A microdigestion procedure directly performed in the autosampler cups for the determination of trace elements in biological samples by GF AAS

SHORT REPORT

A microdigestion procedure directly performed in the autosampler cups for the determination of trace elements in biological samples by GF AAS

Reinaldo C. CamposI, ^*; Sergio F. Jerez Vegueria^{I, II}; Rodrigo A. Gonçalves^I; Ângela L. R. Wagener^I

^IDepartamento de Química, Pontifícia Universidade Católica do Rio de Janeiro, CP 38097, 22453-900 Rio de Janeiro-RJ, Brazil

^IIInstituto de Química, Universidade Federal Fluminense, 24020-150 Niterói-RJ, Brazil

ABSTRACT

A microdigestion procedure for the determination of Cd and Cu in biological samples by graphite furnace atomic absorption spectrometry (GF AAS) is described. Masses up to 5 mg are directly weighed in the autosampler cup and 100 µL of the digestion solution (1:1 v/v HNO₃-H₂SO₄ or concentrated HNO₃) are added. The cups are closed and the digestion is performed, at 60 ºC overnight in a specially designed digestion block. After cooling, 900 µL of ultrapure water is added, the solution is homogenized and the cups are transferred to the autosampler tray. Since the digestion is performed in a sealed environment and the whole procedure uses only one flask, the risks of contamination and losses are minimized. Calibration was performed with external calibration curves, in the same medium as the reagents blank. The analysis of nine different standard reference materials permitted the assessment to the accuracy of the procedure. Considering a 5 mg sample mass, the limits of quantification in the original samples calculated from ten successive measurements of the blank solution (k=10) were 0.07 and 1.7 and 0.02 and 0.3 µg g^-1 for Cd and Cu respectively, using the HNO₃-H₂SO₄ mixture or concentrated HNO₃ for the digestion. The procedure was used for the determination of Cu in human liver biopsy samples.

Keywords: microdigestion procedure, trace analysis, graphite furnace atomic absorption spectrometry

RESUMO

Um procedimento de microdigestão para a determinação de Cd e Cu em amostras biológicas por espectrometria de absorção atômica em forno de grafite (GF AAS) é descrito. Massas de até 5 mg são pesadas diretamente na cubeta do amostrador automático e 100 µL de solução digestora (HNO₃-H₂SO₄ 1:1 v/v ou HNO₃ concentrado) são adicionados. As cubetas são fechadas e a digestão é realizada a 60 ºC, por 12 h, em um bloco de digestão especialmente desenhado; seguem-se a adição de 900 µL de água ultrapura, a homogeneização e transferência das cubetas ao amostrador automático. O ambiente fechado e o uso de apenas um único frasco durante todo o processo minimizam os riscos de contaminação e perdas. Curvas analíticas externas, no mesmo meio do branco, mostraram-se adequadas para a calibração. A análise de nove diferentes materiais de referência certificados permitiu a avaliação da exatidão do procedimento. Os limites de quantificação na amostra original (5 mg), calculados a partir de dez sucessivas medições do branco (k = 10) foram 0,07 e 1,7 ou 0,02 e 0,3 µg g^-1 para Cd e Cu, respectivamente, usando cada uma das misturas. O procedimento foi utilizado, com sucesso, para a determinação de Cu em amostras de biópsia de fígado humano.

Introduction

The sample dissolution or digestion is still the most common sample pre-treatment in total trace analysis, since a low viscosity liquid (preferably an aqueous solution) is the more adequate way for presenting samples to most available instrumentation.¹ The introduction of liquid samples is simpler and faster, also allowing the full automation of this step. However, when the sample amount is a limitation sample dissolution or digestion may lead to difficulties, since these procedures usually need sample amounts at the 0.1-1 g order, leading to final volumes from 10 to 100 mL. Solid sampling (SS) is an alternative and techniques such as solid sampling electrothermal vaporization associated to inductively coupled plasma mass spectrometry (SS-ETV-ICP-MS) or solid sampling graphite furnace atomic absorption spectrometry (SS-GF AAS) are examples of such possibility.^2,3 Solid sampling is claimed to avoid the risks of contamination and losses that are related to sample digestion, and since no dilution occurs, excellent limits of detection in the original samples can be obtained. However, typical problems related to solid sampling still impair the spread of its acceptance in routine analysis: Due to the small sample masses usually used ^4,5 problems related to sample non-homogeneity may be experienced; since the use of aqueous calibration solutions is not always possible, calibration problems may also be observed.

An alternative for dealing with small sample masses are microdigestion procedures.^6-19 They can be performed by direct acid addition or vapor phase digestion.^{7-10,12,14,15,19-25} Contamination risks can be minimized if a single vessel is used for the whole procedure.^{6,8,11,15,19-23,25-30} For instance, Sperling has proposed a microdigestion procedure for the determination of Cd in environmental samples.³¹ He used 50 µL of a 1+4 v/v H₂SO₄:HNO₃ mixture to digest 5 mg of biological materials in 1.5 mL polypropylene (eppendorf) vials. The solution was then made up to 1 mL with deionized water before ammonium pyrrolidinedithiocarbamate (APDC) extraction and GF AAS determination in the organic extract. Later on, Campos et al.³² have used the same strategy as a comparison procedure for the analysis of small masses of solid powdered vegetable samples, but the GF AAS determination was performed directly in the aqueous solution derived from the acid digestion. An interesting variation was presented by Flores and co-workers, who determined As in 10 mg hair samples, after microwave assisted digestion in 1.5 mL polypropylene vials; determination was performed by hydride generation atomic absorption spectrometry, and the digestion flask was used as reduction vessel, as well.³³ However, if GF AAS is to be used, as in the former cases, the final sample solution has still to be transferred to the autosampler cups. Thus, in order to overcome this step, the present work proposes and investigates the direct weighing and digestion of biological samples in the autosampler cups of the GF AAS instrument itself. The digestion was performed in a sealed system using a specially designed digestion block, avoiding any sample transference, aiming at minimizing contact with exogenous surfaces.

Experimental

Instrumental

The GF AAS measurements were performed in a model ZEEnit 60 (Analytik Jena, Jena, Germany) atomic absorption spectrometer, equipped with a transversally heated graphite atomizer, and an AS-52 autosampler. Cadmium and Cu hollow cathode lamps (Analytik Jena) operated at 228.8 and 324.8 nm were respectively used as line sources. The lamp currents and slits were those recommended by the manufacturer. Pin platform pyrolitically coated graphite tubes were used, as well as Zeeman effect based background correction with the 2-field mode at 0.8 T. Measurements were performed in peak area, and were the average of at least 3 replicates. The injected volumes were always 10 µL. An AD-4 microbalance (Perkin Elmer, Bodenseewerk, Germany, Part No. C655-001, 0.1 µg sensitive) was used for the sample weighing. For the digestion, a specially designed cylindrical aluminum digestion block (Ø = 140 mm; h = 40 mm), with 18 drilled holes (Ø = 14 mm) were used. The cups stoppers were kept in place during the digestion by an aluminum cover (Ø = 140 mm; h = 12 mm), tightened by three screw-nuts (Figure 1). The autosampler cups (Sarstedt, Numbrecht, Germany, part number 73.641) are made of polystyrene, and the stoppers (Sarstedt, part number 65.649) are made of low density polyethylene.

Materials, reagents, solutions, certified reference materials and samples

Argon 99.99% (AGA, Rio de Janeiro, Brazil) was used as a protective and carrier gas. Ultra pure water, obtained from a Gehaka Master System apparatus (Gehaka, Sao Paulo, Brazil) was used throughout. Analytical grade HNO₃ (Vetec, Rio de Janeiro, Brazil) was purified by sub boiling distillation using a teflon^R sub boiler apparatus (Hans Kuerner, Rosenheim, Germany). Sulfuric acid (Merck, Rio de Janeiro, Brazil) was of analytical reagent grade and 1000 mg L^-1 Cd and Cu stock solutions were respectively prepared by adequate dilution of Titrisol ampoules (Merck, Darmstadt, Germany) with 0.2% v/v HNO₃. Calibration solutions were prepared by further convenient dilutions of the stock solutions in the same acid concentration as the digestion blanks. Two digestion solutions were used: 1+1 v/v HNO₃:H₂SO₄ and concentrated HNO₃. Palladium nitrate (10000 mg L^-1) and Mg(NO₃)₂ (10000 mg L^-1), both from Merck were used for preparing the modifier solution. A series of certified reference materials (CRMs) was analyzed and they are listed throughout the work. Two biopsy human liver samples were also analyzed. All plastic ware was washed with tap water, immersed in 10% v/v neutral Extran solution (48 h), rinsed in sequence with tap and deionized water, and immersed in 20% v/v HNO₃ for, at least, 24 h. Before handling, these materials were thoroughly rinsed with ultrapure water and oven dried at 40 ºC, avoiding any contact with metallic surfaces and dust contamination. Contamination was always checked up by a strict blank control.

Proposed procedure

Sample aliquots weighing between 0.5 and 5 mg were directly weighed in the autosampler vials (conical bottom). The acid digestion solution (100 µL) was then added to the vials. The cups were tightly closed with the plastic stoppers and placed in the digestion block. The cover of the digestion block was then screwed on the body of the block, pressing the stoppers and sealing the cups. The digestion block was transferred to an oven, and heated to 60 ºC remaining at this temperature overnight. All the digestion was performed in a hood; afterwards, the digestion block was let to cool down to the room temperature, the cover of the digestion block was removed and the cups (still closed) were removed from the block. In this way, no oxidation of the block was observed along the experiments. The cups were opened, and 900 µL of ultrapure water was added to each vial. Homogenization was achieved by aspirating/dispensing the solution in the vials many times. This operation was manually performed with the micropipette used for adding the ultrapure water, using a unique tip for each cup. The vials were then transferred to the autosampler tray and the GF AAS analysis was performed according to the optimized graphite furnace programs displayed in Table 1. Cadmium determination was performed with the aid of Pd and Pd+Mg as modifiers. The modifier masses dispensed onto the platform were 10 µg (Pd) and 10 + 15 µg (Pd+Mg(NO₃)₂) and the injected volumes (sample and modifier solutions) were 10 µL. Palladium alone was used for the samples digested with the acid mixture; Pd+Mg when only HNO₃ was used. The modifier was injected in the conventional way that is after the sample solution and before the drying steps. The water contents of the CRM samples were determined in separate aliquotes, by heating them at 105 ºC overnight. The calculations took the water content into consideration.

Results and Discussion

Temperature program optimization

Optimum pyrolysis and atomization temperatures were obtained from pyrolysis and atomization temperatures curves performed in the blanks, prepared by the 1+9 (v/v) dilution of the digestion solutions (1+1 v/v HNO₃:H₂SO₄ and concentrated HNO₃). They are displayed in Table 1 as well as other temperature programs parameters. Before the determinations, the vicinities (± 100 ºC) of the pyrolysis and atomization temperatures chosen were investigated for both the calibration solutions and each kind of sample solution. This was due to the possibility of differences between set and real temperatures. This also permitted to verify the adequacy of the pyrolysis and atomization temperatures to the real samples.

Calibration and figures of merit

External calibration was performed with aqueous calibration solutions prepared using the same media as the blanks. No statistically significant difference was observed between the slopes derived from these calibration curves and those obtained from analyte addition curves, for the various matrices and the two elements studied. Correlation coefficients were always better than 0.99 and typical coefficients of variation between 1 and 3% were observed if the same sample solution was analyzed in sequence (n = 5). The limits of detection (LODs) were calculated from 10 successive measurements of the blank solutions (k = 3) as recommended by IUPAC. They were 0.1 and 2.5 µg L^-1, for Cd and Cu respectively, if the acid mixture had been used for the digestion. For the digestion with HNO₃, they were 0.03 and 0.5 µg L^-1. Considering sample masses of 5 mg, the limits of quantification in the original samples were 0.07 and 1.7 µg g^-1 using the digestion mixture, and 0.02 and 0.3 µg g^-1 using the concentrated HNO₃, for Cd and Cu, respectively.

Accuracy

Accuracy was assessed by the analysis of certified reference materials. They are listed in Tables 2 and 3, as well as their respective certified values and confidence ranges. Table 2 also shows the results, and their respective confidence ranges, obtained after digestion with the 1+1 v/v HNO₃:H₂SO₄ mixture, while Table 3 refers to the HNO₃ digestion. In relation to Cd, the digestion with the 1+1 v/v HNO₃:H₂SO₄ solution (Table 2) led to good agreement between found and certified values for the four CRMs that showed Cd values above the limit of quantification of the procedure. Cd values in Dogfish Muscle, Non Fat Milk Powder, Peach, Citrus and Apple Leaves were below this limit. For Cu, its content in only one CRM was below the limit of quantification (Non Fat Milk Powder). For all other CRMs, good agreement between found and certified values was observed. For the digestion with concentrated HNO₃ only (Table 3), better limits of quantification could be observed due to the lower blanks obtained. The concentrated HNO₃ was purified by sub boiling distillation while this purification procedure proved to be ineffective for H₂SO₄. The lower blanks permitted the determination of Cd in two of the CRMs (Peach Leaves and Citrus Leaves) that were below the limit of quantification using the previous digestion mixture. Acceptable agreement between found and certified values was verified, especially considering that their values are very close to the limit of quantification. On the other hand, low Cd recovery was now observed for Dogfish Muscle. In contrast, for Cu, a good agreement was observed in all cases, and the new limit of quantification was low enough to permit the Cu determination even in the Non Fat Milk Powder CRM.

Confidence ranges of the found values larger than those correspondent to the certified values can be explained by the small sample masses used in the proposed procedure in comparison to those used in the certification of these materials. However, even in these cases the coefficients of variation of the proposed procedure are adequate for trace analysis. Note that in Tables 2 and 3 the n = 5 value is related to the number of independent analysis performed for the same sample, which includes the sample weighing. As expected, a tendency to larger coefficients of variation was observed in the cases which concentration values were close to the limits of quantification.

Application

A significant application for the proposed procedure arose when two liver biopsy samples came to the laboratory in order to be investigated for their Cu content, for a possible Wilson disease diagnostic. They were presented in small pieces about 2 mm³ in size, implicating that any physical pre-treatment (grinding, homogenization) would be technically difficult and lead to prohibitive mass losses. Their very small masses also impaired the use of conventional digestion procedures. The use of direct solid sampling GF AAS would imply cutting the samples in even smaller pieces, a difficulty and risky operation, due to the very small sample size. Thus, the samples were analyzed as they were received: Each small piece was directly introduced and weighed in the cup for digestion. They weighed 5.222 and 5.960 mg (wet weight), respectively. They were submitted to the proposed microdigestion procedure, using the 1+1 v/v HNO₃:H₂SO₄ acid mixture, and Cu values of 11 and 38 µg g^-1, wet weight were found in the two biopsy samples, respectively. A parallel Bovine Liver CRM analysis was run, for quality assurance leading to good agreement between the found and certified value.

Conclusions

The proposed method proved to be feasible for the digestion of different kinds of biological samples. Good agreement between found and certified values using the 1+1 v/v HNO₃:H₂SO₄ digestion mixture was observed in the determination of Cd in those investigated CRMs that presented Cd values above the limit of quantification. The digestion with concentrated HNO₃ alone led to poorer Cd recoveries in the analysis of Dogfish Muscle. However, it permitted the assessment of less concentrated CRMs due to lower limit of quantification found in this case, a consequence of the lower blank. For Cu, good agreement between found and the certified values was observed in all investigated CRMs by both digestion procedures. However, the digestion with HNO₃ also permitted the assessment to lower concentrations due to the lower blanks observed. These results underline the importance of a detailed optimization of the digestion mixture composition for a full exploitation of the proposed procedure. Concerning the background attenuation, it was always comfortably in the range of the background corrector.

The proposed digestion procedure is simple, performed in a closed environment, and actually uses only one vessel from weighing till the instrumental measurement, minimizing the risks of contamination or losses. The small size of the digestion vessel (the autosampler cup, itself) makes it possible to design small heating blocks with a large number of places. These blocks are easy to handle, heat in normal ovens, and cool down in a short time, due to their relatively small mass. The final sample solution homogenization is easily performed with the same automatic pipette used for making up the final volume, and the cups are ready to be transferred to the autosampler tray. The temperature of the digestion procedure could not be increased, otherwise the autosampler cups would deform, impairing their proper adjustment in the autosampler tray. This led to a somewhat large digestion time. However, the possibility of batches with a large number of places can compensate for this disadvantage if a large number of samples are to be analyzed. The investigation of other digestion mixtures may also enlarge the applicability of the method. The limits of quantification were low enough to permit Cu determination in all samples and Cd determination in all but two CRMs. To the best of our knowledge, this is the first really one vessel digestion-instrumental determination procedure described for GFAAS in the literature. The method also aligns itself with the principles of a green analytical methodology.^34,35 It is important to note that certified values and their ranges in certified reference materials are calculated for sample masses much larger than those used in the present work. Thus one can expect that an important contribution to the coefficients of variation presently found is related to the sample non homogeneity, due to the small masses used. However, even with such low masses, the investigated CRMs have shown themselves sufficient homogeneous to permit acceptable coefficient of variations in trace analysis. This is also observed in other micro sampling techniques, such as solid sampling GF AAS.^36-42

Received: June 26, 2008

Web Release Date: October 29, 2009

• 1. Butler, O. T.; Cook, J. M.; Harrington, C. F.; Hill, S. J.; Rieuwerts, J.; Miles, D. L.; J. Anal. At. Spectrom. 2006, 21, 217.
• 2. Resano, M.; Aramendia, M.; Devos, W.; Vanhaecke, F.; J. Anal. At. Spectrom 2006, 21, 891.
• 3. Vale, M. G. R.; Oleszczuk, N.; dos Santos, W. N. L.; Appl. Spectrosc. Rev. 2006, 41, 377.
• 4. Kurfürst, U.; Appl. Spectrosc. Rev 1991, 63, 1205.
• 5. Belarra, M. A.; Resano M.; Castillo, J. R.; J. Anal. At. Spectrom. 1998, 13, 489.
• 6. Croteau, M.; Hare, L; Tessier, A.; Can. J. Fish. Aquat. Sci 2001, 58, 1737.
• 7. Barkacs, K.; Varga, A.; Gál-Solynos, Zaray, G.; J. Anal. At. Spectrom 1999, 14, 577.
• 8. Araújo, G. C. L.; Nogueira, A. R.; Nóbrega, J. A.; Microchim. Acta 2004, 144, 81.
• 9. Dash, K; Thangavel, S.; Dhavile, S. M.; Rao, S. V.; Chaurasia, S. C.; Arunachalam; Anal. Chim. Acta 2005, 546, 229.
• 10. Amarasiriwardena, D.; Analyst 1994, 119, 1017
• 11. Nieuwenhuize, J.; Poley-Vos, C. H.; Goud, A.; Hemminga, M. A.; At. Spectrosc. 1988, 9, 204.
• 12. Dombovári, J.; Becker, J. S.; Dietze, H. J.; Fresenius J. Anal. Chem 2000, 367, 407.
• 13. Anderson, K.; At. Spectrosc. 1996, 17, 30.
• 14. Krushevska, A.; Waheed, S.; Nóbrega, J. A.; Amarisiriwardena, D.; Barnes, R. M.; Appl. Spectrosc. 1998, 52, 205.
• 15. Bohlen, A.; Klockenkamper, R.; Messerschimidt, J.; Alt, F.; Anal. Chim. Acta 2002, 451, 279.
• 16. Silva, M. M.; Vale, M. G. R.; Damin, I. C. F.; Welz, B.; Mandaji, M.; Fett, J. P.; Anal. Bioanal. Chem 2003, 377, 165.
• 17. Marcó, L. M; Capote, T.; Hernández, C.; Greaves, E. D.; Spectrochim. Acta 2001, 56B, 2187.
• 18. Cain, D. J.; Buchwalter, D. B.; Luoma, S. N.; Environ. Toxicol. Chem 2006, 25, 1042.
• 19. Araújo, G. C. L.; Nogueira, A. R. A.; Nóbrega, J. A.; Analyst 2000, 125, 1861.
• 20. Dash, K.; Thangevel, S.; Dhavile, S. M.; Chandrasekaran, K; Chaurasia, S. C.; At. Spectrosc 2003, 24,143.
• 21. Eilola, K.; Peramaki, P.; Analyst 2003, 128, 194.
• 22. Czégény, Z.; Berente, B.; Óvári, M.; Tapia, M. T.; Záray. G.; Microchem. J 1998, 59, 100.
• 23. Eilola, K.; Peramaki, P.; Fresenius J. Anal. Chem 2001, 369, 107.
• 24. Nóbrega, J. A.; Trevizan, L. C.; Araújo, G. C. L.; Nogueira, A. R. A.; Spectrochim. Acta 2002, 57B, 1855.
• 25. Niemela, M.; Kola, H.; Eilola, K.; Peramaki, P.; J. Pharm. Biomed. Anal 2004, 35, 33.
• 26. Silva, W. G. P.; Campos, R. C., Miekeley, N.; Anal. Lett 1998, 31, 1061.
• 27. Momen, A.; Zachariadis, G. A.; Anthemidis, A. N.; Stratis, J. A.; Anal. Chim. Acta 2006, 565, 81.
• 28. Dhindsa, H. S.; Battle, A. R.; Mierzwa, J.; Fresenius J. Anal. Chem 1998, 362, 374.
• 29. Padilla, L. K.; Anderson, K. A.; Chemosphere 2004, 49, 575.
• 30. Dierenfeld, E. S.; tkinson, S.; Craig, M.; Walker, K. C.; Strich, W. J.; Clauss, M.; Zoo Biol. 2005, 24, 51.
• 31. Sperling, K. R. In Fortschiritte in der Atomspektrometrischen Spurenanalytik; Welz, B., ed., VCH: Weiheim, Germany, 1984, p. 385.
• 32. Campos, R. C.; Curtius, A. J.; Berndt, H.; J. Braz. Chem. Soc 1990, 1, 66.
• 33. Flores, E. M. M.; Saidelles, A. P.; Barin, J. S. ; Mortari, S. R.; Martins, A. F.; J. Anal. At. Spectrom 2001, 16, 1419.
• 34. Lawrence, H. K.; Gron, L.U.; Young, J. L.; Chem. Rev 2007, 107, 2695.
• 35. Armenta, S.; Garrigues, S.; de la Guardia, M.; Trends Anal. Chem 2008, 27, 197.
• 36. Nowka, R.; Müller, H.; Fresenius J. Anal. Chem 1997, 359, 132.
• 37. Silva, M. M.; Vale, M. G. R.; Damin, I. C. F.; Welz, B.; Mandaji, M.; Fett, J. P.; Anal. Bioanal. Chem 2003, 377, 165.
• 38. Resano, M.; Garcia-Ruiz, E.; Vanhaecke, F.; Crespoband, C.; Belarra, M. A.; J. Anal. At. Spectrom. 2004, 19, 958.
• 39. Kurfurst, U.; Rehnert, A.; Muntau, H.; Spectrochim. Acta 1996, 57B, 229.
• 40. Ribeiro, A. S.; Vieira, M. A.; da Silva, A. F.; Borges, D. L. G.; Welz, B.; Heitmann, U.; Curtius, A. J.; Spectrochim. Acta 2005, 60B, 693.
• 41. Resano, M.; Briceno, J.; Aramend, M.; Belarra, M. A.; Anal. Chim. Acta 2007, 582, 214.
• 42. Detcheva, A.; Grobecker, K. H.; Spectrochim. Acta 2006, 61B, 454.

Publication Dates

• Publication in this collection
  14 Oct 2011
• Date of issue
  2009

History

• Accepted
  29 Oct 2009
• Received
  26 June 2008