of major importance. Due to the lack of studies using ROTEM in cats, the extent to which prior sedation may have influenced results in the present study is unclear. In addition, ROTEM measurements were started after 15 min resting time at 37 °C instead of 30 min at room temperature, as recommended by the PROVETS guidelines . This was done in order to perform all analyses within 60 min of blood collection and avoid temperature variations, but may have affected results in some samples. Furthermore, the effects of transendothelial fluid shifts was excluded due to the in vitro character of the study. In addition, vasoactive effects of fluids, endogenous release of fibrinolytic factors, clot dissolution, excretion or degradation of HES, and extraneous factors, such as stress response, tissue damage, and endothelial injury are not taken into account in an in vitro model. Results of the current and other in vitro studies do not therefore mimic in vivo conditions. A further limitation was the dilution of citrated blood samples with citrate-free study solutions, which may have resulted in an excess in calcium concentrations following the standardized recalcification in the ROTEM cup. This in turn could impact thrombin generation and diminished the hypocoagulable effects of HES. Finally, only healthy cats were enrolled in this study, and the effects of fluid therapy on coagulation may be more pronounced in cats with pre-existing coagulopathies.
Data from the present study suggest that an in vitro 1:6 dilution with HES 130/0.42 affects feline whole blood coagulation to a greater extent than a similar dilution with RA. However, the magnitude of the observed changes was small, and only a single parameter was outside of the established reference interval after dilution with HES. Further studies are necessary to evaluate the in vivo risk of hemostasis impairment following administration of HES in healthy cats and those with naturally occurring disease and pre-existing coagulopathies.
CFT, clot formation time; CT, clotting time; ex-tem, extrinsic thromboelastometry; fib-tem, fibrinogen function thromboelastometry; HES, hydroxyethyl starch; in-tem, intrinsic thromboelastometry; MCF, maximal clot firmness; RA, Ringer’s acetate; ROTEM, rotational thromboelastometry
The authors would like to thank Axon Lab AG, Täfernstrasse 15, 5405 Baden, Switzerland for provision and service of the ROTEM machines.
Parts of the results were presented in abstract form at the 14th European Veterinary Emergency and Critical Care Society Annual Congress, Lyon, France, June 2015.
The expenses were funded by resources of the Division of Emergency and Critical Care, Small Animal Clinic, Department of Clinical Veterinary Medicine, Vetsuisse Faculty, University of Bern, Switzerland.
Availability of data and materials
The datasets supporting the conclusions of this article are included within the article.
NAA did the clinical examination and sedation of the cats, blood collection, carried out all ROTEM analyses, and helped to draft the manuscript; AK did the echocardiographic examination of the cats; JH performed the statistical analyses and helped to draft the manuscript. KNA designed the study, assisted at sample collection, interpreted the data and drafted the manuscript. All authors read and approved the final manuscript.
The authors declare that they have no competing interests that could inappropriately influence or bias the results.
Consent for publication
Consent from the owners was obtained.
Ethics approval and consent to participate
The study protocol was approved by University of Bern and the Animal Experiment Committee of the Swiss Federal Veterinary Office (No. 37/14). Informed owner consent was obtained before study enrollment.
Open AccessThis article is distributed under the terms of the Creative Commons Attribution 4.0 International License (http://creativecommons.org/licenses/by/4.0/), which permits unrestricted use, distribution, and reproduction in any medium, provided you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The Creative Commons Public Domain Dedication waiver (http://creativecommons.org/publicdomain/zero/1.0/) applies to the data made available in this article, unless otherwise stated.
- Davis H, Jensen T, Johnson A, Knowles P, Meyer R, Rucinsky R, Shafford H, American Association of Feline P, American Animal Hospital A. 2013 AAHA/AAFP fluid therapy guidelines for dogs and cats. J Am Anim Hosp Assoc. 2013;49(3):149–59.View ArticlePubMedGoogle Scholar
- Murphy K, Hibbert A. The flat cat: 1. a logical and practical approach to management of this challenging presentation. J Feline Med Surg. 2013;15(3):175–88.View ArticlePubMedGoogle Scholar
- Adamik KN, Yozova ID, Regenscheit N. Controversies in the use of hydroxyethyl starch solutions in small animal emergency and critical care. J Vet Emerg Crit Care. 2015;25(1):20–47.View ArticleGoogle Scholar
- Glover PA, Rudloff E, Kirby R. Hydroxyethyl starch: A review of pharmacokinetics, pharmacodynamics, current products, and potential clinical risks, benefits, and use. J Vet Emerg Crit Care. 2014;24(6):642–61.View ArticleGoogle Scholar
- Finfer S, Liu B, Taylor C, Bellomo R, Billot L, Cook D, Du B, McArthur C, Myburgh J, Investigators ST. Resuscitation fluid use in critically ill adults: an international cross-sectional study in 391 intensive care units. Crit Care. 2010;14(5):R185.View ArticlePubMedPubMed CentralGoogle Scholar
- Perner A, Haase N, Guttormsen AB, Tenhunen J, Klemenzson G, Aneman A, Madsen KR, Moller MH, Elkjaer JM, Poulsen LM, et al. Hydroxyethyl starch 130/0.42 versus Ringer’s acetate in severe sepsis. N Engl J Med. 2012;367(2):124–34.View ArticlePubMedGoogle Scholar
- Myburgh JA, Finfer S, Bellomo R, Billot L, Cass A, Gattas D, Glass P, Lipman J, Liu B, McArthur C, et al. Hydroxyethyl starch or saline for fluid resuscitation in intensive care. N Engl J Med. 2012;367(20):1901–11.View ArticlePubMedGoogle Scholar
- Brunkhorst FM, Engel C, Bloos F, Meier-Hellmann A, Ragaller M, Weiler N, Moerer O, Gruendling M, Oppert M, Grond S, et al. Intensive insulin therapy and pentastarch resuscitation in severe sepsis. N Engl J Med. 2008;358(2):125–39.View ArticlePubMedGoogle Scholar
- Press release: European Medicined Agency (EMA) PRAC Hydroxyethyl-starch solutions (HES) no longer to be used in patients with sepsis or burn injuries or in critically ill patients, HES will be available in restricted patient populations [http://www.ema.europa.eu/ema/index.jsp?url=pages/news_and_events/news/2013/10/news_detail_001930.jsp&mid=WC0b01ac058004d5c1]. Accessed 19 Dec 2013.
- Cazzolli D, Prittie J. The crystalloid-colloid debate: Consequences of resuscitation fluid selection in veterinary critical care. J Vet Emerg Crit Care. 2015;25(1):6–19.View ArticleGoogle Scholar
- Kozek-Langenecker SA. Effects of hydroxyethyl starch solutions on hemostasis. Anesthesiology. 2005;103(3):654–60.View ArticlePubMedGoogle Scholar
- Westphal M, James MF, Kozek-Langenecker S, Stocker R, Guidet B, Van Aken H. Hydroxyethyl starches: different products--different effects. Anesthesiology. 2009;111(1):187–202.View ArticlePubMedGoogle Scholar
- Franz A, Braunlich P, Gamsjager T, Felfernig M, Gustorff B, Kozek-Langenecker SA. The effects of hydroxyethyl starches of varying molecular weights on platelet function. Anesth Analg. 2001;92(6):1402–7.View ArticlePubMedGoogle Scholar
- Classen J, Adamik KN, Weber K, Rubenbauer S, Hartmann K. In vitro effect of hydroxyethyl starch 130/0.42 on canine platelet function. Am J Vet Res. 2012;73(12):1908–12.View ArticlePubMedGoogle Scholar
- Falco S, Bruno B, Maurella C, Bellino C, D’Angelo A, Gianella P, Tarducci A, Zanatta R, Borrelli A. In vitro evaluation of canine hemostasis following dilution with hydroxyethyl starch (130/0.4) via thromboelastometry. J Vet Emerg Crit Care. 2012;22(6):640–5.View ArticleGoogle Scholar
- Wierenga JR, Jandrey KE, Haskins SC, Tablin F. In vitro comparison of the effects of two forms of hydroxyethyl starch solutions on platelet function in dogs. Am J Vet Res. 2007;68(6):605–9.View ArticlePubMedGoogle Scholar
- Smart L, Jandrey KE, Kass PH, Wierenga JR, Tablin F. The effect of Hetastarch (670/0.75) in vivo on platelet closure time in the dog. J Vet Emerg Crit Care. 2009;19(5):444–9.View ArticleGoogle Scholar
- Wurlod VA, Howard J, Francey T, Schweighauser A, Adamik KN. Comparison of the in vitro effects of saline, hypertonic hydroxyethyl starch, hypertonic saline, and two forms of hydroxyethyl starch on whole blood coagulation and platelet function in dogs. J Vet Emerg Crit Care. 2015;25(4):474–87.View ArticleGoogle Scholar
- Smith SA, McMichael M, Galligan A, Gilor S, Hoh CM. Clot formation in canine whole blood as measured by rotational thromboelastometry is influenced by sample handling and coagulation activator. Blood Coagul Fibrinolysis. 2010;21(7):692–702.PubMedGoogle Scholar
- Reuteler A, Howard J, Axiak-Flammer S, Adamik KN. Comparison of a balanced versus a saline-based tetrastarch on canine whole blood coagulation and platelet function. J Vet Emerg Crit Care. 2014;24(S1):S27 (abstract).Google Scholar
- Alwood AJ, Downend AB, Brooks MB, Slensky KA, Fox JA, Simpson SA, Waddell LS, Baumgardner JE, Otto CM. Anticoagulant effects of low-molecular-weight heparins in healthy cats. J Vet Intern Med. 2007;21(3):378–87.View ArticlePubMedGoogle Scholar
- Banerjee A, Blois SL, Wood RD. Comparing citrated native, kaolin-activated, and tissue factor-activated samples and determining intraindividual variability for feline thromboelastography. J Vet Diagn Invest. 2011;23(6):1109–13.View ArticlePubMedGoogle Scholar
- Bjornvad CR, Wiinberg B, Kristensen AT. Obesity increases initial rate of fibrin formation during blood coagulation in domestic shorthaired cats. J Anim Physiol Anim Nutr (Berl). 2012;96(5):834–41.View ArticleGoogle Scholar
- Hall DJ, Rush JE, deLaforcade AM, Shaw SP. Kaolin-activated thromboelastography in echocardiographically normal cats. Am J Vet Res. 2012;73(6):775–8.View ArticlePubMedGoogle Scholar
- Marschner CB, Bjornvad CR, Kristensen AT, Wiinberg B. Thromboelastography results on citrated whole blood from clinically healthy cats depend on modes of activation. Acta Vet Scand. 2010;52:38.View ArticlePubMedPubMed CentralGoogle Scholar
- Doderlein E, Mischke R. Reference intervals for thromboelastometry with the ROTEM((R))delta in cats. Res Vet Sci. 2015;100:271–6.View ArticlePubMedGoogle Scholar
- Kol A, Borjesson DL. Application of thrombelastography/thromboelastometry to veterinary medicine. Vet Clin Pathol. 2010;39(4):405–16.View ArticlePubMedGoogle Scholar
- Wellmann ML, DiBartola SP, Kohn CW. Applied Physiology of Body Fluids in Dogs and Cats. In: DiBartola S, editor. Fluid, Electrolyte, and Acid–base Disorders in Small Animal Practice. 4th ed. St. Louis: WB Saunders CO; 2012. p. 2–25.View ArticleGoogle Scholar
- Hartog CS, Reuter D, Loesche W, Hofmann M, Reinhart K. Influence of hydroxyethyl starch (HES) 130/0.4 on hemostasis as measured by viscoelastic device analysis: a systematic review. Intensive Care Med. 2011;37(11):1725–37.View ArticlePubMedGoogle Scholar
- Russel KE. Platelet Kinetics and Laboratory Evaluation of Thrombocytopenia. In: Weiss DJ, Wardrop KJ, editors. Schalm’s Veterinary Hematology. 6th ed. Ames: Wiley-Blackwell; 2010. p. 576–85.Google Scholar
- Estrin MA, Wehausen CE, Jessen CR, Lee JA. Disseminated intravascular coagulation in cats. J Vet Intern Med. 2006;20(6):1334–9.View ArticlePubMedGoogle Scholar
- Stokol T. Laboratory diagnosis of disseminated intravascular coagulation in dogs and cats: the past, the present, and the future. Vet Clin North Am Small Anim Pract. 2012;42(1):189–202.View ArticlePubMedGoogle Scholar
- Paige CF, Abbott JA, Elvinger F, Pyle RL. Prevalence of cardiomyopathy in apparently healthy cats. J Am Vet Med Assoc. 2009;234(11):1398–403.View ArticlePubMedGoogle Scholar
- Tarnow I, Falk T, Tidholm A, Martinussen T, Jensen AL, Olsen LH, Pedersen HD, Kristensen AT. Hemostatic biomarkers in dogs with chronic congestive heart failure. J Vet Intern Med. 2007;21(3):451–7.View ArticlePubMedGoogle Scholar
- Davis CJ, Gurbel PA, Gattis WA, Fuzaylov SY, Nair GV, O’Connor CM, Serebruany VL. Hemostatic abnormalities in patients with congestive heart failure: diagnostic significance and clinical challenge. Int J Cardiol. 2000;75(1):15–21.View ArticlePubMedGoogle Scholar
- Stokol T, Brooks M, Rush JE, Rishniw M, Erb H, Rozanski E, Kraus MS, Gelzer AR. Hypercoagulability in cats with cardiomyopathy. J Vet Intern Med. 2008;22(3):546–52.View ArticlePubMedGoogle Scholar
- Reynolds BS, Geffre A, Bourges-Abella NH, Vaucoret S, Mourot M, Braun JP, Trumel C. Effects of intravenous, low-dose ketamine-diazepam sedation on the results of hematologic, plasma biochemical, and coagulation analyses in cats. J Am Vet Med Assoc. 2012;240(3):287–93.View ArticlePubMedGoogle Scholar
- Flatland B, Koenigshof AM, Rozanski EA, Goggs R, Wiinberg B. Systematic evaluation of evidence on veterinary viscoelastic testing part 2: Sample acquisition and handling. J Vet Emerg Crit Care. 2014;24(1):30–6.View ArticleGoogle Scholar