Services on Demand
- Cited by SciELO
- Access statistics
Print version ISSN 1415-4757
Genet. Mol. Biol. vol.27 no.2 São Paulo 2004
GENETICS OF MICROORGANISMS
Carlos Henrique S. CarvalhoI; Usha B. ZehrII; Nilupa GunaratnaII; Joseph AndersonII; Halina H. KononowiczII; Thomas K. HodgesII; John D. AxtellII
IEmbrapa Milho e Sorgo, Sete Lagoas, MG, Brazil
IIPurdue University, West Lafayette, IN, USA
The results presented in this work support the hypothesis that Agrobacterium-mediated transformation of sorghum is feasible, analogous to what has been demonstrated for other cereals such as rice, maize, barley and wheat. The four factors that we found most influenced transformation were: the sensitivity of immature sorghum embryos to Agrobacterium infection, the growth conditions of the donor plant, type of explant and co-cultivation medium. A major problem during the development of our protocol was a necrotic response which developed in explants after co-cultivation. Immature sorghum embryos proved to be very sensitive to Agrobacterium infection and we found that the level of embryo death after co-cultivation was the limiting step in improving transformation efficiency. The addition of coconut water to the co-cultivation medium, the use of vigorous and actively growing immature embryos and the removal of excess bacteria significantly improved the survival rate of sorghum embryos and was critical for successful transformation. Hygromycin phosphotransferase (hpt) proved to be a good selectable marker for sorghum. We also found that b-glucuronidase (GUS) activity was low in most of the transgenic plant tissues tested, although it was very high in immature inflorescences. Although promising, the overall transformation efficiency of the protocol is still low and further optimization will require particular attention to be given to the number of Agrobacterium in the inoculum and the selection of sorghum genotypes and explants less sensitive to Agrobacterium infection.
Key words: Agrobacterium tumefaciens, GUS, transformation, sorghum.
Successful Agrobacterium-mediated transformation has been reported in rice (Aldemita and Hodges, 1996; Hiei et al., 1997; Hiei et al., 1994; Rashid et al., 1996; Toki et al., 1997), maize (Ishida et al., 1996), barley (Tingay et al., 1997), wheat Cheng et al., 1997) and, recently, sorghum (Zhao et al., 2000).
The multiplicity of factors that influence transformation is probably the reason why Agrobacterium-mediated transformation in monocotyledonous plant species has been difficult to achieve (Hiei et al., 1997; Ishida et al., 1996). Several factors are important in transformation, the type and developmental stage of the infected plant tissues, the concentration of Agrobacterium tumefaciens, the composition of the media used for co-cultivation infection and tissue culture, the selectable marker genes used, the type of vector and the plant genotype being among the factors that influence transformation (reviewed by Hiei et al., 1997). A critical point in developing an efficient transformation protocol is to find the right combination of the many factors that act together during transformation.
In this paper we discuss several factors that influence transformation efficiency, including the sensitivity of sorghum explants to Agrobacterium infection, type of explant, inoculation method and co-cultivation media. We found that the addition of coconut water to the co-cultivation medium together with the use of vigorous and actively growing immature embryos as explants for infection and the removal of excess Agrobacterium significantly improved the survival rate of explants and were critical for the success of transformation. The sensitivity of immature embryos to Agrobacterium infection was considered by us to be the limiting step to increase transformation efficiency. We also evaluated the use of b-glucuronidase (GUS) expression as a tool for monitoring transformation events and found that under the conditions of this study GUS expression was higher in specific sorghum tissues.
Materials and Methods
Sorghum genotype P898012 was used for most experiments because of its ease for tissue culture, although the genotypes Feterita Gesish (Early Feterita from Sudan), SRN 39 (Striga resistant African line), P967083 (Purdue University developed line), IS2329 (PI# 217837 Lwalli White), Rio (Sweet sorghum), Sugar drip (Sweet sorghum), B-Wheatland (Commercial B line), RTx430 (Commercial R line) and Candystripe (Mutable pericarp land race from Sudan) were also evaluated for tissue culture response. Plants cultivated either in greenhouse or in field conditions were used as a source of explants. Seeds containing immature sorghum embryos at the milk stage of endosperm development (usually 1.2 to 2.5 mm long) were harvested and washed thoroughly with running water for 10 min, surface sterilized for 25 min in 20% bleach with approximately 0.1% Tween 20, and then rinsed four times with sterile water before embryo extraction. Embryo harvesting and plating onto the tissue cultured medium or inoculation with Agrobacterium were done in the same day. Immature embryos were used as explants for most experiments, although pre-cultured immature embryos cultured in medium I8 (Table 1) for 1 to 5 days, immature inflorescences (0.5 to 5 cm long) and callus derived from immature embryos and inflorescences were also tested. The pre-cultured of immature embryos, co-cultivation and selection after transformation were done in 100x15 mm petri dishes.
We obtained Agrobacterium tumefaciens strain LBA4404, containing the 'super virulent' binary vector pTOK233, from Japan Tobacco Inc. (Hiei et al. 1994) and used this strain in all experiments. The pTOK233 vector contains the virB, virC and virG genes, the hygromycin-resistance hygromycin phosphotransferase gene (hpt), a kanamycin-resistance gene (npt) and a gene for b-glucuronidase (gusA) (Figure 1). Hpt was used as a selectable marker. The Agrobacterium was prepared for inoculation by streaking one loop of the bacterial stock kept at -70 °C onto yeast extract peptone (YP) agar (containing (g/L) yeast extract, 10; agar, 8; NaCl, 5; peptone, 5; pH 6.8) plates supplemented with 50 mg/L hygromycin, and incubated at 28 °C for 3 days. Cultures were collected with a scoop, suspended in inoculation medium (IM, Table 1), adjusted to the required optical density (l = 600 nm) using a Spectronic 21D spectrophotometer (Milton Roy, USA) and used for inoculation within 30 min. In most of the experiments 0.03% (w/v) Pluronic F-68 was added to IM medium to try to improve transformation efficiency (Cheng et al. 1997).
We studied three different inoculation protocols: 1) Immature embryos were soaked in IM medium containing the Agrobacterium cells for 5 to 10 min, blotted dry with filter paper to remove excess bacteria and plated on I6As co-cultivation agar in 100x15 mm petri dishes. (Table 1); 2) A drop of the IM medium containing the Agrobacterium cells [I presume this is what you mean.] was applied to individual embryos lying on I6As co-cultivation agar ; 3) Immature embryos were placed in a 2 mL microtube with 1 mL of IM medium, sonicated for 15 or 30 s in a Cole Parmer sonicator (Chicago, IL), vortexed for 10 s, allowed to stand for 5 min, blotted with filter-paper and plated onto co-cultivation agar. In one experiment a toothpick and a needle were used to inoculate restricted sectors of the embryos.
In all cases, co-cultivation was allowed to proceed for 2 to 5 days at 25 °C, after which the embryos were transferred to I8+C medium. (Table 1) containing cefotaxime to kill the Agrobacterium and calli proliferation allowed to take place for 6 to 12 days at 27 °C. Some experiments were also carried out to test the effectiveness of the addition of antioxidants and the effects of coconut water (see below). After proliferation calli were transferred to the first selection medium, I8+15H+C agar (Table 1), for two weeks after which they were cut into 1 to 3 mm pieces and transferred to a second selection medium, S10+25H+C agar (Table 1), on which they were grown for 3 to 4 months, being subcultured onto fresh S10+25H+C agar every 2 weeks. All callus induction and selection was carried out at 27 °C. The growth of the embryos and Index of Agrobacterium growth during co-cultivation was assessed using a visual index with 0 representing no growth and 5 maximum growth.
Two regeneration protocols were tested: 1) resistant calli were taken from the S10+25H+C agar and transferred to 100x25 mm petri plates containing pre-regeneration medium (PR; Table 1) for two weeks and then to plates of regeneration medium 6 (R6; Table 1) until the plantlets reached about 2 cm in length when they were transferred to appropriate jars containing fresh R6 medium for further growth under fluorescent light (± 50 mE m2/s) at 27 °C; 2) calli with visible immature embryo-like structures were transferred from S10+25H+C agar to 100x25 mm petri dishes containing R8 medium and cultured in the dark at 25 °C for 2-3 weeks. The mature, opaque embryo-like structures were then transferred to regeneration medium 9 (R9; Table 1) and kept under high intensity light (± 120 mE m2/s) until plantlet formation. Calli with no visible somatic embryos were first cultured in regeneration medium 7 (R7; Table 1) at 28 °C for two to three weeks and then transferred to R8 medium and then treated the same as in regeneration protocol 1, above.
The regenerated seedlings produced by the protocols described above were transplanted to pots contained a peatmoss mixture, transferred to a greenhouse, and covered with a plastic bag to prevent dehydration. The plastic bags were gradually lifted to decrease humidity, allowing hardening-off of the plants. After one week the plastic bags were removed and the plants allowed to grow to maturity.
Effects of antioxidants, Murashige and Skoog salts and coconut water
Polyvinylpyrrolidone (PVP, Sigma) and polyvinylpolypyrrolidone (PVPP, Sigma) were both tested for their ability to act as antioxidants and reduce explant browning and death. To test the antioxidant activity of these compounds we conducted other experiments in which we added 0.5 or 1% (w/v) PVP or PVPP to the I6As co-cultivation medium along with 0.2% (w/v) dithiothreitol (DTT). Following co-cultivation the embryos were cultured for seven days on I8+C medium or I8+C medium supplemented with 0.5% PVPP and covered with sufficient liquid I8+C medium (i.e. I8+C medium without agarose) containing 0.2% (w/v) DTT to cover the embryos (Perl et al., 1996).
The effects of replacing the MS salts in medium I8 with N6 salts to produce medium I9 (Table 1) were tested in experiments in which medium I8 was replaced by medium I9 for callus induction and cultivation.
Experiments were also made to observe the effects of coconut water by comparing the results produced with medium I8 (containing coconut water) and those produced when medium I8 was substituted by medium I10 (Table 1), which was identical to medium I8 except the coconut water was omitted.
In one experiment, timentin (150 mg/L) and carbenicillin (500 mg/L) instead of cefotaxime were used to kill Agrobacterium after co-cultivation.
Scanning electron microscopy (SEM) was used to study embryos inoculated with Agrobacterium. Samples of immature embryos used for transformation were inoculated with Agrobacterium and co-cultivated for 32 h and then vigorously washed five times by vortexing for 15 s in 0.2 M phosphate-buffer (pH 6.8) containing 0.9% (w/v) NaCl to remove bacteria that were not firmly attached. An attachment deficient Agrobacterium (strain At701 chvA:lacZ, provided by Stanton Gelvin, Purdue University) was used as a control to check if the washing procedure removed all non-attached bacteria. Immature embryos were prepared for SEM using a standard protocol for the fixation of biological material.
Inheritance of hygromycin resistance in T1 progeny
To test for the inheritance of the hygromycin phosphotransferase hpt gene we self-pollinated T1 sorghum plants and 20 days after pollination harvested the seeds, surface sterilized them with by washing with 20% bleach and extracted the immature embryos and plated them onto germination medium G (Table 1) and allowed them to grow at 28 °C for 3-6 days. Germinated embryos with active root and shoot growth were then transferred to germination medium containing hygromycin (G+25H; Table 1) and the plantlets evaluated for hygromycin resistance 10 days after transfer.
DNA isolation and Southern blot analysis
Sorghum genomic DNA was extracted from leaf tissue, digested with HindIII and analyzed by Southern hybridization (Gardiner, 1998). A gusA DNA probe was prepared from a BamHI-EcoRI restricted fragment of pBI221 (Clontech) and the hpt DNA fragment probe was obtained from the pHYG plasmid (Thomas Hodges, Purdue University) after restriction digestion with SalI.
Beta-glucuronidase (GUS) expression assays
We investigated the expression of GUS in actively growing roots, stem sections, young leaves at the rolled stage, mature leaves and young (5 to 15 cm long) inflorescences from the T1 transgenic plant number 687. Samples were divided into two sub-samples, one for histochemical assay and one for fluorogenic assay.
Expression of GUS was assayed by histochemical staining according to (Rueb and Hensgens, 1989) and by the fluorogenic 4-methyl umbelliferyl glucuronide (MUG) assay.
For the fluorogenic assay, 100 mg fresh weight of tissue was homogenized using a pestle and mortar in 1 mL of extraction buffer (150 mM sodium phosphate, pH 7.0, 10 mM Na2 EDTA, 10 mM b-mercaptoethanol, 0.1% (w/v) Triton X-100, 0.1% (w/v) N-laurylsarcosine, 25 mg/mL PMSF (Phenylmethylsulfony fluoride). The homogenates were centrifuged at 10,000 rpm for 3 min and the supernatant (extract) collected and stored on ice until use. A sample of 40 mL of the extract was then mixed with 460 mL of extraction buffer containing 1 mM MUG and incubated at 37 °C for 60 min, after which 100 mL aliquots were removed and mixed with 1500 mL of 0.2 M Na2CO3 to stop the reaction and the fluorescence measured in a fluorometer (Hoefer Scientific).
Protein concentration was determined by using the Bio-Rad Protein Assay reagent (Bio-Rad Laboratories, CA).
The effect of PVPP on GUS activity was determined by homogenizing 100 mg (fresh weight basis) of sorghum leaves with 12.5, 25 or 50 mg (dry weight basis) of PVPP (soaked overnight in extraction buffer) and assaying aliquots of the homogenate fluorometrically as described above. Experiments were also carried out using successively larger aliquots of leaf-homogenate to check whether or not chlorophyll was affecting the fluorometer readings.
As a control, the effect of sorghum leaf extracts on E. coli GUS activity was determined using the same fluorometric assay, except that 2.4 U/mL E. coli GUS was added during sorghum leaf homogenization.
In preliminary experiments, medium I6 (Cai and Butler, 1990) was used for callus induction but in this medium the immature embryos usually produced black pigments which seemed to delay callus growth and also to interfere with the identification of GUS activity. This problem was reduced by adding 3 g/L proline and 2 g/L asparagine as suggested by Elkonin et al., 1995, to produce medium I8, callus grown in this medium producing much less pigment and growing faster than in medium I6. We tested the replacement of the MS salts in medium I8 with N6 salts (Chu et al., 1975) by producing medium I9 (Table 1) but found that medium I8 produced more embryogenic callus than medium I9 (Table 2) which supports the work of Zhao et al., 2000 who also found that MS-based medium resulted in better embryogenic callus response from immature embryos of P898012.
The addition of coconut water to the medium seemed to increase the percentage of embryos that formed callus, reduced pigment production and improve callus growth (Table 2).
Plant regeneration was easily attained with 2-4 week old callus, but older callus showed much less regenerative capacity. Regeneration Protocol 2 appeared to be more efficient than regeneration protocol 1, although it was not very efficient for the regeneration of callus more than 2 months old.
Effect of donor plant growing conditions
The tissue-culture response of immature embryos during co-cultivation and callus formation after co-cultivation depended on the growth conditions of the donor plant. Immature embryos isolated from donor plants growing under sub-optimal conditions, such as water stress and low temperature, did not show any apparent growth during co-cultivation and often died after co-cultivation. Immature embryos isolated from donor plants growing under good environmental conditions responded more promptly to tissue culture, showing some growth during co-cultivation and were less adversely affected by inoculation with Agrobacterium. These embryos also had a better chance of survival after co-cultivation and usually showed bigger spots in the histochemical GUS assays.
Toxic effect of some explants to Agrobacterium
When cut or injured, immature inflorescence of most sorghum genotypes tested produced toxic compounds that inhibited Agrobacterium growth during co-cultivation. A halo without bacterial growth was often observed around inflorescences and plates having a large inflorescence showed no growth of Agrobacterium. Sorghum is well known for its high content of phenolic compounds, but whether they were responsible for the bactericidal effect was not investigated. This bactericidal effect was also observed in immature embryos, with immature embryos showing good growth under co-cultivation frequently producing black pigments around which Agrobacterium would not grow and no bacterial growth occurred in these areas even when the embryos were removed from the plates. Apparently only embryos in certain stages of development were able to produce substances that prevented bacterial growth, since Agrobacterium was able to grow (as assessed visually) on most embryos sampled. This toxic effect has also been observed in immature maize embryos where it was more pronounced when the embryos were less resistant to infection by Agrobacterium (Schalappi and Holn, 1992).
Sensitivity of immature embryos to Agrobacterium
A browning phenomenon was observed following co-cultivation of Agrobacterium and sorghum explants, particularly in immature embryos. During co-cultivation immature embryos usually maintained a good appearance, white and smooth. However, when the embryos were transferred to a bacteria-free medium containing cefotaxime but no hygromycin they became brown and shrunk within 48 h and died. Non-inoculated immature embryos produced normal callus in the presence of cefotaxime, suggesting that cefotaxime was not responsible for the necrotic effect. Furthermore, the browning phenomenon was not diminished by the use of timentin (150 mg/L) and carbenicillin (500 mg/L) instead of cefotaxime. The necrotic process was apparently a result of an Agrobacterium-explant interaction, immature embryos from tan plant sorghum genotypes (PP290 and SRN39) showing less browning than immature embryos from red or purple plant sorghum genotypes (P898012 and Feterita) although most of these embryos died after co-cultivation.
Immature embryos observed by SEM during co-cultivation were coated with a layer of Agrobacterium cells embedded and trapped in a crust of material probably produced by the Agrobacteria (Figure 2D). This coat could not be removed even after washing by vortexing the immature embryos several times in liquid medium. Almost the whole embryo surface was covered with this material, except the edge, where clumps or individual Agrobacterium cells could be seen attached to each other and to the walls of the embryo cells by a mesh of fibrils (Figure 2C). Some of the embryos with this coating started to develop a coleoptile instead of forming callus. When embryos were inoculated with a toothpick or needle, even without injuring the embryo, only those sectors that received Agrobacterium became brown, indicating a localized necrotic effect. Reducing the number of Agrobacterium did not eliminate the problem. At 5.0 x 109 colony forming units (cfu)/mLGUS expression was higher but 60 to 100% of the embryos died after co-cultivation (Table 3). With a 10-fold dilution (5.0 x 108 cfu/mL) GUS activity was observed only in a very few experiments, although embryo death was still very high. Infection solutions with less than 1.0 x 108 cfu/mL reduced embryo death to acceptable levels, but no GUS activity was observed. A similar necrotic process elicited by Agrobacterium has been reported in grape (Perl et al., 1996; Pu and Goodman, 1992) and Catharanthus roseus cells (Garner et al. 1996). In grapes it was assumed that necrogenesis was due to a hypersensitive response of the grape cells to the Agrobacterium (Perl et al., 1996).
The addition of PVPP or PVPP+DTT to the inoculation, co-cultivation or post-co-cultivation media slightly reduced browning of immature embryos, but did not improve embryo survival rate after co-cultivation. Moreover, DTT seemed to be toxic to the embryos, which did not produce callus when DTT was added during or after co-cultivation.
Pre-cultured immature embryos and callus derived from immature embryos or inflorescence were less affected by Agrobacterium infection. The more time in tissue culture the explant had before co-cultivation, the higher its survival rate after co-cultivation. Immature embryos cultured in medium I8 for three to five days before co-cultivation and callus which was two to four weeks old showed a much higher survival rate than immature embryos. Most of the pre-cultured immature embryos and callus continued to grow after co-cultivation, although transient GUS expression in pre-cultured immature embryos and callus was rare and usually much lower than that observed in immature embryos. Immature embryos were used for most experiments because they showed higher transient GUS expression than pre-cultured embryos and callus, thus allowing monitoring of the transformation events.
Effect of Pluronic F-68 on GUS expression
The addition of 0.03% Pluronic F68 to the inoculation medium (Cheng, et al., 1997) dramatically increased transient GUS expression by up to 100-fold (Table 4). Figure 5A shows that GUS staining in immature embryos varied from single spots to large patches of blue on the edge and scutelum, although GUS expression in immature embryos was not consistently observed in the same treatment and only about 40% of the experiments showed some GUS expression. Apparently, the greenhouse and field growth conditions of the donor plants affected transformation efficiency and/or GUS expression. Pluronic F-68 did not increase transient GUS expression in pre-cultured embryos or callus.
Effect of co-cultivation media
Co-cultivation media significantly affected transient GUS expression and embryo survival after co-cultivation. The use of 3 g/L proline and 2 g/L asparagine during co-cultivation, which had the best response for callus induction, promoted bacterial overgrowth on the embryos and reduced GUS expression and embryo survival after co-cultivation (Table 5). The use of 1/10 MS salts tended to increase the percentage of embryos with blue spots but reduced embryo survival and callus formation after co-cultivation. Although it stimulated the growth of Agrobacterium, the addition of coconut water to the co-cultivation medium promoted a fast embryo response to tissue culture which increased embryo survival. Only immature embryos that showed some growth during the co-cultivation period were able to form callus. The best results were obtained when embryos were immersed in the bacteria inoculation medium for 5 to 10 min, blotted with a filter-paper to remove excess bacteria and co-cultivated on medium I6As containing coconut water. The combination of coconut water in the co-cultivation medium, vigorous, actively growing immature embryos and the removal of excess bacteria significantly improved embryo survival rate and was critical for the success of transformation.
Selection and regeneration of transformed plants
After co-cultivation the explants were allowed to grow for 6 to 12 days in a medium without hygromycin but with cefotaxime to kill Agrobacterium. This period without selection seemed to help the explants to recover from infection and apparently did not affect embryo selection with hygromycin. Hygromycin phosphotransferase (Hpt) seemed to be an acceptable selectable marker for sorghum transformation, since in some experiments putatively transformed calli or transgenic plants resistant to hygromycin were produced from a small number of explants (Events 91, 177: Table 6).
Seven transgenic plants originating from three transformation events were produced in three independent experiments. Five plants grew to maturity as normal fertile plants, while one plant showed stunted growth and stiff leaves and one died in the greenhouse. In two other experiments, calli resistant to hygromycin were produced but no plants were regenerated. Table 6 lists only the experiments where transgenic plants or callus resistant to hygromycin were produced. The transformation efficiency in these experiments ranged from 0.8 to 3.5%, indicating the potential of Agrobacterium-mediated transformation for sorghum. However, the overall transformation efficiency was much lower because the majority of the explants did not survive Agrobacterium infection. Approximately 2000 embryos were inoculated under the same conditions without producing transgenic plants.
Molecular analysis of T0 and T1 transgenic plants
Stable gene integration was confirmed by Southern blot analysis of T0 and T1 plants. Histochemical and fluorogenic assays detected GUS expression in several tissues of stable transformed plants, and the segregation ratio of hygromycin-resistant plants in T1 progenies was able to be determined. Although one advantage of Agrobacterium-mediated transformation is the tendency to insert a low copy number of transgenes, all three events produced plants with more than one copy of the inserted gene (Figure 3).
The segregation ratio of the T0 progeny (Plant 687) was 118 hygromycin- resistant plants to 6 hygromycin susceptible plants (19.6:1), which was close to the expected Mendelian segregation ratio of 15:1 for duplicate genes.
Effect of sorghum leaf extracts on bacterial b-glucuronidase
We found that E. coli b-glucuronidase activity was reduced by approximately 15% when mixed with sorghum leaf extract during homogenization (Figure 4A). Non-transformed sorghum tissue did not show any significant background activity that could affect the detected GUS activity.
In the experiments to determined whether the addition of PVPP during tissue homogenization increased GUS activity in transgenic sorghum we found that the addition of 25 mg of PVPP/100 mg fresh weight of leaves promoted an increase in GUS activity of about 20% (Figure 4B). Higher amounts of PVPP did not promote any increase in GUS activity and under our conditions it was very difficult to homogenize the samples when the concentration of PVPP was higher than 50 mg PVPP/100 mg of leaf fresh weight. The slight increase in GUS activity promoted by PVPP indicates that phenolic compounds may have been involved in reducing GUS activity in sorghum.
GUS activity assays in transgenic tissues
We found that GUS activity was infrequently observed in putatively transformed callus under selection or in callus produced from transgenic plants. Some calli showed small clusters of cells with intense blue staining but the majority of cells did not stain (Figure 5B). Young leaves at the rolled stage usually produced some blue color along the veins or close to the margins but GUS staining was never detected in roots, mature leaves or stems. In general, GUS staining was easily visualized in floral tissues, such as inflorescences, florets and developing seeds (Figure 5). Inflorescences, particularly young ones, showed levels of GUS activity 30 to 60-fold higher than that found in leaves, stems and roots (Figure 6, vertical bars and pictures). The staining ranged from a strong blue color in inflorescences smaller than 5 cm, up to patches of blue on the rachis nodes (probably regions of active growth) in older inflorescences. The stronger staining in regions of active growth was not due to better stain penetration in these areas, since a longitudinal cut in the inter nodal regions (which would increase stain penetration) did not improve staining. Other floral tissue, such as palea, glume, ovary and seeds also showed GUS staining. These observations suggest that floral tissues, particularly young inflorescences, are better tissues in which to look for GUS activity in putative transformed plants. In mature leaves, stems and roots, GUS activity was detected only by the fluorogenic assay, probably because this method is much more sensitive than the histochemical assay. No blue background was observed in non-transformed sorghum tissues.
Transgenic plant 687 showed GUS activity concentrated in some actively growing tissues such as young leaves and inflorescences, this being particularly evident in inflorescences where GUS activity was detected only in nodal regions undergoing active growth.
The results presented in this work corroborate the assumption that Agrobacterium-mediated transformation of sorghum is certainly feasible, analogous to what has been demonstrated with other cereals such as rice, maize, barley and wheat.
Four factors influenced transformation the most, i.e. sensitivity of immature embryos to Agrobacterium infection, donor plant growing conditions, explant type, and co-cultivation media.
A major problem during protocol development was a necrotic response that the explants developed after co-cultivation. Immature sorghum embryos proved to be very sensitive to Agrobacterium infection and embryo death after co-cultivation was considered a limiting step to improve transformation efficiency. The phenomenon revealed some of the characteristics of a hypersensitivity-like reaction, such as a rapid and localized death of plant cells at the site where Agrobacterium was applied, oxidative burst (browning) and tissue shrinkage. Nevertheless, none of the treatments with antioxidants known to minimize hypersensitivity reaction in other species significantly diminished embryo death, and it is still unclear if embryo death was caused by a hypersensitivity-like reaction.
A large variation in transient GUS expression and immature embryo survival after co-cultivation was found in many experiments under similar conditions. This variation was partly attributable to the influence of the growth conditions of the immature embryo donor plants. Variability in environmental conditions may be associated with reduced plant vigor as a consequence of the sub-optimal lighting and temperature conditions which often occur in greenhouses (Frame et al., 2000). Our results are in agreement with these observations since the best results were obtained with immature embryos collected from more vigorous donor plants.
Transient GUS expression and embryo recovery after infection were also strongly influenced by inoculation conditions and co-cultivation medium. A key point was to maintain the Agrobacterium concentration high enough for transformation and inoculation and use co-cultivation conditions that allowed the embryo to response to tissue culture. Under these conditions GUS expression was usually restricted to a few spots on the scutellum. It is possible that the use of a promoter stronger than the CaMV 35S promoter would enhance GUS activity in sorghum. Similar work also with the genotype P898012 (Zhao et al., 2000) resulted in an average of 60% of immature embryos with blue spots using the ubiquitin promoter. The ubiquitin promoter has been shown to produce higher GUS expression than the CaMV 35S promoter in other cereals such as maize (Schledzewski and Mendel, 1994), rice (Dong et al., 1991) and barley (Schledzewski and Mendel, 1994).
Coconut water in the co-cultivation and callus induction media improved embryo recovery and callus formation. However, considering that P898012 is a genotype very responsive to coconut water, the use of other genotypes may require different media composition because many genotypes do not respond very well to coconut water (Kaeppler and Pederson, 1996).
Pluronic-F68 dramatically improved transient GUS expression in immature embryos but did not have the same effect on pre-cultured immature embryos or callus. This result indicates the usefulness of Pluronic F-68 for immature sorghum embryo transformation, supporting the observations of Cheng et al., (1997) in wheat.
Putatively transformed callus resistant to hygromycin and callus from transgenic plants did not show consistent GUS expression. Some callus pieces showed intense blue staining in localized areas but most of the calli did not stain blue. Thus, GUS expression in callus pieces detected by histochemical assay was not a reliable parameter for assessing transformation. In transgenic plants, GUS activity was stronger in the nodes of young inflorescences, suggesting that this is the best tissue to check for GUS activity. Since the CaMV 35S promoter is preferentially expressed in certain tissues (Dong et al., 1991) it may be that this pattern is common for sorghum.
Sorghum leaf extracts reduced E. coli b-glucuronidase activity by about 15% and this reduction was associated with the presence of phenolic compounds produced by the leaves. Other plants containing high concentrations of phenolics, such as cranberry, also reduce GUS activity (Serres et al., 1997). However, the 15% decrease which occurred in our experiments was not enough to fully explain the very low (sometimes undetectable) levels of GUS activity observed in most of the transgenic sorghum tissues analyzed. Low levels of GUS activity seem to be a prevalent characteristic of several sorghum tissues (Battraw and Hall, 1991; Casas et al., 1993 and 1997; Hagio et al., 1991) and may be caused by more than one factor. Besides promoter strength and specificity and the presence of phenolic compounds, the silencing of gusA may also account for the low levels of GUS activity detected.
The hpt locus proved to be a good selectable marker for sorghum. Selection with hygromycin was very efficient and non-transformed calli and seedlings were easily discriminated against in media containing hygromycin.
Although transgenic plants were produced in three experiments, the overall transformation efficiency was quite low. Several other experiments under similar conditions failed to produce transformed plants. Further protocol optimization will require particular attention to inoculum concentration and the use of sorghum genotypes and explants less sensitive to Agrobacterium infection.
We thank EMBRAPA, Brazil, for financial support, D. Sherman from the Electron Microscopy Center at Purdue University for the help and B. Frame from the Maize Transformation Facility at Iowa State University for helpful suggestions on the regeneration protocols.
Aldemita RA and Hodges TK (1996) Agrobacterium tumefaciens-mediated transformation of japonica and indica rice varieties. Planta 199:612-617. [ Links ]
Battraw M and Hall TC (1991) Stable transformation of Sorghum bicolor protoplasts with chimeric neomycin phosophotransferase II b-glucuronidase genes. Theor Appl Genet 82:161-168. [ Links ]
Cai T and Butler L (1990) Plant regeneration from embryogenic callus initiated from immature inflorescences of several high-tannin sorghums. Plant Cell Tiss Org Cult 20:101-110. [ Links ]
Casas AM, Kononowicz AK, Haan TG, Zhang L, Tomes DT, Bressan RA and Hasegawa PM (1997) Transgenic sorghum plants obtained after microprojectile bombardment of immature inflorescences. In vitro Cell Dev Biol 33:92-100. [ Links ]
Casas AM, Kononowicz AK, Zerh UB, Tomes DT, Axtell JD, Butler LG, Bressan RA and Hasegawa PM (1993) Transgenic sorghum plants via microprojectile bombardment. Proc Natl Acad Sci USA 90:11212-11216. [ Links ]
Cheng M, Fry JE, Pang S, Zhou H, Hironaka CM, Duncan DR, Conner TW and Wan Y (1997) Genetic transformation of wheat mediated by Agrobacterium tumefaciens. Plant Physiol 115:971-980. [ Links ]
Chu CC, Wang CC, Sun SC, Hsu C, Yin KC, Chu CY and Bi FY (1975) Establishment of an efficient medium for anther culture of rice through comparative experiments on the nitrogen sources. Sci Sin 18:658-659. [ Links ]
Dong J-Z, Yang M-Z, Jia S-R and Chua N-H (1991) Transformation of melon (Cucumis melo L.) and expression from the cauliflower mosaic virus 35S promoter in transgenic plants. Bio/Tech 9:858-868. [ Links ]
Elkonin IA, Lopushanskaya RF and Pakhomova NV (1995) Initiation and maintenance of friable, embryogenic callus of sorghum (Sorghum bicolor (L.) Moench) by amino acids. Maydica 40:153-157. [ Links ]
Frame BR, Zhang H, Cocciolone SM, Sidorenko LV, Dietrich CR, Pegg SE, Zhen S, Schnable P and Wang K (2000) Production of transgenic maize from bombarded type II callus: Effect of gold particle size and callus morphology on transformation efficiency. In Vitro Cell Dev Biol Plant 36:21-29. [ Links ]
Gamborg OL, Shyluk JP, Brar DS and Constable F (1977) Morphogenesis and plant regeneration from callus of immature embryos of sorghum. Plant Sci Lett 10:67-74. [ Links ]
Gardiner JM (1998) UMC Maize RFLP Procedures Manual. Unpublished. (A compilation of procedures with modifications, updated 1998). [ Links ]
Garnier F, Label P, Hallard D and Chenieux JC (1996) Transgenic periwinkle tissues overproducing cytokinins do not accumulate enhanced levels of indole alkaloids. Pant Cell Tissue and Org Cult 45:223-230. [ Links ]
Hagio T, Blowers AD and Earle ED (1991) Stable transformation of sorghum cell cultures after bombardment with DNA-coated microprojectiles. Plant Cell Rep 10:260-264. [ Links ]
Hiei Y, Komari T and Kubo T (1997) Transformation of rice mediated by Agrobacterium tumefaciens. Plant Mol Biol 35:205-218. [ Links ]
Hiei Y, Ohta S, Komari T and Kumashiro T (1994) Efficient transformation of rice (Oryza sativa L.) mediated by Agrobacterium and sequence analysis of the boundaries of the T-DNA. Plant J 6:271-282. [ Links ]
Ishida Y, Saito H, Ohta S, Hiei Y, Komari T and Kumashiro T (1996) High efficiency transformation of maize (Zea mays L.) mediated by Agrobacterium tumefaciens. Nat Biotech 14:745-750. [ Links ]
Kaeppler HF and Pederson JF (1996) Media effects on phenotype of callus cultures initiated from photoperiod-insensitive, elite inbred sorghum lines. Maydica 41:83-89. [ Links ]
Li Z, Upadhyaya NM, Meena S, Gibbs AJ and Waterhouse PM (1997) Comparison of promoters and selectable marker genes for use in Indica rice transformation. Mol Breed 3:1-14. [ Links ]
Murashige T and Skoog F (1962) A revised medium for rapid growth and bioassays with tobacco tissue culture. Physiol Plantarum 15:473-497. [ Links ]
Perl A, Lotan O, Abu-Abied M and Holland D (1996) Establishment of an Agrobacterium-mediated transformation system for grape (Vitis vinifera L.): The role of antioxidants during grape-Agrobacterium interactions. Nat Biotech 14:624-628. [ Links ]
Pu XA and Goodman RN (1992) Induction of necrogenesis by Agrobacterium tumefaciens on grape explants. Physiol and Mol Plant Pathol 41:241-254. [ Links ]
Rashid H, Yokoi S, Toriyama K and Hinata K (1996) Transgenic plant production mediated by Agrobacterium in Indica rice. Plant Cell Rep 15:727-730. [ Links ]
Rueb S and Hensgens LAM (1989) Improved histochemical staining for b-glucuronidase activity in monocotyledonous plants. Rice Genet Newsl 6:168-169. [ Links ]
Schalappi M and Holn B (1992) Competence of immature maize embryos for Agrobacterium-mediated gene transfer. Plant Cell 4:7-16. [ Links ]
Schledzewski K and Mendel RR (1994) Quantitative transient gene expression: comparison of the promoters for maize polyubiquitin1, rice actin1, maize-derived Meu and CaMV 35S in cells of barley, maize and tobacco. Trans Res 3:249-255. [ Links ]
Serres R, McCown B and Zeldin E (1997) Detectable b-gluguronidase activity in transgenic cranberry is affected by endogenous inhibitors and plant development. Plant Cell Rep 16:641-646. [ Links ]
Tingay S, McElroy D, Kalla R, Fieg S, Wang M, Thornton S and Brettell R (1997) Agrobacterium tumefaciens-mediated barley transformation. Plant J 11:1369-1376. [ Links ]
Toki S (1997) Rapid and efficient Agrobacterium-mediated transformation in rice. Plant Mol Biol Rep 15:16-21. [ Links ]
Zhao Z, Cai T, Tagliani L, Miller M, Wang N, Pang H, Rudert M, Schroeder S, Hondred D, Seltzer J and Pierce D (2000) Agrobacterium-mediated sorghum transformation. Plant Molec Biol 44:789-798. [ Links ]
EditorAssociado: Darcy Fontoura de Almeida
Carlos Henrique S. Carvalho
Alameda do Café 1000
37026-400 Varginha, MG, Brazil
Received: October 15, 2002;
Accepted: October 21, 2003.