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Service de médecine zoologique, Département de sciences cliniques, Faculté de médecine vétérinaire, Université de Montréal, 3200 rue Sicotte, Saint-Hyacinthe, Quebec J2S 2M2, Canada
Fluid therapy is one of the most important treatments in cases of kidney disorders in birds. The choice between oral, subcutaneous, intravenous, and intraosseous routes depends on the patient and its needs.
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Elevated dietary protein alone does not seem to be the underlying etiology of gout in all avian species because diets as high as 70% protein failed to induce gout in adult cockatiels.
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The efficacy of allopurinol remains controversial in avian medicine and its use has not been reported in many avian species.
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Surgical procedures, such as nephrectomy or renal transplantation, are not advisable in birds owing to the anatomic constraints of the avian kidney.
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No effective therapy is recognized in birds with renal neoplasia.
Introduction
As in mammals, avian renal disease may be classified as acute or chronic. Acute renal failure results from an abrupt decrease in renal function, often caused by an ischemic or toxic insult.
Causes of kidney disease may be classified as prerenal, renal, postrenal, or of mixed origin. A prerenal origin is characterized by hypoperfusion of the kidney. Conditions that commonly lead to the development of prerenal hyperuricemia include dehydration, hypovolemia, and congestive heart failure. Renal origin of kidney disease refers to an intrarenal process, leading to a dramatic decrease in the glomerular filtration rate. In birds, a decrease in glomerular filtration rate can either be a sign of renal disease or an appropriate physiologic response to water restriction.
Plasma exogenous creatinine excretion for the assessment of renal function in avian medicine. Pharmacokinetic modeling in racing pigeons (Columba livia).
Causes of renal disease in the avian patient include infectious nephritis, hypovitaminosis A, heavy metal intoxication, and renal neoplasia. Postrenal hyperuricemia occurs when there is a disruption of the integrity of the urinary tract or an obstruction of urine outflow (eg, urolithiasis).
The treatment of avian renal disease relies on supportive care such as fluid therapy and nutritional support. Analgesia and adaptations of the environment are indicated in cases of renal disease associated with painful joints or spinal nerve compression. Other treatments vary with the underlying etiology and may include systemic antibiotics, antifungal therapy, vitamin A supplementation, chelation therapy, and agents to lower uric acid levels such as allopurinol. Potentially nephrotoxic drugs should be used with extreme caution in patients with renal disease. Additionally, drugs that are excreted through the kidney may fail to reach therapeutic plasma levels in polyuric birds or reach toxic levels if drug excretion and elimination are impaired.
fluid therapy constitutes one of the most important treatments in cases of kidney disorders in birds. Uric acid is eliminated by active tubular secretion
Fluid type is selected based on results of biochemical analyses, evaluation of blood electrolytes, glucose, and acid–base status. When these values are not known, a balanced isotonic crystalloid solution, such as lactated Ringer’s solution may be used for rehydration and hemodynamic support.
Caution is recommended when using colloid fluids in patients with renal disease by extrapolation from mammals.
Route of administration
Depending on the clinical circumstance, fluids can be administered by oral, subcutaneous, intravenous (IV), and/or intraosseous (IO) routes. Fluids are often administered by mouth by gavage with liquid oral nutrition. This route is generally safe and adequate for avian patients that are not in shock or debilitated.
In birds with mild dehydration, fluids can also be provided subcutaneously. Subcutaneous fluids can be administered in the inguinal (Fig. 1), interscapular, or axillary regions. Volumes as great as 20 mL/kg may be administered in 1 location.
Subcutaneous fluids are easily delivered using a butterfly needle, which allows the animal to move without the needle being pulled out. Practitioners unfamiliar with avian anatomy should beware of the thin skin and the presence of abdominal air sacs close to the inguinal region. Thus, it is key to remain steady during the procedure and to firmly hold the leg in extension to avoid inadvertent coelomic puncture. Fluids given subcutaneously and by mouth are poorly absorbed if hypovolemic shock is present.
Fig. 1Subcutaneous injection of fluids in the inguinal region of a Fisher’s lovebird (Agapornis fisheri). An operator manually restrains the bird. The bird’s leg is gently pulled forward, revealing a translucent cutaneous fold between the body and the leg, proximally and medially to the quadriceps muscle.
(Courtesy of O. Cojean, méd vét, IPSAV, Saint-Hyacinthe, Canada).
The choice between these routes depends on patient size, patient temperament, and the volume of fluids needed. IV catheters may be used for initial fluid therapy, but do not have the stability of an IO catheter. Permanent supervision of birds with IV catheters is also required to prevent fatal hemorrhage in case of accidental removal of the catheter.
IO catheters can be placed quickly, are stable and reliable, and are relatively easy to maintain, but placement is more painful. Fluids can also be provided in a larger bolus by the IO route than the IV route.
IV catheterization often requires sedation or general anesthesia to avoid stressful physical restraint. Jugular and ulnar catheters must be sutured in place.
Fig. 3Placement of a 24G catheter in the medial metatarsal vein of an Amazon parrot. The vein is manually occluded at the level of the proximal tibiotarsus.
(Courtesy of I. Langlois, DVM, DABVP, Knoxville, TN.)
Fig. 4A cockatiel (Nymphicus hollandicus) receiving fluid therapy via an IO catheter in the right ulna. The wing has been taped to the body. The patient is weak and thus does not need an Elizabeth collar.
(Courtesy of C. Grosset, méd vét, CES, IPSAV, DACZM, Saint-Hyacinthe, Canada.)
Palpate the styloid process of the distal ulna on the dorsal aspect of the wing.
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Pluck the feathers over the surrounding site and prepare aseptically.
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Ideally use a 20- to 25-gauge short spinal needle.
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Flex the distal wing tip and grasp the ulna between the fingers of one hand. With the other hand, the spinal needle is inserted just ventral to the condyle and directed proximally toward the elbow along the ulnar shaft (Fig. 5A, 5B).
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Apply gentle pressure as the bevel of the needle is rotated, allowing the needle to cut through the cortex of the bone and enter the medullary cavity.
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If the lumen of the needle becomes plugged, the needle may be removed and replaced.
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Check the patency of the catheter with a small amount of heparinized saline. Visualize flow in the ulnar vein as the fluid is injected (Fig. 5C).
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Two orthogonal radiographic views may also be obtained to confirm correct placement.
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Secure the catheter with butterfly taping and by suturing this tape to the skin, if necessary.
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Place a figure-of-eight wing bandage to minimize wing movement.
Placement of an IO catheter in the proximal tibiotarsus
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Flex the stifle, and palpate the cnemial crest at the proximal anterior surface of the tibiotarsus, just distal to the knee joint.
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Insert the needle at the cnemial crest at, or to either side of, the insertion of the patellar tendon, to avoid penetration of the stifle joint.
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Secure the catheter in place with tape.
Fig. 5Placement of an IO catheter in the ulna of an avian patient (see Box 1). (A) Computed tomography scan of an African gray parrot (Psittacus erithacus). Dorsal view of the right wing. The white arrow indicates the site and axis of insertion of the catheter in the ulna. (B) After aseptic preparation of the site and appropriate analgesic protocol administration, the ulna is grasped between the fingers. Palpate the styloid process of the distal ulna on the dorsal aspect of the wing. The needle is inserted in the distal ulna and directed proximally. (C) Check the patency of the catheter by using a small amount of heparinized saline flush. Visualize the flow in the ulnar vein as the fluid is injected.
(Courtesy of [A] S. Larrat, méd vét, MSc, DES, DACZM, Brech, France; and [C] M. Desmarchelier, DVM, MSc, DACVB, DACZM, DECZM, Saint-Hyacinthe, Canada.)
Some birds may benefit from an Elizabethan or cervical restraint collar; however, these devices can be extremely stressful to some birds and may adversely affect patient condition. The ability to tolerate a collar should be assessed in each patient
Daily maintenance fluid requirements have not been determined in birds; however, the recommendations of different authors range from 50 to 150 mL/kg/d, with the higher end of the range expected in smaller species.
Maintenance plus one-half of the estimated fluid deficit is generally administered over the first 12 to 24 hours, with the remainder of the deficit replaced over the following 48 hours.
Fluids should be warmed to body temperature. Depending on the patient’s condition and species, the author will typically give 50 to 100 mL/kg of fluid twice a day subcutaneously, IV, IO, or via a combination of routes.
Owners may offer fruit juice without added sugar or infant electrolyte replacement solution (Pedialyte, Abbott, Saint-Laurent, Quebec, Canada) full strength or diluted with water. Owners can also increase the proportion of fruits and vegetables in the diet or offer moistened seeds or other foods like warm, unsalted vegetable soup. Caretakers may float seeds in the water bowl to encourage drinking behavior. Regular access to a shower or bath can also promote drinking, acknowledging that individual birds vary greatly in the ways they choose to bathe. Some birds love the feeling of a trickling shower, some enjoy daily misting with a spray bottle, and some like to dunk themselves in a pool of water.
If none of these measures prove adequate and the bird is still not drinking in sufficient amounts, the owner can use a plastic eyedropper, syringe, or straw with finger kept over 1 end to slowly offer fluids directly into the beak, followed by positive reinforcement like verbal praise. Reserve this method as a last resort and inform owners of the risk of fluid aspiration.
Nutritional Supportive Care
Patients with renal disease should be monitored for weight loss and appropriate nutritional support should be offered as needed.
By extrapolation, few commercial diets low in proteins have been formulated for birds with renal insufficiency (eg, Roudybush AK formula; Woodland, CA), although evidence-based data on whether protein restriction is beneficial in birds are lacking. Precise protein content and composition is also not disclosed for this diet.
Renal lesions, such as gout, have been associated with excess dietary protein in birds, but only under specific conditions.
In 1 study, a 42.28% protein diet fed to 18-day-old broiler chicks for 15 weeks induced multiple renal abnormalities, primarily nephrosis and visceral gout.
In another study, diets high in urea were linked to outbreaks of nephritis in poultry16, however, cockatiels (Nymphicus hollandicus) fed high dietary protein (up to 70%) for 11 months did not develop renal lesions. The cockatiels were able to upregulate enzymes associated with amino acid catabolism and uric acid synthesis.
Of note, these cockatiels received a gradually increasing protein concentration in their diet over 3 weeks. Uric acid increased linearly with dietary protein levels, but remained within normal limits in these birds, indicating that hyperuricemia is specific of renal disease or severe dehydration in granivorous avian species. Because the nutritional requirements vary among avian species, it is unknown if these conclusions can be extrapolated to other birds. Unlike carnivorous birds, granivorous species have low requirements for dietary amino acids and seem to be able to conserve amino acids by tight regulation of amino acid catabolism.
A safe recommendation is that birds with hyperuricemia should not consume diets with protein levels greater than what is considered normal for the given species.
Omega-3 fatty acid supplementation has been shown to decrease the risk of chronic renal disease and delay the progression of disease in dogs and humans.
These cytokines are proinflammatory and vasoactive, which promotes chronic kidney disease progression, owing to renal free radical production and antioxidant depletion.
In humans, the positive effects of the polyunsaturated fatty acid eicosapentaenoic acid (EPA) are more pronounced than those of α-linolenic acid, another omega-3 fatty acid.
Concentrated sources of longer chain omega-3 fatty acids (such as EPA and docosahexanoic acid) are limited to fish and other marine products and algal-based sources.
Most psittacine diets are highly enriched in omega-6 fatty acids (primarily linoleic acid) and limited in omega-3 fatty acids (Table 1). Of note, diets high in polyunsaturated fatty acids require additional antioxidants to prevent lipid peroxidation during storage.
; however, the palatability of fish oil may be an issue when supplementing psittacine birds at home. Being carnivorous, some birds of prey are more likely to accept fish oil in their diet. In cases of concomitant gout, ensure the patient receives a plant-based source of EPA or docosahexanoic acid rather than a fish oil source, which may have higher purine levels
Severe dehydration and many forms of renal disease, including obstructed ureters, can result in decreased uric acid elimination thus causing hyperuricemia.
Fluid therapy (combined with medications for hyperuricemia if needed) is generally continued until uric acid decreases to either normal or mildly increased levels (10–20 mg/dL) and the bird demonstrates signs of improvement, such as eating or increased activity.
The use of medications for hyperuricemia is extrapolated from human medicine, and the safety and efficacy of these treatments are often lacking in birds. These drugs have been poorly studied in psittacine birds and should only be used with close monitoring of uric acid levels.
Xanthine oxidase inhibitors
Xanthine oxidase inhibitors, such as allopurinol and febuxostat, decrease uric acid synthesis. The efficacy of allopurinol in avian medicine is controversial; information is available for only a limited number of species. In broilers, uricemia was reduced as well as xanthine oxidase and xanthine dehydrogenase activity in the kidney in birds treated with allopurinol (25 mg/kg by mouth).
Toxicity has been reported following administration of allopurinol in red-tailed hawks (Buteo jamaicensis). Vomiting developed at 50 mg/kg by mouth every 24 hours and was attributed to the accumulation of oxypurinol, a metabolite that worsens renal gout.
Allopurinol given at 25 mg/kg by mouth every 24 hours to red-tailed hawks was shown to be safe, but had no significant effect on plasma uric acid concentrations. Based on the lack of response at a dose of 25 mg/kg and the toxic effects at 50 mg/kg, allopurinol is not recommended in the red-tailed hawk.
It is unknown whether this finding should be extrapolated to psittacine birds.
Uricase
Uricase oxidizes uric acid to allantoin in humans. Little information is available in veterinary medicine. Poultry on a high-protein diet developed hyperuricemia, which was reversed with uricase injection.
In a more recent study, the uricolytic properties of uricase were studied in a granivorous bird (pigeon, Columba livia domestica) and a carnivorous avian species (red-tailed hawk). Plasma concentrations of allantoin and uric acid were determined in experimental groups before and after receiving 100, 200, and 600 UI/kg uricase intramuscularly once daily. All regimens caused a significant decrease in plasma uric acid concentrations within 2 days after the first administration, when compared with controls. Plasma allantoin concentrations were also significantly higher when compared with controls, suggesting a similar mechanism of action in these species.
Investigations into the uricolytic properties of urate oxidase in a granivorous (Columba livia domestica) and in a carnivorous (Buteo jamaicensis) avian species.
In turkeys diagnosed with articular gout, colchicine administered at 0.18 mg/kg by mouth every 24 hours for 7 days failed to influence uric acid concentrations.
No controlled study on colchicine has been published in birds.
Uricosuric drugs
Uricosuric drugs, such as probenecid, promote uric acid excretion by the kidneys. Uricosuric drugs are contraindicated when tubular urate crystals are present, which is frequently seen in birds.
Birds with renal disorders may suffer from pain caused by articular gout or nerve compression secondary to renal masses (Fig. 6). Affected birds are likely to spend more time on the cage floor and suffer from impaired locomotion. Husbandry adaptations and pain control are required to improve their quality of life.
Fig. 6Articular gout secondary to renal disease in a budgerigar parakeet (Melopsittacus undulatus).
(Courtesy of C. Grosset, Dr méd vét, CES, IPSAV, DACZM, Saint-Hyacinthe, Canada.)
Water and food dishes can be placed as close to the bird as possible. Containers of different shapes and depths can stimulate consumption. Replace standard perches with perches of a larger diameter and ladders or ramps that allow the bird to use its beak. Once the bird is unable to perch normally, the claws may need to be trimmed and shaped more frequently than in a healthy bird. Patients with gout should not be restricted in their movements, and instead should be housed in as large a cage as possible. The minimum size considered adequate allows the bird enough space to spread its wings without hitting either the sides of the cage or other perches.
Pain management is paramount in birds with articular gout or nerve compression by renal masses (Table 2). Long-term treatment with opioids may be considered. Intra-articular injections of corticosteroids are administered to humans with only 1 joint affected by gout,
but this treatment modality has not been investigated in birds. The effectiveness of intra-articular bupivacaine injections in the suppression of osteoarthritic pain has also been demonstrated in humans.
Evaluation of a protocol for determining the effectiveness of pretreatment with local analgesics for reducing experimentally induced articular pain in domestic fowl.
It was concluded that the optimum intra-articular dose of bupivacaine for the treatment of musculoskeletal pain in the domestic fowl was 3 mg bupivacaine in 0.3 mL saline.
Evaluation of a protocol for determining the effectiveness of pretreatment with local analgesics for reducing experimentally induced articular pain in domestic fowl.
Physical modalities such as thermotherapy and laser may also be used to diminish pain. Low-level laser therapy (660 nm, 9 J/cm2) has been shown to decrease neuropathic pain.
Pharmacokinetics of butorphanol tartrate in a long-acting poloxamer 407 gel formulation administered to Hispaniolan Amazon parrots (Amazona ventralis).
Alternatively, after discussion with owners of the safety versus quality of life balance, the use of nonsteroidal anti-inflammatory drugs may be considered as a palliative treatment. A study in Hispaniolan Amazon parrots (Amazona ventralis) indicated 1.3 mg/kg by mouth every 12 hours of meloxicam to be a therapeutic dosage for relief of arthritic pain.
Both severe gout and renal tumors carry a poor prognosis; therefore, euthanasia must be considered when analgesia and husbandry modifications fail to ensure an appropriate quality of life for the patient.
(1–10 mg/kg by mouth every 12 hours) and sucralfate (25 mg/kg by mouth every 8 hours) staggered 2 hours apart from other oral treatments.
Chronic anemia owing to decreased erythropoietin secretion is challenging to manage because avian erythropoietin is structurally different from that of mammals.
The use of dialysis has not been described in birds and coelomic dialysis is not possible in the avian patient owing to the presence of abdominal air sacs. Renal transplantation has also never been described in avian medicine and is unrealistic given the position of the kidneys immediately ventral to the synsacrum, adjacent to air sacs, and in close relation with pelvic nerves.
Specific therapy for renal disease
In avian species, renal diseases are caused by various etiologies, including infectious nephritis (bacterial, viral, parasitic, fungal), renal neoplasms, toxic exposure, and nutritional disorders.
Specific treatment options vary depending on the cause.
Bacterial Nephritis
Many bacteria have been reported to cause nephritis in birds, including Enterobacteriaceae, Pasteurella spp., Pseudomonas spp., Streptococcus spp., Staphylococcus spp., Listeria monocytogenes, Erysipelothrix rhusiopathiae, and chlamydial organisms.
Cloacal samples may also be used owing to the possibility of ascending infection but may not be reliable. In cats and dogs, bacterial nephritis is treated for at least 4 to 6 weeks.
Pending culture and sensitivity results, empirical broad-spectrum antibiotics that provide excellent therapeutic levels within renal tissue should be initiated such as β-lactams, trimethoprim-sulfamethoxazole, or fluoroquinolones.
Unusual and severe lesions of proventricular dilatation disease in cockatiels (Nymphicus hollandicus) acting as healthy carriers of avian bornavirus (ABV) and subsequently infected with a virulent strain of ABV.
Treatment of viral nephritis usually relies on nonspecific supportive care.
Parasitic Nephritis
Renal coccidiosis is the most common cause of parasitic nephritis. Renal diseases caused by the coccidian Eimeria spp. have been reported in several species, including juvenile waterfowl,
Schizonts of Leukocytozoon spp., Plasmodium spp., and Haemoproteus spp. have been identified in avian renal tissue and associated with lymphoplasmacytic inflammation.
Renal trematodes and cestodes have also been reported in multiple species of bird housed outdoors, including order Columbiformes, Passeriformes, Anseriformes, Psittaciformes, and Galliformes.
Antiparasitic treatments vary greatly depending on the species and life cycle of the parasite, with ponazuril (20 mg/kg by mouth every 24 hours for 7 days) or toltrazuril (25 mg/kg by mouth once a week) being used for coccidia, and praziquantel (10 mg/kg subcutaneously 2 times 10 days apart) for trematodes and cestodes.
its use is not approved in food animal species in many countries. Practitioners should consult local regulations for approved anticoccidial agents. Monensin has been used for the treatment of renal coccidiosis, but is toxic in turkey and guinea fowl.
and rotation of anticoccidial drugs is recommended to minimize the risk of resistance. Natural products, such as cider vinegar, are also emerging as alternative strategies to control avian coccidiosis.
IV administration quickly establishes fungicidal concentrations, making amphotericin B a frequent choice for initial therapy. The use of amphotericin B has been associated with nephrotoxicity in mammals
; however no evidence of nephrotoxicity has been documented in birds. This difference may be associated with the shorter elimination half-life in birds compared with mammals after IV administration of amphotericin B.
In combination with early, systemic antifungal therapy, topical amphotericin B can be administered through a polypropylene tube during endoscopic or surgical procedures.
Topical therapy is recommended when renal lesions can be easily debrided to maximize drug concentrations in tissues; however, in many patients granulomas cannot be reached endoscopically.
Itraconazole, fluconazole, and voriconazole are the most studied azoles in birds. The relative toxicity of an azole depends on the affinity to fungal cytochrome P450 enzyme, compared with its affinity to the avian cytochrome P450.
Regular bile acid monitoring is recommended during treatment for early detection of hepatic adverse effects. Itraconazole is a first-generation triazole antifungal agent, commonly used in birds for treatment of aspergillosis.
Voriconazole is increasingly used to treat invasive aspergillosis in birds, given the broad antifungal spectrum, which includes molds (fungicidal) and yeasts (fungistatic), and its rapid bioavailability.
Studies have documented dose- and species-dependent variability, suggesting that different dosage regimens of antifungals may be required for different species of birds (Table 3).
If itraconazole is used owing to monetary constraints, doses of 2.5 mg/kg PO q12–24 h have been used safely with frequent monitoring of plasma bile acid levels
Voriconazole is usually preferred over itraconazole owing to toxicity reports in African gray parrots
5 mg/kg PO q24 h or 10 mg/kg PO q48 h or 100 mg/L in the drinking water
Fluconazole has the safest therapeutic index of the azoles.
Described doses resulted in plasma levels that exceeded human MIC for most strains of Candida albicans generally less effective against aspergillosis than itraconazole.
Partial response to treatment with fluconazole (15 mg/kg by mouth every 12 hours) and terbinafine (15–20 mg/kg by mouth every 12 hours) was described in an African gray parrot (Psittacus erithacus) with renal cryptococcosis.
but an umbrella cockatoo (Cacatua alba) with keratoconjunctivitis associated with microsporidia was successfully treated with albendazole (25 mg/kg by mouth every 24 hours) for 90 days.
Careful monitoring of renal parameters is important for the duration of chelation therapy. Elevated uric acid levels can be observed with heavy metal poisoning and improvement of hyperuricemia with therapy has been reported.
Succimer (meso 2,3-dimercaptosuccinic acid or DMA) is an oral chelator, derived from British Anti-Lewisite capable of chelating lead from soft tissues, but not from bone.
In an experimental trial with induced lead intoxication in cockatiels, a dose of 40 mg/kg by mouth every 12 hours was found to be safe, whereas a dose of 80 mg/kg by mouth every 12 hours was associated with a high mortality rate.
Evaluation of gastrointestinal tract transit times using barium-impregnated polyethylene spheres and barium sulfate suspension in a domestic pigeon (Columba livia) model.
Fluid therapy and supportive care are also indicated. Some authors recommend the use of activated charcoal (1 g/kg or 1–3 mg/g body weight) as an adsorbent.
This treatment is not recommended for acids or corrosive alkaloid agents because it will be useless and may complicate retrieval from the crop. For more information regarding treatment of avian intoxications, the reader should refer to the excellent review by Lightfoot and Yeager.
Hypovitaminosis A can lead to squamous metaplasia of renal epithelium, ureteral mucosa, and collecting ducts leading to obstruction of the ureters and secondary hydronephrosis, hyperuricemia, and oliguric or anuric renal failure.
Vitamin A may be supplemented at 2000 to 5000 IU/kg intramuscularly, then repeated every 1 to 3 weeks depending on patient condition and response. Of note, fat-soluble vitamin A is considered safer than water-soluble vitamin A.
Vitamin A supplements are also available in powder form. Beta-carotenes and other provitamin A carotenoids can serve as a safer alternative to potentially toxic vitamin A in psittacine birds.
Seeds and nuts are generally low in carotenoids, whereas some orange-colored fruits and vegetables, such as carrots, melon, and butternut squash, can provide large quantities thereof.
Some avian species, such as recessive white canaries (Serinus canaria), are unable to convert ß-carotene to vitamin A and require 3 times as much vitamin A as colored canaries.
Excess vitamin D3 promotes metastatic mineralization of viscera, including the kidneys. Vitamin D3 is considered toxic at 4 to 10 times the recommended dose. Any bird species can potentially be susceptible to hypervitaminosis D
; however the dietary requirements for vitamin D vary among avian species, with optimum levels at 200 IU/kg in poultry, 900 IU/kg in turkey, and 1200 IU/kg in Japanese quail.
In cases of hypervitaminosis D associated with hypercalcemia, fluid therapy and treatments stimulating calciuresis, such as bisphosphonates and corticosteroids, are recommended in dogs and cats.
Unfortunately, the use of corticosteroids is controversial in birds owing to the risk of associated immunosuppression and safe doses of bisphosphonate have not been described in birds. Because metastatic calcifications are irreversible, prognosis is guarded.
Iron overload
Iron storage disease results from the accumulation of iron in various tissues, including the kidneys.
High dietary iron has been implicated in the development of iron storage disease in susceptible species, such as hornbills, toucans, lories, and lorikeets, as well as mynahs and other Sturnidae.
The high vitamin C content of many fruits also enhances dietary iron uptake. Frugivorous species should be offered fruits low in vitamin C to minimize uptake of iron from commercial diets.
Another common strategy is to soak commercial pellets in black tea (first discard the water after initial infusion to avoid caffeine administration, then add water again to the cup and let the pellets soak) to increase the amount of tannins in the food and thereby decrease iron absorption. Soaking should be done every other month to avoid causing other mineral deficiencies.
In case of renal hemochromatosis, treatments described in birds include therapeutic venipunctures to decrease hematocrit, oral deferiprone, or intramuscular deferoxamine injections (Table 4).
Table 4Treatments of hemochromatosis in selected avian species
In rare instances, changes to digestive microbial flora may affect the cloacal environment and contribute to the formation of cloacoliths. A cloacolith composed of 100% uric acid was reported in a blue-fronted Amazon parrot fed a mixture of table food, seeds, and pellets.
Cloacoliths can obstruct the ureteral opening and cause postrenal hyperuricemia. Cloacoliths can usually be disintegrated and removed with forceps via the cloaca with or without endoscopic assistance.
Ureteroliths have also been described in a double yellow-crowned Amazon parrot (Amazona ochrocephala), a chestnut-bellied seed finch (Oryzoborus angolensis), and in poultry.
Machado C, Mihm F, Buckley DN. Disintegration of kidney stones by extracorporeal shockwave lithotripsy in a penguin. Proceeding of first international conference of zoological avian medicine. Oahu Hawaii, September 6–11, 1987. p. 343–9.
Renal carcinoma is the most common renal neoplasm reported. Other renal neoplasms reported include renal adenoma, nephroblastoma, cystadenoma, and lymphoma.
in: Kahn C.M. Line S. The Merck veterinary manual. Non-infectious diseases of the urinary system in small animals. 9th edition. John Wiley and Sons,
Summerset, (South Dakota)2005: 1249-1288
In birds, unless the renal neoplasm is contained and pedunculated, surgical removal is virtually impossible because of the kidney’s dorsal location, its intricate relationship with adjacent vessels and nerves,
the limited access to the renal arteries, and the short distance between the renal artery and the aorta, which make ligation or hemostasis difficult if not impossible.
in: Kahn C.M. Line S. The Merck veterinary manual. Non-infectious diseases of the urinary system in small animals. 9th edition. John Wiley and Sons,
Summerset, (South Dakota)2005: 1249-1288
Chemotherapy has not been thoroughly evaluated for avian renal tumors. Carboplatin was used to treat renal adenocarcinoma in a budgerigar, resulting in a short-lived clinical improvement but the mass continued to grow.
Radiation therapy for renal tumors has been rarely performed owing to questionable tolerance of adjacent tissues. In the case of a black swan (Cygnus atratus) presented with chronic T-cell lymphocytic leukemia affecting the kidneys, whole body radiation therapy with 2 Gy was performed over 31 days, in addition to chemotherapy with chlorambucil, followed by lomustine, l-asparaginase, and prednisone.
The swan survived more than 1 year after treatment initiation and was euthanized owing to hyperviscosity syndrome associated with the leukemia. The white blood cell count decreased after radiation therapy and no adverse effects to radiation were detected clinically or at necropsy in this swan. The dose received was much lower than tolerable radiation doses evaluated in ring-necked parakeets (Psittacula krameri).
Further studies are needed on the use of radiation therapy in birds for radiosensitive neoplasms.
Summary
The clinical management of bird with renal disease may prove challenging. Treatment choice is highly impacted by the cause and chronicity of the disease. The specific physiology of avian kidneys, and the large variety of species encountered in clinic implies that only a small part of the knowledge about mammalian therapeutics can be extrapolated to birds. More studies on renal disease treatments and their specific applications are warranted.
References
Grauer G.F.
Management of acute renal failure.
in: Elliott J. Grauer G.F. Manual of canine and feline nephrology and urology. 2nd edition. BSAVA,
Gloucester (England)2007: 215-222
Plasma exogenous creatinine excretion for the assessment of renal function in avian medicine. Pharmacokinetic modeling in racing pigeons (Columba livia).
Investigations into the uricolytic properties of urate oxidase in a granivorous (Columba livia domestica) and in a carnivorous (Buteo jamaicensis) avian species.
Evaluation of a protocol for determining the effectiveness of pretreatment with local analgesics for reducing experimentally induced articular pain in domestic fowl.
Pharmacokinetics of butorphanol tartrate in a long-acting poloxamer 407 gel formulation administered to Hispaniolan Amazon parrots (Amazona ventralis).
Unusual and severe lesions of proventricular dilatation disease in cockatiels (Nymphicus hollandicus) acting as healthy carriers of avian bornavirus (ABV) and subsequently infected with a virulent strain of ABV.
Evaluation of gastrointestinal tract transit times using barium-impregnated polyethylene spheres and barium sulfate suspension in a domestic pigeon (Columba livia) model.
Machado C, Mihm F, Buckley DN. Disintegration of kidney stones by extracorporeal shockwave lithotripsy in a penguin. Proceeding of first international conference of zoological avian medicine. Oahu Hawaii, September 6–11, 1987. p. 343–9.
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