Rebecca A. Johnson Department of Surgical Sciences, School of Veterinary Medicine, University of Wisconsin, Madison, Wisconsin, USA The kidneys are responsible for numerous essential biological functions, such as maintaining acid–base, electrolyte, and endocrine balance, regulating blood pressure, and forming urine by filtering hematologic nitrogenous end‐products while retaining solutes, proteins, and blood cells [1]. Acute kidney injury (AKI) and chronic kidney disease (CKD) are common clinical entities that are associated with impaired kidney function (see Chapter 43). Depending on etiology and chronicity, patients may exhibit clinical signs such as vomiting, diarrhea, oral ulceration, anorexia, weight loss, polydipsia, and urine output changes such as polyuria, oliguria, or anuria. Patients also commonly present with electrolyte and acid–base disturbances (e.g., hyperkalemia and metabolic acidosis) and/or volume overload. To relieve these severe clinical signs, stabilize patient condition, improve quality of life, and extend lifespan, renal replacement therapies are utilized, especially if medical therapy has been unsuccessful. Renal replacement therapies include both intracorporeal (renal transplantation and peritoneal dialysis [PD]) and extracorporeal (intermittent hemodialysis [IHD] and continuous renal replacement therapy [CRRT]) techniques. Although these therapies are associated with significant financial, ethical, and emotional considerations, they have progressed from non‐traditional, infrequent clinical entities to more common, progressive therapeutic options for companion animals with renal impairment. In this chapter, first, the unique principles used in the critical anesthetic management of dogs and cats undergoing renal transplantation are discussed, followed by a brief discussion of anesthetic considerations for specific dialysis techniques. In the mid‐1950s, Guild et al. performed the first successful renal transplantation on identical twin humans [2]. Although the first renal transplant in clinical veterinary medicine occurred in 1984, only in the last few decades has renal transplantation gained popularity in clinical veterinary medicine as a therapy for companion animals with CKD [3]. Morbidity and mortality rates associated with renal transplantation differ significantly between dogs and cats. For example, mean survival time for clinical canine patients is variable, reported to be from 18 days [4] up to 8 months [5]. In contrast, 70–93% of cats are discharged after surgery [3], and mean survival times in clinical feline patients are between 360 and 653 days, with 59–79% still alive after 6 months and 32–45% after 3 years [3,6–8]. The exact reasons for lower success rates in dogs compared with cats are not entirely clear. However, strong canine host immune responses require that potent immunosuppressive therapy is administered to prevent rejection, thereby increasing the possibility of adverse events [4,9–11]; thromboembolism, allograft rejection, and respiratory, neurologic, skin, and urinary tract infections are commonly reported [3]. Although thromboembolism is associated with immunosuppression (among other factors) and is reported as a complication in human transplantation, it is infrequently seen in cats [11,12]. Increasing age of both canine and feline patients is associated with decreased survival rates following transplantation [4,8,13], whereas severe preoperative azotemia, hypertension, and increased left ventricular wall thickness are also associated with increased mortality in cats [8]. Thus, although renal transplantation appears to be a promising treatment for CKD in animals, discriminant patient selection and preoperative risk assessment may enhance the survival of kidney transplant recipients. Since the majority of current clinical patients undergoing transplantation are cats, this chapter focuses on feline techniques. Currently, debate exists concerning the ethics surrounding renal transplantation in veterinary medicine (for review, see [14] and [15]). For example, in 2003, the Royal College of Veterinary Surgeons (RCVS) in the United Kingdom approved guidelines for feline renal transplantation based on procedures being done in other countries such as the United States, New Zealand, and Australia [14]. The guidelines were set up using strict standards and included using source animals that were siblings or cohorts screened for compatibility to the recipient. However, in 2013, the procedure was suspended in the UK pending review and in 2016 deliberations were ongoing, as the RCVS began considering feline renal transplantation as a possible “mutilation” procedure in the living source cat making it less “cat‐like.” In addition, the Royal Society for the Prevention of Cruelty to Animals suggests that renal transplantation is potentially illegal as it causes unnecessary feline suffering, among various other debatable issues [14]. The term “donor cat” is also under debate by the RCVS as the source cat cannot freely make the choice to give up the organ themself [15]. Thus, although renal transplantation in cats appears to be medically feasible and advantageous in some instances as cats may live longer following renal transplantation when compared with cats medically managed for CKD [8], many perspectives and much debate still exist regarding its place in veterinary medicine. Many patients with CKD that present for renal transplantation will have acid–base and electrolyte abnormalities. A complete blood count and serum biochemistry should be performed as the magnitude of the elevations in blood urea nitrogen (BUN) and creatinine levels is associated with increased mortality in cats [8], but not in dogs [4]. In addition, urinalysis and urine culture, blood typing, thoracic and abdominal radiographs, cardiac and abdominal ultrasound, and systemic blood pressure measurements should be performed to screen for any pre‐existing comorbidities and to ensure compatible blood types. Comorbidities such as hypertension and cardiovascular disease are common and are associated with a higher postoperative mortality in feline patients as previously mentioned [8]. Thus, perioperative treatment of these disorders may reduce complication rates and patients should be medically managed before transplantation. Preoperative patient preparation includes placement of a double‐ or triple‐lumen central venous catheter for chronic administration of balanced electrolyte solutions to correct electrolyte and acid–base abnormalities, to measure central venous pressure (CVP), and to facilitate blood sampling (Fig. 44.1). The right jugular is preferred in the event that an esophagostomy tube is required to facilitate nutritional support following surgery. Immunosuppressive and antihypertensive therapy may also be instituted, and hemo‐ or peritoneal dialysis may be performed prior to transplantation, particulary in anuric, profoundly azotemic, and edematous cats (see below) [3]. Depending on patient needs, red blood cell transfusion, whole blood transfusion, or erythropoietin, replacement therapy may also be administered to enhance oxygen‐carrying capacity if the patient is severely anemic (PCV < 20%). However, the transfusion trigger point for patients with CKD is often lower than for healthier patients owing to compensatory mechanisms associated with chronic disease; therefore, patients should be assessed on an individual basis. The use of autogenous mesenchymal stem cells to improve long‐term outcomes by reducing the possibility of acute rejection and/or systemic infection is currently under investigation [3]. Although stem cell work is promising in humans [16] and in vitro feline studies are favorable [17], additional in vivo feline investigations are needed, especially since complications associated with the addition of a surgical harvesting procedure in an already compromised cat may preclude its use [3]. Figure 44.1 An example of a triple‐lumen intravenous catheter inserted in the right jugular vein of a cat. These catheters may be placed preoperatively under sedation using the Seldinger technique and are subsequently used for hemodialysis techniques, fluid therapy, blood administration, and blood sampling perioperatively. Source: Dr. Rebecca Johnson, with permission. Donor animals are routinely screened with a serum chemistry, complete blood count, blood typing, urinalysis and culture, and infectious disease testing (toxoplasmosis, feline leukemia virus, and feline immunodeficiency virus in cats; heartworm in dogs). Computed tomography to characterize renal tissue and vasculature is frequently performed. Approximately 84% of feline donors had no associated long‐term effects associated with nephrectomy, whereas 7% developed renal insufficiency or died of urinary tract disease [18]. The ultimate goal of the anesthetic period is to provide acceptable anesthesia, analgesia, and muscle relaxation to patients without compromising existing renal function or function of the new kidney. Hence, the anesthetic plan includes agents that have minimal cardiovascular depression, are not directly nephrotoxic, and minimally rely on the kidneys for their excretion. In addition, prudent anesthetic techniques required for any patient anesthetized for prolonged periods such as adequate padding, generous and repeated application of ocular lubricant, consistent core body temperature monitoring, and active warming with a forced‐air warmer to reduce hypothermia should be employed for both the donor and the recipient. All attempts to reduce anesthetic time should be made, and good communication between the anesthetic and surgical teams is imperative throughout the perioperative procedures as prolonged anesthetic times (median = 300 min) are associated with reduced overall survival rates in cats [13]. Currently, live kidney donors are already owned or are adopted by the recipient’s owner prior to any surgical procedure. They are young, healthy animals with normal cardiovascular and renal function; anesthetic procedures for kidney removal are generally routine and are chosen based on the individual donor’s disposition and anesthetic needs while minimizing any cardiovascular depression (Table 44.1). Specific to the donor, acepromazine is frequently used pre‐ or intraoperatively to promote renal vasculature dilation through α1‐adrenergic receptor blockade [19,20]; any associated hypotension must be quickly addressed to ensure that kidney perfusion pressure is supported. Vasoconstrictive agents such as α2‐adrenergic receptor agonists are avoided if possible to reduce potential increases in vascular resistance [21–26]. Appropriate analgesic techniques are used as required; epidurals with preservative‐free morphine, with or without a local anesthetic such as bupivacaine or ropivacaine, and other systemic μ‐opioid receptor agonists are commonly used as adjunctive analgesic agents. Other agents to improve renal perfusion such as mannitol can also be administered. Anesthetic monitoring is routine but focuses on the cardiovascular system; pulse oximetry, electrocardiography, direct (dorsal pedal, coccygeal, or femoral arterial catheter) or indirect (oscillometric or Doppler ultrasonic) arterial blood pressure, end‐tidal carbon dioxide/anesthetic gases, and core body temperature are monitored continuously. Blood gas analyses, including electrolytes, and packed cell volumes are performed perioperatively. Table 44.1 Suggested anesthetic and analgesic agents for renal replacement therapy patients. IV, intravenous; IM, intramuscular; TM, transmucosal. Kidney recipient anesthesia is handled similarly to that for other patients with CKD (see Chapter 43). However, recipients present unique challenges as they accept a new kidney (graft) that has been removed from a donor and stored in hypoxic conditions for minutes to hours (Fig. 44.2A) (for microsurgical and storage techniques, see [3,4,27–30]). Although few currently used anesthetic agents are directly nephrotoxic, and no specific anesthetic agents are associated with changes to short‐term or overall survival rates [13], many anesthetics alter renal function through decreases in cardiac output, systemic vascular resistance and blood pressure, neuroendocrine status, and renal blood flow (RBF), which will subsequently affect the glomerular filtration rate (GFR). The stress response to surgery can release aldosterone, vasopressin, renin, and endogenous catecholamines, which can increase renal vascular resistance and subsequently reduce GFR [31–33]. Hence, the objectives of the anesthetic period include reducing patient stress and maintaining systemic blood pressure (and, therefore, GFR) to the greatest extent possible via the use of anesthetic agents with minimal cardiovascular depression. Figure 44.2 Intraoperative renal transplantation. A. Donor kidney (white arrow) placed in the abdomen of the recipient following extracorporeal storage. Note the pale color of the stored kidney as the anastomoses are not yet completed in this photograph. B. Donor kidney (gray arrow) following renal artery and vein anastomoses and application of chlorpromazine to the renal artery. Note the pink (perfused) color of the kidney compared with the kidney in A. Source: Dr. Jon McAnulty, Department of Surgical Sciences, School of Veterinary Medicine, University of Wisconsin, Madison, WI, USA, with permission. Similar to the kidney donor, anesthetic and analgesic agents must be chosen according to the individual patient’s physiologic status and signalment as each transplant patient is unique; there is no universal protocol that can be used for every patient. Preoperative medication using a combination of the μ‐opioid receptor agonist, fentanyl, and a benzodiazepine is common since neither fentanyl nor the benzodiazepine class of drugs substantially affects cardiovascular function at clinically acceptable doses (Table 44.1) [34–37]. For example, fentanyl or a fentanyl analog (including sufentanil, alfentanil, and remifentanil) and midazolam are commonly used intravenously to facilitate anesthetic induction, provide analgesia, and reduce the stress response to surgery. Fentanyl is also advantageous since it has a relatively short duration of action, which facilitates rapid adjustments, does not release histamine, and is minimally excreted (< 10%) unchanged by the kidneys [38–40]. Although other opioids, such as hydromorphone, may be acceptable for use as analgesics, systemic morphine is not recommended. Systemic morphine administration increases plasma histamine levels, which can be associated with systemic hypotension [38]. In addition, morphine‐6‐glucuronide is an active metabolic product of morphine in dogs and humans, and delayed elimination of this metabolite in patients with renal insufficiency may prolong drug effects [41–45]. Although cats have low levels of glucuronyl transferase and morphine undergoes a different type of conjugation reaction in this species, the pharmacokinetics of morphine are somewhat similar to those of dogs and humans, but clearance rates may be slightly slower [46–48]. Hence, systemic morphine administration in feline kidney recipients is not routinely recommended when other opioids are available. Similarly, α2‐adrenergic receptor agonists, such as dexmedetomidine, should be avoided as they reduce cardiac output with increases in systemic vascular resistance [21–26]. Phenothiazines are also not recommended as a routine premedication in recipients since administration can reduce systemic vascular resistance and potentially decrease arterial blood pressure in dogs and cats via peripheral α‐adrenergic receptor blockade [20,49,50]. Anesthetic induction can be accomplished with slow administration of small doses of propofol as it is rapidly metabolized by both hepatic and extra‐hepatic means and RBF and GFR are minimally affected (Table 44.1) [51,52]. Although the effects of alfaxalone on RBF and GFR are not specifically reported in cats, small boluses of alfaxalone may also be used since postinduction cardiovascular effects appear similar to those of propofol (for review, see [53]). Although significantly metabolized in the liver, ketamine is usually avoided since its active metabolite, norketamine, is excreted unchanged by the kidney [54] and may contribute to prolonged drug effects in animals with decreased renal function. If ketamine is required as a premedication or induction agent (for example, due to animal behavior or lack of an alternative), doses should be reduced as much as possible by combination with appropriate coinduction agents. Etomidate may be used but is not commonly recommended since, although it has minimal cardiovascular effects, it induces transient adrenal suppression, which has been associated with increased postoperative mortality in critically ill humans [55,56]. Etomidate’s effect on postoperative mortality in compromised cats is unknown. During anesthetic maintenance (Table 44.1), most inhalant anesthetics reduce GFR (isoflurane, sevoflurane, and desflurane), and attempts to reduce levels and maintain systemic blood pressure should be made [52,57]. Therefore, it is common to use a constant rate infusion of fentanyl or another fentanyl analog throughout the surgical procedure to reduce inhalant levels and enhance antinociception [58–60]. In addition, an epidural containing preservative‐free morphine may be used; addition of local anesthetics to the epidural is usually avoided to reduce any further hypotension from profound decreases in vascular resistance due to sympathetic nervous system blockade. Following such epidural techniques, cats should be closely monitored for associated hypotension. Although there have been concerns that sevoflurane may not be safe for use in AKI or CKD due to the production of potentially nephrotoxic compound A (in rodents) and inorganic fluoride, no adverse effects have been shown in clinical patients and sevoflurane can be used in these patients, as can isoflurane and desflurane [57,61–63]. Intraoperative anesthetic monitoring is essential for the risk management of renal transplant patients. For example, intraoperative hypoxemia is associated with reduced overall survival rates [13]. Thus, monitoring includes pulse oximetry, capnometry, inhalant agent levels, electrocardiography, and core body temperature. In addition, intraoperative hemodynamic monitoring and management are imperative to ensure reasonable organ perfusion pressure, yet not subject the patient to fluid overload. Although CVP does not always correlate well with the patient’s overall fluid status, acute CVP changes may indicate impending fluid overload. However, this relationship is still debated [64]. Pulse pressure variation or pleth variability index may be better indices of fluid status in the mechanically ventilated patient, although their usefulness in cats have not been fully investigated [65]. Invasive blood pressure should be closely monitored since patients may experience normo‐, hypo‐, or hypertension throughout the procedure and into the postoperative period. An arterial catheter should be placed in the dorsal pedal or femoral artery; however, the descending aorta or its major branches may be occluded during renal artery anastomosis, and the signal will be lost during this period. The coccygeal artery may be used but can be difficult to keep clean postoperatively, which may negate its use in an immunosuppressed patient. Care in handling these catheters is essential as patients may be purposely heparinized and excessive bleeding at the puncture site may occur. Indirect blood pressure measurement using an ultrasonic Doppler flow detector or oscillometric technique applied to the front limb should be performed concurrently with invasive monitoring as these indirect techniques can be used during aortic occlusion and/or if an artery cannot be catheterized; however, they can be less accurate depending on circumstances [66–70]. Intravenous fluid therapy in human transplant surgeries has recently been addressed [71]. Large crystalloid volumes are not recommended, but accelerated fluid administration during the initial period of graft ischemia may improve subsequent kidney function. Thus, feline fluid rates of 3–5 mL/kg/h based on the individual patient’s needs and comorbidities (e.g., heart disease) with small, accelerated (3–5 mL/kg) fluid boluses over approximately 15 min as needed during ischemia are recommended. These guidelines also suggest that a balanced electrolyte solution should be used; 0.9% sodium chloride is not recommended due to extracellular shifts in serum potassium, increases in serum chloride, and a decrease in pH (hyperchloremic acidosis) [71–74]. In fact, hyperkalemia does not worsen with balanced solutions, and 0.9% sodium chloride can actually result in significant metabolic disorders [71–74]. Synthetic colloids such as hydroxyethyl starches should not be used due to potential adverse effects such as coagulopathies, reticuloendothelial system dysfunction, and delayed or impaired renal function [71,75]. If patients are normovolemic during surgery, yet remain hypotensive under general anesthesia, β‐adrenergic receptor agonists, such as dobutamine, can be used to increase cardiac output. The use of dopamine remains controversial because of species differences in receptor pharmacology and potential increases in systemic vascular resistance with higher doses [45]. If the patient cannot tolerate further fluid loading, titrated vasopressors, such as norepinephrine, may be considered to treat hypotension, despite the risk of renal vasoconstriction. In humans, norepinephrine use does not have a negative effect on recipient graft function since the harmful effects of systemic hypotension likely outweigh the potential renal vasoconstriction caused by norepinephrine [76,77]. However, this has yet to be tested in clinical veterinary transplant patients.
44
Anesthetic Considerations for Renal Replacement Therapy
Introduction
Intracorporeal techniques
Renal transplantation
Ethical considerations
Preoperative considerations
Anesthetic management
Kidney donor management
Agent
Dose/Route
Preanesthetic sedatives/analgesics
Benzodiazepines
Midazolam
0.05–0.2 mg/kg IV, IM
Diazepam
0.05–0.2 mg/kg IV
Opioids
Fentanyl
1.0–5.0 μg/kg IV
Hydromorphone
0.05–0.1 mg/kg IV, IM
Methadone
0.2–0.5 mg/kg IV, IM
Induction agents
Propofol
1.0–6.0 mg/kg IV to effect
Alfaxalone
0.5–2.0 mg/kg IV to effect
Maintenance agents
Inhalants
Desflurane
Minimal concentrations to effect
Isoflurane
Sevoflurane
Opioids
Fentanyl
2–20 μg/kg/h IV
Postoperative analgesics
Opioids
Fentanyl
1–2 μg/kg/h IV with careful monitoring
Buprenorphine
20–30 μg/kg IV, TM
Methadone
0.2–0.5 mg/kg IV, IM
Kidney recipient management

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