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Tree Physiology 20, 467–475 © 2000 Heron Publishing—Victoria, Canada Changes in cellular structures and enzymatic activities during browning of Scots pine callus derived from mature buds HANNA LAUKKANEN, LEA RAUTIAINEN, ERJA TAULAVUORI and ANJA HOHTOLA Department of Biology/Botany, University of Oulu, PO Box 3000, FIN-90401 Oulu, Finland Received March 29, 1999 Summary Visible browning is a typical feature of callus cultures derived from shoot tips of mature Scots pine (Pinus sylvestris L.). Because the ability of callus to regenerate is low, we determined the effect of browning on growth and changes in cellular structure during culture. Striking alterations in cellular structure were detected by LM (light microscopy), EM (electron microscopy) and SEM (scanning electron microscopy). Accumulation of phenolic substances was shown by histochemical staining. Staining for $-glucosidase activity of soluble proteins that had been subjected to polyacrylamide gel electrophoresis indicated lignification of cells. The measured growth rate of callus was low compared with a hypothetical growth curve. Peroxidase activity increased rapidly soon after the start of the culture period, but especially between the second and third weeks of culture. At this time, the degradation of cell membranes and browning began coincident with the loss of chlorophyll. We conclude that browning is associated with cell disorganization and eventual cell death, making tissue culture of mature pine especially difficult. Keywords: extracellular matrix, growth, $-glucosidase, phenolics, Pinus sylvestris, peroxidase, recalcitrance, tannin. ameliorative effect on browning of Scots pine callus derived from mature pine buds. Peroxidases have many roles in plant growth and development. Campa (1991) reported that peroxidases were associated with chlorophyll degradation and lipid peroxidation in senescent plant tissues. The presence of phenol compounds accelerates this degradation (Kato and Shimizu 1985). Elevated peroxidase activity is often associated with the production of polyphenols, e.g., lignins and tannins, which may also act as antioxidants against oxidative stress (Sakagami et al. 1995). Although Scots pine callus showed oxidative activity when catechol was used as a substrate for polyphenol oxidase (Laukkanen et al. 1999), addition of catalase revealed that the oxidation was mainly (60–70%) caused by peroxidases. Catechol oxidation activities did not correlate with the onset or progress of browning. Because of the recalcitrance of mature Scots pine in tissue culture, we investigated changes in growth, cytoplasmic and extracellular structures during browning to assess the effect of browning on the regeneration ability of tissue cultures of mature pine. The roles of peroxidase, lipid peroxidation, pigment degradation, lignification and onset of browning were also investigated. Introduction Browning or blackening is frequently observed in tissue cultures of woody plants. Browning is caused by the oxidation of phenols after cellular disorganization. Disorganization of cellular components is often a result of the degradation of membranes by the toxic forms of oxygen (Lee and Whitaker 1995). Oxidation of phenols may occur nonenzymatically, or may be catalyzed by phenol oxidases or peroxidases (Webb 1966, Rhodes and Wooltorton 1978, Vaughn and Duke 1984, Ke and Saltveit 1988). The brown polymers of phenols have been reported to hamper tissue culture of many high-tannin plants, such as Sorghum (Cai et al. 1987), Quercus (Tóth et al. 1994) and Pinus (Laukkanen et al. 1997) species. Attempts have been made to prevent the browning of many food plants, especially fruits and vegetables, by various chemicals, to enhance preservation (Vámos-Vigyázó 1995). Hohtola (1988) tested a range of concentrations of various oxidase inhibitors and antioxidants in the growth medium and found that they had no conclusive Materials and methods Plant material and culture conditions Twigs were collected in April and November from 15- to 20-year-old Scots pine (Pinus sylvestris L.) trees growing in natural stands in Oulu, northern Finland (65o N; 25o30¢ E). The buds were surface-sterilized in 5–6% calcium hypochlorite for 20 min and rinsed three times in sterile distilled water, after which the scales were removed aseptically. The bud tips (2–3 mm), including the apical meristem, were placed on MS medium (Murashige and Skoog 1962) modified as described by Hohtola (1988), except that the only inorganic nitrogen source was ammonium nitrate (2 mM), the concentration of sucrose was 2%, and arginine and glucose were not used. The growth regulators 2,4-D (2,4-dichlorophenoxy acetic acid, 4.5 m M), BA (N 6-benzyladenine, 1.7 m M) and kinetin (1.8 m M) were used. The pH was adjusted to 5.7. The medium was solidified with 0.6% Phytagel (Sigma, St. Louis, MO). All 468 LAUKKANEN, RAUTIAINEN, TAULAVUORI AND HOHTOLA tissues were cultured in test tubes for the first 2 weeks and then transferred to fresh medium in test tubes, and finally transferred to petri dishes after 4 weeks. The cultures were maintained in a 16-h photoperiod (white fluorescent Osram 18 W tubes (Germany), at 1.6 W m –2, 400–700 nm) at 24 ± 2 oC. Suspension cultures were initiated by transferring 2-week-old callus to liquid growth medium including the same salts as the solid growth medium and agitated on an orbital shaker (130 rpm). On the days of measurement, 1 ml of suspension culture was taken for dry weight estimation. It was filtered through a preweighed filter paper and washed with deionized water. The filter with the culture was dried overnight at 100 oC before weighing. Color and pigment estimation Color changes in callus were followed visually and spectrophotometrically during culture. The color changes were classified into the following categories: green, yellow-green, yellow-brown, brown and dark brown. Samples (0.5 g) were collected at the beginning of the culture period and at weekly intervals throughout the 7 weeks of culture and homogenized in liquid nitrogen. Pure acetone was used to extract green and yellow pigments from the samples. The extracts were centrifuged (12 000 g, 5 min) and the supernatants were measured spectrophotometrically at 435 (chlorophylls) and 665 (carotenoids) nm (Goodwin 1976). Preparation of samples for LM, EM and SEM During callus culture, small pieces of tissue (3–5 mm) were collected weekly and fixed in 10:5:85 (v/v) FAA (formalin:acetic acid:94% ethanol). The fixed tissues were dehydrated in an ethanol series, infiltrated with 1:1 (v/v) Historesin:95% EtOH and embedded in Historesin (Reichert-Jung, Heidelberg, Germany). Sections were cut with an LKB Historange microtome at 4 m m thickness from 10 blocks. Fresh pieces or LM (light microscopy) sections of callus were stained with 0.05% toluidine blue (Feder and O’Brien 1968), 10% acidic vanillin (Mueller-Harvey et al. 1987), 2% acidic phloroglucinol (Harris et al. 1994) and 0.01% acridine orange (Oparka and Read 1994), or a solution for phenolic compounds containing 2% K3Fe(CN)6 and 2% FeCl3 in water (100 ml) plus 10 crystals of KMnO4 (Mueller-Harvey et al. 1987). The colors of the cell walls after toluidine blue staining indicate the viability of the cells. The cell wall is reddish purple in a viable cell and blue to greenish blue in a dead cell without cytoplasm. Polyphenolic material gives a green coloration and lignified matter a blue coloration (Feder and O’Brien 1968, Harris et al. 1994). Vanillin–HCl characteristically produces a bright cherry red product in the presence of flavan-3-ol monomers (catechin) and polymers. Unstained sections and fresh suspension cells were examined with a fluorescence microscope with UV excitation (Nikon Optiphot 2 with a 100-W HG lamp and an automatic Nikon Microflex UFX 35 DX camera, filter combination Ex 365/10, DM 400, BA 400). Samples for EM (electron microscopy) were prepared according to Kupila-Ahvenniemi and Hohtola (1979), except that pieces of callus tissue were fixed overnight in cold 3% glutaraldehyde in sodium phosphate buffer (pH 7.0), rinsed three times in sodium phosphate buffer, post-fixed in cold 1% osmium tetroxide for 3 h, rinsed three times in sodium phosphate and embedded in Ladd’s epon. For scanning electron microscopy (SEM), the samples were fixed in FAA, dehydrated by ethanol series, dried with a critical point dryer, covered with gold, and viewed in a JEOL JEM 100B scanning electron microscope. Peroxidase assay Vegetative buds (0.3 g) were transferred to an ice-cold beaker after quick removal of the scales. Enzymatic activities were measured in buds (Day 0) and in callus during culture (14, 28 and 42 days after the initiation of culture). For the assay of peroxidase (POD), buds and callus (0.3–0.5 g) were frozen in liquid N2 and ground to a fine powder with a mortar and pestle. The powder was homogenized (45 s, on ice) in 3 ml of extraction buffer, with an electric grinder (Heidolph Elektro KG, Kelheim, Germany). The extraction buffer for POD was 0.167 M potassium phosphate (pH 7.8). After homogenization, 2.5 ml of the extraction buffer containing insoluble PVPP (polyvinyl polypyrrolidone, final concentration 2.5% w/v, soaked for 24 h in buffer) was added to the sample and the mixture allowed to stand for 40 min in the dark with occasional stirring. The mixture was centrifuged at 25,000 g (25 min, 4 oC) and filtered. One hundred m l of the filtrate was added to 100 ml of 0.167 M potassium phosphate buffer (pH 5.5) containing 10 mM guaiacol and 20 mM H2O2. The mixture was incubated at room temperature and the change in absorbance at 470 nm monitored for 5 min. Soluble protein content was measured as described by Bradford (1976). Lipid peroxidation analyses Lipid peroxidation was measured in 2- to 7-week-old callus (0.5 g) by determining malondialdehyde (MDA, a product of lipid peroxidation) content by the thiobarbituric acid (TBA) reaction according to Dhindsa et al. (1981). Protein analyses Soluble proteins were extracted from 0.5-g samples that were ground in liquid nitrogen and homogenized with a mortar and pestle in 2 ml of extraction buffer (50 mM Tris-HCl, pH 8.6, 20 mM KCl and 10 mM MgCl2) containing 1.5% (w/v) of insoluble PVPP. The homogenate was centrifuged at 13 000 g for 15 min. The supernatant was subjected to one-dimensional SDS-PAGE (ExcelGel ™ SDS), as recommended in the Pharmacia (Upsala, Sweden) instruction manual. After electrophoresis, the proteins were visualized by silver staining (Bio-Rad, silver staining kit). The molecular mass standards were from Amersham gradient 8-18 (Pharmacia). Soluble proteins obtained from 1 g samples of callus were separated by non-denaturing PAGE and stained for $-glucosidase activity as described by Dharmawardhana et al. (1995) by incubating with 0.2 mM MUG (4-methylumbelliferyl $-glucoside). Electrophoresis was performed at 4 ° C according to the Laemmli (1970) procedure but without SDS and 2-mercaptoethanol. TREE PHYSIOLOGY VOLUME 20, 2000 BROWNING OF PINE CALLUS For glycoprotein analysis, 1.0 g samples of callus were ground in liquid nitrogen and homogenized with a mortar and pestle in sterile water, after which 2.5 volumes of ethanol were added and the mixture allowed to stand overnight at 4 oC. The ethanol-insoluble residue was precipitated by centrifugation at 15 000 g for 10 min and resuspended in 100 ml of buffer containing 20 mM Tris-HCl (pH 7.4), 100 mM NaCl, 1 mM MgCl2 and 1 mM MnCl2. Glycoproteins were purified according to Gavish et al. (1992). The purified glycoproteins were analyzed by one-dimensional SDS-PAGE (Pharmacia) and stained with Coomassie Brilliant Blue G-250 (Neuhoff et al. 1988). Results Color changes of tissues The rate of browning varied among the different callus tissues, but in most cases the callus changed from green to yellow-green after three days of culture and thereafter changed gradually through yellow-brown to dark brown. The first sign of brown color usually appeared as small yellow-brown spots on the surface of callus after 2 weeks of culture, or after 1 week on the cut surface of the explant. Several dark brown calli were found among the 4-week-old callus samples, and browning was often complete after 8 weeks of culture, though color variations among similar callus masses and among areas of the same callus were evident. The color of suspension cultures derived from callus remained green for 2 weeks, but thereafter the cultures gradually turned to yellow-brown and brown. Concentrations of green and yellow pigments The amounts of green (chlorophylls) and yellow pigments (carotenoids) decreased during culture, but the reduction in chlorophylls usually started after 2 weeks of culture, whereas a decrease in carotenoids was already evident after 1 week (Table 1). The yellow pigments disappeared more slowly than the green pigments, and this was manifest as a color change from green to yellow-green in young callus. The water content of the explants increased after 1 week (Laukkanen et al. 1997), which partly explains the difference in pigment concentrations 469 between the 1-week-old culture and the buds. The peeling of buds probably also affected the amounts of pigments detected. Changes in peroxidase activity and lipid peroxidation during culture Peroxidase activity increased during culture. The activity in 6-week-old callus was 5-fold higher than in buds (Table 1). The rate of increase slowed after 4 weeks of culture. Lipid peroxidation was maximal after 2 weeks of culture, but the process decreased gradually during aging of the callus. Growth of callus and suspension cultures Figures 1A and 1B show the growth of callus and cell suspensions during culture. The fresh weight of callus increased in parallel with the increase in dry weight (cf. Lindfors et al. 1990). The increase in callus production was 2.6-fold from the first to the second week, whereas from the sixth to the seventh week it was only 1.1-fold. The standard deviations of the growth curve increased during culture, reflecting differences in growth among individual calli. The relative growth rate of the callus cultures declined over time, so that there was no exponential growth phase (Figure 1A) (King et al. 1972). The growth curve of the suspension culture showed a large decline in dry weight after 2 weeks of culture (Figure 1B), coinciding with the onset of browning. Alterations in cellular structure during browning The vanillin–HCl test for tannin gave a positive but variable pink-red reaction in a fresh, crushed callus sample. The red color was usually weak in green tissues and bright cherry red in dark brown tissues. Fresh brown callus reacted with phloroglucinol–HCl and acridine orange, indicating lignification of the cells. The cell walls of brown callus also showed a positive blue color after staining with a solution for phenolic compounds (results not shown). The proportion of greenish blue cells increased during the culture, and approximately 50% of the cells were without cytoplasm after 4 weeks of culture (Figure 2A). Fibrillar material (phenolics) was observed in vacuoles of fixed (Figure 2A) and fresh callus cells (Figure 2C) and between the cells (Figure 2D). The young green callus tissue expressed blue Table 1. Changes in the amounts (± SD) of chlorophylls, carotenoid, peroxidase (POD) activity and lipid peroxidation during callus culture. Standard deviations < 10 –1 are not shown. There were three (n) samples for pigment analysis (except Week 1, n = 1); POD = activity of guaiacol peroxidase, n = 3–11; and MDA = malondialdehyde, a product of lipid peroxidation, n = 2–3. Culture time (Weeks) Chlorophylls (A435) Carotenoids (A665) POD (A min –1 mg prot –1) 0 1 2 3 4 5 6 7 2.05 1.58 1.22 1.15 0.80 0.63 0.42 0.36 2.68 1.01 1.07 0.84 0.43 0.34 0.25 0.21 58.7 ± 5.6 121.4 ± 19.8 180.5 ± 50.7 263.3 ± 39.2 307.2 ± 98.4 TREE PHYSIOLOGY ON-LINE at http://www.heronpublishing.com Peroxidation of lipids (m M MDA gFW –1) 27.2 ± 32.4 ± 16.7 ± 21.3 ± 19.5 ± 21.8 ± 6.4 2.5 6.5 1.5 1.7 5.4 470 LAUKKANEN, RAUTIAINEN, TAULAVUORI AND HOHTOLA The cells with thin walls were rich in starch, whereas the yellow-brown cells often lacked cytoplasm. Under the light microscope, sections of old callus usually showed bright white fluorescence in the intercellular spaces (Figure 2F). The cytoplasm of dark brown pine callus was completely disorganized and rich in tannin (Figure 3F, 4A and 4B) or devoid of cytoplasm. Osmiophilic material was seen in the cytoplasm (Figure 3F) and in the intercellular spaces in dying brown callus (Figure 4B). The number of microvesicles (Figure 4B) and other membraneous structures, such as multivesicular bodies (Figure 4C), increased during culture. The number of fibrillar structures increased during culture, and the brown tissues often had very dense fibrillar areas (Figure 4D). Polypeptide analyses Figure 1. (A) Growth curve based on fresh mass (FW, mg) determinations of calli (n = 10) initiated from bud apices. Symbols: 䊉 = measured growth curve; 䊏 = exponential growth curve. (B) Dry weight determinations of suspension cultures (n = 3) derived from pine callus. Symbols: 䊉 = dry mass (mg), measured six times during the culture period (18 days). autofluorescence on UV excitation, whereas the cells just before browning emitted bright white fluorescence (Figure 2B). Unstained fresh suspension cells that were yellow-brown under the light microscope exhibited white fluorescence on UV excitation (Figure 2E). In the SEM image of callus, membrane-like structures were seen (Figure 3A), resembling those found in the superficial cells of Coffea arabica L. callus (Nakamura and Maeda 1990). Well-organized organelles, such as mitochondria and chloroplasts (Figure 3B), were visible in the cytoplasm of green callus. Other plastids without grana, such as amyloplasts, were also present, as shown in Figure 3C. The amount of starch increased during culture, as did the osmiophilic material (tannins) in vacuoles (Figure 3E). Myelin-like structures were found within the cytoplasm and vacuoles of young callus that had apparently formed as a result of ER activity or through tonoplast folding (Figure 3D). The fresh unstained cells of completely dark brown callus had thick cell walls that emitted a yellow-brown fluorescence typical of phenol substances on UV excitation, or thinnish cell walls with white fluorescence. The concentration of a polypeptide with a molecular mass of 24 kDa (Figure 5) was high after 2 weeks of culture. In a previous study, Laukkanen et al. (1997) reported that the concentration of a 24 kDa protein increased from the beginning of culture and was highest after 12 to 14 days of culture. Polypeptides of 28, 14 and 10 kDa were abundant, whereas the 24 kDa glycoprotein was seen as a faint band. This polypeptide can be detected better by silver staining of purified glycoproteins (Laukkanen et al. 1997). When soluble proteins were subjected to PAGE and then stained for $-glucosidase, a single fluorescent band of approximately 60 kDa was observed in UV (Figure 5). This fluorescent band had a similar molecular mass to the coniferin-specific $-glucosidase of lodgepole pine reported by Dharmawardhana et al. (1995). Discussion Scots pine, like several other pine species, is recalcitrant in tissue culture. To determine if this is associated with tissue browning, we studied the relationship between browning and growth, cellular structure and enzyme activity during in vitro culture of callus derived from mature pine buds. The dry mass growth curve of cell suspension cultures showed that deterioration of cells began after about 2 weeks in culture. Similarly, the first visible signs of browning in callus were usually seen after 2 weeks in culture when peroxidase (POD) reached its maximum activity and the growth rate started to decrease. At the same time, the amount of chlorophyll started to decline and lipid peroxidation reached its maximum. Earlier work on pine callus has shown that PODs, and to some extent polyphenol oxidases (PPOs), are able to oxidize catechol producing dark brown quinones (Laukkanen et al. 1999). However, we found that after 2 weeks of culture, POD activity with catechol as substrate was considerably lower (approximately 11,000´ ) than POD activity with guaiacol as substrate. Furthermore, POD activity with catechol as substrate did not correlate with the onset of browning. Our results are in agreement with the finding that some peroxidases function as phenol oxidases by oxidizing hydroxycinnamic derivatives and flavans (see references in Siegel 1993 and Richard-Forget and Gauillard 1997). TREE PHYSIOLOGY VOLUME 20, 2000 BROWNING OF PINE CALLUS 471 Figure 2. (A) Callus tissue after 4 weeks of culture. The reddish blue color indicates viable cells and the blue to greenish blue color indicates degraded cells without cytoplasm (arrow); 175´ . (B) Autofluorescent material (arrow) inside young (10-day) callus; 85´ . (C) Fibrillar structures (arrow) of fresh callus cells, CW = cell wall; 345´ . (D) Fibrillar structures (arrow) between callus cells (UV fluorescence); 85´ . (E) Unstained fresh cells from suspension culture. The cell (left) with a yellow-brown tone under a light microscope showed bright white autofluorescence on UV excitation, whereas the normal-looking cell (right) showed blue; 175´ . (F) Fluorescence of a microscope section of brown callus (42 days). Note the white autofluorescence in the intercellular spaces; 175´ . Scots pine callus is able to produce ethylene during the first 2 or 3 weeks; thereafter the amount of ethylene decreases in parallel with browning (Lindfors et al. 1990). Ethylene is known to induce de novo synthesis of peroxidase and phenylalanine ammonia-lyase (PAL), an enzyme involved in lignification and phenylpropanoid synthesis of cells (Abeles et al. 1988, Hyodo and Fujinami 1989). An increase in PAL activity during the first 2 or 3 weeks of culture has been detected in pine callus (Laukkanen et al. 1997). The enzyme activity staining for $-glucosidase in Scots pine callus revealed a single fluorescent band of 60 kDa indicating lignification of cells. Lignification was confirmed by histochemical staining of cells. The 60-kDa fluorescent band has a similar molecular mass to the purified coniferin $-glucosidase isolated from lignifying xylem of lodgepole pine by Dharmawardhana et al. (1995). Coniferin $-glucosidase is a homodimer of 28 kDa subunits, although a subunit of 24 kDa was also seen on SDS-PAGE after purification. Similarly, we observed polypeptides of 28 and 24 kDa when a soluble protein extract from Scots pine callus was subjected to SDS-PAGE. The 24 kDa band may represent subunits of methyltransferase, an enzyme associated with lignin synthesis (Pakusch et al. 1991). The production of lignin compounds in callus of pine species may be a result of stress reac- TREE PHYSIOLOGY ON-LINE at http://www.heronpublishing.com 472 LAUKKANEN, RAUTIAINEN, TAULAVUORI AND HOHTOLA Figure 3. Bars = 5 m m. (A) A tions because several stresses are known to induce the synthesis of phenylpropanoids (cf. Dixon and Palva 1995, Lange et al. 1995). The amount of (+)catechin, a precursor of tannin, was 10-fold higher and that of condensed tannins approximately 3-fold higher in 4-week-old callus of Scots pine compared with buds (Laukkanen et al. 1997). These compounds contributed to the formation of the red color in callus that was stained with vanillin–HCl. Because Scots pine callus produces large amounts of ethylene (Lindfors et al. 1990, Laukkanen and Sarjala 1997), we suggest that the production of ethylene, rather than the browning process, resulted in the accumulation of (+)catechin, as in the russet spotting of iceberg lettuce, Lactuca sativa L. (Ke and Saltveit 1988). The toxicity of large tannin deposits has been observed in other tissues in addition to Scots pine callus. For example, large tannin deposits were reported to be toxic in brown tissues of slash pine (Hall et al. 1972, Baur and Walkinshaw 1974). The results from slash pine suggested that the foam-like tannin is significantly more soluble and causes more pronounced cellular degradation than the dense spherule type. The foam-like tannin was also observed in our Scots pine TREE PHYSIOLOGY VOLUME 20, 2000 BROWNING OF PINE CALLUS 473 Figure 4. Bars = 5 m m. (A) The fine structure of dark brown callus. Note the large starch granules (arrows) and the dark tannin deposits (T) in the absence of cytoplasm. (B) Dark osmiophilic material (arrow) in the intercellular space of brown callus. Note the numerous small vesicles (small arrow) in the cytoplasm (C). (C) Multivesicular bodies inside the cell wall (CW) of brown callus. (D) A dense fibrillar network between the cell walls (CW) of brown callus. callus culture. Our EM studies indicated that accumulation of large amounts of tannin and starch in cells precedes the browning Figure 5. Polyacrylamide gel electrophoresis of soluble proteins extracted from 3-week-old callus. Lane A: SDS-PAGE of soluble proteins stained with silver. Arrow indicates a 24 kDa polypeptide. Lane B: Purified glycoproteins stained with Coomassie blue. Arrows indicate polypeptides of 28, 14 and 10 kDa. Lane C: Enzyme activity staining for $-glucosidase after native PAGE. Arrow indicates an approximately 60 kDa polypeptide. and deterioration of tissues. The results are in accordance with the idea that the accumulation of tannins in the cytoplasm leads to cell death (Baur and Walkinshaw 1974, Barnett 1978, Hall et al. 1992). We observed cellular alterations similar to those observed during aging of callus derived from hypocotyl segments of Pinus radiata D. Don (Barnett 1978), where cell aging was accompanied by increases in the amount of osmiophilic material, probably tannins, in the vacuoles, and in the size of the starch grains. The final stage of tannin accumulation in callus cells appears to be its incorporation into the cytoplasm with accompanying degeneration of the cytoplasm and its organelles. At this stage, tannin may also be observed in the intercellular spaces. The increase in lipid peroxidation during browning suggests that browning of Scots pine callus and cell suspensions markedly reduced their regeneration capacity. Hall et al. (1972) observed a relationship between cytoplasmic disorganization and oxygen consumption in slash pine callus derived from embryos. Oxygen consumption was lower in brown and dark brown calli compared with green, yellow-green, yellow or yellow-brown calli. Although proembryos have been found in suspension cultures derived from buds, no further differentiation into somatic embryos has been observed (Hohtola 1995). There is evidence that autofluorescence of the cell wall in UV light, together with the presence of a large central nucleus (Blervacq et TREE PHYSIOLOGY VOLUME 19, 1999 474 LAUKKANEN, RAUTIAINEN, TAULAVUORI AND HOHTOLA al. 1995) and extracellular fibrillar structures of proembryos (Rohr et al. 1989, Dubois et al. 1992, Jasik et al. 1995, Šamaj et al. 1995) indicate embryogenic potential in tissue cultures. However, because autofluorescence can also be a sign of incipient lignin synthesis under stress, we conclude that the autofluorescence and fibrillar structures found in browning Scots pine callus reflect high oxidative stress in the cells rather than the potential development of somatic embryos. In conclusion, microscopic studies revealed that, during browning, large changes occurred in the cellular structure of callus derived from mature Scots pine buds. Accumulation of tannins in the cell walls, intercellular spaces and cytoplasm was observed in brown tissues. Disorganization or absence of cytoplasm and lignified cell walls were typical of dark brown callus. This type of browning is a consequence of high oxidative stress and causes serious disorganization in the cytoplasm and eventual cell death, thereby reducing the regeneration capacity of callus and suspension cultures. High peroxidase activity precedes and stimulates the deterioration of tissues leading to rapid browning. 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