Print version ISSN 0103-3131
Rev. Bras. Fisiol. Veg. vol.12 no.3 Lavras 2000
Departamento de Biologia/Faculdade de Filosofia, Ciências e Letras de Ribeirão Preto/Universidade de São Paulo Ribeirão Preto SP
ABSTRACT - Seed composition and reserve mobilization were investigated in wild poinsettia (Euphorbia heterophylla L.). Lipids, around 60% of seed dry mass, are the major reserve. Proteins, including albumins (49%), salt insoluble globulins (30%), salt-soluble globulins (21%) and prolamins (0.3%), comprise about a quarter of seed dry mass. Soluble sugars comprise about 3.6% of seed dry mass, sucrose being the predominant sugar. Starch was not detected in the endosperm of E. heterophylla. Lipid depletion starts after initial imbibition, and is completed between 72 and 96 hours. Protein fractions exhibit different degradation patterns, salt-soluble globulins being continuously degraded after the start of imbibition whereas salt insoluble fractions are degraded between 36 and 72 hours, and albumins between 60 and 84 hours. Globulin depletion is accompanied by an increase in free amino acids in the endosperm whereas intense albumin depletion is not. This result suggests that during albumin depletion there is a rapid transfer of amino acids to the growing embryo. Histochemical studies indicated that light accelerates protein degradation in the micropylar area of the seed. Soluble sugars increase in the embryo with no concomitant decrease in the endosperm, suggesting that sugars are mostly originated from the catabolism of lipids.
ADDITIONAL INDEX TERMS: weed, wild poinsettia, Euphorbiaceae, proteins, lipids, carbohydrates.
COMPOSIÇÃO E MOBILIZAÇÃO DE RESERVA DA SEMENTE DE Euphorbia heterophylla DURANTE A GERMINAÇÃO E DESENVOLVIMENTO INICIAL DA PLÂNTULA
RESUMO A composição e a mobilização de reservas da semente de amendoim-bravo (Euphorbia heterophylla L.) foi investigada. Os lipídios constituem cerca de 60% da massa seca da semente, sendo o principal material de reserva. As proteínas constituem aproximadamente a quarta parte da massa seca da semente distribuídas entre as frações de albuminas (49%), globulinas insolúveis (30%), globulinas solúveis em solução salina (21% ) e prolaminas (0,3%). Os açúcares solúveis constituem cerca de 3,6% da massa seca da semente, sendo a sacarose o açúcar predominante. O amido não foi detectado no endosperma de E. heterophylla. A degradação dos lipídios inicia-se logo após a embebição inicial da semente sendo completada entre 72 e 96 horas. As frações protéicas têm diferentes padrões de degradação: as globulinas solúveis são continuamente degradadas após o início da embebição da semente, as globulinas insolúveis entre 36 e 72 horas e as albuminas entre 60 e 84 horas. A degradação das globulinas é concomitante com o aumento nos níveis de aminoácidos no endosperma, mas a degradação de albuminas não é. Esse resultado sugere que durante a degradação de albuminas ocorre uma rápida transferência de aminoácidos do endosperma para o embrião. Estudos histoquímicos indicaram que a luz acelera a degradação das proteínas na região micropilar da semente. Os açúcares solúveis aumentam no embrião sem uma concomitante diminuição no esdosperma, sugerindo que os açúcares são originados do catabolismo de lipídios.
TERMOS ADICIONAIS PARA INDEXAÇÃO: Planta invasora, amendoim-bravo, Euphorbiaceae, proteínas, lipídios, carboidratos.
Euphorbia heterophylla L. (wild poinsettia), a native plant of tropical and subtropical America (Hutchinson and Dalziel, 1958), is now widely spread as an important weed in at least 28 tropical countries and is present in 37 more (Wilson, 1981). In Brazil it has become a major weed mainly in soybean fields (Cerdeira et al., 1981; Lorenzi, 1982; Santos and Corso, 1986; Pinto and Panizzi, 1994; Barreto and Evans, 1998). In the United States it has been recognized as a major weed in soybean in Louisiana since the late 1970s (Bannon et al., 1978; Moore et al., 1990; Bridges et al., 1992; Willard and Griffin, 1993a, b; Brecke, 1995) and has continued to increase in distribution and prevalence during recent years. It is now considered a weed of major economic importance in both peanut and cotton in Georgia and Florida (Bridges et al., 1992).
Research on E. heterophylla has been mainly directed toward finding suitable methods for its control (Gusman et al., 1990; Moore et al., 1990; Willard and Griffin, 1993a, b; OMakinwa and Akinyemiju, 1993; Brecke and Tobola, 1996). However, it has persisted as an agricultural problem probably resulting from widespread adoption of chemical weed control, coupled with the weeds resistance to most herbicides; high seed production and the fact that seed germination can occur at any time throughout the growing season (Egunjobi and Kupoluyi, 1973; Wilson, 1981; Barreto and Evans, 1998). The germination of E. heterophylla seed has been investigated (Bannon et al., 1978; Suda et al., 1989; Brecke, 1995; Suda and Pereira, 1997) but there is no information available on the physiological and biochemical aspects of reserve composition and mobilization in the seed.
The main purpose of the present work is to analyze lipids, proteins and carbohydrates in the endosperm of E. heterophylla during germination and initial seedling development and thus contribute to the knowledge on seed metabolism in this species.
MATERIAL AND METHODS
Mature fruits of Euphorbia heterophylla L. were collected from local plants and dried until dehiscence; seeds were harvested by hand and stored in air-tight flasks at 5 ºC. At this temperature seeds remain viable for several months (Bannon et al., 1978); however, lots were renewed every 3 months for use in our experiments.
Seeds were germinated in 9-cm Petri dishes on two sheets of Whatman No. 1 filter paper moistened with distilled water (3 mL). The dishes were placed in a growth chamber at 25 or 30 ºC under continuous light or total darkness. For all biochemical analyses the seeds were germinated at 30 ºC. Darkness was maintained by wrapping the Petri dishes with black polyethylene. For germination tests three dishes, each containing 25 seeds, were used for each treatment. For the growth study and biochemical analyses, material was sampled from a large population of seeds or seedlings. Seed germination measurements under darkness were made in a light-proof room under a green safe-light. Germination was defined as elongation of the radicle to at least 5 mm.
Estimation of endosperm degradation and embryo growth
At various times after imbibition, 15 seeds or seedlings were harvested and the embryo (cotyledons plus embryo-axis) separated from the endosperm. For cotyledon dry mass determination 20 pairs of cotyledons were excised from 20 embryos. Dry matter was determined by weighing the parts after a period until dry weight remained constant (at least 24 h at 80 ºC).
Determination of chlorophyll
Chlorophyll was determined using the method of Arnon (1949) after extracting the cotyledons with 80% acetone (v/v). Triplicate samples of 20 pairs of cotyledons were used for each determination.
Determination of lipids, soluble sugars, proteins, amino acids and starch
The seeds and seedlings were harvested and the parts were separated as described above. Triplicate samples of 20 endosperms or embryos were used for each determination.
For total lipid determination endosperm was ground in a mortar and pestle in 5 mL of chloroform:methanol (2:1, v/v) and the next steps were carried out according to the procedure described by Becker et al. (1978), except that the combined organic phases were shaken with 0.1 mol.L-1 KCl, which permitted a better separation of the phases (Radin, 1969). All procedures were done at room temperature.
For soluble sugars and free amino acids determinations endosperms or embryos were ground in a mortar and pestle in 10 mL of 80% ethanol (v/v) and the mixture boiled for 10 min. Following centrifugation at 2,000 x g for 10 min, the supernatant was collected and the pellet reextracted in 10 mL of hot 80% ethanol. Supernatants from both extractions were combined, and total soluble sugar and reducing sugars were then determined by the phenol sulfuric acid (Dubois et al., 1956) and Nelson-Somogy (Somogy, 1952) methods, respectively, using glucose as standard. Free amino acids were determined in the final supernatant by the ninhydrin method (Moore and Stein, 1954) using leucine as standard. In some embryo supernatants chlorophyll removal was necessary before sugar or amino acid determinations. These supernatants were shaken with an equal volume of petroleum ether and, after phase separation, the chlorophyll containing phase (petroleum ether) was discarded and alcoholic phase used for determinations.
Proteins were extracted according to their solubility (García-Agustín and Primo-Millo, 1989) at 4 ºC. Endosperms were subjected to consecutive extraction with distilled water (albumins), 5% (w/v) sodium chloride (globulins), 60% (v/v) ethanol (prolamins) and 0.4% (w/v) sodium hydroxide. The alkali-soluble protein, formerly named glutelin (Shewry and Tatham, 1990), is referred to in the present study as "salt insoluble protein". Extracts were centrifuged at 15,000 x g for 2 min and the supernatant filtered. An aliquot of each extract was taken for the quantification of the proteins by the method of Lowry et al. (1951) using bovine serum albumin as the standard.
Starch was determined by the colorimetric method of Allen et al. (1974) which utilizes KI and KIO3.
Determination of soluble sugars by thin-layer chromatography
Sugar solutions (1 mL) were concentrated at 30 ºC during 24 h by evaporation of solvent (80% ethanol) and aliquots were spotted on silica-gel plates (Whatman, 250 mm layer).
Chromatography was performed according to the method of Lato et al. (1968) using a solvent system of n-buthanol-ethyl acetate-isopropanol-acetic acid-water (7:20:12:7:6). Sugars were stained with naphthoresorcinol.
Anatomical and histochemical analysis
For observations under the light microscope, seeds were collected 0, 24, 48, 72, and 96 hours after the onset of imbibition. For lipids, seeds were sectioned 25-30 m m thick with a freezing microtome and stained in oil red O (Cardemil and Reinero, 1982). Sections which were extracted with acetone were also stained with oil red O, as control. For proteins, the seeds were fixed in FAA (95% ethanol-acetic acid-formaldehyde-water, 10:1:2:7). The seeds were dehydrated in a graded ethanol series and embedded in Paraplast. The sections (25 mm) were stained with 0.25% (w/v) Coomassie Blue G in 50% methanol (v/v) containing 10% (v/v) acetic acid (Cawood et al., 1978).
Gel electrophoresis of protein fractions
Prior to electrophoresis, extracts of salt-soluble globulins and salt insoluble proteins were dialyzed against water and centrifuged at 15,000 x g for 2 min. The pellet was resuspended in 62.5 mmol.L-1 Tris-HCl buffer (pH 6.8) containing 2% (w/v) SDS, 10% (w/v) glycerol, 5% (v/v) b-mercaptoethanol and 0.01% (w/v) bromophenol blue and boiled for 90 s. Albumin extracts were mixed with an equal volume of the above buffer twice concentrated.
Electrophoresis was carried out in 10% (w/v) SDS-polyacrylamide slab gels, according to the method of Laemmli (1970). Gels were stained with Coomassie Brilliant Blue G. The molecular masses of the proteins were estimated in relation to the mobilities of the molecular mass standard proteins (Dalton Mark VII-L, Sigma).
RESULTS AND DISCUSSION
The literature on light affecting the germination of E. heterophylla seeds is in some cases contradictory. Bannon et al. (1978) observed that light promotes germination when the seeds are maintained at constant temperatures. However, Brecke (1995) reported that the seeds are insensitive to light under the same conditions. Suda and Pereira (1997) showed that light sensitivity during germination in this species may be influenced both by the conditions in which the parent plants were grown and by the time interval during which seeds were stored. In the present work (Figure 1) light caused a highly significant increase in germination over the dark control. At 30 ºC this difference became less apparent after 72 h; however it was still significant even at 120 h as determined by Student t test (P<0.05). The average germination time ± confidence interval (95%) was calculated according to Labouriau and Osborn (1984). At 30 ºC under light or darkness mean germination times were 48.0 ± 2.4 or 74.4 ± 21.6 h, respectively. At 25 ºC under light, the mean germination time was 79.2 ± 28.8 h.
Table 1 summarizes the composition of E. heterophylla seeds. Lipids were the main reserve materials stored in the endosperm. Seeds of species belonging to the family Euphorbiaceae are usually rich in lipids (Rizk, 1987), e.g. castor-bean (Ricinus communis) seeds where the lipid content (Copeland and McDonald, 1995) approaches that found for E. heterophylla. According to Earle et al. (1960), linolenic and linoleic acids constitute the main fatty acids in E. heterophylla seeds.
Seed storage proteins were initially classified by Osborne (1924) according to their solubility into albumins (water soluble), globulins (saline soluble), prolamins (alcohol soluble) and glutelins (acid or alkali soluble). However, on the basis of currently available evidence, glutelins are now considered to be prolamins (Shewry and Tatham, 1990). The results from the sequential extraction procedure of proteins indicated that in E. heterophylla the albumins, the salt insoluble and the salt-soluble fractions comprised the major fraction, and prolamins accounted for only 0.3% of the seed protein. The salt-insoluble fraction could be dissolved in 0.1N NaOH or in the presence of SDS (sample buffer for SDS-PAGE). In this respect this fraction is similar to castor bean crystalloid protein (Tully and Beevers, 1976; Gifford et al., 1982). However, the protein from castor bean was also soluble in 0.37 mol.L-1 NaCl (Youle and Huang, 1976) whereas the similar fraction from E. heterophylla was not, even using a more concentrated solution (0.87 mol.L-1 NaCl). According to Gifford and Bewley (1983) and Lalonde et al. (1984) there are two major types within 11S globulins: those which are soluble in salt solutions (e.g., legumins) and those which require the addition of urea or SDS for total solubility (e.g., crystalloids). Thus the insoluble protein of E. heterophylla seed may be included in the second group of globulins. The prolamin fraction is essentially absent in E. heterophylla seeds, confirming the idea that prolamins are restricted to one family, the grasses (Shewry et al., 1995).
The changes in dry matter of the endosperm and embryo (or seedling) are presented in Figure 2. In seeds maintained under light at 30 ºC or 25 ºC (Figure 2 A, C) or in the dark at 30 ºC (Figure 2 B), endosperm depletion occurred between 48 and 120 h from the start of imbibition with a concomitant increase in seedling dry matter. In seeds maintained under darkness at 25 ºC, there was no significant variation in these parameters (Figure 2 D).
The changes in dry matter and chlorophyll content of the cotyledons of light-grown seedlings are shown in Figure 3. There was an initial increase in dry matter between 48 and 72 h followed by a slower increase thereafter. Chlorophyll content increased from 48 h.
Biochemical changes in the endosperm were investigated under light or darkness, at 30 ºC. Degradation of stored lipids began immediately after imbibition (Figure 4). A rapid decline of the oil reserves was observed within 72 to 96 h in both dark and light-grown seedlings, when around 70% of the total lipids were digested. This pattern is unusual compared to some other oil rich seeds. In castor bean endosperm (Muto and Beevers, 1974), maize scutellum (Lin et al., 1983), and cucumber cotyledons (Slack et al., 1977; Becker et al., 1978), the total lipid content remained unchanged during early periods of germination but declined quickly thereafter.
The total sugar (Figure 5 A) in the endosperm remained essentially constant up to 72 h, declining thereafter. Reducing sugars (Figure 5 B) showed rapid increases until 48 h and declined sharply after 72 h. In the embryo (Figure 5 C, D) sugars increased after 36 h. Chromatographic analysis of soluble sugars indicated that sucrose may be the major component of the free sugars fraction in the endosperm tissue (Figure 6 A, lines 5 to 8). Glucose and fructose could be seen in these chromatograms, however, only in trace amounts. This may be not the case in the embryo after 48 h of imbibition, which presented apparently higher amounts of glucose and fructose (Figure 6 B, lines 6 to 8). These results were also in agreement with the colorimetric analysis of sugars (Figure 5 D) where the embryos exhibited increasing amounts of reducing sugars after 48 h. The correlation between the increase in reducing sugars and the appearance of glucose and fructose suggests that the hydrolysis of sucrose may be intense in the embryo over that period. In castor bean sucrose is the sugar actually transported from endosperm and hydrolysis occurs subsequently in tissues to which the sucrose is moved (Kriedemann and Beevers, 1967a,b). The total sugar level in the endosperm did not decrease when embryo sugar levels were increasing (Figure 5 A, C). Probably in the endosperm the conversion of stored lipids to carbohydrates occurred, maintaining sugar levels. This idea is supported by the fact that embryos also exhibit a similar increase in total sugar levels when seeds are maintained in the dark, and photosynthesis may then be excluded as the main source of sugars from the embryo. The conversion of reserve lipids to sugars has been extensively investigated in castor bean seeds (Kornberg and Beevers, 1957; Canvin and Beevers, 1961; Beevers, 1961). However, another source of sugar from the endosperm may be from amino acids derived from the breakdown of protein occurring at the same time. Gluconeogenesis from amino acids was demonstrated in germinating castor bean endosperm (Stewart and Beevers, 1967).
Starch and raffinose, which serve as reserve carbohydrates in a number of seeds (Bewley and Black, 1985), were not detected in E. heterophylla seeds (Table 1 and Figure 6 A, lines 4 to 8). This finding is consistent with another study which indicated that another member of Euphorbiaceae, castor bean, does not contain raffinose (Amuti and Pollard, 1977).
Quantitative changes in the protein reserves are presented in Figure 7. The main periods of degradation occurred between 60 and 84 h for albumins and between 36 and 72 h for salt insoluble proteins when these fractions decreased respectively by 80% and 98% of their initial values. Salt-soluble globulins exhibited a slower decrease over the entire period.
Electrophoretic profiles of endospermic protein fractions obtained from quiescent seeds at several periods after the start of imbibition are presented in Figure 8. The major bands of albumins exhibited molecular masses between 29.5 to 66 kDa and 20 to 22 kDa; salt-soluble globulins between 43 to 47 kDa, 31 to 36 kDa and 18 to 26 kDa; salt insoluble proteins ranged between 29 to 36 kDa and 18 to 20.5 kDa. Lalonde et al. (1984) reported for the insoluble protein (reduced form) from seeds of several Euphorbiaceae, including E. heterophylla, the predominance of two groups of polypeptides (20 to 25 kDa and 29 to 35 kDa). The polypeptides between 20 to 25 kDa were not prominent in our insoluble fraction (Figure 8) but were present in the salt-soluble fraction. This difference may be due to the methods of extraction since our insoluble fraction is the residue of high salt extraction which was included in our work as an additional step. Moreover, the molecular mass ranges obtained for E. heterophylla globulin subunits are in agreement with Marcone et al. (1998), who conducted detailed characterization of 21 purified seed globulins from dicotyledonous and monocotyledonous plants and concluded that the majority of subunits fell within two molecular mass ranges: 20 to 27 kDa and 30 to 39 kDa. In addition, we observed that in the case of E. heterophylla the low molecular mass globulin subunits were found mainly in the salt-soluble fraction, whereas the high molecular mass subunits were found in both salt-soluble and insoluble fractions. After 48 h the albumin fraction exhibited a predominance of smaller polypeptides (around 20 kDa) (Figure 8). These results suggest that the albumin fraction may be subject to gradual hydrolysis in this process.
Quantitative changes in free amino acids are presented in Figure 9. In the endosperm there was a peak between 24 and 60 h under light, and between 36 and 96 h under dark conditions. Most of the free amino acids which increase and accumulate in the endosperm (until 60 h under light or 72 h under darkness) may come from the degradation of globulins (salt-soluble and insoluble), since the amount of amino acids which are released by albumin degradation in this period may be low because limited proteolysis releases low amounts of amino acids (Müntz, 1996). In seeds maintained under light, the level of free amino acids rapidly decreased in the endosperm and simultaneously increased in the embryo over the period which coincided with the degradation of albumins (between 60 to 72 h) (Figures 7 and 9). These results suggest that amino acids derived from albumins could be rapidly transferred from the endosperm into the embryo, owing to a source sink relationship. The translocation in the dark was slower because the embryo could not be a fully active metabolic sink.
Histochemical analysis showed that lipid reserves in E. heterophylla endosperm are laid down in oil-bodies (Figure 10 A). The morphology of those bodies was modified 24 h after the onset of imbibition with swelling and apparent loss of integrity followed by their gradual disappearance (Figure 10 B). These oil-bodies disappeared from the cells when the tissue was previously washed with acetone as control (not shown).
Sections from the endosperm of quiescent seeds exhibited protein bodies in abundance (Figure 11 A). Their fusion was observed at 24 h after the onset of seed imbibition, and their disappearance occurred gradually until 72 h (under light) (Figures 11 B, C, D) or 96 h (under darkness, not shown).
Protein degradation in seed storage tissues during germination does not occur at once in the entire organ, the region where degradation starts varying according to species (Harris and Chrispeels, 1975; Harris et al., 1975; Davies and Chapman, 1981; Asghar and DeMason, 1990; Dias et al., 1993). In the present case, storage protein degradation was initiated in the micropylar region before emergence had occurred (Figure 12) and was accelerated by light. The disappearance of protein bodies occurred 24 h earlier in the light than in the dark (not shown). A similar phenomenon was observed in red light-treated lettuce (Lactuca sativa) achenes, where reserve materials of the micropylar end of the endosperm were mobilized prior to visible germination (Psaras et al., 1981).
The results presented here suggest that light may influence both degradation and translocation of reserves in the endosperm of E. heterophylla during germination and early seedling establishment. The observed decreases in dry mass were about 40% under light and about 20% under darkness between 48 and 72 h after the start of imbibition. Lipids, total protein and amino acids decreased over the same period at higher rates under light (about 47%, 80% and 77%, respectively) when compared to the dark condition (about 20%, 66% and 1%, respectively). On the other hand, decreases in total sugars and reducing sugars did not exhibit notable differences between light and dark germination conditions.
We thank Mr. Antônio J. Colusso, Mr. Marcelo Gonçalves, and Mr. Jaime L. Zeotti for technical assistance. We are grateful to Dr. João K. Kajiwara, Departamento de Morfologia, Faculdade de Medicina de Ribeirão Preto, Universidade de São Paulo for suggestions with respect to histochemical detection of lipid bodies. This work was partially supported by grants 92/3176-4 and 96/8069-2 to JFG, Fundação de Amparo à Pesquisa do Estado de São Paulo.
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Received: 02/02/00 Accepted: 10/10/00
1. Graduate student, Departamento de Bioquímica, Faculdade de Medicina de Ribeiro Preto, Universidade de São Paulo, Ribeirão Preto SP, 14.049-900, Brasil. E-mail:email@example.com
2. Corresponding author. E-mail: firstname.lastname@example.org