Skip to main content
NCBI home page
Saudi Journal of Biological Sciences logoLink to Saudi Journal of Biological Sciences
. 2015 Jan 19;22(5):543–550. doi: 10.1016/j.sjbs.2015.01.002

Haematological and biochemical parameters and tissue accumulations of cadmium in Oreochromis niloticus exposed to various concentrations of cadmium chloride

Nasser A Al-Asgah a, Abdel-Wahab A Abdel-Warith a,b,⁎, El-Sayed M Younis a, Hassan Y Allam b
PMCID: PMC4537862  PMID: 26288556

Abstract

Oreochromis niloticus, weighing 36.45 ± 1.12 g were exposed to 10%, 20% and 30% of the LC50 of CdCl2 which represents treatments (T1)1.68, (T2)3.36 and (T3)5.03 mg/l, respectively, for a period of 10, 20 and 30 days. It was found that, compared to a control group reading of 0.19 ± 0.03 μg/g dry weight, accumulation of Cd in the gills was significantly (p < 0.05) increased in samples ranging between 7.64 ± 0.86 and 61.73 ± 0.82 μg/g dry weight from T1 at 10 days to T3 at 30 days. The accumulation of Cd in the liver, meanwhile, was also observed to significantly increase (p < 0.05) with increasing time and concentrations with results ranging between 3.21 ± 0.12 and 181.61 ± 1.32 compared to the control group results of 0.29 ± 0.04 μg/g dry weight. Although muscles exhibited lower levels of accumulation than the gills and liver they still showed the same pattern of increase compared to the control group, with a significant difference ranging between 0.32 ± 0.02 and 2.16 ± 0.08 compared to the control group results of 0.03 ± 0.001 μg/g dry weight. Also, haematological parameters such as red blood cells (RBCs), haemoglobin (Hb) and haematocrit (Hct) were reduced in fish exposed to Cd at all periods, with significant differences (p < 0.05). Plasma glucose concentration showed a significant increase. Total protein levels of fish showed a significant reduction (p > 0.05) for all exposed treatments. Also, the total lipid level increased significantly as fish were exposed to increasing cadmium concentrations, compared to control fish. Finally, the activities of aspartate aminotransferase (AST IU/l) and alanine aminotransferase (ALT IU/l) showed a significant increase (p < 0.05) with increasing time and concentrations.

Keywords: Nile tilapia, Blood parameters, Heavy metals, Physiological, Toxicity

1. Introduction

Oreochromis niloticus is an important species in commercial fisheries in the world. It is also a species commonly found in brackish water in estuaries around the world (Vijayan et al., 1996) and responds promptly to environmental alterations. Cadmium is widely used in modern industry (Novelli Filho et al., 2000) and, along with other heavy metals; it is known to exert a wide range of pathological effects on fish and other aquatic organisms (Iger et al., 1994). In particular, metal accumulation in fish has been linked to the damage to organ structure (Giari et al., 2007), various changes in the indices of red blood cells (Vosyliené, 1999), changes in the levels of glucose, osmotic regulation (Fu et al., 1990) and alteration in enzyme activities (Lionetto et al., 2000). Furthermore, Cd is known to have severe toxic effects on aquatic organisms when present in excessive amounts (Novelli et al., 1999), including damage to essential biochemical and physiological functions (Heath, 1995).

Chronic sub-lethal exposure to waterborne Cd leads to accumulation of this metal mainly in the fish kidneys, liver and gills (Hollis et al., 1999; McGeer et al., 2000), with the level of accumulation in distinct organs depending on uptake and elimination rates, which are different from one tissue type to other (Lange et al., 2002). Some organs, such as the liver, intestines, gills and kidney are often investigated for metal accumulations. Moreover, these tissues have been identified as the main storage sites for Cd (Kim et al., 2004). Haematological parameters are used as an index to detect physiological changes in a number of fish species and to assess structural and functional health during stress conditions (Adhikari et al., 2004; Suvetha et al., 2010). Fish blood is sensitive to pollution-induced stress, and changes to the haematological parameters, such as haemoglobin content, haematocrit and the number of erythrocytes, can be used to monitor stress caused by pollutants such as heavy metals (Romani et al., 2003; Barcellos et al., 2004).

Biochemical parameters in fish are also sensitive for detecting potential adverse effects of metal accumulations. The activities of various enzymes are considered to be sensitive biochemical indicators before hazardous effects occur in fish and are important parameters for testing water for the presence of toxicants (Gül et al., 2004). Determination of enzymes, such as aspartate alanine aminotransferase (AST, ALT) and lactate dehydrogenase (LDH), is considered a useful biomarker to determine pollution levels during chronic exposure (Basaglia, 2000; Ozman et al., 2006; Younis et al., 2012).

The aims of this study were to investigate the effects of exposure to three concentrations of Cd for varying durations on the Cd accumulation in the gill, liver and muscle tissues of the freshwater fish O. niloticus, as well as on some haematological and biochemical parameters.

2. Materials and methods

2.1. Experimental fish

Fingerlings of Nile tilapia, O. niloticus, were collected from the fish seed hatchery of King Abdulaziz City for Sciences and Technology Mozahmiya, Riyadh, Saudi Arabia. Fish were acclimatised to laboratory conditions for two weeks prior to experiments.

2.2. Experimental design

One hundred and sixty acclimatised fish, weighing 36.45 ± 1.12 g, were divided into four groups. Three of these groups were exposed to 10%, 20% or 30% of the LC50 of CdCl2, which represents 1.68(T1), 3.36(T2) and 5.04(T3) mg/l CdCl2, respectively, for 10, 20 and 30 days. The fourth, unexposed, group served as the control. Glass aquaria with a capacity of 80 l (100 × 50 × 40 cm) were used, with replicates for each concentration. The water was changed once a week to maintain the environmental conditions and CdCl2 concentrations (Proença and Bittencourt, 1994). Dissolved oxygen was added with diffused air at the top of the biological filter. Fish were fed twice daily with a 32% crude protein diet at a rate of 2% of body weight. Mortalities within each group were recorded.

2.3. Experimental exposure

After acclimatisation, 20 fish were transferred to experimental tanks (80 l) containing dechlorinated tap water. Duplicate cultures were established for each concentration tested, adding calculated amounts of a 1000 mg/l stock solution of CdCl2 prepared in deionised water, with an unexposed group serving as the control fish. The cadmium treatment level was based on the 96-h LC50 of CdCl2 in O. niloticus, which was previously determined to be 16.8 mg/l by Zirong and Shijun (2007).

2.4. Tissue analysis

After the fish were decapitated, the gills, liver and muscle tissues were collected and freeze-dried. Tissues were washed in fresh water three times and briefly rinsed in double-deionised water; the water left on the tissue surface was blotted dry with filter paper. Tissues were dried at 80 °C overnight, weighed (approx. 0.3 g dry) and then digested. The digested solutions were diluted with double-deionised water and subjected to atomic absorption spectrophotometry. The tissue digestion was conducted according to the method described by Allen (1989). Cd concentration was measured using an Atomic Absorption spectrometer (Varian – Spectra, 220 FS).

2.5. Haematological and biochemical analysis

After each experimental period, samples of the blood, liver, gills and muscle were taken from five fish specimens from each aquarium. Fish were not fed for 24 h before sampling and were anaesthetised with buffered MS222 (50 mg/l). Blood samples were taken from the caudal vein of an anaesthetised fish with a sterile syringe containing heparin solution as an anticoagulant. Plasma was obtained by centrifugation of blood at 3000 rpm for 15 min and non-haemolysed plasma was stored in a deep freezer for further biochemical analyses. These blood samples were used for determining the count of red blood cells (RBCs) following the method of Dacie and Lewis (1984), and the haemoglobin content (Hb) (Van Kampen and Zijlstra, 1961). The haematocrit value (Hct) was calculated according to the formulae mentioned by Britton (1963).

Plasma glucose (mg/l) was determined using assay kits supplied by Human Diagnostics Worldwide according to Trinder (1969). Total protein (g/100 ml) content was determined according to the method of Henry (1964). Total lipid (g/l) content was determined colorimetrically according to Joseph et al. (1972). The activity levels of aspartate aminotransferase (AST) and alanine aminotransferase (ALT) were determined colorimetrically according to Reitman and Frankel (1957).

2.6. Statistical analysis

The statistical analysis of the data was done using a one way analysis of variance (ANOVA) technique. The means were separated by Fisher’s LSD test and compared using Duncan’s Multiple Range Test (DMRT) as described by Snedecor and Cochran (1989). Significant differences were defined at p < 0.05.

3. Results

3.1. Cd accumulation in gills

Table 1 shows the concentration of Cd in fish exposed to T1, T2 and T3 CdCl2, with the significantly (p < 0.05) increased accumulation of this element in the gills being especially noteworthy. After 10, 20 and 30 days accumulations in the gills were 7.64, 24.52 and 31.65 μg/g dry weights for the T1 group, 15.83, 32.42 and 42.16 for the T2 group, and 28.96, 40.81 and 61.73 for the T3 group compared to the control group which showed lower accumulations of 0.19, 0.28 and 0.32 mg/l after all the exposed periods, with significant differences (p < 0.05) among all groups.

Table 1.

Cadmium accumulation (μg/g dry weight) in some tissues of O. niloticus exposed to cadmium chloride for 10, 20 and 30 days.

Tissues Cd Concentrations Exposure time (days)
10 20 30
Gills Control⁎ 0.19 ± 0.03a 0.28 ± 0.06a 0.32 ± 0.05a
T1(10%LC50) 7.64 ± 0.86b 15.83 ± 0.93b 28.96 ± 0.87b
T2(20%LC50) 24.52 ± 0.67c 32.42 ± 0.74c 40.81 ± 0.68c
T3(30%LC50) 31.65 ± 0.81d 42.61 ± 0.61d 61.73 ± 0.82d



Liver Control 0.29 ± 0.04a 0.41 ± 0.02a 0.96 ± 0.05a
T1(10%LC50) 3.21 ± 0.12b 17.01 ± 0.32b 32.51 ± 0.51b
T2(20%LC50) 28.16 ± 0.61c 36.81 ± 0.72c 57.67 ± 0.64c
T3(30%LC50) 68.41 ± 0.96d 138.12 ± 1.03d 181.61 ± 1.32d



Muscles Control 0.03 ± 0.001a 0.08 ± 0.006a 0.12 ± 0.004a
T1(10%LC50) 0.32 ± 0.02b 0.64 ± 0.06b 0.77 ± 0.06b
T2(20%LC50) 0.68 ± 0.04bc 0.91 ± 0.09c 1.12 ± 0.06bc
T3(30%LC50) 0.88 ± 0.06cd 1.41 ± 0.04d 2.16 ± 0.08d
Open in a new tab

Values in the same column for each period separately with the same superscript are not significantly different (p > 0.05).

⁎

Control (not exposed 0 mg/l CdCl2).

3.2. Cd accumulation in the liver

The highest bioaccumulation of cadmium was observed in the organs mainly implicated in metal intoxication; thus, bioaccumulation was higher in the liver followed by the gills and muscles. The highest amount of Cd residue was found in the liver after 30 days of exposure. Table 1 also shows that the accumulation of Cd in the liver after 10 days was 3.21 ± 0.12, 28.16 ± 0.61 and 68.41 ± 0.96 respectively for the fish exposed to T1, T2 and T3 CdCl2,with significant differences (p < 0.05) between the treatments and control group (0.29 ± 0.04 μg/g dry weights). The accumulations increased significantly (p < 0.05) as the concentration of Cd increased. After 20 days accumulations showed the same trend, being 17.01 ± 0.32, 36.81 ± 0.72 and 138.12 ± 1.03 respectively with this increase showing a significant difference (p < 0.05) between exposed and control fish (0.41 ± 0.02 μg/g dry weights). Also, after 30 days the results illustrated in Table 1 for different concentrations were 32.51 ± 0.51, 57.67 ± 0.64 and 181.61 ± 1.32 respectively, again with significant differences (p < 0.05) between the exposed and control group 0.96 ± 0.05 μg/g dry weights (Table 1).

3.3. Cd accumulation in muscles

Table 1 shows a similar trend with respect to fish muscles exposed to concentrations of Cd for 10 days. This exposure resulted in 0.32 ± 0.02, 0.68 ± 0.04 and 0.88 ± 0.05 μg/g dry weights respectively, a significant increase (p < 0.05) in response to increasing Cd concentrations between the treatments and control groups (0.03 ± 0.001). After a 20 day exposure period the data obtained were 0.64 ± 0.06, 0.91 ± 0.09 and 1.41 ± 0.04 respectively, again showing a significant difference (p < 0.05) in the increase between the treatment and control groups (0.08 ± 0.006 μg/g dry weights). A similar trend was evident in the data obtained after the 30 day exposure period, in which the dry weights were 0.77 ± 0.06, 1.12 ± 0.06 and 2.16 ± 0.08 respectively compared to control group figures of 0.12 ± 0.004 μg/g (Table 1).

3.4. Haematological parameters

Table 2 shows that the RBCs, HB and HCT were reduced in fish exposed to Cd in all periods, as well as being in each case lower than in the control (p < 0.05). The RBC count decreased significantly (p < 0.05) in T1, T2 and T3 CdCl2 at 10 days with counts of 1.82 ± 0.06, 1.76 ± 0.07, 1.65 ± 0.03 and 1.30 ± 0.05 count × 106 mm3 for the control, T1, T2 and T3 respectively. Also, data obtained for HBs were 5.29 ± 0.18, 5.11 ± 0.41 and 4.96 ± 0.22 respectively with a significant decrease (p < 0.05) evident between the treated and control fish 6.00 ± 0.71 g/100 ml. In the same way, the HCT% showed a significant difference (p < 0.05) between exposed fish and the control: 33.26 ± 0.32 31.70 ± 0.32, 28.41 ± 0.62 and 27.58 ± 0.53% for control, T1, T2 and T3 respectively (Table 1).

Table 2.

Haematological and biochemical parameters of O. niloticus exposed to different concentrations of cadmium chloride for 10 days.

Parameters Concentrations
Control⁎ T1(10%LC50) T2(20%LC50) T3(30%LC50)
RBC (count × 106/mm3) 1.82 ± 0.06cd 1.76 ± 0.07c 1.65 ± 0.03b 1.30 ± 0.05a
Hb (g/100 ml) 6.00 ± 0.30d 5.29 ± 0.18c 5.11 ± 0.41ab 4.96 ± 0.22a
Hct (%) 33.26 ± 0.32d 31.70 ± 0.32c 28.41 ± 0.62ab 27.58 ± 0.53a
Glucose (mg/l) 60.32 ± 0.57a 66.42 ± 0.68b 72.50 ± 0.71c 76.38 ± 0.92d
TP (g/100 ml) 2.85 ± 0.09d 2.26 ± 0.07c 2.03 ± 0.03ab 1.97 ± 0.06a
TL (g/l) 10.96 ± 0.08a 15.31 ± 0.06b 16.06 ± 0.07c 17.11 ± 0.09d
AST (IU/l) 81.65 ± 1.06a 123.04 ± 1.36b 127.40 ± 1.46c 129.60 ± 1.61cd
ALT (IU/l) 30.95 ± 0.26a 49.24 ± 0.83bc 51.31 ± 1.06c 56.74 ± 1.01d
Survival (%)⁎⁎ 100.00 81.62 73.65 64.86
Open in a new tab

Values in the same row with the same superscript are not significantly different (p > 0.05).

⁎

Control (not exposed 0 mg/l CdCl2).

⁎⁎

Survival during all experimental periods.

3.5. Biochemical parameters

Plasma glucose (mg/l) concentrations, meanwhile, showed significantly (p < 0.05) higher values (Tables 2–4) which increased as the concentration and exposure periods increased compared to the control group. The total protein levels of O. niloticus for the 10, 20, and 30 day periods are given in Table 2–4. A highly significant reduction (p < 0.05) in cadmium is evident for all exposure periods and concentrations compared to the control group. The total lipid levels (g/l) for the fish for the different exposure periods are given in Table 2–4. Increased cadmium concentrations led to a highly significant increase in total lipids (p < 0.05) for all periods of exposure.

Table 3.

Haematological and biochemical parameters of O. niloticus exposed to different concentrations of cadmium chloride for 20 days.

Parameters Concentrates
Control⁎ T1(10%LC50) T2(20%LC50) T3(30%LC50)
RBC (count × 106/mm3) 1.73 ± 0.04d 1.26 ± 0.07c 1.18 ± 0.05b 1.13 ± 0.08a
Hb (g/100 ml) 7.30 ± 0.12d 4.87 ± 0.09c 4.86 ± 0.18b 4.79 ± 0.11a
Hct (%) 31.56 ± 0.23d 26.91 ± 0.41c 25.38 ± 0.24b 24.61 ± 0.39a
Glucose (mg/l) 55.85 ± 0.66a 88.20 ± 0.56b 93.75 ± 0.84c 100.21 ± 0.88d
TP (g/100 ml) 3.05 ± 0.04d 1.69 ± 0.08c 1.53 ± 0.06b 1.42 ± 0.03a
TL (g/l) 11.62 ± 0.02a 17.46 ± 0.05b 18.23 ± 0.08c 20.07 ± 0.06d
AST (IU/l) 72.62 ± 1.03a 132.10 ± 1.05b 138.60 ± 1.11c 143.50 ± 1.64d
ALT (IU/l) 32.65 ± 0.35a 59.11 ± 0.51b 64.30 ± 0.66c 70.24 ± 0.98d
Open in a new tab

Values in the same row with the same superscript are not significantly different (p > 0.05).

⁎

Control (not exposed 0 mg/l CdCl2).

Table 4.

Haematological and biochemical parameters of O. niloticus exposed to different concentrations of cadmium chloride for 30 days.

Parameters Concentrations
Control⁎ T1(10%LC50) T2(20%LC50) T3(30%LC50)
RBC (count × 106/mm3) 1.81 ± 0.04d 1.11 ± 0.07c 1.09 ± 0.06bc 1.03 ± 0.03a
Hb (g/100 ml) 7.85 ± 0.11d 4.61 ± 0.09c 4.44 ± 0.07ab 4.38 ± 0.08a
Hct (%) 32.21 ± 0.41d 23.73 ± 0.52c 22.41 ± 0.33ab 22.51 ± 0.65a
Glucose (mg/l) 54.66 ± 0.48a 107.30 ± 0.67b 115.61 ± 0.56c 125.23 ± 0.44d
TP (g/100 ml) 3.11 ± 0.03d 1.33 ± 0.07c 1.21 ± 0.06b 1.11 ± 0.72a
TL (g/l) 12.05 ± 0.04a 20.96 ± 0.05b 22.11 ± 0.07c 23.01 ± 0.08d
AST (IU/l) 76.52 ± 1.04a 148.7 ± 1.05b 151.20 ± 1.04bc 160.13 ± 1.08d
ALT (IU/l) 35.62 ± 0.4a 72.21 ± 0.39b 79.81 ± 0.65c 88.62 ± 0.46cd
Open in a new tab

Values in the same row with the same superscript are not significantly different (p > 0.05).

⁎

Control (not exposed 0 mg/l CdCl2).

There are significant differences in AST and ALT activity levels (IU/l) in the serum of fish exposed to cadmium in comparison with the control fish (Tables 2–4). Cadmium appeared to induce a highly significant increase in the levels of these two liver enzymes for all exposure periods as the concentrations of Cd increased. Therefore, survival rates (%) were recorded which decrease by increasing cadmium concentration and time with data ranging between 100 (no mortality) for the control group to 81.62%, 73.65% and 64.86% for T1, T2 and T3 respectively Table 2.

4. Discussion

Many studies have investigated Cd accumulation and distribution among organs. The distribution of accumulated Cd in organs differs between these studies, however (Cattani et al., 1996). The inconsistencies in these previous studies may be ascribed to the differences in the cadmium concentrations and exposure times used (Wu et al., 1999). A few papers, however, have compared Cd accumulation among organs in relation to Cd exposure time. Differential responses of Cd exposure and cadmium resistance may be related to oxidative stress biomarkers, increasing the activities of antioxidant enzymes. When the metal concentration increased and overcame the capacity of natural detoxifying systems, various adverse effects occurred and we observed increased mortality. These results were in agreement with data obtained by Nishiyama et al. (1998), who also recommended that oxidative stress, which is defined as the imbalance between oxidant fluxes and antioxidant defences, this might be related with cadmium exposure and mortality. In fish that survived, there were increases in antioxidant defences.

The present data showed that the highest content of Cd was found in the tissues of the liver, gills and muscles, and that these accumulations increased 626, 324, and 72-fold, respectively, after 30 days of exposure, compared to the control group. Results found in carp (Cyprinus carpio) indicated that more than 10-fold higher levels of Cd accumulated in the kidneys than in the liver (Kraal et al., 1995). According to the present data, however, in O. niloticus, it is the gills that are the temporary target organ of Cd accumulation, with the Cd then being transferred to the digestive tract and organs such as the liver and kidneys via the circulatory system or the enterohepatic circulation. In addition, compared to the organs, the accumulation rate of Cd after 30 days’ treatment was the lowest in muscle. In the present study, across all concentrations and periods, the accumulation pattern of cadmium follows the order; the liver > gills > muscles and these results are in full agreement with the data obtained by Cogun et al. (2003), who found a similar distribution pattern for cadmium and copper in tissues of O. niloticus. In the marine fish, Sparus aurata, however, Souid et al. (2013) reported that the source of Cd-uptake in sea water, metal accumulation in different tissues decreased in the following order: intestine > gills > kidney > liver > muscles for short term exposures of 2, 4 and 24 h. This result might be related to the short term exposure to the metal, which might not have permitted transference of Cd through the portal system from the digestive tract to the liver, which is involved in storage and metal detoxification (Handy, 1993). In bass (Dicentrarchus labrax) and flounder (Scophthalmus maximus), meanwhile, Cd accumulation followed the order kidneys > liver > gills (Cattani et al., 1996). The finding of the present study is in congruence with (Brown et al., 2006) who suggested that the pollutants may be distributed uniformly within the body tissues of fish but accumulate differently. Overall, fish exposed to Cd leads to accumulate the metal in a concentration–dependent manner (Isani et al., 2009). These results also are in congruence with the finding of the present study. This is in agreement with our data, suggesting that metal accumulation depends largely on the period of exposure and the type of organ. Overall, given long term exposure, the liver accumulates Cd strongly when compared to other studied tissues.

Many studies on fish have demonstrated that the distribution of Cd is tissue specific and depends on the exposure route, as reported by Kraal et al. (1995) and Guinot et al. (2012). Moreover, the results in the present study are in accordance with data obtained by Filipović Marijić and Raspor (2006), who argued that after long term exposure metals, are transferred to storage organs such as the liver or kidney. Studies carried out with different aquatic fish species have shown that the liver is the prime organ for metal accumulation and also plays an important role in storage, redistribution, detoxification or transformation of metals (Erdem and Kargin, 1992; Evans et al., 1993). In accordance with our data Cogun et al. (2003) who observed that muscle in O. niloticus generally accumulates the lowest concentrations of metals during exposure of fish for 30 days to cadmium and copper.

The present study reveals that the O. niloticus exposed to Cd exhibited a significant reduction in their RBCs, Hb and Hct in comparison with the control. These results are in agreement with Gill and Epple (1993) and Karuppasamy et al. (2005) who each found a significant reduction in the RBCs, Hb and Hct in American eel Anguilla rostrata and the air breathing fish, Channa punctatus, after exposure to 150 μg and 29 mg Cd/l, respectively. Our results are also in full agreement with data obtained by Mekkawy et al. (2011), who reported that fish exposed to 4.64 mg/l (25% of 96 h LC50) Cd showed a significant decrease in their RBCs Hb and Hct in O. niloticus when exposed to 4.64 mg/l cadmium for 15 and 30 days. Shalaby (2007), found similar results for O. niloticus exposed to 10 ppm Cd for 15 and 45 days. The reduction in these parameters at sub-lethal levels of cadmium might be due to the destruction of mature RBCs and the inhibition of erythrocyte production due to a reduction of haemosynthesis that affects haematopathology or causes acute haemolytic crisis which in turn results in severe anaemia in most vertebrates, including fish species, exposed to various environmental contaminants (Khadre, 1988).

Blood glucose is a sensitive and reliable indicator of pollutants causing environmental stress in fish. Our results are in agreement with data obtained by Shalaby (2007) and Mekkawy et al. (2011) who showed that Cd elevated blood glucose levels in Nile tilapia exposed to 4.64 mg/l (25% of 96 h LC50) for 15 and 30 days. Sastry and Subhadra (1985) reported that Cd induced hyperglycaemia with an associated decrease in liver glycogen in catfish, Heteropneustes fossilis. Soengas et al. (1996), meanwhile, suggested that hyperglycaemia occurred in Atlantic salmon Salmo salar due to cadmium toxicity, possibly associated with changes in liver carbohydrate metabolism which causes activation of liver glycogenolysis and glycolysis as well as increased levels of plasma glucose and lactate.

The decrease in plasma total protein level (hypoproteinemia) shown in this study was in agreement with the findings of Mekkawy et al. (2011). They recorded that O. niloticus exposed to 4.64 mg/l (25% of 96 h LC50) Cd for 15 and 30 days showed a reduction in serum protein levels. This decrease of total protein may be due to the destruction of protein-synthesising subcellular structures and inhibition of the hepatic synthesis of blood protein (Fontana et al., 1998). Loss of protein from damaged kidneys could contribute further to the observed hypoproteinemia (Gad, 2005). Our data are in accordance with Shalaby (2001), who suggested that Cd-induced increase in serum total lipids in comparison with the control of O. niloticus may be due to a disturbance in the metabolism of lipids after fish were exposed to Cd for 15 and 45 days.

The activity of AST and ALT enzymes in blood may also be used as a stress indicator. The significant changes in the activities of these enzymes in blood plasma indicate tissue impairment caused by stress (James et al., 1991; Svoboda, 2001). The increase of AST and ALT values in the fish reveal enzymes exporting from liver into the blood stream (Yang and Chen, 2003; Perez-Rostro et al., 2004). According to Chen et al. (2004) increased levels of these two enzymes in tilapia are associated with hepatic injury. In the present study, there were significant changes in AST and ALT activities in plasma of O. niloticus exposed to cadmium for 10, 20 and 30 days compared to the control group. The increased levels of AST and ALT in blood plasma indicate impairment of the liver. In addition, the increase of plasma AST and ALT may be related to hepatocellular damage or cellular degradation caused by cadmium, probably in the liver, heart or muscle (Yamawaki et al., 1986). These results are in agreement with those of Shalaby (2007) who found that sub-lethal concentrations of Cd caused significant increases in AST and ALT of O. niloticus after 15 and 45 days of exposure to cadmium. Also, Mekkawy et al. (2011) confirmed similar data for these enzymes in O. niloticus exposed to cadmium for 15 and 30 days.

5. Conclusion

The observations of our data showed that metal accumulation depends largely on three factors; the concentration of metal, period of exposure and the type of organ. Overall, given exposure, the liver accumulates Cd strongly when compared to other studied tissues of Nile tilapia (gills and muscles). Haematological and biochemical parameters indicated that cadmium acts as a stressor leading to changes in some blood parameters and accumulation in important tissues.

Acknowledgment

The authors would like to extend their sincere appreciation to the Deanship of Scientific Research at King Saud University for its funding of this research through the Research Group Project No. RGP-VPP-304.

Footnotes

Peer review under responsibility of King Saud University.

References

  1. Adhikari S., Sarkar B., Chatterjee A., Mahapatra C.T., Ayyappan S. Effects of cypermethrin and carbofuran haematological parameters and prediction of their recovery in a freshwater teleost, Labeo rohita (Hamilton) Ecotoxicol. Environ. Saf. 2004;58:220–226. doi: 10.1016/j.ecoenv.2003.12.003. [DOI] [PubMed] [Google Scholar]
  2. Allen S.E. 2nd ed. Blackwell Scientific Publications; Oxford: 1989. Chemical Analysis of Ecological Materials. [Google Scholar]
  3. Basaglia F. Isozyme distribution of ten enzymes and their loci in South American lung fish, Lepidosirenparadoxa (Osteichtyes, Dipnoi) Comp. Biochem. Physiol. 2000;B126:503–510. doi: 10.1016/s0305-0491(00)00224-8. [DOI] [PubMed] [Google Scholar]
  4. Barcellos L.J.G., Kreutz L.C., Souza C., Rodriguez L.B., Fioreze I., Quevedo R.M., Cericato L., Soso A.B., Fagundes M., Conrad J., Lacerda L.A., Terra S. Haematological changes in Jundia (Rhamdia quelen) after acute and chronic stress caused by usual aquacultural management, with emphasis on immunosuppressive effects. Aquaculture. 2004;237:229–236. [Google Scholar]
  5. Britton C.J. 9th ed. I. A. Churchill, Ld.; London: 1963. Disorders of the Blood. [Google Scholar]
  6. Brown L., Werner I., Johnson M.L. Physiological and behavioural effects of zinc and temperature on coho salmon (Oncorhynchus kisutch) Hydrobiologia. 2006;559:161–168. [Google Scholar]
  7. Cattani O., Serra R., Isani G. Correlation between metallothionein and energy metabolism in sea bass Dicentrarchus labrax exposed to cadmium. Comp. Biochem. Physiol. 1996;C113:193–199. [Google Scholar]
  8. Chen C., Wooster G.A., Bowser P.R. Comparative blood chemistry and histopathology of tilapia infected with Vibrio vulnificus or Streptococcus iniae or exposed to carbon tetrachloride, gentamicin or copper sulfate. Aquaculture. 2004;239:421–443. [Google Scholar]
  9. Cogun H.Y., Yuzereroglu T.A., Kargın F. Accumulation of copper and cadmium in small and large Nile tilapia Oreochromis niloticus. Bull. Environ. Contam. Toxicol. 2003;71:1265–1271. doi: 10.1007/s00128-003-8523-8. [DOI] [PubMed] [Google Scholar]
  10. Dacie J.V., Lewis S.M. Churchill Living Stone; London: 1984. Practical Haematology. [Google Scholar]
  11. Erdem C., Kargin F. A comparative study on the accumulation of copper in liver, spleen, stomach, intestine, gill and muscle tissues of Cyprinus carpio and Tilapia nilotica. Biyokim. Derg. 1992;1:13–27. [Google Scholar]
  12. Evans D.W., Doo D.K.D., Hanson P. Trace element concentration in fish livers: implication of variations with fish size in pollution monitoring. Mar. Pollut. Bull. 1993;26:329–354. [Google Scholar]
  13. Filipović Marijić V., Raspor B. Age-and tissue dependent metallothionein and cytosolic metal distribution in a native Mediterranean fish, Mullus barbatus, from the Eastern Adriatic Sea. Comp. Biochem. Physiol. 2006;143:382–387. doi: 10.1016/j.cbpc.2005.05.019. [DOI] [PubMed] [Google Scholar]
  14. Fontana L., Moreira E., Torres M., Ferna‘ndez I., Rios A., Sanchezde Medina F., Gil A. Dietary nucleotides correct plasma and liver microsomal fatty acids alterations in rats with liver cirrhosis induced by oral intake of thioacetamide. J. Hepatol. 1998;28:662–669. doi: 10.1016/s0168-8278(98)80291-2. [DOI] [PubMed] [Google Scholar]
  15. Fu H., Steinbach O.M., Vanden Hamer C.J.A., Balm P.H.M., Lock R.A.C. Involvement of cortisol and metallothionein-like proteins in the physiological responses of tilapia (Oreochromis mossambicus) to sublethal cadmium stress. Aquat. Toxicol. 1990;16:257–270. [Google Scholar]
  16. Gad N.S. Impact of environmental pollution in the southern region of Lake Manzalah Egypt on some biochemical parameters of Tilapia Zilii. J. Egypt. German Soc. Zool. 2005;48A:279–298. [Google Scholar]
  17. Giari L., Manera L.M., Simoni E., Dezfuli B.S. Cellular alterations in different organs of European sea bass Dicentrarchus labrax (L.) exposed to cadmium. Chemosphere. 2007;67:1171–1181. doi: 10.1016/j.chemosphere.2006.10.061. [DOI] [PubMed] [Google Scholar]
  18. Gill T.S., Epple A. Stress-related changes in the hematological profile of the American eel (Anguilla rostrata) Ecotoxicol. Environ. Saf. 1993;25(2):227–235. doi: 10.1006/eesa.1993.1021. [DOI] [PubMed] [Google Scholar]
  19. Guinot D., Urena R., Pastor A., Varo I., Ramo J., Torreblanca A. Long-term effect of temperature on bioaccumulation of dietary metals and metallothionein induction in Sparus aurata. Chemosphere. 2012;87:1215–1221. doi: 10.1016/j.chemosphere.2012.01.020. [DOI] [PubMed] [Google Scholar]
  20. Gül S., Belge-Kurutas E., Yildiz E., Sahan A., Doran F. Pollution correlated modifications of liver antioxidant systems and histopathology of fish (Cyprinidae) living in Seyhan Dam Lake, Turkey. Enviro. Int. 2004;30:605–609. doi: 10.1016/S0160-4120(03)00059-X. [DOI] [PubMed] [Google Scholar]
  21. Handy R.D. The effect of acute exposure to dietary Cd and Cu on organ toxicant concentrations in rainbow trout, Oncorhynchus mykiss. Aquat. Toxicol. 1993;27:1–14. [Google Scholar]
  22. Heath A.G. CRC Press; Boca Raton, FL: 1995. Water Pollution and Fish Physiology. [Google Scholar]
  23. Henry R.J. Harper and Row; New York: 1964. Colorimetric determination of Total Protein: Clinical Chemistry; p. 181. [Google Scholar]
  24. Hollis L., McGeer J.C., McDonald D.G., Wood C.M. Cadmium accumulation, gill Cd binding, acclimation, and physiological effects during long term sublethal Cd exposure in rainbow trout. Aquat. Toxicol. 1999;46:101–119. [Google Scholar]
  25. Iger Y., Lock R.A.C., Van Der M., Wendelaar Bonga S.E. Effects of water-borne cadmium on the skin of the common carp Cyprinus carpio. Arch. Environ. Contam. Toxicol. 1994;26:342–350. doi: 10.1007/BF00203561. [DOI] [PubMed] [Google Scholar]
  26. Isani G., Andreani G., Cocchioni F., Fedeli D., Carpené E., Falcioni G. Cadmium accumulation and biochemical responses in Sparus aurata following sub-lethal Cd exposure. Ecotoxicol. Environ. Saf. 2009;72:224–230. doi: 10.1016/j.ecoenv.2008.04.015. [DOI] [PubMed] [Google Scholar]
  27. James R., Sivakumar V., Sampath K., Rajendran P. Individual and combined effects of zinc; cadmium and copper on growth of Oreochromis mossambicus. Indian J. Fish. 1991;38:198–200. [Google Scholar]
  28. Joseph A., Knight M., Anderson S., James M., Rawie H. Chemical basis of the sulfophospho-vanillin reaction for estimating total serum lipid. Clin. Chem. 1972;18(3):198–201. [PubMed] [Google Scholar]
  29. Karuppasamy R., Subathra S., Puvaneswari S. Haematological responses to exposure to sublethal concentration of cadmium in air breathing fish, Channa punctatus (Bloch) J. Environ. Biol. 2005;26(1):123–128. [PubMed] [Google Scholar]
  30. Khadre S.E.M. The effect of experimentally induced inflammation on the blood pattern and haemopoietic organs of the teleost, Clarias lazera. Bull. Inst. Oceano. Fish. ARE. 1988;14:191–203. [Google Scholar]
  31. Kim S.G., Jee J.H., Kang J.C. Cadmium accumulation and elimination in tissues of juvenile olive flounder, Paralichthys olivaceus after sub-chronic cadmium exposure. Environ. Pollut. 2004;127:117–123. doi: 10.1016/s0269-7491(03)00254-9. [DOI] [PubMed] [Google Scholar]
  32. Kraal M.H., Kraak M.H.S., DeGraat C.J., Davids C. Uptake and tissue distribution of dietary and aqueous cadmium by carp (Cyprinus carpio) Ecotoxicol. Environ. Saf. 1995;31(2):179–183. doi: 10.1006/eesa.1995.1060. [DOI] [PubMed] [Google Scholar]
  33. Lange A., Ausseil O., Segner H. Alterations of tissue gulathione levels and metallothionein mRNA in rainbow trout during single and combined exposure to cadmium and zinc. Comp. Biochem. Physiol. C Pharmacol. Toxicol. 2002;131:231–243. doi: 10.1016/s1532-0456(02)00010-8. [DOI] [PubMed] [Google Scholar]
  34. Lionetto M.G., Giordano M.E., Vilella S., Schettino T. Inhibition of eel enzymatic activities by cadmium. Aquat. Toxicol. 2000;48:561–571. doi: 10.1016/s0166-445x(99)00056-9. [DOI] [PubMed] [Google Scholar]
  35. McGeer J.C., Szebedinszky C., McDonald D.G., Wood C.M. Effects of chronic sublethal exposure to waterborne Cu, Cd or Zn in rainbow trout. 1:iono-regulatory disturbance and metabolic costs. Aquat. Toxicol. 2000;50:231–243. doi: 10.1016/s0166-445x(99)00105-8. [DOI] [PubMed] [Google Scholar]
  36. Mekkawy A.A., Mahmoud U.M., Wassif E.T., Naguib M. Effects of cadmium on some haematological and biochemical characteristics of Oreochromis niloticus (Linnaeus, 1758) dietary supplemented with tomato paste and vitamin E. Fish Physiol. Biochem. 2011;37:71–84. doi: 10.1007/s10695-010-9418-3. [DOI] [PubMed] [Google Scholar]
  37. Nishiyama Y., Ikeda H., Haramaki N., Yoshida N., Imaizumi T. Oxidative stress is related to exercise intolerance in patients with heart failure. Am. Heart J. 1998;135:115–120. doi: 10.1016/s0002-8703(98)70351-5. [DOI] [PubMed] [Google Scholar]
  38. Novelli E.L.B., Lopes A.M., Rodrigues A.S.E., Novelli Filho J.L.V.B., Ribas B.O. Superoxide radical and nephrotoxic effect of cadmium exposure. Int. J. Environ. Health Res. 1999;9:109–116. [Google Scholar]
  39. Novelli Filho J.L.V.V., Novelli E.L.B., Manzano M.A., Lopes A.M., Cataneo A.C., Barbosa L.L., Ribas B.O. Effect of tocopherol on superoxide radical and toxicity of cadmium exposure. Int. J. Environ. Health Res. 2000;10:125–134. [Google Scholar]
  40. Ozman M., Gungordu A., Kucukbay F.Z., Guler R.E. Monitoring the effects of water pollution on Cyprinus carpio in Karakaya Dam Lake, Turkey. Ecotoxicology. 2006;15:157–169. doi: 10.1007/s10646-005-0045-1. [DOI] [PubMed] [Google Scholar]
  41. Perez-Rostro C.I., Racotta I.S., Ibarra A.M. Decreased genetic variation in metabolic variables of Litopenaeus vannamei shrimp after exposure to acute hypoxia. J. Exp. Mar. Biol. Ecol. 2004;302:189–200. [Google Scholar]
  42. Proença, C.E.M., Bittencourt, P.R.L., 1994 Manual de piscicultura tropical. Brasília: Ibama, (78 pp.).
  43. Reitman S., Frankel S. Colorimetric determination of glutamic oxaloacetic and glutamic pyruvic transaminases. Am. J. Clin. Pathol. 1957;28:53–56. doi: 10.1093/ajcp/28.1.56. [DOI] [PubMed] [Google Scholar]
  44. Romani R., Antognelli C., Baldracchini F., Santis A., Isani G., Giovannini E., Rosi G. Increased acetylcholinesterase activities in specimens of Sparus auratus exposed to sublethal concentrations. Chem. Biol. Interact. 2003;145:321–329. doi: 10.1016/s0009-2797(03)00058-9. [DOI] [PubMed] [Google Scholar]
  45. Sastry K.V., Subhadra K. In vivo effects of cadmium on some enzyme activities in tissues of the freshwater catfish, Heteropneustes fossilis. Environ. Res. 1985;36(1):32–45. doi: 10.1016/0013-9351(85)90005-2. [DOI] [PubMed] [Google Scholar]
  46. Shalaby A.M.E. Effect of EDTA on toxicity reduction of cadmium in relation to growth, some haematological and biochemical profiles of Nile tilapia (Oreochromis niloticus) J. Fish. Aquatic Sci. 2007;2(2):100–109. [Google Scholar]
  47. Shalaby A.M.E. Protective effect of ascorbic acid against mercury intoxication in Nile tilapia (Oreochromius niloticus) J. Egypt. Acad. Soc. Environ. Develop. (D-Environ. Stud.) 2001;2(3):79–97. [Google Scholar]
  48. Snedecor G.W., Cochran W.G. The Lowa State University Press; Ames, IA: 1989. Statistical Methods; p. 476. [Google Scholar]
  49. Soengas J.L., Agra-Lago M.J., Carballo B., Andres M.D., Veira J.A.R. Effect of an acute exposure to sublethal concentration of cadmium on liver carbohydrate metabolism of Atlantic salmon (Salmo salar) Bull. Environ. Contam. Toxicol. 1996;57:625–631. doi: 10.1007/s001289900236. [DOI] [PubMed] [Google Scholar]
  50. Souid G., Souayed N., Yaktiti F., Maarouf K. Effect of acute cadmium exposure on metal accumulation and oxidative stress biomarkers of Sparus aurata. Ecotoxicol. Environ. Saf. 2013;89:1–7. doi: 10.1016/j.ecoenv.2012.12.015. [DOI] [PubMed] [Google Scholar]
  51. Suvetha L., Ramesh M., Saravanan M. Influence of cypermethrin toxicity on ionic regulation and gill Na+/K+-ATPase activity of a freshwater teleost fish Cyprinus carpio. Environ. Toxicol. Pharmacol. 2010;29(1):44–49. doi: 10.1016/j.etap.2009.09.005. [DOI] [PubMed] [Google Scholar]
  52. Svoboda M. Stress in fish – review. Bul. VURH Vodnany. 2001;37:69–191. [Google Scholar]
  53. Trinder P. Determination of glucose concentration in the blood. Ann. Clin. Biochem. 1969;6:24. [Google Scholar]
  54. Van Kampen E.J., Zijlstra N.C. Determination of haemoglobin. Clin. Chem. Acta. 1961;5:719–720. [Google Scholar]
  55. Vijayan M.M., Morgan J.D., Sakamoto T., Grau E.G., Iwama G.K. Food deprivation affects seawater acclimation in tilapia: hormonal and metabolic changes. J. Exp. Biol. 1996;199:2467–2475. doi: 10.1242/jeb.199.11.2467. [DOI] [PubMed] [Google Scholar]
  56. Vosyliené M.Z. The effect of heavy metals on haematological indices of fish (Survey) Acta. Zool. Litu. 1999;9:1392–1657. [Google Scholar]
  57. Wu S.M., Weng C.F., Yu M.J., Lin C.C., Chen S.T., Hwang J.C., Hwang P.P. Cadmium-inducible metallothionein in tilapia Oreochromis mossambicus. Bull. Environ. Contam. Toxicol. 1999;62:758–768. doi: 10.1007/s001289900937. [DOI] [PubMed] [Google Scholar]
  58. Yamawaki K., Hashimoto W., Fujii K., Koyama J., Ikeda Y., Ozaki H. Hematological changes in carp exposed to low cadmium concentration. Bull. Japan. Soc. Sci. Fish. 1986;59(3):459–466. [Google Scholar]
  59. Yang J.L., Chen H.C. Serum metabolic enzyme activities and hepatocyte ultrastructure of common carp after gallium exposure. Zool. Stud. 2003;42:455–461. [Google Scholar]
  60. Younis E.M.1., Abdel-Warith A.A., Al-Asgah N.A. Hematological and enzymatic responses of Nile tilapia Oreochromis niloticus during short and long term sublethal exposure to zinc. Afr. J. Biotechnol. 2012;11(19):4442–4446. [Google Scholar]
  61. Zirong X., Shijun B. Effects of waterborne Cd exposure on glutathione metabolism in Nile tilapia Oreochromis niloticus liver. Ecotoxicol. Environ. Saf. 2007;67:89–94. doi: 10.1016/j.ecoenv.2006.04.006. [DOI] [PubMed] [Google Scholar]

Articles from Saudi Journal of Biological Sciences are provided here courtesy of Elsevier

RESOURCES