Comparing the Effects of Stage and Duration of Retinoic Acid Exposure on Amphibian Limb Development: Chronic Exposure Results in Mortality, Not Limb Malformations

Sigmund J. Degitz1, Gary W. Holcombe, Patricia A. Kosian, Joseph E. Tietge, Elizabeth J. Durhan and Gerald T. Ankley

U.S. Environmental Protection Agency, Mid-Continent Ecology Division, 6201 Congdon Boulevard, Duluth, Minnesota 55804

Received January 11, 2003; accepted March 25, 2003


    ABSTRACT
 TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Recently, high frequencies of malformations have been reported in amphibians across the United States. It has been suggested that the malformations may be the result of xenobiotic disruption of retinoid signaling pathways during embryogenesis and tadpole development. Therefore, a series of experiments were undertaken to examine life-stage specific effects of continuous retinoid exposure on Xenopus laevis. Continuous all-trans retinoic acid (RA) concentrations were delivered using a column saturator and a flow-through diluter system. Stage 8 embryos were exposed to RA concentrations ranging from 0.013 to 2 µg/l. At the onset of hindlimb bud emergence (NF stage 48), a subset of tadpoles was moved to clean water, and remaining organisms were exposed continuously through metamorphosis. In addition, early limb-bud–stage tadpoles were exposed for 1 week, 2 weeks, or until tail resorption was complete, to eight concentrations of RA in the range of 0.031–3 µg/l. RA exposure resulted in a concentration-dependent increase in mortality and dysmorphogenesis in embryos at concentrations of 0.24 µg/l and above. However, this early embryonic exposure did not result in hindlimb abnormalities in surviving tadpoles allowed to mature in clean water. RA did not induce limb malformations in any surviving tadpole exposed during larval stages. We are confident that the concentrations used were high enough, given that the highest concentration used resulted in 100% mortality within 2 weeks of initiating the exposure. This result suggests that other aspects of growth and development, which are not externally obvious, are more sensitive to retinoids than skeletal development. From these experiments and our previous work, we conclude that it is unlikely that retinoid mimics would produce the spectrum of limb malformations which recently have been observed in amphibians collected from the field.

Key Words: retinoic acid exposure; amphibian limb development, retinoid signaling pathways; limb malformations.


    INTRODUCTION
 TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Within the last decade, there has been increasing concern over reports of malformed amphibians (primarily Ranid) across North America. The most striking and of greatest public concern are malformations of the hindlimbs. These malformations can be grouped into two broad categories: supernumerary limbs or truncated/missing limbs. These observations have stimulated considerable research aimed at diagnosing the ultimate cause for the observed increases. The proposed causes include trematode infection, ultraviolet radiation, and xenobiotic chemicals. Although the cause of these malformations remains rather controversial, there is convincing experimental evidence that trematode infection and UV radiation can produce malformations characteristic of those observed in the field (Ankley et al., 1998Go, 2000Go, 2002Go; Johnson et al., 1999Go, 2001Go, 2002Go). Laboratory UV radiation and natural sunlight have both been shown to produce partial to near-complete truncation of the hindlimb (Ankley et al., 1998Go, 2000Go, 2002Go). In several studies, trematode infection has been shown to produce both supernumerary limbs and limbs with distal truncation (Johnson et al., 1999Go, 2001Go, 2002Go). More recently it was reported that trematode-induced malformations are more common in areas of agricultural runoff (Kiesecker, 2002Go), possibly suggesting an interaction between parasites and xenobiotic compounds. Further, it has been proposed that xenobiotic disruption of the retinoid signaling pathway may be involved (Gardiner and Hoppe, 1999Go). The hypothesis is based primarily on the striking similarities between the malformations observed in field specimens and those that can be produced in amphibians in the laboratory by retiniods (Degitz et al., 2000Go; Scadding and Maden, 1986aGo,bGo).

Retinoids are metabolic derivatives of vitamin A, which act as signaling molecules that regulate many processes critical to early embryonic development, including axial patterning, cellular differentiation, tissue induction, proliferation, and apoptosis (Sucov and Evans, 1995Go). Retinoids elicit their effects through binding to members of the steroid-thyroid nuclear receptor superfamily and regulating transcription of specific target genes. Alterations in retinoid levels, whether it is a condition of excess or deficiency, result in developmental anomalies in nearly all vertebrate species studied. The role of retinoids in vertebrate limb development has received considerable attention. When administered to regenerating amphibian limbs, retinoids induce proximo-distal and mirror-image duplications (Maden, 1983Go; Scadding and Maden, 1986aGo,bGo; Thoms and Stocum, 1984Go). In the chick, local application of retinoids affects limb pattern regulation by mimicing the effects of the zone of polarizing activity causing, anterior-posterior duplication (Summerbell, 1983Go; Tickle et al., 1982Go, 1985Go). One common feature of these amphibian and chick experiments is the employment of surgical manipulation of the limb tissue. In contrast, systemic pulsed exposure of developing limbs to retinoids does not result in limb duplication. Rather, treatment of developing bud-stage-stage mice (Kochhar, 1977Go; Kochhar et al., 1984Go) and amphibians (Degitz et al., 2000Go; Scadding and Maden, 1986aGo,bGo), in the absence of physical manipulation, results in concentration and developmental stage-dependent deletions and reduction of hindlimb skeletal segments.

Ideally, native Ranid species would be used to evaluate the potential for environmental retinoid mimics to affect embryonic and larval development. However, conditions for extended culture and breeding of Ranid species are not well defined, and the use of field collected embryos is limited to the natural breeding season. As an alternative, Xenopus laevis is a well-studied model of vertebrate development, for which a great deal of baseline data are available. In addition, previous studies suggest that the response to retinoids between native Ranids and X. laevis are similar (Degitz et al., 2000Go).

In the current study, we asked the following question. Does chronic exposure to retinoids during amphibian limb development cause malformations characteristic of those observed in the field specimens? RA was used because it is a potent ligand for the retinoic acid receptors and is the standard retinoid to which nearly all others are compared. We exposed X. laevis to RA continuously, either from stage 8 (Nieuwkoop and Faber 1994Go) to completion of metamorphosis, or for 1-week periods at critical stages of limb development. We found that RA produces obvious malformations when administered during embryogenesis, as would be expected. However, exposure during embryogenesis or limb development does not produce limb malformations in tadpoles not killed by the exposure to RA.


    MATERIALS AND METHODS
 TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Organisms.
Xenopus laevis adults (Carolina Biological, Burlington, NC) were injected with human chorionic gonadotropin (HCG; Carolina Biological, Burlington, NC) and allowed to go into amplexus. The eggs were collected, the gel coat removed by washing in 2% cysteine (pH 8.1) (Sigma Chemical, St. Louis, MO), and screened at stage 6 to determine viability. At stage 8, embryos were placed in 20 tanks in an electronic diluter (described below) at a rate of 60 embryos per tank. All organisms were maintained in a continuous flow of Lake Superior water at 22°C until exposures were initiated. After hatching, all tadpoles, regardless of treatment were fed a diet of trout starter/algae Tetrafin/brine shrimp three times daily.

Experimental Design
Embryonic exposure.
Starting at stage 8, Xenopus embryos were exposed to a range of nominal all-trans retinoic acid (Sigma Chemical Co., St Louis, MO) concentrations (0.012, 0.031, 0.052, 0.086, 0.144, 0.24, 0.6, and 2 µg/l) or Lake Superior water (two controls). Each treatment group consisted of 60 organisms. After 3 days of exposure 10 organisms from each treatment were removed and placed in fixative for later characterization of structural abnormalities by comparing exposed animal to controls. We sampled at 3 days because we found, in preliminary experiments, that several of the treatments resulted in mortality by 3 days, making it impossible to characterize the RA-induced malformations. After 9 days (when controls reached stage 48), 20 organisms for each treatment were removed and maintained in continuous flow of Lake Superior until tail resorption was complete (stage 65). The remaining organisms were continuously exposed to RA until stage 65. When tadpoles reached stage 65, they were removed from the test system, weighed, measured (snout-vent length), examined for gross malformations (controls were used for reference), and preserved in 95% ethanol.

Larval exposure.
At stage 48, X. laevis tadpoles were exposed to a range of nominal RA concentrations (0.031, 0.052, 0.086, 0.114, 0.24, 0.6, 2, and 3 µg/l) or Lake Superior water (controls). Each treatment group consisted of 60 organisms. After 7 or 14 days of exposure, 20 organisms from each treatement were removed and maintained in continuous flow of Lake Superior until stage 65. The remaining organisms were continuously exposed to RA until stage 65. Upon removal from the test system, organisms were weighed, measured (snout-vent length), examined for gross malformations (controls were used for reference), and preserved in 95% ethanol. The limb segments and digits of exposed animals were compared to controls

Exposure system.
Glass wool columns were constructed and as described by Kahl et al., 1999Go. Five hundred mg of RA was dissolved into ~70 ml of high-pressure liquid chromatography (HPLC)-grade acetone and stirred on a magnetic stir plate until dissolved. One half of the dissolved chemical was poured into one leg of a U-shaped column packed with glass wool. Columns were maintained under a nitrogen atmosphere while the chemical was added to the column leg and while the acetone was being evaporated. The solution containing the RA was pulled up and down the column leg (using a vacuum pump) until the acetone was completely evaporated and the RA coated onto the glass wool. This process was repeated using the remainder of the acetone/chemical solution on the other column leg. After evaporation was complete, neoprene stoppers were inserted in both ends of the column, and the stoppers were taped in place with duct tape. The columns were wrapped in aluminum foil (to limit photodegradation), and placed in a freezer until used for testing. Prior to testing, columns were flushed (using Lake Superior water that had been deoxygenated using nitrogen) at 11.0 ml/minute for 1 hour and at 5.0 ml per minute for an additional 23 hours to remove residual compound.

The delivery system consisted of two columns in series, with a new column being added to replace the oldest column every third day. Deoxygenated water was pumped through the columns at a rate of 1.5 ml/minute into a 30-ml pre-dilution cell. Of this volume, 0.36 ml/minute was pumped to the toxicant dilution cell of a computerized electronic delivery system. In this system, four high-volume Fluid Metering, Incorporated (FMI) pumps supplied water (two supplied control water, and two supplied water containing RA) to four sets of electronic solenoids. The computer fired each solenoid for a preprogramed amount of time to provide the amount of diluent water (control tanks) and diluent plus toxicant-laden water necessary to achieve the desired concentration in each exposure tank. All delivery lines were made of Teflon and kept in the dark to minimize the breakdown of the RA. Exposure tanks were glass aquaria (22.5 x 14.0 x 16.5 cm deep) equipped with 13-cm standpipes, which resulted in an actual tank volume of 4.0 l. The continuous flow rate to each tank was 85 ml/minute. Fluorescent lamps provided a light intensity that ranged from 61 to 139 lumens at the water surface. The photoperiod was 12 h light : 12 h dark.

Water analysis.
All laboratory procedures were conducted under amber lighting. Water samples (10 to 75 ml), were collected from the embryo and larval exposures three times the first week of the test and then once a week until test completion. The samples were placed in amber bottles; acetic acid was added to a strength of 20 mM; acetonitrile was added to a final volume of 45%. Samples were concentrated by processing through solid phase extraction (SPE). Briefly, 3-ml C18 SPE columns (J. T. Baker, Phillipsburg, NJ), fitted with 50-ml reservoirs, were precleaned with 10 ml dichloromethane, activated with 25 ml methanol, and rinsed with 5 ml of deionized water. The samples were then applied to the columns under mild negative pressure (5 mm Hg). Following sample addition, each column was washed with 3 ml aqueous acetonitrile (60:40 v/v) and lightly dried. The adsorbed RA was slowly eluted under vacuum (1 mm Hg) with four 500-µl aliquots of methanol. The eluate was evaporated under nitrogen to a known volume (e.g., 100 µl), transferred to an amber vial containing a microinsert, capped, and immediately analyzed for RA.

The SPE methanol concentrates and methanol-diluted samples were analyzed by reversed-phase HPLC. The HPLC system consisted of a Hewlett-Packard (HP) model 1100 pump and automatic liquid sampler (Hewlett-Packard, Avondale, PA) and a BAS model LC-4B amperometric electrochemical detector (Bioanalytical Systems, Lafayette, IN). An aliquot of each sample (30 µl) was injected directly onto an Adsorbosphere HS C18 5-µm column (Alltech, Deerfield, IL) and eluted isocratically with 100 mM sodium acetate in 65% acetonitrile and 2.5 % methanol (pH = 5, acetic acid) at a flow rate of 1.5 ml/min. Data were collected with HP ChemStation software, and RA concentrations were determined using the external standard method of quantification with a five point linear calibration curve. Routine (i.e., ~10 %) quality assurance analyses (blanks, duplicates, and matrix spikes) were conducted with each SPE sample set. Concentrations of RA in the water samples were corrected based on recovery data. The analytical quantification limit was 0.004 ng/ml. No RA was detected in the blanks from the X. laevis embryo (n = 10) or larval exposures (n = 8). The mean (± SD) percentage agreement among duplicate samples was 91 ± 7.5 % (n = 10) and 93 ± 6.7 % (n = 8) from the X. laevis embryo and larval exposures, respectively. The mean (± SD) recovery of RA in the spiked water samples was 89 ± 11.6 % (n = 23) and 90 ± 8.5 % (n = 19) from the X. laevis embryo and larval exposures, respectively.

Data analysis.
The experimental design of this experiment is unique in that we choose to test a relatively large number of concentrations at the expense of tank replication. This was a necessary step, given the number of different exposure durations tested. With the data available in the literature (stage sensitivity differences) we did not feel that we could test several different life stages with a limited number of test concentrations. The principle objective of these experiments was to determine if continuous RA exposure would result in hindlimb malformations, and the experiments were designed to maximize the potential to do so. Given the steep dose-response curves observed (absence of several treatments with partial effects compared to controls) for mortality and dysmorphogenesis in these experiments, curve fitting models were not applicable in all exposures scenarios. Instead we calculated cumulative probability of survival, and ultimately, mortality as described by (Kaplan, 1958Go) and present the data as percent mortality in a given treatment. The effects were quite obvious, and presentation would not be enhanced by curve fitting.


    RESULTS
 TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
RA Concentrations
RA concentrations were measured three times during the first week of the test and then once a week until test completion. A summary of the measured concentrations can be found in Table 1Go. The measured test concentrations were very close to the target concentrations, and the nominal concentrations are referred to below.


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TABLE 1 Summary of Measured Water Concentrations
 
Embryonic Exposure
Stage 8 embryos were exposed for 3 days (stages 8–41), 9 days (stages 8–48) or until tail resorption was complete (stages 8–65), and mortality was recorded daily. After three days of exposure (stage 41), a random subset of 10 organisms were removed and examined for externally obvious dysmorphogenesis. There were no obvious signs of gross dysmorphogenesis observed at concentrations of 0.24 µg/l RA and below. At the 0.6 µg/l RA concentration and above, 100% of the organisms developed abnormally. Dysmorphogenesis, at 0.6 µg/l, was restricted to the craniofacial region and consisted of micropthalmia, reductions in the prosencephalon, mesencephalon, and edema (Fig. 1Go). At 2 µg/l the effects were more severe, ranging from holoprosencephaly and anophthalmia to near complete absence of procephalic tissue (Fig. 1Go). At this concentration there were also dramatic effects on posterior development (Fig. 1Go).



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FIG. 1. Images showing malformations induced by 3-day RA following exposure. (A) control larva, (B) larva exposed to 0.6 µg/l RA, and (C) larva exposed to 2 µg/l RA.

 
Continuous exposure to RA through completion of metamorphosis resulted in a concentration-dependent increase in mortality (Table 2Go). The control mortality in this treatment group was relatively low (10.4 and 0 % for control 1 and control 2, respectively), given that these experiments covered nearly the entire period of development (Table 2Go). High levels of mortality (100%) were observed at concentrations of 0.24 µg/l RA and above in the tadpoles exposed through tail resorption (Table 2Go). The time to 100% mortality for these groups was 51, 18, and 15 days for treatments 0.24, 0.6, and 2 µg/l, respectively. At the 0.144 µg/l RA treatment level 60% mortality was observed. Mortality at all other test concentrations were similar to control. In addition to mortality we examined the effects of RA treatment on growth (length and weight) and developmental rate (time to stage 64) (Table 2Go). We did not observe dramatic effects on these endpoints at concentrations which did not produce mortality above control levels.


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TABLE 2 Mortality, Length, Weight, and Time to Metamorphosis Data for Exposure Initiated at Stage 8 (Embryonic Exposures)
 
In the group exposed from stage 8–48 (9 day exposure), followed by clean water grow out until metamorphosis was complete, control mortality was low (2.2 and 5.0 % for control 1 and 2, respectively). RA treatment resulted in 60.6% mortality at 0.24 µg/l and 100% mortality at 0.6 µg/l RA. By day 9, when sub-sampling occurred, mortality in the 2 µg/l RA had reduced the number of tadpoles remaining to a point that transferring tadpoles to clean water was not practical. Time to 100% mortality in the 0.6 µg/l RA treatment was 21 days. Mortality at all other test concentrations were similar to control.

The most important finding of the embryonic exposures is the lack of hindlimb malformations in any of the tadpoles surviving until tail resorption from either the 9-day pulse exposure or the chronic exposure. Both exposure paradigms had at least on experimental concentrations in which partial mortality was observed. At these concentrations we did not observe malformations in the survivors. Further, we monitored the test system several times a day and examined all dead animals for evidence of malformations. We did not observe hindlimb malformations in any of these dead organisms removed from the test system.

Larval Exposure
The larval exposures were initiated at stage 48, tadpoles were exposed for 1 week or 2 weeks and were moved to clean water grow out, or were exposed in the test system until tail resorption was complete. We observed high control mortality (29%) in the chronic larval control 4 and larval chronic control 3 was terminate early due to high mortality (Table 3Go). However, because the controls for the chronic embryonic and chronic larval exposure were maintained under identical conditions and were collected from that same spawn we used embryonic chronic controls for making comparison in the treatment group exposed until tail resorption. In this group exposure to concentrations of 0.24 µg/l and below did not result in mortality greater than in controls, however 0.6, 2, and 3 µg/l RA caused 100% mortality. Time to 100 % mortality in these three treatments was 35, 18, and 11 days, respectively.


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TABLE 3 Mortality, Length, Weight, and Time to Metamorphosis Data for Exposure Initiated at Stage 48 (Larval Exposure)
 
In the group exposed for 7 day starting at stage 48, we observed 0 and 10.2 % mortality in the two control tanks (Table 3Go). Tadpoles exposed for 7 days to 2 µg/l experienced 46.8 % mortality. A mechanical failure resulted in the premature loss of all tadpoles transferred at 3 µg/l RA. At all of the lower concentrations, mortality was similar to controls. Tadpoles exposed for 14 days to the two highest treatments were not transferred because of high levels of mortality experienced during the exposure, which is consistent with the short time to 100% mortality reported above for the chronic portion of the larval study. At lower concentrations, RA did not cause mortality appreciably greater than the two control groups (12 and 5.5%).

Similar to the embryonic exposures, we examined the effects of RA on growth (length and weight) and developmental rate (time to stage 64) (Table 2Go). We did not observe dramatic effects on these endpoints at concentrations that did not produce mortality above control levels. Thus, these endpoints appear to be only slightly more sensitive to RA treatment.

In contrast to the embryonic exposures, only one of the exposure durations that were tested resulted in partial mortality (7-day exposure). In both the 14-day and chronic exposures, mortality appeared to be an all-or-none situation. Similar to embryonic exposures, RA treatment, regardless of duration, did not produce hindlimb malformations in surviving or dead animals removed from the test system.


    DISCUSSION
 TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Previously, we examined the developmental toxicity of the model retinoid, RA, in X. laevis and four native species of Ranids (Degitz et al., 2000Go). In those experiments, we showed that all five species responded qualitatively and quantitatively similarly. This was the basis for using X. laevis for the present experiments focused on the determining the effects of longer-term, continuous, RA exposure on hindlimb development.

In the current experiments, we have compared the effects of both life-stage sensitivity and duration of RA exposure on development. The developmental toxicity of RA has been the subject of considerable experimentation in a number of vertebrate species. In mice and rats, exposure to retinoids during gastrulation results in a broad spectrum of craniofacial defects (Sulik et al., 1988Go, 1995Go; Vickers, 1985Go). With progression of the mammalian embryo into organogenesis, there is a decrease in the sensitivity to retinoids (Kochhar et al., 1984Go). In amphibians there are considerable data on the effects of retinoids on embryonic development (Creech Kraft and Juchau, 1995Go; Creech Kraft et al., 1995Go; Dawid et al., 1993Go; Leroy and De Robertis, 1992Go) and on hindlimb development and regeneration (Maden, 1983Go, 1985Go). Synthesis of these studies suggests a significant stage-specific difference in sensitivity. Previously, we reported a difference in sensitivity of several orders of magnitude when comparing early embryos and tadpoles (Degitz et al., 2000Go). In those experiments, stage 48 and 52 tadpoles tolerated concentrations as high as 1250 µg/l RA, while stage 8 embryos showed severe dysmorphogenesis and, ultimately, mortality in nearly all of the animals exposed at 25 µg/l RA. However, all of the studies reported in the literature, including our previous work, were conducted using 24-h static exposure paradigms. In our studies, we showed that RA has a short half-life in aqueous solution and that target concentrations were only achieved for a few hours. In the current study, in which a constant flow-through exposure was used, effects were observed at much lower RA concentrations. This result demonstrates the significance of exposure duration in the ultimate outcome. Further, stage sensitivity differences were not as great as one may have predicted from the pulse exposure paradigm. We chose this approach because it more accurately represents potential environmental exposure to retinoid mimics (i.e., chronic or long-term pulse) rather than a few-hour "pulse."

Yet another unanticipated finding was that RA did not result in malformations in animals surviving until stage 65. Exposure starting at stage 8 resulted in a concentration-dependent increase in the frequency and severity of dysmorphogenesis. This was determined by collecting a subsample three days after the exposure was initiated (stages 40–42). However, all organisms in these treatment groups died very early in the study. This mortality was apparently caused by gross abnormalities induced by RA. The spectrum of effects included microphthalmia and reductions in the prosencephalon. With increasing concentration, the effects were more severe, ranging from holoprosencephaly and anophthalmia to complete absence of procephalic tissue. At these higher concentrations, there were also dramatic effects on posterior development. These results are consistent with those previously described for amphibians (Creech Kraft and Juchau, 1995Go; Creech Kraft et al., 1995Go; Dawid et al., 1993Go; Degitz et al 2000Go; Leroy and De Robertis, 1992Go) and mammalian species exposed to retinoids (Sulik et al., 1988Go, 1995Go). Interestingly, we observed high levels of mortality in treatment groups that did not show obvious signs of dysmorphogenesis following three days of embryonic exposure. There are several possible explanations for these observations: developmental events which follow embryogenesis may be more sensitive to RA; lengthier exposure duration may have accumulative impact; or effects which were not externally obvious caused the mortality. We observed partial mortality in both the 9-day (at 0.24 µg/l) and the chronic embryo (at 0.144 µg/l) exposure paradigms. However, we did not observe externally obvious skeletal malformations in the surviving tadpoles. These results suggest that other aspects of growth and development are more sensitive to excessive retinoid concentrations than skeletal development.

It has been proposed that hindlimb malformations observed in amphibians across North America may be attributed to xenobiotic disruption of retinoid signaling pathways (Gardiner and Hoppe, 1999Go). This proposal was based on the phenotypes observed in Rana septentrionalis specimens collected from an unnamed lake in central Minnesota. Malformations included reductions, deletions, and supernumerary structures. The current studies were designed with a primary objective of examining the impact of chronic RA exposure on limb development. In mice, duplications of posterior structures, including the pelvis and hindlimb, have been reported following retinoid exposure at the blastula stage of development (Rutledge et al., 1994Go). Retinoids have been shown to have the ability to mimic the effects of the zone of polarizing activity in developing limbs, causing anterior-posterior duplication (Summerbell, 1983Go; Tickle et al., 1982Go, 1985Go). When administered to regenerating amphibian limbs, retinoids induce proximo-distal and mirror-image duplications (Maden, 1983Go; Scadding and Maden, 1986aGo,bGo; Thoms and Stocum, 1984Go). Given the ability of retinoids to alter normal limb patterning, it is not surprising that systemic exposure of developing limb-bud-stage mice (Kochhar, 1977Go; Kochhar et al., 1984Go), X. laevis (Scadding and Maden, 1986bGo), and axolotl (Scadding and Maden, 1986aGo) results in concentration- and developmental stage-dependent deletions and reductions of hindlimb skeletal segments. Given this knowledge base, we proposed that there may be two critical windows for producing limb defects: early embryogenesis and during the period of limb pattern formation. Exposure starting at stage 8, regardless of duration, did not result in limb malformation in surviving organisms. To assess the impact during the period of pattern formation, we exposed tadpoles starting at stage 48 for 1 week, 2 weeks, or until stage 65. Similar to the finding of the embryonic exposures, RA did not induce limb malformation in any surviving tadpole. We are confident that the concentrations used were high enough to produce malformations, given that the highest concentration used resulted in 100% mortality within 2 weeks of initiating the exposure. Further, in the 1-week exposure group, we observed partial mortality at 2 µg/l, but we did not observe limb malformations in surviving tadpoles at stage 65. Again, these results suggest that other aspects of growth and development, which are not externally obvious, are more sensitive to retinoids than skeletal development.

From these experiments and our previous work (Degitz et al., 2000Go), we conclude that it is unlikely that retinoid mimics are playing a significant role in the recently observed hindlimb malformations in Ranids from the field. We cannot rule out the possibility that short-term exposures at high concentrations could cause limb malformation. However, it is difficult to put forth a pulse exposure scenario that would be at a high enough concentration to produce skeletal malformations yet short enough in duration not to cause mortality. Further, there have been no published reports of retinoid mimics being found at any affected site. If, however, at some point retinoid mimics are found, data from the present study and our previous work will provide a basis for determining if exposure patterns and concentrations are consistent with those necessary to produce hindlimb malformations in amphibians.


    ACKNOWLEDGMENTS
 
The authors would like to thank Mike Hornung and Sidney Hunter for their helpful comments on the manuscript.


    NOTES
 
The information in this document has been funded wholly (or in part) by the U.S. Environmental Protection Agency. It has been subjected to review by the National Health and Environmental Effects Research Laboratory and approved for publication. Approval does not signify that the contents reflect the views of the Agency, nor does mention of trade names or commercial products constitute endorsement or recommendation for use.

1 To whom correspondence should be addressed at U.S. EPA, Mid-Continent Ecology Division, Duluth, MN 55804-2595. Back


    REFERENCES
 TOP
 ABSTRACT
 INTRODUCTION
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
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